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Research Collection
Doctoral Thesis
Living cell adhesion measured by force spectroscopy
Author(s): Weder, Gilles
Publication Date: 2010
Permanent Link: https://doi.org/10.3929/ethz-a-006092558
Rights / License: In Copyright - Non-Commercial Use Permitted
This page was generated automatically upon download from the ETH Zurich Research Collection. For moreinformation please consult the Terms of use.
ETH Library
DISS. ETH NO. 18943
LIVING CELL ADHESION MEASURED BY FORCE SPECTROSCOPY
a dissertation submitted to
ETH ZURICH
for the degree of
Doctor of Sciences (Dr. sc. ETH Zurich)
presented by
Gilles WEDER
Master of Science in Biology, University of Neuchâtel, Switzerland, 2006
born on June 13, 1983
citizen of Au (SG)
accepted on the recommendation of
Prof. Dr. Janos Vörös, examiner
Dr. Martha Liley, co-examiner
Dr. Harry Heinzelmann, co-examiner
Dr. Mathis Riehle, co-examiner
2010
Table of contents
iii
SUMMARY VII
RÉSUMÉ XI
CHAPTER 1 INTRODUCTION 1
1.1. CELL ADHESION 1 1.1.1. CONCEPT 1 1.1.2. AT THE MOLECULAR LEVEL 1 1.1.3. AT THE CELL LEVEL 3 1.1.4. APPLICATIONS 5 1.2. CURRENT TECHNIQUES FOR CELL ADHESION STUDIES 6 1.2.1. LIGHT MICROSCOPE-BASED TECHNIQUES 6 1.2.2. MECHANICAL APPROACHES FOR CELL POPULATION STUDIES 7 1.2.3. MECHANICAL APPROACHES FOR SINGLE CELL STUDIES 8 1.3. ATOMIC FORCE MICROSCOPY FOR CELL ADHESION STUDIES 14 1.3.1. PRINCIPLE 14 1.3.2. FORCE SPECTROSCOPY MODE 15 1.3.3. SINGLE BIO-MOLECULE FORCE SPECTROSCOPY 17 1.3.4. SINGLE CELL FORCE SPECTROSCOPY (SCFS) 20 1.4. SCFS CONFIGURATIONS 23 1.5. DISSERTATION OBJECTIVES 25 1.6. ORGANIZATION OF THE DISSERTATION 26
CHAPTER 2 MATERIALS AND METHODS 29
2.1. SUBSTRATE PREPARATION 30 2.1.1. CLEANING PROTOCOL 30 2.1.2. SURFACE MODIFICATION WITH POLYELECTROLYTES 30 2.1.3. PREPARATION OF PNIPAM-GRAFTED SURFACES 31 2.1.4. PREPARATION OF PATTERNED PNIPAM-GRAFTED SURFACES 31 2.1.5. MICRO-FABRICATION OF LOW ASPECT-RATIO PILLARS IN QUARTZ 31 2.1.6. MICRO-FABRICATION OF HIGH ASPECT-RATIO PILLARS IN QUARTZ 32 2.1.7. STERILIZATION PROTOCOL 33 2.2. CELL CULTURE 33 2.2.1. SAOS-2 OSTEOSARCOMA CELLS 33 2.2.2. 3T3 MOUSE FIBROBLASTS 33 2.2.3. PRIMARY EMBRYONIC MOUSE FIBROBLASTS 34 2.2.4. CELL CYCLE SYNCHRONIZATION 34 2.2.5. CELL PROLIFERATION ASSAY 34 2.2.6. CELL SEEDING 35 2.3. INSTRUMENTATION 35 2.3.1. ATOMIC FORCE MICROSCOPE (AFM) 35 2.3.2. FLUORESCENCE ACTIVATED CELL SORTER (FACS) 37 2.3.3. CONFOCAL MICROSCOPE 38 2.3.4. SCANNING ELECTRON MICROSCOPE (SEM) 38
Table of contents
iv
2.4. FORCE-DISTANCE CURVES 39 2.4.1. CANTILEVERS FOR SHORT-TERM ADHESION 39 2.4.2. CELL CAPTURE FOR SHORT-TERM ADHESION 39 2.4.3. SHORT-TERM ADHESION MEASUREMENTS 40 2.4.4. CANTILEVERS FOR LONG-TERM ADHESION 40 2.4.5. LONG-TERM ADHESION MEASUREMENTS 41 2.4.6. CANTILEVERS FOR INDENTATION 41 2.4.7. ELASTICITY MEASUREMENTS 42 2.5. AFM IMAGING 42 2.6. CELL PREPARATION 42 2.6.1. FACS 42 2.6.2. CONFOCAL MICROSCOPY 42 2.6.3. SEM 43 2.7. DATA PROCESSING AND STATISTICAL ANALYSIS 43 2.7.1. FACS 43 2.7.2. ANALYSIS OF FORCE-DISTANCE CURVES 43 2.7.3. STATISTICAL ANALYSIS 45
CHAPTER 3 CELL ADHESION DURING THE CELL CYCLE 47
3.1. INTRODUCTION 48 3.1.1. THE CELL CYCLE 48 3.1.2. ADHESION OF MITOTIC CELLS 49 3.1.3. SHORT-TERM ADHESION MEASUREMENTS 49 3.2. CELL CYCLE SYNCHRONIZATION 51 3.2.1. G1, S AND G2M 51 3.2.2. NATIVE MITOTIC CELLS 52 3.3. SHORT-TERM ADHESION 52 3.3.1. PRESENCE OF ADHESION PROTEINS THROUGHOUT THE CELL CYCLE 52 3.3.2. POSITION OF THE UNBINDING EVENTS 55 3.3.3. ADHESION PER PROTEIN COMPLEX IN THE DIFFERENT CELL CYCLE PHASES 55 3.3.4. MAXIMUM FORCE OF DETACHMENT 56 3.3.5. WORK OF DETACHMENT 57 3.3.6. HIGHER STIFFNESS OF MITOTIC CELLS 58 3.4. DISCUSSION 60 3.4.1. CELL ADHESION BETWEEN M-PHASE AND INTERPHASE 60 3.4.2. STATISTICS 61 3.4.3. THE USE OF TRYPSIN 62 3.4.4. THE SHORT CONTACT TIME 62 3.5. CONCLUSION 62
CHAPTER 4 CANTILEVER FUNCTIONALIZATION FOR CELL DETACHMENT 65
4.1. INTRODUCTION 66 4.1.1. LONG-TERM ADHESION 66 4.1.2. CANTILEVER FUNCTIONALIZATION FOR CELL DETACHMENT 67 4.2. DETACHMENT OF ADHERENT CELLS 68 4.2.1. PERCENTAGE OF CELL DETACHMENT 68 4.2.2. MAXIMUM FORCE OF DETACHMENT 70
Table of contents
v
4.2.3. WORK OF DETACHMENT 70 4.3. DISCUSSION 72 4.3.1. SELECTION OF THE CANTILEVER FUNCTIONALIZATION 72 4.3.2. LIMITATION OF THE CONTACT TIME 73 4.3.3. THE EFFECT OF CANTILEVER FUNCTIONALIZATION ON CELL ADHESION 73 4.4. CONCLUSION 74
CHAPTER 5 CELL ADHESION ON FUNCTIONALIZED SURFACES FOR CELL SHEET ENGINEERING 77
5.1. INTRODUCTION 78 5.1.1. TISSUE ENGINEERING 78 5.1.2. CELL SHEET ENGINEERING 79 5.2. LONG-TERM ADHESION TO GLASS AT 37 °C AND 27 °C 80 5.3. CELL ADHESION ON POLYELECTROLYTES AT 37 °C 84 5.3.1. ADHESION FORCES 84 5.3.2. CHARACTERIZATION OF PLL/HA SUBSTRATES 85 5.3.3. DISCUSSION OF POLYELECTROLYTE COATED SURFACES 86 5.4. CELL ADHESION ON PNIPAM AT 37 °C & 27 °C 87 5.4.1. PRINCIPLE 87 5.4.2. ADHESION FORCES 87 5.4.3. DISCUSSION OF PNIPAM FUNCTIONALIZED SURFACES 89 5.5. CONTROLLING CELL ADHESION USING A PATTERNED PNIPAM COATING 89 5.5.1. PRINCIPLE 89 5.5.2. ADHESION FORCES 90 5.5.3. DISCUSSION OF PNIPAM PATTERNED SURFACES 92 5.6. DISCUSSION 93 5.6.1. DETACHMENT OF ADHERENT CELLS 93 5.6.2. LIMITATION OF THE SAMPLE SIZE 94 5.7. CONCLUSION 94
CHAPTER 6 EFFECT OF SUB-MICRON TOPOGRAPHY ON CELL ADHESION 97
6.1. INTRODUCTION 98 6.1.1. TOPOGRAPHY AND CELL ADHESION 98 6.1.2. TOPOGRAPHY AND CELL TYPE 98 6.1.3. DESCRIPTION OF THE SUB-MICRON TOPOGRAPHY 99 6.2. LONG-TERM ADHESION TO FLAT QUARTZ 100 6.3. EFFECT OF SUB-MICRON TOPOGRAPHY 101 6.4. COMPARISON WITH PRIMARY MOUSE FIBROBLASTS 103 6.4.1. CELL ADHESION 104 6.4.2. CELL PROLIFERATION 104 6.4.3. CELL MORPHOLOGY 105 6.5. DISCUSSION 107 6.5.1. DETACHMENT OF ADHERENT CELLS 107 6.5.2. CELL ADHESION TO QUARTZ AND GLASS 107 6.6. LIMITATION OF THE CELL TYPE 108 6.7. CONCLUSION 109
Table of contents
vi
CHAPTER 7 CONCLUSIONS & OUTLOOK 111
ACKNOWLEDGEMENTS 115
CURRICULUM VITAE 117
REFERENCES 121
Summary
vii
Summary
Cell adhesion is the binding of a cell to another cell, extracellular matrix or a surface, using cell
adhesion molecules. Many of these interactions involve transmembrane integrin receptors.
Integrins cluster to provide dynamic links between extracellular and intracellular environments,
by bi-directional signaling and stabilization of the focal adhesion points. The interactions involve
complex couplings between cell biochemistry, structural mechanics, and surface bonding.
Adhesive interactions play a major role in the development of multicellular organisms, by
guiding and anchoring cells into their appropriate locations. Adhesion is also important in the
maintenance of the body: changes in the expression or function of cell adhesion molecules are
implicated in all steps of tumor progression. Tumor cells are able to loosen their attachment to
leave their original location and become lodged at distant tissues (metastasis). Implantology
research and tissue engineering are directly focused on cell-surface interactions, since events
leading to integration of an implant into bone and to long performance of the device take place at
the interface formed between tissue and implant. Modifying the surface of an implant either by
providing chemical and/or topographical cues encourages bone cell attachment. Cell adhesion is
one way to increase osteointergration and to stabilize the implant. Tissue engineering aims to
replace or restore the anatomic structure and function of damaged or missing tissue. Cell
adhesion is a crucial parameter in the development of biodegradable scaffolds and cell sheet
engineering techniques.
Summary
viii
It is not easy to measure and quantify cell adhesion. Cell adhesion has been investigated using
many techniques. The combination of cell biology with force spectroscopy provides a powerful
tool for exploring the complexity of cell adhesion. The main objective of this work is to use force
spectroscopy to quantify the long-term global adhesion between cells and surfaces and their
response to modified surfaces. Atomic force microscopy-based force spectroscopy is capable of
resolving individual cell binding events as well as global cell adhesion of living cells under
physiological condition. It was used to study and quantify the adhesion of living cells to their
growing substrate.
In order to determine if cell adhesion has to be studied independently of cell cycle or not, cell
adhesion at different phases was measured. The adhesion of osteosarcoma cells to a glass surface
was measured at different phases of the cell cycle. The cells were synchronized in three phases of
the cell cycle: G1, S and G2M. Cells in these phases were compared with unsynchronized and
native mitotic cells. Individual cells were attached to an atomic force microscope cantilever,
brought into brief contact with the glass surface and, then pulled off again. The force-distance
curves obtained allowed the work and maximum force of detachment as well as the number,
amplitude, and position of discrete unbinding steps to be determined. The properties of the
binding proteins present at the cell surface remained similar throughout the cell cycle, including
mitosis. Therefore, next cell detachment experiments were allowed to be studied independently
of cell cycle.
Long-term cell adhesion involves living adherent cells. The challenge was to find a method of
attachment, between cells and atomic force microscope cantilevers, that allows their detachment
from the surface. Fibronectin-coated cantilevers were used to detach individual immortalized
fibroblasts from their growing substrate. The detachment of living adherent cells by force
spectroscopy was tested on a number of chemically functionalized surfaces in order to validate
the technique. The forces involved in the adhesion of fibroblasts were quantified. The cells were
grown on glass surfaces as well as on surfaces used for cell sheet engineering: glass surfaces
coated with polyelectrolyte multilayers (poly-L-lysine and hyaluronic acid) and thermally-
responsive poly(N-isopropylacrylamide) brushes. Large differences in cellular adhesion were
observed on polyelectrolyte coatings, depending on the number of polyelectrolyte bilayers. On
poly(N-isopropylacrylamide)-grafted surfaces, changes of more than an order of magnitude were
observed in cell adhesion above and below the lower critical solution temperature. Glass surfaces
Summary
ix
patterned with periodic poly(N-isopropylacrylamide) microdomains were also investigated. In
this last case, it was shown that cellular adhesion could be reduced while keeping cellular
morphology unchanged.
Finally, in order to investigate the potential and limitations of this technique, two important
experimental parameters were altered: the topography and the cell type. Immortalized and
primary fibroblasts were studied on flat and topographically structured quartz surfaces. Using a
fibronectin-coated AFM cantilever, it was possible to detach a large proportion of the
immortalized cells from the quartz surfaces. Their adhesion to the quartz surface, and the effects
of topography on this adhesion, could be quantified. In contrast, few primary cells were detached
under the same experimental conditions. A qualitative analysis of their behavior showed that
immortalized fibroblasts adhered less strongly than primary fibroblasts to at least one quartz
surface.
The potential and limitations of single cell force spectroscopy in the study of the adhesive
properties of cells are discussed. Quantitative data of this nature should open the way for more
rigorous investigation and comparison of the influence of different parameters on cell/substrate
adhesion.
Summary
x
Résumé
xi
Résumé
L’adhérence cellulaire correspond à la liaison d’une cellule à une autre cellule, à la matrice
extracellulaire ou à une surface, en utilisant des molécules spécifiques d’adhésion. La plupart de
ces interactions impliquent des récepteurs transmembranaires de type intégrines. Les intégrines se
regroupent et s’organisent afin d’établir des liens dynamiques entre le milieu extracellulaire et
intracellulaire, pour la signalisation moléculaire et la stabilisation des points d’adhésion focaux.
Les interactions sont le résultat de couplages complexes entre la biochimie cellulaire, la structure
mécanique et les liaisons de surface.
Les interactions d’adhésion jouent un rôle majeur dans le développement des organismes
pluricellulaires, en guidant et fixant les cellules dans leur emplacement approprié. L’adhésion est
également importante dans l’homéostasie du corps ; des changements dans l’expression et la
fonction des molécules d’adhésion cellulaire sont impliqués dans toutes les étapes de la
progression de tumeurs. Les cellules tumorales sont capables de se détacher et de quitter leur
emplacement d’origine afin de coloniser d’autres tissus (métastases). La recherche sur les
implants et le génie tissulaire sont directement intéressés par les interactions cellule-surface, car
la réussite d’une bonne intégration d’un implant dans l’os et l’efficacité à long terme se joue à
l’interface du tissue et de l’implant. Des modifications chimiques et/ou topographiques de la
surface d’un implant peuvent favoriser l’attachement des cellules osseuses. L’adhésion cellulaire
est responsable de l’ostéo-intégration de l’implant. L’adhésion cellulaire est aussi un paramètre
Résumé
xii
crucial dans le développement des prothèses biodégradables et des feuillets cellulaires.
L’adhésion cellulaire n’est pas facile à mesurer et quantifier. L’adhésion cellulaire a été
investiguée par de nombreuses techniques. La combinaison de la biologie et de la spectroscopie
de force offre un outil puissant pour l’exploration de la complexité de l’adhésion cellulaire.
L’objectif principal de ce travail est d’utiliser la spectroscopie de force pour quantifier les forces
globales d’adhésion à long terme entres des cellules et des surfaces, ainsi que leur réponse à des
surfaces modifiées. La spectroscopie de force issue de la microscopie à force atomique est
capable de mesurer aussi bien des liaisons d’adhésion individuelles que l’adhésion globale de
cellules vivantes en condition physiologique. Elle a été utilisée pour étudier et quantifier
l’adhésion de cellules vivantes à leur substrat de croissance.
L’adhésion cellulaire a été mesurée à différentes phases du cycle cellulaire afin de déterminer si
elle pouvait être étudiée indépendamment, ou non, du cycle cellulaire. L’adhésion entre des
cellules provenant d’un ostéo-sarcome et une surface en verre a été mesurée à différente phases
du cycle cellulaire. Les cellules ont été synchronisées dans trois phases du cycle cellulaire : G1, S
et G2M. Dans ces phases, les cellules ont été comparées avec des cellules non synchronisées et
des cellules naturellement en mitose. Des cellules individuelles ont été attachées à un levier de
microscope à force atomique, mises en bref contact avec la surface en verre et, ensuite retirées à
nouveau. Les courbes de force obtenues en fonction de la distance ont permis de déterminer le
travail et la force maximale de détachement aussi bien que le nombre, l’amplitude et la position
des étapes de détachement. Les propriétés des protéines d’adhésion présentes à la surface de la
cellule sont restées similaires au travers du cycle cellulaire entier, y compris en mitose. Par
conséquent, les mesures suivantes de détachement cellulaire ont été étudiées indépendamment du
cycle cellulaire.
L’adhésion cellulaire à long terme implique des cellules adhérentes vivantes. Le défi a été de
trouver une méthode d’attachement, entre les cellules et les leviers de microscope à force
atomique, capable de supporter leur détachement de la surface. Des leviers recouverts de
fibronectine ont été utilisés pour détacher des fibroblastes individuels immortalisés de leur
surface de croissance. Le détachement de cellules adhérentes vivantes, en utilisant la
spectroscopie de force, a été testé sur de nombreuses surfaces fonctionnalisées chimiquement afin
de valider la technique. Les forces impliquées dans l’adhésion des fibroblastes ont été quantifiées.
Résumé
xiii
La croissance des cellules a été réalisée sur des surfaces en verre ainsi que sur des surfaces
utilisées pour le génie tissulaire : des surfaces en verre fonctionnalisées avec des multi-couches
de polyélectrolytes (poly-L-lysine et acide hyaluronique) et avec le polymère thermo-sensible
poly(N-isopropylacrylamide). De grandes différences en terme d’adhésion cellulaire ont pu être
observées sur les revêtements de polyélectrolytes, en fonction du nombre de bicouches de
polyélectrolytes. Concernant les surfaces fonctionnalisées avec le poly(N-isopropylacrylamide),
des changements de plus d’un ordre de magnitude ont pu être observés au niveau de l’adhésion
cellulaire au-dessus et au-dessous de la température critique inférieure de solution. Des surfaces
en verre modifiées avec des micro-domaines de poly(N-isopropylacrylamide) ont également été
investiguées. Dans ce dernier cas, il a été montré que l’adhésion cellulaire pouvait être réduite
tout en gardant une morphologie cellulaire identique.
Finalement, deux paramètres expérimentaux importants ont été modifiés, la topographie et le type
cellulaire, afin d’investir le potentiel et les limites de cette technique. Des cellules immortalisées
et primaires ont été étudiées sur des surfaces en quartz plates et avec une topographie. Grâce à
l’utilisation d’un levier fonctionnalisé avec de la fibronectine il a été possible de détacher une
grande proportion des cellules immortalisées des surfaces en quartz. Leur adhésion aux surfaces
en quartz, et les effets de la topographie sur cette adhésion, ont pu être quantifiés. En revanche,
seules quelques cellules primaires ont pu être détachées en utilisant les mêmes conditions
expérimentales. Une analyse qualitative de leur comportement a montré que les fibroblastes
immortalisés adhéraient moins fortement que les fibroblastes primaires sur au moins une surface
en quartz.
L’aspect du potentiel et des limites de la spectroscopie de force avec des cellules individuelles
pour l’étude des propriétés d’adhésion est discuté. Des données quantitatives de ce genre
devraient ouvrir le chemin pour des investigations et comparaisons plus rigoureuses de
l’influence de différents paramètres sur l’adhésion entre une cellule et son substrat.
Résumé
xiv
Chapter1 Introduction
1
Chapter 1
Introduction
1.1. Cell adhesion
1.1.1. Concept
One prerequisite for the evolution of multicellular organisms was the development of
mechanisms by which cells could adhere to one another. Cell adhesion is the binding of a cell to
another cell, extracellular matrix or a surface using cell adhesion molecules (CAMs). Many cell
adhesion processes occur in two steps. First, single cell adhesion proteins bind to their respective
ligands at the cell surface and then the interaction is consolidated by the recruitment of
hierarchically assembled protein complexes called focal adhesions (FAs).
1.1.2. At the molecular level
Cell-cell and cell-substrate interactions are mediated through several different families of
receptors. In addition to targeting cell adhesion to specific extracellular matrix proteins and
ligands on adjacent cells, these receptors influence also many processes in cell regulation, tissue
Chapter1 Introduction
2
homeostasis and morphogenesis. Most of the CAMs belong to five families or superfamilies1:
integrins, immunoglobulins (Ig), cadherins, selectins and homing receptors. These proteins are
typically transmembrane receptors that interact either with similar CAMs (homophilic binding)
or with different CAMs or the extracellular matrix (heterophilic binding). Integrins are
heterophilic molecules that mediate both cell-cell and cell-substratum adhesion2. The
immunoglobulin superfamily is involved in cell-cell adhesion via homo- and heterophilic
interactions. Cadherins are calcium-dependant homophilic cell-cell adhesion proteins3. Selectins
(or LEC-CAMs) mediate white blood cell/endothelial cell adhesion4 and finally homing receptors
target lymphocytes to specific lymphoid tissues. The CAM family that plays a key role in
mediating cell-surface or cell-matrix interactions is the integrin family5.
Integrins are a family of cell adhesion receptors that bind to extracellular matrix ligands, cell-
surface ligands and soluble ligands. They are transmembrane αβ heterodimers and at least
eighteen α and eight β subunits are known in humans, generating twenty-four heterodimers6. The
RGD sequence (arginine-glycine-aspartic acid) in fibronectin was originally identified as an
integrin-binding motifs7. This sequence and related sequences in extracellular matrix molecules
do act as integrin-binding motif. However, integrins also recognize many non-RGD sequences as
ligands8. As far as ligand specificity is concerned, mammalian integrins can bind to, among
others, fibronectin, collagen, laminine, vitronectin, tenascin, thrombospondin, osteopontin or
fibrilin. Some integrins are limited to certain cell types or tissues and other integrins are widely
distributed. Normally, each cell expresses several types of integrins.
Integrins mediate the attachment of the cell to its surroundings and play a role in cell signalling.
They couple the extracellular matrix outside the cell to the cytoskeleton inside the cell. Integrins
are the transducers that directly transmit mechanical stress from the extracellular matrix to the
cytoskeleton and inversely9. This linkage is not only important to stabilize cell adhesion and
morphology but is also involved in cell signalling. The signals received through the integrins
have been shown to be related to cell growth, proliferation, differentiation, viability and
apoptosis10. Table 1.1 shows that the deletion of individual genes coding for integrin subunits, by
gene knockout in mice, plays a critical role in their morphogenesis6. Almost all organs can be
affected.
Chapter1 Introduction
3
Integrin subunit Viability Phenotype
α3 perinatal lethal kidney, lung and skin defects11
α4 embryonic lethal placental and heart defects12
α5 embryonic lethal mesodermal and vascular defects13
α6 perinatal lethal epidermal detachment and neurogenesis defects14
α7 viable muscular dystrophy15
α8 perinatal lethal kidney defect16
αE viable skin inflammation17
β1 embryonic lethal failure to gastrulate18
β3 viable platelet defect19
β4 perinatal lethal epidermal detachment20
β6 viable inflammation of skin and lungs21
β7 viable gut-associated lymphocyte defects22
Table 1.1 Phenotypes of deletions of integrin subunits in the mice6.
1.1.3. At the cell level
FAs serve as stabilizers of the attachment of the cell to its surrounding and as regulators of cell
signalling. Primary adhesion is dominated by single molecule binding23. These connections of the
integrins with the extracellular matrix or a surface induce intracellular signalling cascades leading
to the formation of hierarchically assembled protein complexes called focal adhesions or focal
contacts24,25. FAs usually measure a few square microns across and are located along the ventral
plasma membrane of adherent cultured cells. Recently, it was shown that layilin, a
transmembrane protein, also interacts with the extracellular matrix notably with hyaluronic
acid26,27.
On their cytoplasmic side, FAs are composed of numerous proteins with and without enzymatic
activity that play the role of stabilizer elements, transducers, modulators and adaptors. They are
also associated with the bundles of actin microfilaments of the cytoskeleton. The main
Chapter1 Introduction
4
components of FAs are cytoskeletal proteins such as vinculin, paxilin, tensin, α-actinin, actopaxin
or talin that show no enzymatic activity. Kinases, phosphatases, modulators of small GTPases
and other enzymes are also very important. Many of these components may be expressed in a cell
type specific manner. Figure 1.1 illustrates the complexity of focal adhesions connecting the
extracellular matrix via integrins to the actin fibres of the cytoskeleton28.
Fig. 1.1. Illustration of the components of focal adhesions28. On the extracellular face, integrins engage extracellular
matrix macromolecules and on the cytoplasmic face, integrins coordinate the assembly of focal adhesions.
When cells let go of a surface, they don’t let go of all their integrins29. A substantial proportion of
the integrins is left behind on the substrate as the cell detaches while another fraction is collected
into vesicles30. It has been shown that cells use the endocytic protein clathrin to reabsorb the
integrin receptors that attach them to surfaces, instead of simply leaving the molecules behind31.
Cells may use the reabsorbed integrins to build new FAs but this has not yet been demonstrated.
Chapter1 Introduction
5
1.1.4. Applications
Both cell-cell and cell matrix adhesions are important in multicellular organisms during
morphogenesis and in a variety of basic processes such as proliferation, differentiation, motility,
cellular trafficking, tissue architecture or apoptosis32. Cell adhesion plays an essential role in the
homeostasis of healthy tissues. Unfortunately, cell adhesion can be disrupted and cause a great
variety of diseases.
Some cancers involve mutations in genes for adhesion proteins that result in abnormal cell-cell
interactions. Indeed, changes in the expression or function of cell adhesion molecules have been
implicated in all steps of tumour progression, including the detachment of tumour cells from the
primary site, their intravasation into the blood stream, their extravasation into distant target
organs, and the formation of secondary lesions33. Some people have "blistering diseases" that
result from inherited molecular defects in genes for adhesion proteins. These diseases involve the
formation of a bubble of fluid beneath a thin layer of dead skin. The blisters may start in the
deeper layers of the skin and cover widespread areas. Cell adhesion proteins are also important
for interactions that allow viruses and bacteria to cause damage to humans. Many
pharmaceuticals target the adhesion proteins of viruses and bacteria. Cell adhesion proteins hold
synapses together and the regulation of synaptic adhesion is involved in learning and memory. In
Alzheimer’s disease, there is abnormal regulation of synaptic cell adhesion. The study of cell-
surface interactions allows the indirect study of disturbed cell-cell and cell-matrix interactions in
such diseases.
In contrast, implantology research and tissue engineering are directly focussed on cell-surface
interactions. A goal in the design of bone and dental implants is the development of devices that
induce controlled, guided and rapid healing34. Thus, a better understanding of events at the
interface and of the effects that biomaterials have on bone and bone cells is needed. In tissue
engineering, cells are placed on or within matrices in order to develop functional substitutes for
damaged tissues35.
Cell adhesion has widespread applications. It has been shown that the expression of adhesion
molecules on the surface of cells may change in various diseases. In conclusion, cell adhesion is
fundamental in cancer progression, implantology research, wound healing and against infection
by pathogens.
Chapter1 Introduction
6
1.2. Current techniques for cell adhesion studies Cell adhesion has been investigated using many techniques. Microscope-based techniques
provide qualitative cell adhesion measurements whereas mechanical approaches quantify semi-
quantitatively or quantitatively cell adhesion. The techniques are not described in chronological
order according to their appearance.
1.2.1. Light microscope-based techniques
Light microscopy was used since the earliest examination of cellular structures. Modern light
microscopy provides a variety of imaging techniques and also the capability to perturb biological
structures in living cells in order to study their functions36,37.
Interference reflection microscopy (IRM) has been used to study the adhesion of cells in contact
with planar substrates38. The technique provides information on the separation of the plasma
membrane of the substrate. The interference between the reflected light waves from the substrate-
medium interface and the plasma membrane-medium interface generate an image with high
contrast. IRM allows the visualization of cell-substratum adhesion in living tissue culture cells
continuously for long periods of time without the use of fluorescent markers39.
The use of fluorochrome-conjugated antibodies and green fluorescent protein (GFP)-fusion
proteins produces high-resolution images of the distribution of binding proteins in cells40. Cells
expressing GFP-fusion proteins have been used to determine the compositional dynamics of the
cell adhesion structures. However, the comparison of the relative distributions of the labeled
components in function of the time is not accurate. This problem was partially solved by a
calculation of the pixel by pixel ratio of two fluorescent images41,28. It is particularly suitable for
colocalization studies of proteins forming distinct and defined structures such as focal adhesions.
This spatiotemporal information is important for structure-function studies in cell adhesion.
However, relative change in protein concentration can be estimated but the absolute
concentration of the specific adhesion protein cannot be calculated.
Microscope-based-techniques can also be used for the detection of close protein-protein
interactions using fluorescence resonance energy transfer (FRET)42,43,44. This is a process
involving the radiationless transfer of energy from a donor fluorophore to an appropriately
positioned acceptor fluorophore. FRET can occur when the emission spectrum of a donor
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7
fluorophore significantly overlaps the absorption spectrum of an acceptor and when they are in
favourable mutual orientation. This technique allows the determination of molecular associations
of adhesive components such as the details of the fibronectin fibril assembly process43.
Alternatively, photobleaching techniques have been used to measure the transport of molecules in
living cells or at their surface45,46. The fluorescence of defined regions of the cell was destroyed
and the recovery of fluorescence into those regions reflected the type of transport such as
diffusion or flow. It was used to study the trafficking of cytoskeletal proteins47. The exchange of
α-actinin between the cytoplasmic pool and the focal adhesions was observed. The advantage of
the light-directed technique is the temporal control in the molecular perturbation when compared
to genetic approaches.
In summary, light microscopy-based techniques can be used in situ to study molecular
interactions involved in cell adhesion and dynamics. Specific molecular perturbation in cellular
structures can also be induced. However, cell adhesion is never measured quantitatively.
Although light microscope-based techniques are limited to qualitative images, they are essential
for the implementation of mechanical approaches to measure cell adhesion.
1.2.2. Mechanical approaches for cell population studies
The mechanical behaviour of a living cell cannot be characterized simply in terms of fixed
properties, as the cell structure is a dynamic system that adapts to its local mechanochemical
environment48. An large number of experimental tools have been developed to measure and apply
forces and displacements to probe entire cells as well as individual molecules. Some tools allow
the detection of forces down to the pN regime and displacements down to the Å regime.
In the past, studies were focussed on the mechanical response or mechanical manipulation of
entire cell populations49. A direct manipulation of the substrate to which cells adhere provided a
means of mechanical manipulation50. This approach was used in an attempt to impose cyclic
deformation representative of in vivo conditions for cell adhesion studies. Strains were imposed
and measured via low-resolution displacement sensors and global forces were calculated from
substrate stiffness.
An alternative of providing mechanical stimuli to a cell population through substrate
manipulation was done by controlling the chemical composition. Responses of cells to
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8
mechanical properties of the adhesion substrate were examined by varying the concentration of
one component or the degree of crosslinking in polymeric gels51. The forces imposed by the cells
were not quantified.
Techniques based on force-application measurements have also been developed in order to
detach the cells from their growing substrate. Cells were allowed to adhere on substrates that
were placed in a centrifuge52 (Fig. 1.2A). The centrifugal (normal) force allowed the detachment
of cells and the absolute strength of adhesion varied in function of the cell type. The centrifugal
assay was restricted to comparative cell adhesion measurements. The ratio of cells between the
top and the bottom of the chamber of centrifugation was quantified at a particular spin speed but
no information was obtained at the single cell level.
Fig. 1.2. Schematic of a centrifugal assay52 for cell adhesion studies.
1.2.3. Mechanical approaches for single cell studies
Numerous mechanical approaches for single cells have been used to study the interaction
between cells and substrates. Extensive uses of flexible substrates were used for the detection and
the measurement of traction forces exerted by cells including embedded particle tracking,
micropatterned substrates and microfabricated substrates53.
Marker beads were embedded within a polymeric substrate in order to characterize the traction
forces by two-dimensional displacements of the beads54 (Fig. 1.3A). The displacement of the
beads was measured optically and the corresponding force was calculated via the experimentally
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9
determination of the stiffness of the substrate. Bead-displacement values were translated into a
traction force map using specialized algorithms. In addition, polyacrylamide gels with variable
degrees of cross-linking allowed the modification of the rigidity of the substrate55,56 (Fig. 1.3B).
Micropatterned substrates were fabricated to allow pointwise control of cell adhesion and traction
measurement through displacement of the pattern features57,51,58. Alternatively, micro-fabricated
arrays containing force-sensing elements were developed59,60,61 (Fig. 1.3C). Silicon substrates
were prepared with flexible cantilevers of known bending stiffness with small pads to grow the
cells. The forces exerted by cells on these pads were directly computed by the deflection of the
cantilevers. Otherwise, silicon elastomeric substrates, that were micropatterned to give a regular
array of surface indentations, were also used to measure the surface distortion of the micropattern
caused by cells62.
Fig. 1.3. (A) Schematic of the embedded particle tracking assay reporting cell tractions as displacements of beads
firmly anchored in the film54. (B) Polyacrylamide-based traction assay after mapping the magnitude of stress in
different colors (dyn/cm2)55. (C) Schematic of a force sensitive substrate with an attached cell on the pads of the
flexible cantilevers61.
Traction forces analysis represents a powerful tool that can easily be combined with light
microscope-based techniques to allow experimentation at high spatial and temporal resolution.
There are a number of measurements that are resulting in increasingly accurate estimates of
traction forces in order to correlate the stresses with the adhesive structures. Basically, traction
forces are generated by actomyosin interactions and actin polymerization whereas adhesion
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forces by focal adhesions63. Cell traction forces and adhesion forces can be correlated. However,
none of these approaches quantifies the adhesion forces, or only in a semi-quantitative way via
traction forces. Finally, the resolution of the forces and displacements of these techniques (10-9 N
and 10-7 m) limits the measurements to the single cell level, rather than to the single molecule.
The micropipette aspiration technique was originally developed to study time-dependent
deformation of living individual cells subjected to extracellular pressure. Cells were allowed to
spread for varying amounts of time on glass surfaces and then their free extremity was aspirated
into a micropipette at given pressure levels64 (Fig. 1.4A). Applied aspiration pressure ranged
from 0.1-1000 Pa, with resolution of 0.1 Pa65,66. Displacement of the cell membrane was tracked
by light microscopy with a claimed resolution of ± 25 nm. Then dual pipette assays were used to
pull cells apart and quantify the strength of cadherin-dependent cell-cell adhesion67,68. Cells were
manipulated in suspension, an approach that eliminates matrix-mediated signalling and bypasses
the initiation of intercellular adhesion through filopodial activities occurring during adhesion on a
substrate. Alternatively, one of the two cells could adhere on a surface. The weak point of this
technique is the indirect measurement of the adhesion force via the measurement of the aspiration
pressure and the cell deformation in the micropipette. Computational models of the cell
deformation differ in their interpretation and the cell deformation can also interfere in the
adhesion properties. Although the instrumentation is not commercially available, the technique
has been used successfully for cell-cell interactions.
In contrast to static cell adhesion assays, hydrodynamic shear stress was used to analyze the
immobilization and release of non-adherent cells on surfaces (Fig. 1.4B). Parallel and radial flow
chambers as well as capillaries were used to control the hydrodynamic stress level. The problem
is the development of hydrodynamic shear methods in which there is a clear dose-response
relationship between the number and strength of the adhesion bonds and the measured
hydrodynamic parameter69. The application of a hydrodynamic flow is very useful in analysing
catch bond interactions70,71. A catch bond is a bond that becomes stronger or longer lived when
subjected to tensile mechanical force. This adhesion assay was used to mimic the conditions in
the blood vessel under which leucocytes adhere to vascular endothelial cells72,73. The indirect
computation of the adhesion forces via the hydrodynamic forces involves laborious mathematical
models. Moreover, this technique is limited to short-term adhesion. However, it is useful to
simulate what occurs in blood or lymph vessels.
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Fig. 1.4. Schematic of (A) a micropipette aspiration and (B) a hydrodynamic flow assay74 used for cell adhesion
studies.
Optical tweezers employ light to trap and manipulate cells (Fig. 1.5A). The basic physical
principle underlying optical tweezers is the radiation pressure exerted by light when colliding
with matter75. For transparent materials, light passes through the material but changes direction
upon entering and leaving the material by refraction. A fraction of the light momentum is
imparted onto the refracted material. When a laser beam is focussed tightly by a strong lens, the
effective radiation pressure pulls refractive objects towards the focus and holds it there: an optical
trap. If the laser focus is moved through space, the trapped object is forced to follow. When the
refractive object is pulled away from the laser focus by an external force, the object will scatter
the trapping light, yielding a slight deflection of the ongoing laser light. This allows for three-
dimensional tracking of the position or the force on the trapped object to sub-nanometer or sub-
picoNewton accuracy. Several experimental approaches developed to investigate single cell
mechanics are based on the controlled displacement of dielectric objects that are either attached
to the cell membrane or placed inside the cell. Optical tweezers have been used to study, for
example, short-term adhesion of cells to fibronectin76,77. One drawback is the potential damage to
the cell via radiation. Photo-damage may influence the results because such irradiation levels
were observed to induce a loss of filopodia and a general inhibition of motility78. Moreover,
optical tweezers are limited to the detection of forces in the pN regime and cannot be therefore
employed for the investigation of the global cell adhesion.
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A similar approach to the optical trap is the magnetic trap. Magnetic tweezers that use a magnetic
field gradient can exert and measure forces on magnetic particles coupled to cells (Fig. 1.5B).
The coupling of the magnetic beads to cells was achieved by phagocytosis or covalent
linkage79,80. Magnetic tweezers have been used to measure integrin interactions in initial cellular
adhesion processes81. Two advantages of this approach over optical tweezers are that out-of-plane
rotations and thus torque can be applied, and the elimination of possible damage to the cell via
radiation. A limitation of this technique is that the magnetic susceptibility of the magnetic beads
varies widely, so that these experiments can be difficult to calibrate accurately. Magnetic
tweezers provide great sensitivity but the maximal vertical force of 200 pN that can be applied
greatly restricts their use in studying global cell adhesion, which requires forces in the nN regime.
Optical and magnetic tweezers are unique tools for force microscopy at the cellular level and the
non-contact nature of both techniques removes complicating surface interactions. The low force
regime available with optical and magnetic tweezers means that the nN regime (and higher) can
only be investigated using contact probe methods.
Fig. 1.5. (A) Schematic of optical tweezers48 and (B) magnetic tweezers81 used for cell adhesion studies.
Thus, other techniques such as the microneedle technique were developed to apply and quantify
large forces (in the nN regime) for global cell adhesion investigations. The instrument applies a
mechanical force normal to the cell/substrate interface via a cantilevered probe. The position of
the probe is monitored within an inverted optical microscope via a position-sensitive photodiode
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and the force is calculated from this deflection. Fine glass needles were employed to quantify the
forces needed to displace single adherent cells82. This cytodetachment technique is restricted to
horizontal displacements: only shear stress can be applied instead of normal stress for cell
detachment. Therefore, there is no direct measurement of the normal (vertical) adhesion and the
risk to perforate the cell is not negligible.
Fig. 1.6. (A) Fine glass microneedle82 for cell adhesion studies.
In summary, several methods have been developed for measuring the forces that cells exert on
their substrate, mainly involving the use of deformable substrates. These methods provide
quantitative evaluations of the forces, and some combine this with visualization of the adhesion
sites83,84. However, their capacity to compare the forces applied at the focal adhesions of a cell is
limited. The micropipette assay can be used for simultaneous measurement of separation force
between two cells and detection of fluorescent proteins involved in adhesion. However, the
separation force is not monitored in function of the distance of separation because the position of
the micropipette is controlled by a micromanipulator. Force-distance curves cannot be obtained.
Moreover, this instrumentation is not commercially available and therefore, it is difficult to
establish controls that demonstrate the specificity of the molecular interaction being studied.
Hydrodynamic flow assays are especially useful for cells in suspension such as blood cells.
Optical and magnetic tweezers are very sensitive but they are restricted to the detection of low
forces (pN regime) while global cell adhesion requires the detection of high forces (nN regime).
Finally, the microneedle technique doesn’t have a direct measurement of the vertical adhesion.
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1.3. Atomic force microscopy for cell adhesion studies One of the most promising techniques for the quantification of the adhesion forces is force
spectroscopy, an AFM-based method (Atomic Force Microscopy). The AFM was originally
developed for high-resolution imaging but it has also become a powerful tool to manipulate
biomolecules and cells in a very wide force range. The AFM allows direct force and
displacement measurements from the single cell down to the single molecule level. Force
spectroscopy can be performed in numerous commercially available instruments.
1.3.1. Principle
The atomic force microscope85 is a scanning probe microscope that was developed in 1986. The
AFM can be used to study non-conducting materials, such as insulators and semi-conductors, as
well as electrical conductors. The AFM can operate under ultra high vacuum, ambient air
conditions or in liquid, which is highly useful for biological systems.
The AFM uses a flexible cantilever as a spring to measure the force between the tip of the
cantilever and the sample. The basic principle is that the local attractive or repulsive force
between the tip and the sample is converted into a deflection of the cantilever (Fig. 1.7A). The
deflection of the cantilever is detected via a laser beam that is reflected from the back of the
cantilever onto a detector. A small change in the deflection angle of the cantilever is converted
into a large deflection in the position of the reflected spot. Most AFMs use a photo-sensitive
detector (PSD) that is composed of four quadrants, so that the laser spot deflection can be
determined precisely in two directions.
Originally, the AFM was developed for high-resolution imaging. The detection system measures
the cantilever deflection when the tip is moved over a surface by a scanning system. Different
imaging modes are available: constant height imaging consists of measuring the deflection signal
without changing the height of the cantilever. This is not the most common solution because the
force applied by the cantilever depends on the deflection, so higher parts of the sample will
experience higher applied forces. In contrast, it is much more common to use constant force
imaging. In this mode, a feedback loop monitors the cantilever response and adjusts the
cantilever (or sample) height to take account of the changes in surface height. Thus, all parts of
the probed sample should experience the same force.
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Several forces typically contribute to the deflection of an AFM cantilever, the most common
being relatively weak, attractive van der Waals forces as well as electrostatic repulsive forces.
The general dependence of these forces upon the distance between the tip and the sample is
shown schematically in figure 1.7B. When the tip is less than a few Angströms from the sample
surface, the interatomic force between the cantilever and the sample is predominantly repulsive,
due to the overlap of electron clouds associated with atoms in the tip with those at the sample
surface. In contrast to this contact regime, there is the non-contact regime where the tip is
somewhere between ten to a hundred Angströms from the sample surface. In this case, the
interatomic force between the tip and the sample is attractive as a result of long-range attractive
van der Waals interactions.
Fig. 1.7. Schematic diagram of (A) an atomic force microscope and (B) the tip-sample separation forces86.
1.3.2. Force spectroscopy mode
AFM is also a powerful tool for sensitive force measurements87. Basic force spectroscopy curves
are obtained with a cantilever in air approaching a hard and incompressible surface (such as
glass) (Fig. 1.8). Initially, the cantilever approaches the surface and the forces are too small to
give a measurable deflection. At some point, the attractive forces overcome the cantilever spring
constant and the tip jumps into contact with the surface. Then, the tip remains on the surface and
the separation between the piezo and the sample decreases further causing a deflection of the
cantilever. During the retraction of the cantilever from the surface, the tip remains in contact with
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the surface due to adhesion. At some point, the force from the cantilever will be sufficient to
overcome the adhesion and the tip will break free.
Fig. 1.8. Schematic force curve on a hard surface with (A) approach and (B) retraction curves.
For a soft and compressible biological sample in liquid, the approach force curve shows a gradual
increase in force without the sharp onset of the interactions seen in air (Fig. 1.9A). It is often
difficult to define a single point where the tip and sample come into "contact" since the initial
compression of the surface causes a very little deflection of the cantilever88,89.
Forces curves are obtained directly from the simple relationship between the force and the
cantilever deflection, Hooke’s law:
F = -k dc, where F: force k: spring constant of the cantilever dc: deflection of the cantilever
The interpretation of a force curve relies almost entirely on established force laws. These force
laws describe force as a function of the probe-sample separation distance rather than as a function
of the z-piezo position. Thus, the force curves must be transformed into descriptions of force as a
function of distance. However, current AFMs do not have an independent measure of the probe-
sample distance. Instead, the transformation to distance is achieved by subtracting the cantilever
deflection from the z-piezo movement. A corrected force curve is called a force–distance curve
(Fig. 1.9B).
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Fig. 1.9. Schematics of (A) an uncorrected force curve and (B) a corrected force curve (force-distance curve)90. At
the beginning of the curve (i), the tip is far from the sample and there is no interaction and no cantilever deflection.
The approach brings the tip closer to the sample, and long- and short-range tip-sample interactions cause the
cantilever to deflect (ii). When the tip contacts the surface, the stage movement and cantilever deflection become
coupled (iii). The retracting curve displays hysteresis due to a variety of tip-sample interactions.
1.3.3. Single bio-molecule force spectroscopy
Force spectroscopy can be used to examine rupture forces of molecular bonds and ligand-receptor
interactions, unfolding and folding of various proteins in a stepwise process, extraction of a
protein from a membrane, DNA mechanics or polysaccharide stetching91,92,93,94,91,95. Such an
approach to measuring forces is unique in that components of a single unbinding or unfolding
event can be directly monitored. The flexibility of the AFM is such that force spectroscopy can
be conducted on samples ranging from individual membrane proteins to complex and
heterogeneous whole cells in their native environment. At the cell level, the bond rupture events
represent a combination of the unbinding of ligand-receptor complexes and the disruption of non-
specific binding events.
Adhesion forces between individual ligand-receptor pairs were already quantified more than
fifteen years ago using force spectroscopy on biotin and avidin96. This ligand-receptor pair was
chosen as a model system because of its high affinity and the availability of thermodynamic and
structural data on it. The bond rupture forces were reported for fixed pulling velocities and spring
constants. Further details about the interaction potential of the biotin-avidin pair were revealed by
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18
dynamic force spectroscopy97. Similar experiments were reported on the protein A-IgG bond98,99.
The analysis and interpretation of these experiments can be complex, since bond dissociation is a
non-equilibrium dynamical process100. Bonds in cell adhesion are therefore being continually
created, loaded over some period of time and then failing. They will fail under any level of
pulling force if held for sufficient time101. The kinetics of the anchoring process during the
adsorption of fibrinogen molecules on silica surfaces was for example explored102.
In single molecule unfolding experiments, the force applied to a single protein acts as a
denaturant leading to complete unfolding of its three-dimensional structure103. In an early study,
Rief and co-workers applied single molecule force spectroscopy to the giant muscle protein titin
which consists of repeats of globular immunoglobulin and fibronectin domains104,105. The
continuous mechanical extension of the protein resulted in the subsequent unfolding of the
globular domains allowing the unfolding force and pathway of each domain to be detected.
Similarly, individual bacteriorhodopsin molecules were unfolded and extracted from purple
membrane patches from Halobaterium106,107,108. Force spectroscopy was also employed to unfold
single sodium-proton antiporters of Escherichia membrane patches. Some fundamental
differences have to be considered when the forced unfolding by mechanical manipulation is
compared with the classical experiment in which a protein is unfolded by means of chemical
denaturants or by exposure to heat109. As mentioned for receptor-ligand pairs, the unfolding force
of proteins depends also on the force loading rate110. Secondly, mechanically forced unfolding
may proceed via a different path along the protein’s configurational energy landscape than the
thermal process111.
DNA molecule mechanics has also been investigated. Sequence-dependent mechanical properties
of DNA have been measured by stretching individual DNA double strands attached between a
surface and an AFM tip112 (Fig. 1.10). The forces needed to open the double strands showed
variations between 10 and 20 pN on a length scale of 10 bases.
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Fig. 1.10. Complementary DNA oligonucleotides are chemically attached to an AFM tip and a glass surface. As the
tip is brought in contact with the surface a double strand forms, which can subsequently be unfolded upon retraction
of the tip113.
Single molecule force spectroscopy has also been used to study DNA-protein interactions114.
Overstreched structures of DNA were shown to be stabilized by a protein. Alternatively, direct
force measurements were performed to mechanically unbind a transcriptional regulator protein
that binds to promoter regions in a gene cluster115,116.
The AFM has been used to stretch individual molecules of polysaccharides. Deflections in the
force extension curves for certain polysaccharide molecules were shown to be due to conversion
of the polysaccharide rings in the chain from the energetically favoured “chair” conformation to
the longer “boat” conformation117,118. Dextran molecules were also manipulated and probed by
vertical stretching revealing details of the molecular basis of the mechanical properties of the
polysaccharide that could not have been obtained otherwise. At low forces, the deformation of
dextran was found to be dominated by entropic forces and at elevated forces the strand elongation
was governed by a twist of bond angles119.
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Force spectroscopy has rapidly evolved and is now on the verge of becoming a standard
technique for the structural and functional investigations of bio-molecules120,121. It allows the
characterization of interactions that stabilize functional membrane proteins as well as those that
destabilize them, leading to malfunction and misfolding. This new tool has more recently been
used to investigate bio-molecules in their native environment using entire living cells as probes:
single cell force spectroscopy.
1.3.4. Single cell force spectroscopy (SCFS)
Living single cell force spectroscopy allows the adhesion of cells and single adhesion proteins to
be studied under near-physiological conditions122. The advantage of using living cells rather than
single proteins is that the receptors probed are under physiological conditions and that they can
interact with the cytoskeleton or other components of the cell. It also ensures the correct
orientation, surface density and posttranslational modification of the proteins.
The first single cell force spectroscopy experiment to investigate cell adhesion in vivo at the
single molecule level was reported by Benoit and co-workers123 in 2000. It should be noted that
previously force spectroscopy had been widely used for cell mechanics measurements such as
estimations of Young’s moduli124,125 (more details in section 2.7.2). Benoit’s measurements were
focussed on the interaction of the glycoprotein contact site A (csA) between two eukaryotic cells
of Dictyostelium. CsA is expressed in aggregating cells of Dictyostelium which are engaged in
the development of a multicellular organism. Using a light microscope, a Dictyostelium cell was
captured on the end of a tipless AFM cantilever. The end of the cantilever was functionalized
with a lectin to give a firm attachment of the cell to the cantilever. A target cell was positioned
underneath the cantilever-mounted cell and was approached until a repulsive contact force was
established. This contact force was held constant for a predefined time interval to allow the
establishment of cell adhesion. Upon retraction of the cantilever, the force was recorded as a
function of the distance that the cantilever was moved until contact between the cells were broken
(Fig. 1.11). A de-adhesion force of 23 pN was quantified which may be due to discrete molecular
entities.
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21
Fig. 1.11. Force spectroscopy of adhesion between individual Dictyostelium cells123.
The use of living cells as probes to study receptor-ligand interactions has been carried out using
many cell types. Several studies have focussed on the characterization of integrin interactions
with their ligands on a surface. The unbinding forces of integrins with fibronectin126,127,
collagen128, V-CAM1129,130 (V: vascular), I-CAM1131,132,133 (I: intercellular) and I-CAM2134 have
all been determined. The integrin-fibronectin adhesion forces obtained range from 35 to 80 pN.
The wide range of values obtained might indicate that the strength of the receptor-ligand
interaction depends on the experimental conditions. Indeed, it has been reported that α5β1-
integrin-fibronectin adhesion force on K562 cells varied depending on the force-loading rate
from 40 to 140 pN135. The unfolding and detachment of fibronectin from surface may also
interfere. Other possible influences on the forces measured include non-specific binding of
fibronectin to the cell, extraction of integrins from the cell membrane, temperature, or changes in
cell properties such as membrane fluidity that could result in altered integrin mobility. However,
there is close agreement about the scale of forces required to rupture the bond between integrins
and their ligands. Unfortunately, experimental conditions have not been standardized and are
often not sufficiently documented to allow rigorous comparisons between experiments.
Several CAMs mediate only cell-cell adhesion such as cadherins and selectins. It has proved
difficult to characterize individual cell-cell adhesion events given the heterogeneous and complex
nature of cell surfaces. AFM-based force spectroscopy is capable of resolving such individual
cell-cell binding events but is limited in these kind of applications due to insufficient effective
pulling distances136. Long range force spectroscopy has been made possible by the development
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22
of two AFM instruments by Asylum Research (USA) and JPK Instruments (Germany) with
extended vertical ranges of 40 and 100 µm respectively. Using these instruments, homophilic and
heterophilic binding capabilities of E-cadherin and N-cadherin have been compared137. Individual
E- and N-cadherin displayed different biochemical and biophysical properties. The kinetic of
cadherin pairwise bonds formation was also probed138. Similarly, it has been shown that the
visually distinct rolling patterns of leukocytes over selectin substrates are a consequence of the
kinetic and mechanical properties of the participating adhesive groups139.
The use of living cells to study global cell adhesion has been poorly investigated. It is
fundamental to distinguish affinity-based from avidity-based studies. The affinity describes the
strength of a single bond between an individual receptor on the surface of a cell and its ligand on
another cell or a surface. The avidity describes the global adhesion between two cells or between
a cell and a surface. The affinity of all the individual receptors to their ligands control the overall
adhesiveness (avidity) and for that reason, it is also important to investigate the global cell
adhesion. The interpretation of global cell adhesion is much more complex because avidity
depends on a multitude of biochemical and biophysical parameters. There is certainly the
possibility to extrapolate multiple-bond avidity to evaluate single-bond affinity but the
assumptions are not realistic. Avidity may depend on the density and affinity of the receptors for
their ligands as well as on their spatial arrangement and orientation. The surface area with the
probed cell, the duration of contact, the local geometry and stiffness of the plasma membrane,
and the rate of surface diffusion of cell receptors play also important roles140.
Short-term global cell adhesion has been used to compare the global cell adhesion properties of
wild-type embryonic cells from mutant embryonic cells, that carry a loss-of-function mutation in
a gene involved in gastrulation movements141,142. These findings suggested that the Wnt11 gene
is needed for the adhesion of zebrafish mesendodermal progenitor cells to fibronectin during
gastrulation.
Finally, long-term global cell adhesion has never been successfully reported in the literature. It
has been partially explored in a PhD thesis143. Fibroblasts were allowed to adhere to substrates
and then detached with a functionalized cantilever. The fraction of the probed cells that were
successfully detached was not sufficient (less than forty percent) to quantify significantly the
cellular adhesion forces.
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23
1.4. SCFS configurations Cell-surface interactions can be investigated using SCFS in several configurations144,145,94,91.
Figure 1.12 summarizes the feasible SCFS configurations. Firstly, the contact time of the
interaction between a cell and a surface can be either short (I-IV) or long (V-VIII). In this thesis,
short-term adhesion is defined as contact times from seconds to minutes whereas long-term
adhesion is defined as contact times from hours to days. Therefore, short-term adhesion
measurements involve cells showing a round morphology in contrast to long-term adhesion
where cells have time to spread and to react to the surface. Secondly, the interaction surface that
is studied can be either the substrate or the cantilever. Finally, the cell can either stay on its initial
surface or be captured and transferred to the opposite surface. The study of cell-surface
interactions can be categorized in eight configurations:
(I) Short-term adhesion measurements have been widely investigated for receptor-
ligand interactions using living cells as probes with the cell on the
cantilever129,135,128,134,132,130,133. To date, global short-term adhesion has been poorly
quantified141,142.
(II) The transfer of a cell from the surface to the cantilever is used to perform short-
term adhesion measurements with the cell on the cantilever (configuration I).
(III) Short-term adhesion measurements have also been widely investigated for
receptor-ligand interactions using living cells as probes with the cell on the
substrate126,131,127.
(IV) The transfer of a cell from the cantilever to the substrate can happen during a
prolonged contact time between the cell and the substrate.
(V) In contrast, long-term adhesion measurements have been very little explored.
Long-term measurements with adherent cells on the substrate were restricted to the
analysis of the mechanical properties of cells124,125.
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Fig.
1.1
2. S
ingl
e ce
ll fo
rce
spec
tros
copy
con
figur
atio
ns fo
r cel
l-sur
face
inte
ract
ions
.
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(VI) The detachment of living single adherent cells has never been successfully
reported in the literature. It was partially explored in a PhD thesis but only a small
fraction of the probed cells were successfully detached from their growing
substrate143. This fraction was not sufficient to quantify the cellular adhesion
forces.
(VII-VIII) Finally, the direct growth of cells on the cantilevers for long-term adhesion in
order to quantify their adhesion forces has not been reported.
1.5. Dissertation objectives The main objective of this work is to use force spectroscopy to quantify the long-term global
adhesion between cells and surfaces and their response to modified surfaces. Long-term adhesion
measurements are important to allow the cells to spread and their adhesion proteins to be renewed
in order to react to their growing substrate.
Many techniques have been proposed for the quantification of cell adhesion. AFM-based force
spectroscopy has been shown to be a versatile tool allowing the quantification of receptor-ligand
interactions in living cells.
The quantification of long-term cell adhesion involves adherent cells. The first objective of this
work is to determine if the cell cycle influences cell adhesion or not. Cells in interphase all show
the same morphology under the microscope and therefore cannot be selected as a function of their
progression through the distinct phases of the cell cycle.
The quantification of long-term adhesion requires the detachment of adherent cells from their
culture substrate. The challenge is to find a method of attachment, between cells and atomic force
microscope cantilevers, that allows their detachment from the surface. The establishment of the
attachment has to be quick in order to avoid cell adhesion modifications.
The next step is to validate the technique for the detection of the effects of surface modification
on cell adhesion. The application of the technique in tissue engineering and implantology is
particularly interesting because both research fields are directly focused on cell-surface
Chapter1 Introduction
26
interactions. The objective is to determine if long-term adhesion measurements might be useful in
the development of surfaces for tissue engineering. Long-term cell adhesion forces are quantified
on chemically modified surfaces used in cell sheet engineering in order to correlate the results
with the qualitative effects already reported.
In order to investigate the sensitivity and limitations of the detachment of adherent cells by force
spectroscopy, different experimental parameters can be altered. Surface topography is easily
tunable and its effects on cell adhesion have been widely studied. Another objective therefore is
to analyze the effects of topographical surface modifications on cell adhesion and to evaluate the
possible contribution to bone implant applications. Here cell type is especially important since
both immortalized and primary cells have been studied and very different results have been found
for different cell lines and primary cells. An objective therefore is to compare the detachment of
different cell types in order to determine the potential of the technique in this respect.
1.6. Organization of the dissertation
The dissertation starts with one chapter describing the materials and the experimental techniques
used in the next four chapters focussed on cell adhesion measurements.
Chapter 3 describes the short-term adhesion of Saos-2 human osteosarcoma cells to a glass
surface during the cell cycle. This first experimental chapter examines the effects of the different
phases of the cell cycle on cell adhesion in order to determine if cell adhesion has to be studied
independently of cell cycle or not. The cells were synchronized in three phases of the cell cycle,
trypsinized to release them from the culture surface and captured on a cantilever. Cell adhesion
was compared with unsynchronized cells. Short-term adhesion was used to study the adhesion
proteins already exposed at the cell surface in each phase of the cell cycle without influence of
the glass surface.
Chapter 4 focuses on long-term adhesion measurements with adherent cells. The challenge is to
find a method of attachment, between cells and atomic force microscope cantilevers, that allows
their detachment from the surface. Long-term adhesion on a glass surface was used and several
cantilever functionalizations were tested. Saos-2 osteoblasts were replaced by immortalized 3T3
and primary mouse fibroblasts.
Chapter1 Introduction
27
Chapter 5 presents the quantification of 3T3 cell adhesion to chemically modified glass surfaces
used for cell sheet engineering. This chapter studies the effects of surfaces modifications on cell
adhesion in order to validate the technique. The cells were grown on different polyelectrolyte
multilayers and on poly(N-isopropylacrylamide) films before their detachment.
Chapter 6 presents the quantification of 3T3 and primary fibroblasts to topographically modified
quartz surfaces in order to investigate the sensitivity, the potential and limitations of the
technique. Two cell types were grown on different topographies and their properties of
detachment were compared.
Finally, the last chapter recaps the objectives in their context and summarizes the main
conclusions of the dissertation with an outlook for future work.
Chapter1 Introduction
28
Chapter 2 Materials and Methods
29
Chapter 2
Materials and Methods
The materials and experimental techniques used in this thesis are described in this chapter. In
some cases more detailed explanations about the specific experiments are included in the
individual chapters.
Chapter 2 Materials and Methods
30
2.1. Substrate preparation The substrates used were either glass or quartz surfaces.
2.1.1. Cleaning protocol
Glass coverslips (Milian, Switzerland) and quartz wafers (Si-Mat, Germany) were cleaned in
Piranha solution (H2SO4/H2O2) (4: 1)v/v for 10 min at 120 °C. The substrates were rinsed in
flowing water (MilliQ 185 plus, Millipore AG, Switzerland) and dried in a nitrogen flow. Piranha
solution reacts violently with all organics and should be handled with care.
2.1.2. Surface modification with polyelectrolytes*
The cleaned glass coverslips were treated with an oxygen plasma for 2 min. Poly-L-lysine
hydrobromide (PLL, Mw ~15 - 30 kDa, Sigma, Switzerland) and hyaluronic acid sodium salt
from bovine vitreous humor (HA, Mw ~300 kDa, Sigma, Switzerland) were used at a
concentration of 0.5 mg/ml in buffer solution. The buffer solution was 10 mM 4-(2-
hydroxyethyl)-1-piperazine ethanesulfonic acid (HEPES) with 150 mM NaCl, pH adjusted to 7.4
with NaOH.
The polyelectrolyte multilayers were built up on the substrates by spray deposition, using a
custom-made automated spraying system. Four parallel Paasche VLS airbrushes (Paasche
Airbrush Co., IL, USA) connected to a compressor with pressure control allowed for the spraying
of each polyelectrolyte or buffer solution at a constant pressure of 1 bar, with one airbrush for
each different solution. A Lego Mindstorms NXT programmable robotics kit (Lego Group,
Denmark) was used to fabricate a spraying device with programmable spraying time, pause time
and sequence order. The cleaned substrates were placed on a sample holder allowing for drainage
of the solutions, fixed at a distance of 19 ± 2 cm from the airbrush aperture and tilted at 45°. Each
solution was sprayed according to the following sequence: 5 s polyelectrolyte spraying, 15 s
pause, 5 s buffer spraying, 5 s pause. In this way, the deposition of each bilayer required one
minute. The substrates were rinsed and conserved in the buffer solution.
______________________________________________________________________________*The surface modification with polyelectrolytes was done by O. Guillaume-Gentil at ETH Zurich (Switzerland).
Chapter 2 Materials and Methods
31
2.1.3. Preparation of PNIPAM-grafted surfaces
A thin layer of chromium (2 nm) and another of gold (20 nm) were deposited on the cleaned
glass coverslips by evaporation (Auto 306 Turbo, Edwards, France). A self-assembled monolayer
of 11-mercaptoundecanoic acid (SAM-COOH) was prepared on the gold surface by immersion of
the coverslips in a 2 mM ethanolic solution of 11-mercaptoundecanoic acid (Sigma, MO, USA)
overnight. Finally, the samples were sonicated for 30 s in ethanol and dried in a nitrogen stream.
Amine-terminated poly(N-isopropylacrylamide) (NH2-PNIPAM) with an average molecular
weight of 41 000 g/mol (Polymer Source, Canada was grafted under melt onto anhydride reactive
SAMs (SAM-ANH). The activated anhydride groups were obtained by immersion of the SAM-
COOH in a solution of dimethylformamide containing 0.1 M of trifluoroacetic acid (Sigma, MO,
USA) and 0.2 M of triethylamine (Sigma, MO, USA) for 20 min followed by several washing
steps in dimethylformamide. A PNIPAM film was spin-coated from a 1% w/v ethanolic solution
onto the reactive SAMs at 3000 rpm for 20 s. The substrates were then placed in an oven and
annealed at 150 °C for 5 h. The PNIPAM-grafted surfaces were finally rinsed in ethanol for 1 h
and in deionized water overnight to eliminate the excess of polymer.
2.1.4. Preparation of patterned PNIPAM-grafted surfaces
Patterned PNIPAM-grafted surfaces were obtained using the same method except that the
uniform layer of gold was replaced by a pattern of squares of gold. The squares, 3 x 3 µm, with
an inter-space of 6 µm were obtained by classical photolithography and lift-off. The height of the
gold structures was 20 nm.
2.1.5. Micro-fabrication of low aspect-ratio pillars in quartz*
Low aspect-ratio (270nm high) quartz pillars were fabricated using a modified procedure
previously reported for silicon146. In a first step, a polymer blend thin film was deposited on the
four inch quartz wafers. Poly(methyl methacrylate) (PMMA, Mw=106 kDa, Polymer Standard
Services, Germany) and polystyrene (PS, Mw=101 kDa, Polymer Standard Services, Germany)
were dissolved in dioxane at a concentration of 15 mg/mL to give stock solutions. These were
mixed to obtain a PS/PMMA ratio of (30: 70)w/w. The polymer blend solution was then spin-
______________________________________________________________________________*The microfabrication of pillars in quartz was done by N. Blondiaux & M. Klein at CSEM Neuchâtel (Switzerland).
Chapter 2 Materials and Methods
32
coated onto the substrate under a controlled atmosphere (T °C=21 °C and RH=35 %) using a two
step spin-coating procedure: 2 s at 500 rpm followed by 60 s at 2000 rpm. The resulting thin film
was structured in two phases, one of which (PS) was removed by rinsing the sample in
cyclohexane to reveal the quartz surface underlying the PS areas.
In the second step a durable etch mask was fabricated from the thin polymer film. The polymer-
coated surface was first exposed to an oxygen plasma (O2, 50 sccm, 0.05 torr, 15 W) for 90 s
using an RIE plasma (Plasmalab 80plus, Oxford Instruments, United-Kingdom) to remove any
residual PS layer and expose the quartz substrate. A 10 nm thick chromium layer was then
deposited on the sample using a thermal evaporator (Lab 600H, Leybold Optics, Germany). The
remaining PMMA phase and its chromium layer were removed by sonication in acetone.
The last step was the etching of the quartz, which was carried out in a deep reactive ion etcher
(DRIE) (AMS 200, Alcatel, France) using fluorine chemistry. After etching, the samples were
dipped for 5 min in a chromium etchant CR-7, then cleaned in SC-1 solution
(H2O/NH4OH/H2O2) (5: 1: 1)v/v for 10 min at 70 °C and finally exposed to an oxygen plasma
(RIE, O2, 100 sccm, 0.2 torr, 100 W) for 1 h.
Prior to cell seeding, the quartz surfaces were activated with an oxygen plasma (Harrick plasma,
NY, USA) for 10 min and then incubated in a solution of 0.01 % poly-L-lysine (MW = 150-300
kDa, Sigma, MO, USA) for 30 min to promote cell attachment.
2.1.6. Micro-fabrication of high aspect-ratio pillars in quartz*
The above procedure could be used to fabricate quartz pillars up to 270 nm high. However,
further etching resulted in mask failure. For this reason, an alternative procedure was developed
for higher aspect-ratio structures. A 200 nm layer of amorphous silicon (a-Si) was first deposited
on the quartz by means of LPCVD (Centrotherm Furnace, Germany). The chromium etch mask
was then fabricated on top of the a-Si layer as described above. The chromium layer was used as
an intermediate etch mask that was transferred into the a-Si layer using DRIE. The good etch
selectivity and the relatively thick (200 nm) a-Si mask, allowed the fabrication of deeper
structures in the quartz. After fabrication, the cleaning procedure was the same as for 270
______________________________________________________________________________*The microfabrication of pillars in quartz was done by N. Blondiaux & M. Klein at CSEM Neuchâtel (Switzerland).
Chapter 2 Materials and Methods
33
nm pillars except that the samples were also exposed to KOH after the chromium etchant step in
order to remove the a-Si layer.
2.1.7. Sterilization protocol
The surfaces were sterilized with ethanol before their use in cell culture experiments. The
surfaces were successively immerged in 70% ethanol for 10 s, absolute ethanol for 10 s and
rinsed thrice in sterile deionised water.
2.2. Cell culture Three cell types were used including immortalized human osteoblasts, immortalized mouse
fibroblasts and primary mouse fibroblasts.
2.2.1. Saos-2 osteosarcoma cells
The human osteosarcoma cell line, Saos-2, was obtained from American Type Culture Collection
(Manassas, VA, USA) and was maintained in continuous culture in McCoy’s 5A medium
supplemented with 10% heat-inactivated standardized fetal bovine serum (Biochrom AG,
Germany), 50 units/ml of penicillin (Sigma, MO, USA), 50 µg/ml of streptomycin (Sigma, MO,
USA) and 1.5 mM of L-glutamine (Sigma, MO, USA) at 37°C in a humidified 5% CO2
atmosphere.
2.2.2. 3T3 mouse fibroblasts
The mouse fibroblast cell line, 3T3, was obtained from Marinpharm GmbH (Luckenwalde,
Germany) and was maintained in continuous culture in Dulbecco’s Modified Eagle Medium
(DMEM) supplemented with 10% heat-inactivated standardized fetal bovine serum (FBS,
Biochrom AG, Germany), 50 units/ml of penicillin (Sigma, MO, USA), 50 µg/ml of streptomycin
(Sigma, MO, USA), 1.5 mM of L-glutamine (Sigma, MO, USA) and 1% of non-essential amino
acids (Bioconcept, Switzerland) at 37 °C in a humidified 5% CO2 atmosphere.
Chapter 2 Materials and Methods
34
2.2.3. Primary embryonic mouse fibroblasts
Primary mouse embryonic fibroblasts (PMEF) were isolated from embryos derived from C57
mothers between 12 and 14 days of gestation. Embryos were cut into small pieces and incubated
with a solution of 2.5 g/l trypsin and 0.38 g/l of ethylenediaminetetraacetic acid (EDTA) for 20
min at 37 °C under agitation after removing extracellular tissue, head and liver. Trypsin was
inactivated by addition of DMEM containing 10% FCS and cells were purified by successive
steps of filtration and centrifugation. Cells were maintained in DMEM supplemented with 10%
heat-inactivated standardized fetal bovine serum (FBS, Biochrom AG, Germany), 50 units/ml of
penicillin (Sigma, MO, USA), 50 µg/ml of streptomycin (Sigma, MO, USA) at 37 °C in a
humidified 5% CO2 atmosphere.
2.2.4. Cell cycle synchronization
Saos-2 cells were grown to about 60% confluency. Cell cycle arrest in late G1 phase was induced
using mimosine (Sigma, MO, USA) synchronization. Mimosine was added to a final
concentration of 0.4 mM and the cells were incubated for 48 h.
Cell cycle arrest in late S phase was induced using thymidine (Sigma, MO, USA)
synchronization. Thymidine was added to a final concentration of 4 mM and the cells were
incubated for 48 h. Cells were then washed twice in PBS and incubated with regular medium for
8 h.
Cell cycle arrest in G2M phase was induced using nocodazole (Sigma, MO, USA)
synchronization. Nocodazole-treated cells enter mitosis where they are blocked since they cannot
form metaphase spindles. Nocodazole was added to a final concentration of 0.6 µg/ml and the
cells were incubated for 48 h. Cells were then purified by gentle shaking and by pipetting them
off the dish.
Native mitotic cells were also studied. These were obtained by agitating unsynchronized cultures
of cells to detach mitotic cells from the polystyrene culture surface and then pipetting off the
resulting cells147,148.
2.2.5. Cell proliferation assay
Cells were incubated for 18 h in complete medium before adding Alamar Blue (dilution 1: 10,
Chapter 2 Materials and Methods
35
Invitrogen, CA, USA) for 6 h. Aliquots were transferred to a spectrofluorimeter (Infinite M200,
Tecan, Switzerland) and the fluorescence intensity (λex= 530 nm and λem= 590 nm) was
measured. The remaining Alamar Blue was removed and replaced with fresh complete medium
for similar measurements at 2, 3 and 4 days.
2.2.6. Cell seeding
Cells were detached from the culture dishes by incubating with a solution of 2.5 g/l trypsin and
0.38 g/l of EDTA for 5 min. The dissociated cells were seeded on the surfaces following the
regular conditions of cultivation. Cell detachment experiments were performed in regular
medium supplemented with 25mM HEPES at 37 °C in a temperature-controlled chamber.
G2M synchronized and native mitotic cells were already partially or completely detached from
the culture dishes but were also exposed to trypsin under identical conditions.
2.3. Instrumentation
2.3.1. Atomic force microscope (AFM)
The atomic force microscope (AFM) is one of the family of scanning probe microscopes and was
invented in 198685. It is widely used in biological applications. The AFM uses a flexible
cantilever as a type of spring to measure the force between the tip and the sample. The attractive
or repulsive force between the tip and the sample is converted into a deflection of the cantilever.
This cantilever deflection is detected with a laser beam that is reflected from the back of the
cantilever onto a detector. A small change in the deflection angle of the cantilever is converted to
a measurable large deflection in the position of the reflected spot on the photodiode-detector.
Piezoelectric elements are used to control the position of the cantilever.
AFM is particularly suited for biological applications because the samples can be probed in
physiological conditions. There is no need for staining or coating. The AFM is best known for its
high-resolution imaging capabilities but it is also a powerful tool for sensitive measurements in
force spectroscopy mode. In this mode, the base of the cantilever is moved in the vertical
direction towards the surface using the piezo and then retracted again.
Chapter 2 Materials and Methods
36
A Nanowizard® II BioAFM (JPK Instruments, Germany) was used .It has been developed for life
science research reaching from cell biology and biophysics to surface science and biomedicine.
The Nanowizard® was mounted on an Axiovert 200 inverted optical microscope (Carl Zeiss,
Germany) (Fig. 2.1). A CellHesion® module expended the vertical travel range of the
Nanowizard® to 100 µm by integrating a precise sample lift mechanism into the AFM stage. An
incubation chamber, the BioCell™ (JPK Instruments, Germany), maintained the sample at the
desired temperature (Fig. 2.2).
The atomic force microscope was mainly used in force spectroscopy mode to study cell/surface
interactions at the both cell and molecule levels.
Fig. 2.1. Pictureof the Nanowizard® II life science setup mounted on an inverted optical microscope. The stage and
AFM head are shown sketched separately. The micropositioners to move the sample, represented by a red glass
slide, are surrounded in red (A) and the micropositioners to move the AFM head are surrounded in blue (B).
Chapter 2 Materials and Methods
37
Fig. 2.2. (A) Pictureof the Nanowizard® II life science setup used in this work and, (B) the BioCell™ as a add-on for
the temperature-dependent study of living cells in their native environment.
2.3.2. Fluorescence activated cell sorter (FACS)
Flow cytometry is a technology that simultaneously measures and analyzes multiple physical
characteristics of single cells flowing in a fluid stream through a beam of light. Size, granularity
and fluorescence intensity are measured. These characteristics are determined using an
optoelectronic system that records how the cells scatter the incident laser light and emit
fluorescence.
A flow cytometer is composed of three systems including fluidics, optics and electronics. The
fluidics system transports the cells in a stream to the laser beam for exposure. The optics system
consists of lasers to illuminate the cells in the sample stream and optical filters to direct the
resulting light signals to the appropriate detectors. The electronics system converts the detected
light signals into electronic signals that are processed by the computer (Fig. 2.3). Some
instruments are equipped with an electronics system capable of sorting the cells as a function of
their characteristics.
Chapter 2 Materials and Methods
38
Fig. 2.3. Scattered and emitted light signals are converted to electronic pulses that are processed by the computer.
A FACSAria cell sorter (Becton Dickinson, CA, USA) was used to determine the relative cellular
DNA content during the various phases of the cell cycle using the fluorescent dye propidium
iodide. The incorporated amount of dye was proportional to the amount of DNA. Three distinct
phases were determined including the G1, S and G2M phases. G2 and M phases have an identical
DNA content and cannot be distinguished.
2.3.3. Confocal microscope
Confocal microscopy offers several advantages over conventional optical microscopy: the depth
of field is controlled and all the out of focus structures are suppressed at image formation. The
confocal approach uses spatial filtering to eliminate out-of-focus light in specimens that are
thicker than the focus plane. The confocal microscope offers also the ability to collect serial
optical sections from thick specimens. The cells were imaged with the confocal Leica TCS SP5
(Leica Microsystems, Germany).
2.3.4. Scanning electron microscope (SEM)
A scanning electron microscope (SEM) is a microscope that uses electrons instead of light to
form an image. The image is produced in vacuum by probing the specimen with a high-energy
focused electron beam. The incident electron beam loses some energy at each point on the
specimen that is converted into emission of secondary electrons, back-scattered electrons,
characteristic X-rays, light and heat. The display maps the varying intensity of any of these
Chapter 2 Materials and Methods
39
signals to generate the image.
The samples were imaged with the XL-30 ESEM (Royal Philips, Netherlands) using secondary
electrons since they are the most sensitive to topography.
2.4. Force-distance curves Throughout this work “short-term adhesion” was defined as short cell-substrate contact time
(tcontact = 1 s). The cell was captured on the cantilever before the measurement. In contrast, “long-
term adhesion” was used for long cell-substrate contact time (tcontact = 24 h). In this case, the cell
was grown on the substrate and then detached with the cantilever.
2.4.1. Cantilevers for short-term adhesion
AFM cantilevers were functionalized with concanavalin A using a protocol adapted from
Wojcikiewicz et al149. 500µm long tipless silicon cantilevers (Arrow TL1, Nanoworld,
Switzerland) with a nominal spring constant of 0.03 N/m were used for all short-term adhesion
measurements. Cantilevers were cleaned in an oxygen plasma (Harrick plasma, NY, USA) for 5
min, and then incubated overnight at 37°C in a solution of 0.6 mg/ml biotinamidocaproyl-labeled
bovine serum albumin (Sigma, MO, USA) in 100 mM NaHCO3, pH 8.6. The cantilevers were
then rinsed twice in PBS, incubated in a solution of 0.6 mg/ml streptavidin (Sigma, MO, USA) in
PBS at pH 7.3 for 30 min. After two further rinses in PBS, they were finally incubated in a
solution of 0.6 mg/ml biotin-labeled concanavalin A (Sigma, MO, USA) in PBS for 60 min.
Cantilevers were calibrated in water before each measurement using the thermal fluctuation
method.
2.4.2. Cell capture for short-term adhesion
Using the AFM in force capture mode, the extremity of a concanavalin A-decorated cantilever
was precisely positioned above one cell. An approach step brought cell and cantilever into
contact for 2 s. This was immediately followed by a retraction step to remove the cell from the
surface. The cell was then left undisturbed on the cantilever for 15 min to ensure strong adhesion
between cell and cantilever.
Chapter 2 Materials and Methods
40
2.4.3. Short-term adhesion measurements
Force distance curves were acquired with an approaching and retracting speed of 5 µm/s using
the maximum z-range of 100 µm. The cell was approached towards the surface until a repulsive
force of 900 pN was reached. It was left in contact with the surface for 1 s before the retract step
was started. There was a pause of 60 s at the maximal retract distance between each measurement
(Fig. 2.4).
Fig. 2.4. Schematic illustrating a short-term adhesion measurement with a contact time of 1 s between the cell and
the substrate.
For each cell the first and last force distance curves were compared to ensure that there were no
gross differences due to cell damage. To ensure that the cell-surface contact areas were similar
for all measurements, the largest and smallest cells of each population – in total no more than
20% of the population – were excluded from measurements.
2.4.4. Cantilevers for long-term adhesion
AFM cantilevers were functionalized with fibronectin to promote cell adhesion143. 130 µm long
silicon tipless cantilevers (NSC12, Mikromasch, Estonia) with a rectangular shape and a nominal
spring constant of 4.5 N/m were used for all long-term adhesion measurements. Cantilevers were
cleaned in piranha solution at 120°C for 10 min and activated with an oxygen plasma (Harrick
Plasma, NY, USA) for 3 min. The cantilevers were then incubated in a solution containing 94 %
acidic methanol (1 mM acetic acid in methanol), 5 % water and 1 % (3-aminopropyl)-
triethoxysilane (Sigma, MO, USA) for 30 min. The cantilevers were extensively rinsed in
methanol and dried before incubation in a solution of 1 % glutaraldehyde for 1 min. They were
finally rinsed in water and incubated in a solution of 10 µg/ml fibronectin (Sigma, MO, USA) for
1 h. The cantilevers were kept in the solution of fibronectin. Cantilevers were calibrated in water
before each measurement using the thermal fluctuation method150.
Chapter 2 Materials and Methods
41
2.4.5. Long-term adhesion measurements
The extremity of a fibronectin-decorated cantilever was precisely positioned above the targeted
adherent cell. To ensure that the cell-cantilever contact area was similar for all measurements,
representative cells of comparable size were selected for each condition. The cantilever was
approached towards the cell until a repulsive force of 1.5 nN was reached. It was left in contact
with the cell in constant height for 30 min before the retract step was started. Force distance
curves were acquired with an approaching and retracting speed of 0.5 µm/s using the maximum
z-range of 100 µm. A new cell sample and a new cantilever were used before each measurement
(Fig. 2.5).
Fig. 2.5. Schematic illustrating a long-term adhesion measurement on an adherent cell with a contact time of 30 min
between the cantilever and the cell.
2.4.6. Cantilevers for indentation
Cell elasticity measurements were performed with the same cantilevers as for short-term
adhesion but without functionalization. Arrow TL1 tipless cantilevers (Nanoworld, Switzerland)
were send to Novascan to be modified by gluing glass spheres (radius = 5 µm, Novascan, IA,
USA) to the end of each cantilever to give well-defined indenters151 (Fig. 2.6).
Fig. 2.6. TL-1 tipless cantilever modified by Novascan with a 10 µm sphere attached (SiO2).
Chapter 2 Materials and Methods
42
2.4.7. Elasticity measurements
Force distance curves were acquired with an approach speed of 2.5 µm/s to minimize
hydrodynamic effects. A maximum applied force of 200 pN resulted in a maximal indentation of
300 nm for the softest samples. There was a pause of 60 s at the maximal retract distance between
each measurement. Measurements were performed only on thicker regions of the cell.
2.5. AFM imaging* Polyelectrolyte layers were imaged on a Nanowizard I BioAFM (JPK Instruments, Germany)
using CSC38/noAl cantilevers (Mikromasch, Estonia) in intermittent-contact (fluid) mode.
2.6. Cell preparation
2.6.1. FACS
Cells were harvested by trypsinization, washed in PBS, collected by centrifugation and fixed in
cooled 70% ethanol for 1h. Cells were collected by centrifugation once more and suspended in
PBS containing 40 µg/ml propidium iodide (Sigma, MO, USA), 0.015% v/v Nonidet P40
substitute (Sigma, MO, USA) and 100 µg/ml RNase A (Sigma, MO, USA). The DNA content
was analyzed after at least 30 min incubation on ice.
2.6.2. Confocal microscopy
Cells were washed with cold PBS and fixed for 20 min in PBS containing 4% paraformaldehyde.
They were then rinsed twice with PBS and incubated for 10 min in a solution of 0.1 M glycine in
PBS. After two further rinses in PBS, the cells were incubated in a blocking solution composed
of 0.05 % saponine and 0.2 % bovine serum albumin in PBS, for 20 min. Cells were stained for
actin filaments with AlexaFluor 488 Phalloidin (dilution 1: 40, Sigma, MO, USA) for 2 h at room
temperature under agitation. The cells were finally washed twice in blocking solution, in PBS and
in water. A mounting medium was used to preserve fluorescence.
______________________________________________________________________________*The AFM images were obtained by O. Guillaume-Gentil at ETH Zurich (Switzerland).
Chapter 2 Materials and Methods
43
2.6.3. SEM
Cells were rinsed with PBS and fixed in a solution of 2.5 % glutaraldehyde in 0.2 M cacodylate
buffer, pH 7.4 overnight. After this incubation, the cells were dehydrated in a series of
ethanol/water mixtures: 20 %, 20 %, 30 %, 40 %, 50 %, 60 %, 70 %, 80 %, 90 %, 100 %, 100 %
ethanol (5 min each incubation), followed by drying in air. The cells were observed after
sputtering with gold.
2.7. Data processing and statistical analysis
2.7.1. FACS
For each cell population, 15’000 cells were analyzed. Each synchronization experiment was
repeated at least 5 times. Data acquisition was performed with the FACSDiva software (Becton
Dickinson, CA, USA) and further analysis of the data was carried out with the WinMDI software
(J. Trotter, Scripps Research Institute, CA, USA).
2.7.2. Analysis of force-distance curves
After completion of a force-distance cycle, the measured changes in piezo z-position and the
corresponding deflection signal in newtons were saved by the Scanning Probe Microscopy
software (JPK Instruments, Germany)152. Force-distance curves were inspected before they were
included in the data analysis. They were discarded if the baseline was too short to ensure that the
cell was completely detached from the surface during cantilever retraction. The baseline was
linear in all curves analyzed. Acoustic noise, mechanical interference, microscopic objects or
other cells floating in the medium may cause unwanted cantilever deflection, which results in
undulating baselines.
For short-term adhesion, data analysis was carried out using ORIGIN 7.5 (OriginLab, MA,
USA). The force-distance curves were complex, usually containing a maximal force peak and
several force steps either preceded by a force plateau or not. The parameters analyzed were the
maximum force of detachment; the number, position and amplitude of the discrete detachment
steps observed along the retraction curve; and the work required to detach the cell from the
substrate. The work of detachment was obtained by integrating the adhesion forces over the
Chapter 2 Materials and Methods
44
distance travelled by the cantilever. For each cell population, 10 force distance curves were
obtained from 10 different cells, giving 100 measurements. Each measurement provided one
maximum force of detachment, one work of detachment and several positions and amplitudes of
the discrete detachment steps.
For long-term adhesion, data analysis was carried out using the Image Processing software (JPK
Instruments, Germany). The force-distance curves were simple and contained one single
maximal force peak. A number of mechanical parameters related to cell detachment were
determined from the force-distance curves including the maximum force, work and distance of
detachment. For each condition, 1 force distance curve was obtained from each of 20 different
cells, giving 20 independent measurements. Each measurement provided one maximum force,
one work and one distance of detachment. The percentage of cells that detached from the surface
was determined by optically examining the end of the AFM cantilever after each measurement.
For elasticity measurements, data analysis was carried out using the Image Processing software
(JPK Instruments, Germany). The software gave the possibility to derive the Young’s modulus
from force curves running through several steps. All operations were applied to the approach
curve. The first step of the processing was to remove any offset or tilt from the curve. The contact
point was calculated automatically. Then the software calculated the indentation depth by taking
the difference between the piezo movement and the cantilever vertical deflection in units of
length. Finally the curve was ready to be fitted to the Hertz model to derive the Young’s
modulus. The formula was adapted for parabolic indenter (Fig. 2.7)153. For each condition, 5
force distance curves were obtained from each of 20 different cells, giving 100 measurements.
The Hertz model assumes linear elastic behaviour as well as homogeneity of the sample.
However, most biological materials are neither homogeneous nor absolutely elastic. The viscous
nature of the cell means that the energy delivered by the indenter is not completely given back by
a cell but dissipates. The variability of the viscous behaviour becomes visible if different
indentation velocities are tested154,155. Each cell type has its own relaxation time. Moreover, the
Hertz model is only valid for small indentations (a maximum of 10% of the cell height) where the
substrate doesn’t influence the measurements and where the geometry of the indentation matches
the geometry of the indenter. The Hertz model is a simple model to have a number in order to
quantify the stiffness of the cells.
Chapter 2 Materials and Methods
45
Fig. 2.7. The Young’s modulus can be fitted using the Hertzian model for parabolic indenter. The model assumes
infinite thickness and linear elasticity of the sample156.
2.7.3. Statistical analysis
The forces, the work and the distances of detachment of the cells were quantified as described in
the previous section. The mean of the values together with its standard error was taken as
characteristic for each mechanical parameter of detachment.
For short-term adhesion, several force distances were obtained from each cell. Therefore, not all
the data were independent: results from any one cell were dependent, while data compared
between cells were independent. For this reason, the median value of each parameter was
determined separately for each cell. The mean of these median values together with its standard
error was then taken as characteristic for each condition.
Chapter 2 Materials and Methods
46
The data obtained were analyzed with the statistical analysis and data analysis software S-PLUS
8.0 (Insightful, Switzerland). The two-sample T-test was used to test whether or not two
population means, m1 and m2, are equal. The samples are assumed to come from Gaussian
(normal) distributions. If it was not the case, logarithmic transformations giving normal
distributions of the mechanical parameters were analyzed. A two-tailed test was used, with a null
hypothesis H0 that is the logical counterpart, mutually exclusive and exhaustive, to an alternative
hypothesis H1. Depending on the outcome of the test, the null hypothesis is either rejected or
retained. Rejection of the null hypothesis logically leads to acceptance of the alternative
hypothesis and retention of the null hypothesis leads to an inability to accept the alternative
hypothesis; H0: m1 – m2 = 0 and H1: m1 – m2 ≠ 0. The Bonferroni correction was used for
multiple comparisons to account for the inflation of the Type I-error.
For all statistical tests, a p-value <0.05 was considered significant. The p-value is the probability
of obtaining a test statistic at least as extreme as the one that is actually observed, assuming that
the null hypothesis is true. The smaller the p-value, the more strongly the test rejects the null
hypothesis, that is, the hypothesis being tested.
Chapter 3 Cell adhesion during the cell cycle
47
Chapter 3
Cell adhesion during the cell cycle‡
In order to determine if cell adhesion has to be studied independently of cell cycle or not, cell
adhesion at different phases was measured. In this chapter, force spectroscopy was used to
measure the adhesion of Saos-2 cells to a glass surface at different phases of the cell cycle.
The cantilevers were functionalized for cell capture in order to perform short-term adhesion
measurements.
The cells were synchronized in 3 phases of the cell cycle: G1, S and G2M. Cells in these phases
were compared with unsynchronized and native mitotic cells. Individual cells were attached to an
AFM cantilever, brought into brief contact with the glass surface and then pulled off again. The
force-distance curves obtained allowed the work and maximum force of detachment as well as
the number, amplitude and position of discrete unbinding steps to be determined.
______________________________________________________________________________‡Part of this chapter was published in Measuring cell adhesion forces during the cell cycle by force spectroscopy.
Weder G., Vörös J., Giazzon M., Matthey N., Heinzelmann H. and Liley M. Biointerphases, 2009, 4(2), 27-34.
Chapter 3 Cell adhesion during the cell cycle
48
3.1. Introduction
3.1.1. The cell cycle
The eukaryotic cell cycle is divided into four phases157. The two most dramatic events are when
the nucleus divides, a process called mitosis, and when the cell splits into two cells, a process
called cytokinesis. These two processes constitute the M phase (M = mitosis) of the cell cycle.
The period between the M phase is called interphase, during which the cell grows in size. The
interphase is divided into the remaining three phases of the cell cycle: G1, S and G2. During the S
phase (S = synthesis), the cell replicates its DNA. The G1 phase (G = gap) is the interval between
the completion of the M phase and the beginning of the S phase. The G2 phase is the interval
between the end of the S phase and the beginning of the M phase.
Fig. 3.1. (A) The four successive phases of a standard eukaryotic cell cycle. (B) The relative amount of DNA per cell
during the cell cycle.
Cell cycle can be analyzed by fluorescence labeling of the DNA of cells in suspension and using
a fluorescence activated cell sorter (FACS). G1 cells have one copy of DNA and have therefore
1X fluorescence intensity. Cells in G2M phase have two copies of DNA and have therefore 2X
fluorescence intensity. Since the cells in S phase synthesize DNA, they have fluorescence values
between the 1X and 2X populations.
Chapter 3 Cell adhesion during the cell cycle
49
3.1.2. Adhesion of mitotic cells
For most adherent cells in vitro, dramatic changes in cell morphology take place during the cell
cycle158. For most of the cell cycle, the cells are spread over the surface of the substrate, then, at
the beginning of mitosis, they round up and lose most of their contact to the substrate in
preparation for cytokinesis. Mitotic rounding up is associated with changes in the cytoskeleton,
plasma membrane and cell volume, while adhesion of the cell to the substrate is greatly
reduced159. However, the underlying mechanisms of these changes are poorly understood.
Adherent cells attach to their surroundings via focal adhesions. These large protein complexes
consist of a variety of cytoskeletal and cytoskeletal-associated proteins providing the primary
stabilizing force for the attachment of cultured cells as well as initiation sites for actin stress
fibres160,161. There have been many studies of the role of individual adhesion proteins in the
rounding up of mitotic cells162. These studies show that various phosphorylation events of
cytoskeletal163 and focal adhesion proteins164,165,166,167,168,169 contribute to the pre-mitotic
disassembly of focal adhesions170, the deconstruction of the actin cytoskeleton of the
interphase171 and the construction of a new mitotic cytoskeleton172. However, despite this
dissociation and deconstruction, the mitotic cell remains attached to the substrate. There is direct
contact between the plasma membrane and the substrate173. In addition, there are a number of
retraction fibres, thin actin filaments, that anchor the cell to the substrate via focal adhesions.
Thus some adhesive elements remain during mitosis.
Not only the cytoskeleton, but also the plasma membrane is remodelled during mitosis. Rounding
up of the cell involves a reduction of the total area of plasma membrane, which has been recently
found to take place via normal endocytosis of the plasma membrane and a reduction in the
recycling of internalized membranes174.
3.1.3. Short-term adhesion measurements
A single cell was attached to an AFM cantilever, brought briefly into contact with a glass
substrate, and then pulled off the substrate175 (Fig. 3.2A). Measurement of the cantilever
deflection during this process allowed the forces between cell and surface to be quantified at each
moment and represented in force distance curves (Fig. 3.2B). Several different mechanical
parameters were extracted from these curves152 including the maximum force of detachment, the
Chapter 3 Cell adhesion during the cell cycle
50
displacement needed to completely remove the cell from the substrate and the work of
detachment. Not only global cellular parameters were studied: it was also possible to identify and
analyze individual unbinding events, discrete steps in the force distance curve that occur on the
release of individual proteins or protein complexes from the surface176.
Fig. 3.2.(A) Schematic of a single-cell force spectroscopy measurement, and (B) a force-distance curve acquired
during approach (I-II in blue) and retracting steps (III-IV in orange). In the initial phase of the approach there is no
contact between the cell and the surface (I). Then the cell is pressed onto the surface until a pre-set maximal force is
attained. During this phase the elastic response of the cell can be observed (II). The position of the cantilever is held
constant for a given contact time. Information on different mechanical parameters can be obtained from the
retraction: the work of detachment, the number, amplitude and position of the unbinding events corresponding to
single proteins or protein complexes and, finally, the maximal force needed to detach the cell from the surface (III).
In the last step, there is no physical contact between cell and surface (IV).
With this approach, the results obtained reflected the composition and organization of the plasma
membrane, for example, concerning the presence, activity and organization of adhesion proteins.
However, the short contact time – one second - between cell and substrate means that no
information could be gained about how the cell responds to the surface on a longer time scale,
thus excluding the effects of, for example, changes in protein expression.
Chapter 3 Cell adhesion during the cell cycle
51
3.2. Cell cycle synchronization
3.2.1. G1, S and G2M
Saos-2 cells were synchronized in 3 phases of the cell cycle, G1, S and G2M. Unsynchronized cell
populations showed the expected distribution of 56% of cells in the G1 phase, 21% in the S phase
and 23% in the G2M phase. Good synchronization was obtained in both the G1 phase with 78% of
cells in G1 and in the G2M phase with 80% of cells in G2M. S phase synchronization was limited
to 62% due to differences in resumption of the cell cycle for individual cells after release from
the thymidine synchronization (Fig. 3.3). A more specific synchronizing agent to synchronize the
cells in the intermediate S phase of DNA replication was not found.
Fig. 3.3.DNA content analysis of the cell cycle measured by flow cytometry of SaOs-2 cells in the presence of
synchronizing agents: (A) unsynchronized, (B) mimosine as a G1 synchronizing agent, (S) thymidine as a S
synchronizing agent and, (D) nocodazole as a G2M synchronizing agent.
Chapter 3 Cell adhesion during the cell cycle
52
3.2.2. Native mitotic cells
When studying synchronized cells, it is important to be aware that the synchronizing agent may
affect several properties of the cell; nocodazole, for example, inhibits the polymerization of the
microtubules. In order to exclude the possibility that any differences observed between G2M cells
and unsynchronized cells were an unexpected artifact due to the use of nocodazole, native mitotic
cells were also investigated. Native mitotic cells were obtained from unsynchronized cell cultures
and were separated from cells in other phases of the cell cycle thanks to their reduced adhesion to
the culture surface. Gentle agitation of the medium or culture support resulted in their release
from the surface into the culture medium while other cells remained firmly attached.
3.3. Short-term adhesion
3.3.1. Presence of adhesion proteins throughout the cell cycle
First experiments carried out with the Saos-2 cells were used to select the experimental
parameters for the short-term adhesion measurements. An applied force of 900 pN was chosen
and a contact time of 1 s was selected to avoid very strong cell-surface interactions that might
result in a failure to totally detach the cell from the surface even at a retraction distance of 100
µm.
Using these experimental parameters, typical force distance curves obtained for each of the
synchronized cell populations are shown in figure 3.4. Qualitatively, the curves look similar, with
discrete unbinding events indicating the presence of adhesion-protein complexes at the cell
membrane in each phase of the cell cycle. A statistical analysis of these events was carried out,
comparing the number of events per curve, the amplitude of the events and the position of the
events along the retraction curve for the three synchronized cell populations and for a population
of unsynchronized cells.
Chapter 3 Cell adhesion during the cell cycle
53
Fig. 3.4. Typical force distance curves showing the detachment of G1, S and G2M synchronized human osteoblasts
from a glass surface (contact for 1 s with an applied force of 900 pN). The step-like features in the curves
correspond to the release of adhesion proteins from the glass and can be observed in all three phases of the cell
cycle.
Histograms showing the number of unbinding events are shown in figure 3.5. In all cell
populations, there were between 4 and 23 unbinding events per curve, reflecting the number of
adhesion protein complexes that bound to the surface. Comparing the mean numbers of
unbinding events for the different populations, the values obtained are 8.9 and 12 in interphase
(G1 and S), while in the two M-phase populations (G2M and native mitotic) the means are 11.3
and 10.9. For the unsynchronized cells, which are expected to be approximately 80% in
interphase (since made up of 56% G1 and 21% S), 12.6 is obtained. The number of unbinding
events in interphase and metaphase are broadly similar: there is no large decrease in unbinding
events that might be associated with a loss of adhesion in M-phase (Table 3.1).
Chapter 3 Cell adhesion during the cell cycle
54
Fig. 3.5. Histograms showing the number of unbinding events of human osteoblasts on a glass surface after an
applied force of 900pN for 1s. The number of unbinding events was measured for unsynchronized cells and
synchronized cells in G1, S and G2M phases. Between 4 and 23 unbinding events were observed in each force
distance curve independently of the cell cycle phase.
Mean (Median) ±SEUnsynchronized 12.6 0.5G1 phase 8.9 0.4S phase 12 1G2M phase 11.3 0.5Native mitotic 10.9 0.8
Number of unbinding events
Table 3.1. Comparison of the number of unbinding events for 5 conditions: unsynchronized cells, G1, S, G2M
synchronized cells and native mitotic cells (SE: standard error).
Chapter 3 Cell adhesion during the cell cycle
55
3.3.2. Position of the unbinding events
The positions (distance from the surface) of the unbinding events in the force distance curves
were also analyzed. Clear differences were observed between the G2M phase and the other
populations, while differences between unsynchronized, G1 and S phases were not significant. A
statistical analysis of the number of events before and after 30 µm displacement of the cantilever
is shown in table 3.2.
● For unsynchronized cells, 78% of unbinding events occur within the first 30 µm and 22% in
the remaining distance. Similar values were obtained for cells in G1 and S.
● For cells in G2M, 93% of unbinding events occur within the first 30 µm and 7% in the
remaining 70 µm of travel.
● For native mitotic cells, 95% of unbinding events occur within the first 30 µm and 5% in the
remaining 70 µm of travel.
Clearly, cells in G1 and S can be stretched further before the cell is released from the surface than
cells in G2M or native mitotic cells.
≤ 30µm (%) > 30µm (%)Unsynchronized 78 22G1 phase 80 20S phase 79 21G2M phase 93 7Native mitotic 95 5
Position of unbinding events
Table 3.2. Comparison of the distribution of the position of unbinding events between 5 conditions: unsynchronized
cells and G1, S, G2M synchronized cells and native mitotic cells.
3.3.3. Adhesion per protein complex in the different cell cycle phases
The amplitudes of the unbinding events are very similar in all the different conditions, with mean
values between 84 and 108 pN (Table 3.3). The size of these events suggests that they correspond
to the rupture or release of either individual proteins or small protein complexes from the glass
surface.
Chapter 3 Cell adhesion during the cell cycle
56
Comparing the values obtained for interphase (G1 and S) with M-phase (G2M and native mitotic),
86 and 84 pN respectively for the interphase populations and 108 and 96 pN for the M-phase
populations are observed. In contrast, the unsynchronized population, which is expected to be
approximately 80% in interphase, gives a value of 104 pN.
The similarity of the unbinding forces obtained for all phases of the cell cycle is perhaps
surprising: there are numerous reports of the phosphorylation of individual proteins associated
with the cytoskeleton and with focal adhesions, which might lead one to expect differences (i.e. a
reduction) in the binding ability of the proteins exposed at the cell membrane.
Mean (Median) (pN) ±SEUnsynchronized 104 17G1 phase 86 6S phase 84 13G2M phase 108 5Native mitotic 96 6
Amplitude of unbinding events
Table 3.3. Comparison of the amplitude of the unbinding events for 5 conditions: unsynchronized cells, G1, S, G2M
synchronized cells and native mitotic cells (SE: standard error).
3.3.4. Maximum force of detachment
The values obtained for the means of the maximum forces of detachment are similar for all
phases of the cell cycle: the values, between 0.88 and 1.2 nN, are shown in table 3.4. Comparing
interphase and M-phase, 0.88 and 0.99 nN for G1 and S populations and 1.2 nN for both G2M and
native mitotic cells were obtained. The unsynchronized population gives a value of 1.2 nN. The
maximum force of detachment is not strictly an independent parameter as it is related to the
number of unbinding events and their amplitude. It is, however, not simply the product of the
number of unbinding events and their amplitude due to contraction and/or relaxation of the cell
during the measurement, particularly the first few microns of retraction. The values obtained for
the unsynchronized cell population are compatible with those obtained for each of the phases
individually. The only statistically significant differences are between the distributions of the G1-
phase and mitotic cells.
Chapter 3 Cell adhesion during the cell cycle
57
Mean (Median) (nN) ±SE
Unsynchronized 1.2 0.1
G1 phase 0.88 0.03
S phase 0.99 0.09
G2M phase 1.2 0.06
Native mitotic 1.2 0.06
Maximum force of detachment
Table 3.4. Comparison of the maximum force of detachment for 5 conditions: unsynchronized cells, G1, S, G2M
synchronized cells and native mitotic cells (SE: standard error).
3.3.5. Work of detachment
The work of detachment – similarly to the maximum force of detachment – is not strictly an
independent parameter as it is related to the amplitude and number of unbinding events and their
position during retraction of the cantilever. The mean works of detachment are similar for the
unsynchronized and synchronized cells with values between 1.9 and 0.94 x 10-14 J (Table 3.5). In
interphase, the values obtained are 1.4 and 1.7 x 10-14 J for G1 and S populations. In M-phase the
values are 1.1 and 0.94 x 10-14 J for G2M and native mitotic. 1.9 x 10-14 J was obtained for
unsynchronized cells. The only statistically significant differences are between the distributions
of the unsynchronized and mitotic cells.
Mean (Median) (J) ±SE
Unsynchronized 1.9 x 10-14 0.2 x 10-14
G1 phase 1.4 x 10-14 0.2 x 10-14
S phase 1.7 x 10-14 0.2 x 10-14
G2M phase 1.1 x 10-14 0.1 x 10-14
Native mitotic 0.94 x 10-14 0.2 x 10-14
Work of detachment
Table 3.5. Comparison of the work of detachment for 5 conditions: unsynchronized cells, G1, S, G2M synchronized
cells and native mitotic cells (SE: standard error).
Chapter 3 Cell adhesion during the cell cycle
58
3.3.6. Higher stiffness of mitotic cells
The analysis of the positions of the unbinding events suggested that G2M and native mitotic cells
were stiffer than cells in the other phases. The increased stiffness of mitotic cells has been
reported by other authors177,124 and is associated with a reorganization of the cytoskeleton (Fig.
3.6).
Fig. 3.6. Comparison of unsynchronized (A) and G2M synchronized cells (B) by optical (I) and confocal microscopy
(II) showing the actin fibres (labeled with AlexaFluor 488 Phalloidin). The cell rounding and reorganization of the
cytoskeletal actin fibres observed in B are characteristic of cytokinesis.
This was verified for Saos-2 cells using force spectroscopy to obtain an estimate of the Young’s
modulus of the cells. For these measurements, the cells were adherent on a glass surface and a
round glass sphere attached to an AFM cantilever was brought into contact with them. Given the
size of the glass sphere and the forces applied during the indentation process it was possible to
calculate a value for the Young’s modulus using a Hertzian model (section 2.7.2). The
indentation is the difference between the piezo movement and the cantilever vertical deflection in
units of length (Fig. 3.7).
Chapter 3 Cell adhesion during the cell cycle
59
Fig. 3.7. Force indentation curves derived from (A) unsynchronized and (B) G2M synchronized Saos-2 cells. The
applied force of 200 pN resulted in an indentation of 210 nm for the unsynchronized cells and of 90 nm for the G2M
synchronized cells.
Values for the Young’s modulus of individual G2M synchronized cells and individual adherent
unsynchronized cells are shown in figure 3.8. Typically, the Young’s moduli of the G2M
synchronized cells (mean value 1.4 kPa) are higher than those of the unsynchronized cells (mean
value 0.4 kPa) confirming the increase of the cell stiffness in mitosis. The data obtained are
within reported values for the Young’s modulus of living cells, (between 0.1 and 10 kPa)178,179. It
is difficult to make close comparisons with literature values, given the range of experimental
parameters that influence the values obtained (e.g. geometry of the indenter, depth of indentation,
speed of measurement). However, studies on osteosarcoma cell lines and on primary human bone
cells including osteoblasts give very similar Young’s moduli: between 1 and 2 kPa for MG-63
cells180, from 0.7 to 2.6 kPa for primary human bone cells and MG-6335, and from 2.1 to 8.8 kPa
for Saos-2 cells181.
Chapter 3 Cell adhesion during the cell cycle
60
Fig. 3.8. Histogram showing the values of the Young’s modulus obtained for individual unsynchronized cells and
cells synchronized in G2M phase. Vertical lines indicate the mean values and the error bar is the standard error. No
native mitotic cells were chosen for measurement in the unsynchronized cell population.
3.4. Discussion
3.4.1. Cell adhesion between M-phase and interphase
The experiments described here show that binding proteins and/or protein complexes at the cell
membrane remain similar both in number and in their binding properties during all the phases of
the cell cycle. Indeed, while some differences are observed in the surface binding properties of
the cells, the variations are, in all cases, less than a factor of two and the lowest values are not
associated with the M phase.
A detailed statistical analysis of the data was used to determine the probability that each
measured parameter of each group of cells is the same (the p-value). Table 3.6 shows that the
statistical differences (see white dots on table 3.6) existing between two cell populations are not
associated with the M phase. However, the statistical analysis cannot determine whether or not
the ten cells selected for analysis are representative of the entire cell population under this
condition. It is almost certainly this limitation that results in some unexpected data points (see
white dots). Despite the difficulty to draw a conclusion for small differences between cell
populations, cell adhesion related to M-phase was not different from those related to interphase.
Chapter 3 Cell adhesion during the cell cycle
61
Unsynchro G1 phase S phase G2M phase Unsynchro G1 phase S phase G2M phaseUnsynchroG1 phase ○ ●S phase ● ○ ● ●G2M phase ● ○ ● ● ○ ○Native mitotic ● ● ● ● ● ● ○ ●
Unsynchro G1 phase S phase G2M phase Unsynchro G1 phase S phase G2M phaseUnsynchroG1 phase ● ●S phase ● ● ● ●G2M phase ● ○ ● ○ ● ●Native mitotic ● ○ ● ● ○ ● ● ●
Amplitude of unbinding events
Work of detachment
Number of unbinding events
Maximum force of detachment
Table 3.6. Comparison of the number and amplitude of unbinding events, and the maximum force and work of
detachment for 5 conditions: unsynchronized cells, G1, S, G2M synchronized cells and native mitotic cells. Data were
compared using the two sample T-test with Bonferroni correction (p-value 0.05). The black dots indicate that the cell
populations are not statistically significantly different (p-value ≥0.05) and the white dots indicate that the cell
populations are statistically significantly different (p-value <0.05).
3.4.2. Statistics
Force spectroscopy is inherently a single cell technique: values for different mechanical
properties are determined individually for each cell of each population studied. Single cell
analyses allow us to study not only the average properties of a sample (an ensemble of cells), but
also the variation and heterogeneity within the sample. While this gives access to qualitatively
new information, it also comes with its disadvantages. In our case, the statistical analysis was
made significantly more complicated: for each cell condition ten cells were selected for study –
this relatively small number was chosen because of the lengthy preparation required for
measurements on each individual cell - and ten force distance measurements were carried out per
cell. This method gave a dataset that was a mix of dependent and independent results. In general,
the analysis required that the data for each cell (dependent results) were analyzed first to obtain a
value characteristic of that cell. The values for each cell in the sample were then analyzed as
independent data points to give a value that was representative of the sample as a whole.
Chapter 3 Cell adhesion during the cell cycle
62
3.4.3. The use of trypsin
A significant limitation of this study is the use of trypsin to detach the cells from the culture
surface before fixing them to the cantilever. Trypsinization clearly damages at least some of the
binding proteins exposed at the cell surface and so may well influence results in a study of these
proteins. The effects have tried to be minimized by using a short, reproducible trypsinization on
all samples and allowing the cells to recover for 30 minutes before measurement. Studies by
other authors have shown that, at least in some cases, trypsinization leaves the binding functions
of surface proteins largely intact128,130. SDS-PAGE analyses also showed no effect of the
trypsinization on either α2 integrin or β1 integrins28. While trypsinization may limit the work to
the observation of relatively large effects, it is believed to have no influence on the conclusions of
this study.
3.4.4. The short contact time
Finally, the short contact time between cell and surface during this study limits the analysis to a
study of proteins and protein complexes that are already present at the cell membrane and to the
gross mechanical properties of the cell. There is insufficient time for the cell to react significantly
to the presence of the surface, for example, by changes in the cytoskeleton or in protein
expression. A more complete study of cell surface interactions requires much longer contact
times between cell and surface. However, increased contact times between SaOs-2 cells and glass
result in increased cell/surface adhesion. The results are either a rupture of the cell as cantilever
and surface are separated, or alternatively, the cell does not rupture, but remains attached to both
surface and cantilever even at separations of 100 microns.
3.5. Conclusion Single cell force spectroscopy was used to study the adhesive and mechanical properties of SaOs-
2 cells in culture. The study focused in particular on the changes in these properties between
interphase, when cells are well spread and firmly attached to culture surface and M-phase, when
the cells round up and are much more loosely attached to the surface. The differences in
cell/surface attachment are striking: in M-phase SaOs-2 cells may be removed by shaking culture
vessels while in interphase attempts to pull SaOs-2 cells off the surface may result in cell rupture.
Chapter 3 Cell adhesion during the cell cycle
63
Because of the short time of contact between cell and surface, the investigation is relevant to cell
surface properties and cell stiffness. The experiments described here show that binding proteins
and/or protein complexes at the cell membrane remain similar both in number and in their
binding properties (amplitude of the unbinding events) during interphase and M phase. While
some differences can be observed in the mean values obtained in the different phases, the
differences are, in all cases, less than a factor of 2 and the extreme values are not associated with
the G2M or native mitotic (M) phase. No large reduction was observed either in number or in
amplitude of the unbinding events that might contribute to the loss of adhesion of M-phase cells.
This may be surprising given the numerous studies showing the phosphorylation of proteins
associated with focal adhesions during mitosis.
A second clear conclusion can be drawn from the position of the unbinding events. As the cell
was stretched during detachment from the surface, unbinding events took place at a smaller
extension for the mitotic/G2M cells than for cells in other phases. These cells cannot be stretched
as far before they are released from the surface. This is due to an increased stiffness of the cell
caused by a reorganization of the cytoskeleton during mitosis as also observed by other
researchers in the field.
The maximum force of detachment and the work of detachment were also studied for all the cells.
These two parameters are not strictly independent as they are related to the number and amplitude
of unbinding events and to their position. Here, again the differences observed between M phase
and interphase were relatively small compared to the differences between cellular adhesion
during the cell cycle.
Chapter 3 Cell adhesion during the cell cycle
64
Chapter 4 Cantilever functionalization for cell detachment
65
Chapter 4
Cantilever functionalization for cell
detachment
Long-term cell adhesion involves adherent cells. The challenge is to establish an attachment
between cells and AFM cantilevers strong enough to allow their detachment. In this chapter,
AFM cantilevers were functionalized for long-term adhesion measurements in order to detach
living adherent 3T3 fibroblasts.
The cantilevers were prepared with 4 different functionalizations: concanavalin A, fibronectin,
poly-L-lysine and zirconium. 3T3 mouse fibroblasts were allowed to grow for one day on a glass
surface. Then the cantilevers were pressed onto the adherent fibroblasts for a given contact time
and withdrawn. The functionalization showing the highest percentage of cell detachment was
selected for the rest of this work.
Chapter 4 Cantilever functionalization for cell detachment
66
4.1. Introduction
4.1.1. Long-term adhesion
The use of force spectroscopy permits the study of adhesion of living cells to be studied. In this
thesis, “short-term adhesion” is defined as short cell-substrate contact times, from seconds to
minutes, whereas “long-term adhesion” is defined as long cell-substrate contact times, from hours
to days. Long-term adhesion allows the cells to form strong adhesion complexes that involves a
large number of receptors bindings cooperatively. Long-term adhesion measurements
characterize the cell-surface interaction because the cells can spread, react to the surface and their
adhesion proteins can be renewed. That is the reason why the main objective of this work is to
detach living single adherent cells in order to quantify their global adhesion forces.
Other authors have reported that single cell force spectroscopy is currently restricted to short
contact times that range from milliseconds to about twenty minutes152. This restriction was
observed using single cells captured on an AFM cantilever and the main limitation was the loss
of the cell from the cantilever at prolonged cell/surface contact times i.e. exceeding one hour
(Fig. 4.1). A single cell was captured on a coated AFM cantilever and allowed to settle on the
cantilever for approximately fifteen minutes away from the surface. Then the cell was pressed
onto the substrate for more than one hour. At long contact times, the adhesion between the
cantilever and the cell was weaker than that between the substrate and the cell. Using
concanavalin A to immobilize the cell on the cantilever, forces of up to 50 nN were measured
before the cells detached from the cantilever. This force was, however, dependent on cell type. In
addition, the authors noticed that the almost unavoidable thermal and mechanical drifts in AFM
complicate those experiments that exceeded thirty minutes.
Fig. 4.1. Schematics illustrating a cell captured on an AFM cantilever for (A) a short cell-substrate contact time and
(B) a long cell-substrate contact time exceeding one hour: the interaction cell-cantilever is weaker than the
interaction cell substrate and there is a loss of the cell from the cantilever.
Chapter 4 Cantilever functionalization for cell detachment
67
One possible solution is to first seed the cell on the surface and then to detach it with
functionalized AFM cantilever (Fig. 4.2). In this way, the cell can be incubated for the desired
time on a specific surface under physiological condition without mechanical stress by the
cantilever on it. In this approach, the challenge is to establish a quick adhesion between cells and
AFM cantilevers capable of supporting their detachment. The establishment of the connection
cell-cantilever has to be fast. This is to avoid a disturbance of the adhesion properties of the cell
on the specific surface, and to limit problems related to the thermal and mechanical drifts at the
system. Another advantage of seeding cells on the surface is the elimination of the use of trypsin.
During the long contact time between cell and substrate, cellular adhesion proteins are renewed.
Fig. 4.2. Schematic illustrating a long-term adhesion measurement. The cell is first incubated on the surface for a
long cell-substrate contact time and then detached with an AFM functionalized cantilever. The interaction cell-
cantilever is stronger than the interaction cell-substrate and the cell is detached from the surface.
4.1.2. Cantilever functionalization for cell detachment
In order to successfully detach cells, the adhesion between cell and cantilever has to be stronger
that between cell and substrate. A wide variety of molecules exposed at the cell surface such as
sugars, proteins or lipids are candidates to establish this strong adhesion.
Several cantilever functionalizations have been used by other authors for cell capture. Lectin-
decorated cantilevers, especially with concanavalin A182,136,183,128 and wheat germ
agglutinin123,175, have been widely used to capture several cell types. Lectins are sugar-binding
proteins that interact with the glycoproteins exposed at the cell surface. Cantilevers have also
been decorated with fibronectin that interacts with integrins that are the major adhesion receptors
that mediate cell-substrate adhesion184,143. Alternatively, a charge-based approach has been
reported to allow capture of cells on a cantilever array (several cantilevers in parallel)185. The
Chapter 4 Cantilever functionalization for cell detachment
68
cantilevers were functionalized with poly-L-lysine and then the cells were added in a low
conductivity medium. The biotin-streptavidin system has been used to capture cells on
cantilevers140,137. Cell surface molecules were biotinylated while the cantilever was decorated
with streptavidin. Finally, antibody-antigen interactions have been used for specific cell capture.
Jurkat cells, an immortalized line of T lymphocytes, were coupled to AFM cantilevers using an
anti-leucosialin functionalization129. All these cantilever functionalizations have been shown to
be efficient for cell capture in order to perform short-term adhesion measurements. In contrast,
cantilever functionalization for long-term adhesion with cell detachment is much more
demanding due to the necessity for a stronger attachment of the cell to the substrate.
In order to determine which cantilever functionalization was the most suitable for cell
detachment, three different cantilever functionalizations, commonly used for cell capture, were
systematically tested. The cantilever functionalizations targetted various molecules exposed at the
cell surface. Concanavalin A was selected to bind sugars, fibronectin to bind proteins and poly-L-
lysine to interact with charges.
In addition, a zirconium cantilever functionalization was tested to interact with the lipids of the
cell membrane. Indeed, tetravalent metal ions such as Zr4+ have been shown to interact strongly
with phosphates and phosphonates186. Recently, the affinity between the metal ion and
phosphates/phosphonates was exploited in the bioanalytical field187: capillary columns188 and
porous wafers189 were coated with zirconium phosphonate for phosphopeptide enrichment for
mass spectroscopy. Zirconium coatings on AFM cantilevers have never been used for cell capture
or cell detachment.
4.2. Detachment of adherent cells
4.2.1. Percentage of cell detachment
Single adherent cells were detached from glass surfaces using different AFM cantilever
functionalizations. 3T3 mouse fibroblasts were grown for 24 hours on a flat glass surface. The
glass sample was placed in a temperature-controlled fluidic chamber and a single adherent cell
was selected. The functionalized-cantilever was positioned above the cell and gently pressed on it
Chapter 4 Cantilever functionalization for cell detachment
69
until a force of 1.5 nN was attained (Fig 4.3A). The cantilever was left in contact for 30 minutes
to allow the cell to interact and bind actively with the functionalized cantilever. Finally, the
cantilever was withdrawn until the cell detached either from the surface or from the cantilever.
For each condition, one force distance curve was obtained from each of twenty different cells.
The cantilevers were coated with concanavalin A, fibronectin, poly-L-lysine or zirconium.
During this process, the forces exerted on the cell were continuously recorded and the values
were represented in a force distance curve (Fig 4.3B). The first qualitative information that was
obtained was the percentage of cells detached from the glass surface. The maximum force,
corresponding to the maximum deflection of the cantilever, and the work of detachment were
quantified for the cells successfully detached from the surface.
Fig. 4.3. (A) Schematic of the detachment of a single adherent cell and, (B) a corresponding force-distance curve.
The cantilever is pressed onto the adherent cell until a preset maximal force of 1.5 nN is attained. The position of the
cantilever is held constant for 30 min before it is withdrawn. A force-distance curve is recorded indicating the
maximum force and work of detachment. On both panels, orange defines the approach and turquoise defines the
retraction.
Chapter 4 Cantilever functionalization for cell detachment
70
The percentages of cell detachment from the glass surface were between zero and seventy-five
percent for all cantilever functionalizations. Fifteen percent of cells were detached using the
concanavalin A-functionalized cantilevers, seventy-five percent with the fibronectin, thirty-five
percent with the poly-L-lysine and zero percent with the zirconium. Native cantilevers without
functionalization didn’t allow the detachment of any cells.
Concanavalin AFibronectinPoly-L-lysineZirconiumNative silicon
Cantilever functionalization
00
Percentage of cell detachment (%)
157535
Table 4.1 Comparison of the percentages of detachment of 3T3 cells detached from glass surfaces using four
cantilever functionalizations: concanavalin A, fibronectin, poly-L-lysine and zirconium.
4.2.2. Maximum force of detachment
The maximum forces of detachment of the cells detached with the different functionalized
cantilevers were not statistically different. The maximum forces were quantified only for the cells
that detached from the glass surface. The mean values for the maximum forces of detachment
were 170 nN with the concanavalin A, 230 nN with the fibronectin and 190 nN with the poly-L-
lysine (Fig. 4.4).
4.2.3. Work of detachment
The works of detachment – similarly to the maximum forces of detachment – were similar. The
mean values for the work of detachment were 2.5 pJ with the concanavalin A, 3.3 pJ with the
fibronectin and 2 pJ with the poly-L-lysine (Fig. 4.5). The works of detachment showed no
statistically significant differences.
Chapter 4 Cantilever functionalization for cell detachment
71
Fig. 4.4. Histogram showing the distribution of the maximum forces of detachment of 3T3 cells that detached from
glass surface using cantilevers functionalized with concanavalin A, fibronectin and poly-L-lysine.
Fig. 4.5. Histogram showing the distribution of the works of detachment of 3T3 cells that detached from glass
surface using cantilevers functionalized with concanavalin A, fibronectin and poly-L-lysine.
Chapter 4 Cantilever functionalization for cell detachment
72
4.3. Discussion
4.3.1. Selection of the cantilever functionalization
The results described in the previous sections demonstrate that it is possible to detach living 3T3
fibroblasts from the surface on which they are growing after 24 hours of culture using
functionalized AFM cantilevers. A functionalization of the AFM cantilever is necessary to
achieve a strong adhesion between cell and cantilever.
A functionalization of fibronectin on the cantilever and 30 minutes contact between cell and
cantilever provided a sufficiently strong cell/cantilever adhesion to detach seventy-five percent of
3T3 cells from glass surfaces. In contrast, a cantilever functionalization of concanavalin A
allowed the detachment of only fifteen percent of cells. A cantilever functionalization of poly-L-
lysine allowed an intermediate percentage of thirty-five percent. The fibronectin was found to be
the best cantilever functionalization for the detachment of adherent 3T3 fibroblasts and was
selected for the rest of this work.
The selection of the cantilever functionalization depends on both the cell type and the SCFS
configuration. For example, fibronectin does not induce spreading in HeLa cells190 and their
formation of focal adhesions is not fibronectin-dependent191. However, while the cantilever
functionalization is crucial to promote the attachment of the cell to the cantilever, it may also
influence the adhesion of the cell to the substrate. For this reason, an interaction with the sugars
exposed at the cell surface, instead of the adhesion proteins, may be advantageous for some
SCFS configurations. A functionalization of concanavalin A was selected in the previous chapter
for cell capture and short-term adhesion measurements. The interaction between the cell and the
cantilever was strong enough to avoid a loss of the cell from the cantilever and probably has only
a limited effect in terms of the reorganization of the cell adhesion proteins. Alternatively, a
functionalization of poly-L-lysine might be more efficient to interact with another cell type. In
this case, the preparation of poly-L-lysine-functionalized cantilevers would be simpler and faster.
The cantilevers coated with a thin layer of zirconium (10 nm) didn’t allow the detachment of any
cells. The interaction of the cantilever with the lipids of the cell membrane was probably not
possible due to the presence of other molecules at the cell surface, notably sugars. However, there
are literature reports of three-dimensional vesicle matrices created using multivalent zirconium
Chapter 4 Cantilever functionalization for cell detachment
73
ion linkers between the liposomes186. For this reason, the approach seems promising for the
manipulation of liposomes.
4.3.2. Limitation of the contact time
Good results were obtained using a fibronectin functionalization and a cell contact time of thirty
minutes. During these thirty minutes of contact, cell/cantilever adhesion increases. This is
presumably due to a reorganization of both the focal adhesion proteins exposed at the cell surface
and the cytoskeleton. This reorganization is one limitation of this functionalization because it will
inevitably modify the adhesion of the cell to the substrate. Thus longer cell/cantilever contact
times will result in stronger cell/cantilever interactions but will increasingly modify the
cell/substrate adhesion measured. For this reason, the preparatory cell/cantilever contact time was
kept to the minimum necessary to successfully detach a reasonable proportion of cells from the
culture surface.
4.3.3. The effect of cantilever functionalization on cell adhesion
During the thirty minutes of contact between the cell and the AFM cantilever, the
functionalization of the cantilever may also influence the adhesion of the cell to the substrate. For
this reason, the detachment forces from glass surfaces were compared using different cantilever
functionalizations to observe possible changes to cell adhesion caused by fibronectin.
The quantification of the global cell adhesion between the 3T3 cells and the glass surface was
similar for all measurements independently of the cantilever functionalization (Table 4.2). The
mean maximum forces of detachment were between 180 and 230 nN with no statistically
significant differences for the different fonctionalizations. The mean works of detachment were
between 2 and 3.3 pJ with no statistically significant differences. While some differences are
observed in the maximum forces and works of detachment, the variations are less than a factor of
two and the lowest values are not associated with the fibronectin. Any effects of the cantilever
functionalization on cell-surface interaction after 30 minutes contact were too small to be
detected.
Chapter 4 Cantilever functionalization for cell detachment
74
Mean ±SE Mean ±SE
Concanavalin A 180 55 2.5 0.8Fibronectin 230 47 3.3 0.7Poly-L-lysine 190 31 2 0.5Zirconium ‒ ‒ ‒ ‒Native silicon ‒ ‒ ‒ ‒
Cantilever functionalizationMaximum force of detachment (nN) Work of detachment (pJ)
Table 4.2 Comparison of the maximum forces and works of detachment of 3T3 cells detached from glass surface
using four cantilever functionalizations: concanavalin A, fibronectin, poly-L-lysine and zirconium.
The acquisition of a sufficiently large data set for a statistically significant analysis of cell/surface
adhesion forces was difficult under these experimental conditions. Force distance curves from
twenty separate cells were used for each condition. Only three cells detached from the surface
using cantilevers functionalized with concanavalin A, so only three values (15% of cell
detachment) were available for analysis. The standard error was taken as characteristic of the
variance in order to consider the sample size because it estimates the standard deviation of the
sample mean of a population mean. The three values obtained for the two mechanical parameters
of detachment using concanavalin A-functionalized cantilevers are probably not representative of
a population mean. However, the results seem to indicate similar detachment forces from the
glass surface for the three cells that were detached.
4.4. Conclusion Force spectroscopy can be used to detach single adherent mouse fibroblasts from glass surfaces.
The necessary strong adhesion between cell and cantilever can be obtained by functionalizing the
cantilever with fibronectin. Fibronectin is recognized by integrins that mediate cell-surface
interactions and therefore promotes cell attachment. Another advantage is that the integrins
transmit the traction forces directly to the cytoskeleton157.
Measurements of the maximum forces and works of 3T3 cells detached from their growing
substrate were used to investigate the influence of the cantilever functionalization on the adhesion
of cells to surfaces. Fibroblast adhesion was shown to be similar on glass surfaces independently
Chapter 4 Cantilever functionalization for cell detachment
75
of the cantilever functionalization. However, incomplete sample detachments led to less precise
characterizations of cell detachment forces.
The contact time between cell and cantilever was minimized to thirty minutes to avoid a major
reorganization of the focal adhesion proteins binding the cells on their growing substrate.
Fibronectin-functionalized cantilevers and a contact time of thirty minutes were used to detach
adherent cells forn the rest of this work.
Chapter 4 Cantilever functionalization for cell detachment
76
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
77
Chapter 5
Cell adhesion on functionalized surfaces
for cell sheet engineering‡
In this chapter, the detachment of living adherent cells by force spectroscopy was tested on a
number of chemically functionalized surfaces in order to validate the technique. The objective is
to determine if long-term adhesion measurements are useful in the development of surfaces for
tissue engineering. The adhesion of living fibroblasts was studied twenty-four hours after seeding.
The cantilevers were functionalized for cell detachment in long-term adhesion measurements.
The cells were grown on glass surfaces as well as on surfaces used for cell sheet engineering:
glass surfaces coated with polyelectrolyte multilayers (of poly-L-lysine and hyaluronic acid) and
PNIPAM films. Individual adherent cells were detached from their culture substrate using an
AFM cantilever coated with fibronectin. The maximum forces of detachment of each cell were
measured and taken as characteristic of the cellular adhesion.
______________________________________________________________________________‡Part of this chapter was included in Quantification and characterization of single cell adhesion on functionalized
surfaces for cell sheet engineering. Weder G., Guillaume-Gentil O., Matthey N., Montagne F., Heinzelmann H.,
Vörös J. and Liley M. (submitted to Biomaterials).
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
78
5.1. Introduction
5.1.1. Tissue engineering
Tissue engineering35 is a multidisciplinary field involving the development of biological
substitutes and/or the fostering of tissue remodelling with the purpose of repairing or enhancing
tissue function192. Tissue engineering includes biomaterials193 that are designed to direct cells in
the formation of functional tissue by providing both physical and chemical cues. Finally,
engineering design aspects are very important for two-dimensional cell expansion and three
dimensional tissue growth.
Cells are often seeded into an artificial structure capable of supporting three-dimensional tissue
formation. These structures, typically called scaffolds194, serve as a synthetic extracellular matrix.
They often mimic the in vivo environment and allow the cells to influence their own
microenvironment. Common scaffolds use natural biopolymers or synthetic polymers. The most
commonly natural biopolymers include demineralised bone matrix195, agarose196, collagen197,
hyaluronan198 and alginate199. Synthetic polymers use mainly polyglycolic acid, polylactic acid
and their copolymers that are hydrolytically degradable polymers200,201,202. As an alternative, a
variety of hydrogels, a class of highly hydrated polymer materials, are also employed as scaffold
materials203,204.
These artificial scaffolds have been used in various tissue engineering applications205 such as
fractures repairing206,207. Ideally, they should not only promote cell adhesion, growth, and
revascularization but also be biodegradable without toxic and inflammatory responses. The
synchronization of the rate of new tissue formation with the rate of scaffold degradation has not
been totally solved208,209,210. In order to avoid some of these limitations of tissue reconstruction
using biodegradable scaffolds, Okano et al. developed “cell sheet engineering”211. This concept is
based on the use of sheets of cells for tissue reconstruction instead of individual cells.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
79
5.1.2. Cell sheet engineering
Cell sheet engineering is based on the control of cell adhesion, so that intact sheets of confluent
cells may be recovered with minimal damage to cell structure and function. Clinical applications
include the repair of ocular trauma by corneal epithelial cell sheet transplantation212,213. Similarly,
multilayered cell sheets have been used in cardiac tissue regeneration in rats214.
Various polymers and copolymers of poly(N-isopropylacrylamide) (PNIPAM) have been used as
coatings to control cell-surface adhesion215,216,217,211,218. These thermally-actuated polymers show
a phase transition between a collapsed state above their lower critical solution temperature
(LCST) and an extended, highly hydrated state below their LCST. Above the LCST, which is
typically around 32 °C, cells adhere, spread and proliferate on a PNIPAM-coated surface, while
below the LCST, cells detach spontaneously from the surface. These coatings have been
successfully applied to produce many types of cell sheets including oral mucosal epithelial212,
aortic endothelial219, urothelial220 as well as periodontal ligament cells221, cardiomyocytes222 and
keratinocytes223.
Polyelectrolyte multilayer films are also being developed, as an alternative to PNIPAM coatings,
to control the adhesion of several cell types224,225,226,227 including human mesenchymal stem
cells228. Polyelectrolyte layers are built up by adsorbing polyions onto oppositely charged
surfaces via electrostatic interactions229,230. Multilayered polyelectrolyte films have been shown
to desorb from conductive substrates on the application of an electrical potential231,232. The first
step in the preparation of cell sheets consist of growing cells to confluence onto polyelectrolyte
thin films. The cell sheets then detach either spontaneously or under electrical control233.
Electrical desorption has been shown to be effective for several cell types. In contrast, it has been
postulated that the spontaneous detachment requires weak adhesion to the substrate and high
cell/cell cohesion.
An extensive literature on these two polymer-based coatings documents their properties.
However, to date, there have been no quantitative investigations of their influence on cell
adhesion.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
80
5.2. Long-term adhesion to glass at 37 °C and 27 °C Direct cell adhesion measurements were carried out by detaching single adherent fibroblasts from
glass surfaces using an atomic force microscope and a temperature-controlled fluidic chamber.
3T3 cells were grown for 24 hours on a glass surface. The glass sample was placed in the fluidic
chamber and a single adherent cell was selected. To ensure that the interaction between cell and
surface was similar for all measurements, cells of comparable size were selected for each
condition. The extremity of a fibronectin-decorated cantilever was precisely positioned above the
targeted cell (Fig. 5.1A). The cantilever was gently pressed onto the single adherent cell with a
predefined contact force of 1.5 nN for 30 min at constant height to allow the cell to bind to the
cantilever. Finally the cantilever was withdrawn at 0.5 µm/s until the cell detached either from
the surface or from the cantilever. The viability of the cell after detachment was assessed by
visually observing its active re-spreading on the cantilever (Fig. 5.1B). For each condition,
twenty different cells were probed. Each time a freshly prepared cantilever and new sample of
cells were used.
The force exerted on the cell during this process was continuously recorded. These forces are
typically displayed as a function of the distance between cantilever tip and surface in a force
distance curve (Fig. 5.1C). The maximum force corresponds to the maximal deflection of the
cantilever. There were two possible outcomes of the cell detachment experiments; detachment of
the cell from the glass surface occurred when the adhesion between cell and cantilever was
stronger than that between cell and substrate. In contrast, when the adhesion between cell and
glass surface was stronger, the cell detached from the cantilever. The percentage of cell
detachment gave qualitative information about the cell/surface interaction. The maximum force
of detachment was evaluated separately for experiments where the cell detached from the surface
and those where it did not.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
81
Fig. 5.1. (A) Schematic of the detachment of a single adherent cell by force spectroscopy. In the initial phase of the
approach there is no contact between the cantilever and the adherent cell (A I-II). The cantilever is pressed onto the
adherent cell until a preset maximal force of 1.5 nN is attained (A III). The position of the cantilever is held constant
for 30 min before it is withdrawn at 0.5 µm/s (A IV). Finally, the cell is either on the cantilever if the cell detaches
from the surface (A V, possibility 1), or on the surface if the interaction between cell and surface is stronger than the
interaction between cell and cantilever (A VI, possibility 2). (B) The living detached cell with the last protrusion of
anchoring (B I) is observed after 3 min (B II) and 30 min (B III) to control the re-spreading of the cell on the
cantilever. (C) During the separation of the cell from the surface (or from the cantilever) a force-distance curve is
recorded indicating the maximum force and distance of detachment. The hatched area shows the work of
detachment. On both panels, red defines the approach and blue defines the retraction.
Detachment experiments on glass were carried out at both 37 °C and 27 °C. Two temperatures
were necessary in order to have a direct comparison with measurements on PNIPAM coatings
above and below the LCST and to exclude any possible effects of a physiological response of the
cells to the change in temperature.
In the detachment experiments carried out at 37 °C, seventy-five percent of the cells were
detached from the glass surface whereas twenty-five percent of the cells were left on the surface.
No qualitative differences were observed between force-distance curves where cells detached and
those where the cells remained on the glass surface (Fig. 5.2).
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
82
Fig. 5.2. Typical force-distance curves showing the detachments of single adherent fibroblasts either from a glass
surface (green and blue) or from the cantilever (red and black) at 37 °C using a fibronectin-decorated cantilever.
The mean values of the maximum forces of detachment were 230 nN for the cells detached from
the surface and 150 nN for the cells detached from the cantilever (Fig. 3 and Table 1).
Surprisingly, no statistically significant differences were observed between cells detaching from
the glass surface or from the cantilever (two sample T-test, p-value 0.05).
The maximum forces of detachment of the cells exposed to a temperature of 27 °C for 1 h were
not statistically different from those of the cells continuously incubated at 37 °C. The mean
maximum force of detachment from glass at 27 °C was 200 nN (Table 1), while the mean
maximum force of detachment from the cantilever was 170 nN. The maximum forces of
detachment from the glass surface and from the cantilever were not statistically different. Eighty
percent of the cells detached from the surface and twenty percent from the cantilever. Any
possible effect of temperature was too small to be observed in this study.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
83
Fig. 5.3. Histogram showing the distribution of the maximum forces of detachment of single adherent 3T3 cells
either from the glass surface (red) or from the cantilever (blue) at 37 °C.
Mean (nN) ±SE
Glass 37°C Glass 27°C
From surface From surface
From surface 230 47 0.8205
From cantilever 150 20 0.4145
From surface 200 27
From cantilever 170 43 0.6324
Glass 37°C
Glass 27°C
Two sample T-test
Table 5.1 Comparison of the maximum forces of detachment of mouse fibroblasts on glass at 37 °C and 27 °C (SE:
standard error). Data were evaluated using the two sample T-test and the limit of significance was fixed at a p-value
of 0.05. The values ≥0.05 indicate that the conditions are not significantly different.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
84
5.3. Cell adhesion on polyelectrolytes at 37 °C
5.3.1. Adhesion forces
Multilayer polyelectrolyte coatings were prepared on glass by alternately spraying dilute
solutions of the polycation poly(L-lysine) (PLL) and the polyanion hyaluronic acid (HA). Two
coating types were tested: coatings with one layer of each polyelectrolyte (PLL/HA)1 and
coatings with nine layers of each polyelectrolyte (PLL/HA)9.
Detachment experiments were carried out on adherent 3T3 cells on the polyelectrolyte surfaces at
37 °C as described for glass. The results of the cell detachments from the surface were similar for
(PLL/HA)1 to those obtained on glass: sixty percent of the cells detached from (PLL/HA)1. The
mean value of the maximum force of detachment was 200 nN (Fig. 5.4 and table 5.2). The two-
sample T-test showed no statistically significant differences between cell adhesion on glass or
(PLL/HA)1. Additionally, no statistically significant differences were observed between the mean
values of the maximum forces of detachment from the (PLL/HA)1 surface or from the cantilever.
Fig. 5.4. Histogram showing the distribution of the maximum forces of detachment of single adherent 3T3 cells on
polyelectrolytes films at 37 °C: (PLL/HA)1 in red and (PLL/HA)9 in blue. The cells detach either from the surface
(dark color) or from the cantilever (light color). All the cells detach from the surface on (PLL/HA)9.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
85
In contrast, the results obtained on (PLL/HA)9 were very different: All the adherent cells were
detached from the surface. The mean maximum force of detachment was 100 nN – approximately
half of the value observed on glass or on (PLL/HA)1 (Fig. 5.4 and table 5.2).
Mean (nN) ±SE
Glass 37°C (PLL/HA)1From surface From surface
From surface 200 22 0.9824
From cantilever 220 53 0.9362
(PLL/HA)9 From surface 100 6 0.0003 0.0000
Two sample T-test
(PLL/HA)1
Table 5.2 Comparison of the maximum forces of detachment of mouse fibroblasts on glass at 37 °C and 27 °C (SE:
standard error). Data were evaluated using the two sample T-test and the limit of significance was fixed at a p-value
of 0.05. Values ≥0.05 indicate that the conditions are not significantly different.
5.3.2. Characterization of PLL/HA substrates*
The buildup of (PLL/HA)n multilayers is characterized by the initial formation of isolated
polyelectrolyte complexes that grow by addition of new polyelectrolyte layers and by mutual
coalescence of the complexes234. The growth and coalescence of these complexes finally leads to
the formation of continuous films, and the number of layer pair depositions required to reach a
continuous coverage of the substrate depends highly on the working conditions. Figure 5 shows
the morphologies of the (PLL/HA) coatings used in this study, which both consisted of randomly
distributed polyelectrolyte complexes. The deposition of (PLL/HA)1 yielded nano-droplets
covering less than 1% of the substrate, with heights ranging from 5 to 20 nm. (Fig. 5.5B) The
surface modification with (PLL/HA)9 resulted in polyelectrolyte complexes covering more than
50% of the substrate, with droplet heights around 100 nm in average. (Fig. 5.5C)
______________________________________________________________________________*AFM characterization of the PLL/HA layers was carried out by O. Guillaume-Gentil at ETH Zurich (Switzerland).
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
86
Fig. 5.5. Characterization of PLL/HA modified substrates by atomic force microscopy. (A) Unmodified glass
substrate. (B) (PLL/HA)1 on glass. (C) (PLL/HA)9 on glass. The graphs show one representative profile for each
AFM images.
5.3.3. Discussion of polyelectrolyte coated surfaces
Cell adhesion on (PLL/HA) multilayers has been shown to be relatively low233,235. In general,
polyelectrolyte multilayers based on biopolymers or polypeptides like PLL/HA are considered
soft, highly hydrated materials, and it has been shown that their cell adhesive properties relate
mainly to their hydration degree and viscoelastic properties, regardless of serum protein
adsorption236. As such, one can consider that (PLL/HA)1 coatings do not significantly affect the
hydration and stiffness of the glass substrate due to the low amount of adsorbed polyelectrolytes
and the low surface coverage. However, (PLL/HA)9 coatings yielded bigger complexes and
higher surface coverage, significantly affecting the substrate properties, and consequently its cell
adhesive properties.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
87
5.4. Cell adhesion on PNIPAM at 37 °C & 27 °C
5.4.1. Principle
The second surface chemistry investigated was a reactive PNIPAM layer. This polymer exhibits a
lower critical solution temperature (LCST) in aqueous solution at approximately 32 °C. Above
the LCST, the PNIPAM layer is present in a compact relatively hydrophobic form, while below
the LCST the layer changes to an expanded, swollen and hydrophilic state.
The PNIPAM layers were produced by grafting PNIPAM chains to a thin layer of gold on glass
substrates using a self-assembled monolayer (SAM-COOH) of thiols (HS(CH2)11CO2H) as an
intermediate coupling agent. The amine-terminated PNIPAM was spin-coated onto the reactive
SAM of thiols and the substrate was then annealed above the glass transition temperature to
enable the amine groups to react with the SAM-COOH.
5.4.2. Adhesion forces
Cell detachment experiments were carried out on adherent 3T3 cells incubated for 24 hours at 37
°C on the PNIPAM-functionalized surfaces as described for the glass and polyelectrolyte
substrates. The results obtained for PNIPAM at 37 °C were similar to those obtained on glass and
on (PLL/HA)1. Sixty percent of the cells detached from PNIPAM at 37 °C. The mean value of
the maximum force of detachment was 270 nN (Fig. 5.6 and table 5.3). No statistically
significant differences were observed in the maximum forces of detachment for the cells detached
from the PNIPAM surface or from the cantilever.
Cell detachment experiments were also carried out at 27 °C. At the start of the experiment the
temperature was reduced to 27 °C for 20 minutes during which time the PNIPAM layer changed
from a compact to an extended configuration215. After twenty minutes, the cells showed a
retracted morphology but were still firmly attached to the surface (Fig. 5.7). The temperature was
maintained at 27 °C for the rest of the detachment experiment, which was carried out as
described for glass and polyelectrolytes. Cell adhesion was dramatically reduced at 27 °C. All the
cells were released from the surface. The mean maximum force of detachment was 10 nN (Table
5.3).
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
88
Fig. 5.6. Histogram showing the distribution of the maximum forces of detachment of single adherent 3T3 cells on
PNIPAM at 37 °C in red and at 27 °C in blue. The cells detach either from the surface (dark color) or from the
cantilever (light color). All the cells detach from the PNIPAM surface at 27 °C.
Fig. 5.7. Schematic and optical images showing the morphological response of single adherent 3T3 cells on thermo-
responsive 100%-PNIPAM layers (A) at 37 °C and, (B )after cooling the sample at 27 °C for 20 min. 100%-PNIPAM
induces a retraction of the cell at 27 °C.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
89
Mean (nN) ±SE
PNIPAM 100% 37°C Glass 37°C Glass 27°CFrom surface From surface From surface
From surface 270 50 0.3829 0.2368
From cantilever 350 83 0.4302
PNIPAM 100% 27°C From surface 10 3 <0.0001 <0.0001 <0.0001
PNIPAM 100% 37°C
Two sample T-test
Table 5.3 Comparison of the maximum forces of detachment of mouse fibroblasts on 100%-PNIPAM and glass at 37
°C and 27 °C (SE: standard error). Data were evaluated using the two sample T-test and the limit of significance
was fixed at a p-value of 0.05. Values ≥0.05 indicate that the conditions are not sig nificantly different whereas
values <0.05 indicate that the conditions are significantly different.
5.4.3. Discussion of PNIPAM functionalized surfaces
The study of PNIPAM layers showed a remarkable switching behavior between the adhesive
state at 37 °C and the non-adhesive state at 27 °C. While this behavior has been extensively
studied and investigated in past years, this is the first study to quantify these changes in adhesion.
The mean maximum force of detachment at 27 °C was around 10 nN indicating a reduction in
cell adhesion of more than an order of magnitude between the adhesive and non-adhesive states.
5.5. Controlling cell adhesion using a patterned
PNIPAM coating
5.5.1. Principle
A patterned PNIPAM coating was used to control cell adhesion by locally detaching the cell from
the surface on lowering the temperature at 27 °C. The patterned film was obtained using the
grafting method previously described except that the uniform layer of gold was replaced by a
patterned gold layer. The gold layer was composed of squares of 3 x 3 µm, and covered
approximately 30% of the glass substrate (Fig. 5.8).
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
90
Fig. 5.8. Single adherent 3T3 cell grown on PNIPAM-patterned glass and cooled to 27 °C for 1h showing the actin
fibres (labeled with AlexaFluor 488 Phalloidin) by confocal microscopy. In average, 29 squares of PNIPAM (in
black) are in contact with each cell.
5.5.2. Adhesion forces
Cell adhesion measurements on PNIPAM-patterned glass surfaces were performed using the
experimental procedure described previously. The results obtained for PNIPAM-patterned glass
at 37 °C were similar to those obtained on plain glass. Eighty-five percent of cells detached from
PNIPAM-patterned glass at 37 °C. The mean value of the maximum force of detachment was 240
nN (Fig. 5.9 and table 5.4).
The results obtained at 27 °C were different from those obtained at 37 °C. Cooling the sample to
27 °C for 1 h did not alter the morphology of the cells (Fig. 5.10). Ninety percent of cells
detached from PNIPAM-patterned glass at 27 °C. The mean value of the maximum force of
detachment was 110 nN (Table 5.4). A statistical comparison of the maximum forces of
detachment showed a clear difference (p-value 0.0007).
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
91
Fig. 5.9. Histogram showing the distribution of the maximum forces of detachment of single adherent 3T3 cells on
PNIPAM-patterned glass at 37 °C in red and at 27 °C in blue. The cells detach either from the surface (dark color)
or from the cantilever (light color).
Fig. 5.10. Schematic and optical images showing the morphological response of single adherent 3T3 cells on
thermo-responsive 33%-PNIPAM layers (A) at 37 °C and, (B )after cooling the sample at 27 °C for 20 min. 33%-
PNIPAM does not induce any major morphological modifications of the cell at 27 °C.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
92
Mean (nN) ±SE
PNIPAM 33% 37°C Glass 37°C Glass 27°CFrom surface From surface From surface
PNIPAM 33% 37°C From surface 240* 35 0.6419 0.4546
PNIPAM 33% 27°C From surface 110** 19 0.0007 0.0035 0.0030
Two sample T-test
Table 5.4 Comparison of the maximum forces of detachment of mouse fibroblasts on 33%-PNIPAM and glass at 37
°C and 27 °C (SE: standard error). Data were evaluated using the two sample T-test and the limit of significance
was fixed at a p-value of 0.05. Values ≥0.05 indicate that the conditions are not sig nificantly different whereas
values <0.05 indicate that the conditions are significantly different. *This value was calculated for the 17 cells that detached from the surface (85% of cell detachment)
**This value was calculated for the 18 cells that detached from the surface (90% of cell detachment)
5.5.3. Discussion of PNIPAM patterned surfaces
A patterned glass/PNIPAM surface has been also studied. The glass adhesive substrate was
covered with an array of small gold squares functionalized with PNIPAM. The array was chosen
so that each adherent cell covered on average 29 squares and one third of the glass surface was
covered with the gold-PNIPAM coating. A reduction in temperature to 27 °C should therefore
result in a local de-adhesion of the cell at each of the 3 x 3 micron squares of PNIPAM under the
cell, while leaving the gross morphology of the cell and, to a large extent, the cytoskeleton
unchanged. Ideally this would reduce the maximum detachment force of the cell by one third, so
that highly adherent cells could be detached using fibronectin-coated AFM cantilevers.
The results reported here show that the 3T3 cells used in this study proliferate well on the
patterned PNIPAM/glass substrates and have similar morphologies to those grown on plain glass
surfaces. In addition, at 37 °C, cellular adhesion to the PNIPAM/glass surfaces is
indistinguishable from that on plain glass. When the temperature is reduced to 27 °C, there is no
observable change in cellular morphology, but there is a clear and significant reduction in mean
detachment forces from 240 nN to 110 nN.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
93
5.6. Discussion
5.6.1. Detachment of adherent cells
The maximum force needed to detach a cell from the culture surface was measured separately for
each individual cell and was taken as characteristic of the adhesion of the cell. On most surfaces,
a very broad distribution of results was obtained, indicating a large heterogeneity in the
attachment of the cells. Despite the wide distribution of individual values, statistically significant
results were obtained. One notable exception was the (PLL/HA)9 surface which had a strikingly
narrow distribution of cell adhesions.
The results for cells detaching from the culture surface or from the cantilever were evaluated
independently. Surprisingly, similar distributions of adhesion strengths were observed between
cell/culture surface and the cell/cantilever for most of the culture surfaces. This can clearly be
seen from the percentage detachments of the cells from the culture surfaces (60-85% of the cells
detached). Only on the two substrates with much lower maximum detachment forces – the
(PLL/HA)9 and the PNIPAM 100% (27 °C) surfaces – was it possible to detach all the cells from
the culture surfaces. These results suggest that the adhesion between cell and cantilever also
varies widely. Thus the exact percentage of cells detaching from the culture surface and the mean
maximum force obtained for a population of cells depends, for most of the surfaces studied here,
on the interplay of the two distributions: cell/surface adhesion and cell/cantilever adhesion.
Moreover, small changes in experimental parameters such as the cell/cantilever contact force or
the retraction speed, may have a strong influence on the percentage of cells that detach from the
quartz surface.
It was possible to quantify cell adhesion on glass, PNIPAM and (PLL/HA) polyelectrolyte
surfaces as well as on mixed glass/PNIPAM surfaces at 37 °C and 27 °C. Very similar mean
maximum detachment forces (200 – 270 nN) were observed on glass (at both 27 °C and 37 °C),
PNIPAM (100% and 33%) at 37 °C and on (PLL/HA)1 surfaces: all substrates on which the 3T3
cells studied proliferate well. On (PLL/HA)9 a very different cellular adhesion was observed,
with a much lower maximum detachment force of 100nN. This reduction in cellular adhesion
associated with an increase in the number of PLL/HA layers has been documented qualitatively
in the literature237,235. It should therefore be possible to correlate cell detachment forces with the
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
94
number of (PLL/HA) layers as well as with initial cellular proliferation and the later detachment
of confluent cell sheets.
5.6.2. Limitation of the sample size
The acquisition of a sufficiently large data set for a statistically significant analysis of cell
behavior is one of the major limitations of the technique. Single cell force spectroscopy is
currently a laborious technique because each cell must be individually bound to a clean freshly-
mounted AFM cantilever. Similarly each cell/substrate sample must be tested at the same time
after cell seeding (24 hours in this case). Force distance curves from twenty separate cells were
used for each experimental condition. In our hands, data from two separate cells could be
acquired per day per atomic force microscope under ideal circumstances.
A significant reduction in the standard errors associated with the means of the different force
distributions would require the number of measurements to be increased by a factor of at least
four. In future studies, an increased cell/cantilever adhesion – giving detachment of all cells from
all surfaces - might allow a more precise characterization of cell detachment forces: a slightly
larger sample size would be available and any skew in the distributions due to incomplete sample
detachment would be eliminated.
5.7. Conclusion Cell adhesion was quantified on a number of different chemically functionalized surfaces: plain
glass, glass coated with polyelectrolyte layers (PLL and HA), homogeneous PNIPAM films and
patterned surfaces with areas of PNIPAM and others of plain glass. On several surfaces,
measurements of cell adhesion were performed at both 37 °C and 27 °C. For most of the cell
culture surfaces very similar values were obtained for the maximum forces of detachment; for
glass at both 37 °C and 27 °C, 100% or patterned PNIPAM surfaces at 37 °C and for (PLL/HA)1
surfaces the mean maximum detachment forces were between 200 and 270 nN. The
measurements of cell adhesion on glass showed that a reduction of the temperature from 37 °C to
27 °C did not induce significant changes in cell adhesion due to physiological changes in the cell.
Very different results were observed on (PLL/HA)9 layers, where mean maximum detachment
forces were 100 nN. This reduced level of cell adhesion is clearly sufficient to allow good initial
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
95
cell proliferation followed, according to literature reports, by detachment of confluent cell sheets.
Reducing the temperature of the homogeneous PNIPAM layers to below the LCST reduced the
cell adhesion by a factor of more than one order of magnitude. This effect has been extensively
studied and reported in the literature. However, this is the first time, to our knowledge, that the
effect has been measured quantitatively.
Finally, preliminary results on patterned glass/PNIPAM surfaces, showed that these substrates
can be used to reduce cell surface adhesion – in this case by a factor of two - while keeping cell
morphology unchanged. It is hoped that these substrates may be used to investigate the adhesion
of highly adherent cells to surfaces in a semi-quantitative way.
Single cell force spectroscopy was used to study the effects of surface modifications on cell
adhesion. These effects of modified surfaces on cell adhesion were quantified. Force
spectroscopy allows unrivalled spatial and temporal control of cells, as well as highly quantitative
force actuation and measurement under physiological condition. Force spectroscopy is a suitable
tool for the development of surfaces in cell sheet engineering.
Chapter 5 Cell adhesion on functionalized surfaces for cell sheet engineering
96
Chapter 6 Effect of sub-micron topography on cell adhesion
97
Chapter 6
Effect of sub-micron topography on cell
adhesion‡
In this chapter, the potential and limitations of force spectroscopy to detach adherent cells were
explored by altering the cell type and the topography of the surface. The adhesion of living
immortalized and primary fibroblasts to their culture substrate was studied twenty-four hours
after seeding.
The cantilevers were functionalized for cell detachment in long-term adhesion measurements.
Both primary fibroblasts and a continuous cell line were studied on flat and topographically
structured quartz surfaces. Individual cells were detached using an AFM cantilever, pressed onto
the cell for thirty minutes and then withdrawn. The force-distance curves obtained allowed the
maximum force, work and distance of detachment to be determined.
______________________________________________________________________________‡Part of this chapter was published in Use of force spectroscopy to investigate the adhesion of living adherent cells.
Weder G., Blondiaux N., Giazzon M., Matthey N., Klein M., Pugin R., Heinzelmann H. and Liley M. Langmuir,
2010, Article ASAP DOI: 10.1021/la904526u.
Chapter 6 Effect of sub-micron topography on cell adhesion
98
6.1. Introduction
6.1.1. Topography and cell adhesion
Adherence-dependent cells are profoundly influenced by the topography of the substrate to which
they adhere. Cellular responses such as adhesion, morphology, alignment, guidance, gene
expression and proliferation are all influenced by topography238,239,240,241,242,243. The effects may
differ widely depending on the dimensions and form of the topography244.
Brunette et al. divided cells into “rugophobic” cells, such as fibroblasts, that prefer smooth
surfaces over rough ones, and “rugophilic” cells, such as osteoblasts245,246. In the last ten years, it
has been shown that the rugophobia/rugophilia classification depends both on the dimensions of
the topography and on the cell type. A large and sometimes contradictory literature on this topic
seems to indicate a number of other poorly-controlled factors that influence cell response to
topography.
Taking the example of fibroblasts, many studies have shown that surface nanotopography affects
fibroblast response, with both increased247,244 and decreased248 adhesion observed. Nanometric
islands have been reported both to speed up initial cell adhesion249 and to have no influence at all
when compared with planar samples250. Numerous studies have shown a reduction in cellular
adhesion and a decrease in spreading when fibroblasts are grown on sub-micron topographies251
such as islands252, columns253 or pits254. In contrast, microtopography has been used to transform
non-adhesive into adhesive substrates for fibroblasts255 by increasing cellular adhesion.
While the effects of nano-sized topography on fibroblast adhesion remain unclear, most authors
report that sub-micron topographies inhibit fibroblast adhesion and result in cell rounding.
6.1.2. Topography and cell type
There are certainly several reasons why studies of cell/surface adhesion are so confused. In many
studies, surface chemistry is poorly controlled, and experimental parameters vary widely between
different research groups. However, the effects of topography on cell adhesion may also differ
widely depending on the cell type256. Immortalized and primary cells from the same tissue origin
have been shown both to exhibit distinct cell morphologies and mechanical properties179. The
effects of surface topography on cell adhesion can be very different for different continuous cell
Chapter 6 Effect of sub-micron topography on cell adhesion
99
lines and different from those of primary cells257. Although the effects of surface topography on
cell adhesion were demonstrated to depend on the cell type, there is a lack of suitable methods to
quantify cell/surface interactions.
Here, force spectroscopy is used to directly measure the adhesion of two cell types to their culture
substrates. The adhesion of immortalized and primary fibroblasts to polylysine-treated quartz
surfaces after 24 hours of growth in situ was first quantified. It was then compared with the
adhesion on identical quartz surfaces that have been structured with a sub-micron pillar motif.
6.1.3. Description of the sub-micron topography
Two different sub-micron topographies on quartz surfaces were tested. Each consisted of quartz
pillars with an average diameter of 400 nm and an approximate surface coverage of 30 %. In one
case the pillars were 270 nm high and in the other 520 nm high. Both topographies are shown in
figure 6.1. The wide distribution of pillar diameters is due to the use of a polymer blend mask in
the fabrication process. Differences in the shape of the pillars are due to differences in the
fabrication process and particularly the lift-off step. After fabrication the samples were
thoroughly cleaned to ensure a controlled and reproducible surface chemistry. All traces of
chromium and amorphous silicon used as etch masks were removed using a chrome etchant and
potassium hydroxide solution. Possible fluorine traces from the dry etching step were removed by
an oxygen plasma.
Fig. 6.1. Scanning electron microscopy pictures of sub-micron pillars in quartz with a height of 270 nm (A), 520 nm
(B) and a flat control surface (C).
Chapter 6 Effect of sub-micron topography on cell adhesion
100
6.2. Long-term adhesion to flat quartz Cell adhesion was measured directly by detaching single adherent 3T3 fibroblasts from quartz
surfaces coated with poly-L-lysine. The forces exerted on the cell during this process were
continuously recorded and the values were represented in a force-distance curve. Each force-
distance curve consisted of one peak independently of whether or not the cell detached from the
quartz surface. Three mechanical parameters were extracted from each curve i.e. the maximum
force, the work and distance of detachment.
The percentage of cells detached from the surface gives the first qualitative information about the
relative adhesion forces. Seventy percent of cells detached from the flat quartz. The maximum
force of detachment was evaluated separately for experiments where the cell was detached from
the surface and those where it did not. No significant statistical differences were observed
between cells detaching from the quartz surface and from the cantilever (two sample T-test, p-
value 0.05) (Fig. 6.2). The mean values of the maximum forces of detachment were 420 nN for
the cells detached from the surface and 310 nN for the cells detached from the cantilever (Table
6.1B)
Fig. 6.2. Histogram showing the mean values of the maximum forces of detachment obtained for the detachments
from the surface (grey) and from the cantilever (black). Vertical lines indicate the means and the error bar is the
standard deviation.
Chapter 6 Effect of sub-micron topography on cell adhesion
101
The mean values for the work of detachment were 7.9 pJ for the cells detached from the surface
and 6.9 pJ for the cells detached from the cantilever (Table 6.1C). Again no significant statistical
differences were observed between the two populations.
The distance of retraction from the surface required to totally detach the cell was also analyzed.
The mean values of the distance of detachment were 33 µm for the detachments from the
substrate and 38 µm for the detachments from the cantilever (Table 6.1D). The two-sample T-test
showed no significant difference between the two populations.
6.3. Effect of sub-micron topography The percentage of cells detached from the quartz surfaces was greatly increased on both pillar
topographies. The percentage of cell detachment was 95 % on the 270 nm pillars and 100 % on
the 520 nm pillars. The maximum forces of detachment were dramatically reduced on the
microstructures, with mean values of 210 nN on the 270 nm pillars and 180 nN on the 520 nm
pillars (Table 6.1B). Wide dispersions in the force values were observed on both flat and
structured surfaces reflecting the heterogeneity of the cell adhesion properties within the same
population (Fig. 6.3).
Similarly, the work of detachment was reduced on the pillars. The mean values on the 270 nm
and 520 nm pillars were 2.6 pJ and 2.7 pJ (Fig. 6.4 and Table 6.1C). The analysis of the distance
of detachment showed that shorter distances were required to totally detach the cells from the
pillars. The values were 22 µm on both 270 nm and 520 nm pillars (Table 6.1D). No statistically
significant differences were observed between the 270nm and 520nm pillars.
Chapter 6 Effect of sub-micron topography on cell adhesion
102
Fig. 6.3. Histogram showing the distribution of the maximum forces of detachment of single adherent 3T3 cells
grown for 24 h on quartz surfaces: Flat (grey), 270 nm pillars (white) and 520 nm pillars (black).
Fig. 6.4. Histogram showing the distribution of the works of detachment of single adherent 3T3 cells grown for 24 h
on quartz surfaces: Flat (grey), 270 nm pillars (white) and 520 nm pillars (black).
Chapter 6 Effect of sub-micron topography on cell adhesion
103
Mean ±SEQuartz flat 70 Quartz flat270 nm pillars 95 From the surface 420 37520 nm pillars 100 From the cantilever 310 50
270 nm pillars* 210 36520 nm pillars 180 29
Mean ±SE Mean ±SEQuartz flat Quartz flatFrom the surface 7.9 1 From the surface 33 3From the cantilever 6.9 1.7 From the cantilever 38 8
270 nm pillars* 2.6 0.7 270 nm pillars* 22 2520 nm pillars 2.7 0.7 520 nm pillars 22 2
A. Percentage of cell detachment (%)
C. Work of detachment (pJ)
B. Maximum force of detachment (nN)
D. Distance of detachment (µm)
Table 6.1 Comparison of the percentages of cell detachment and the mean values of the maximum force of
detachment, the work of detachment, and the distance of detachment of 3T3 cells on three quartz surfaces: flat, 270
nm pillars and 520 nm pillars (SE: standard error). *These values were calculated for the 19 cells that detached
from the quartz surface (95 % of cell detachment).
6.4. Comparison with primary mouse fibroblasts A key point in the study of cell/surface interactions and the role of topography is the choice of
cell type. Both immortalized cell lines and primary cells have been studied and very different
results have been found for different cell lines and primary cells. For this reason, the study was
extended to the more biologically-relevant, but harder to study, primary fibroblasts. The primary
fibroblasts tested were obtained from mouse embryos. As 3T3 cells showed no differences in
adhesion when the height of the submicrometer pillars was changed from 270 nm to 520 nm, the
primary fibroblasts were detached only from the 520 nm pillars.
Chapter 6 Effect of sub-micron topography on cell adhesion
104
6.4.1. Cell adhesion
It was found that – with the experimental parameters used for 3T3 cells – very few primary cells
detached from the flat quartz surface: 90 % of the cells were left on the surface. On the 520 nm
pillars the percentage of detachment increased to 30 %.
Since so few cells detached, the analysis of the force distance curves essentially characterizes the
interaction between cell and cantilever. The mean values of the maximum force of detachment
were 190 nN on the flat quartz and 210 nN on the 520 nm pillars (Table 6.2B). The mean values
obtained for the work of detachment were 1.7 pJ on the flat surface and 3.8 pJ on the 520 nm
pillars (Table 6.2C). The differences between the values obtained on flat quartz and on the pillars
were not statistically significant (two-sample T-test, p-value 0.05) as can be expected from the
fact that they mostly reflect the cell/cantilever interactions. Finally, the mean values for the
distance of detachment were between 13 and 16 µm showing that the primary cells were less
stretched than the 3T3 cells during detachment (Table 6.2D).
Mean ±SEQuartz flat 10 Quartz flat 190 41520 nm pillars 30 520 nm pillars 210 58
Mean ±SE Mean ±SEQuartz flat 1.7 0.5 Quartz flat 13 2520 nm pillars 3.8 1.4 520 nm pillars 16 3
B. Maximum force of detachment (nN)
D. Distance of detachment (µm)
A. Percentage of cell detachment (%)
C. Work of detachment (pJ)
Table 6.2 Comparison of the percentages of cell detachment and the mean values of the maximum force of
detachment, the work of detachment, and the distance of detachment of PMEF cells on two quartz surfaces: flat and
520 nm pillars (SE: standard error).
6.4.2. Cell proliferation
Cell proliferation on the test substrates was investigated to confirm the viability of the cells on
the flat and structured surfaces. The Alamar Blue assay incorporating a non-toxic fluorometric
growth indicator based on detection of metabolic activity was used. The quartz surfaces were
particularly attractive for the 3T3 cells showing an optimal proliferation activity that was not
Chapter 6 Effect of sub-micron topography on cell adhesion
105
modified by the topography (Fig. 6.5A). In contrast, the primary cells were less viable than the
3T3 cells, with a slow and constant proliferation that was reduced on the pillars (Fig. 6.5B).
Fig. 6.5. Alamar Blue assay results from 3T3 mouse fibroblasts (A), and primary mouse embryonic fibroblasts (B).
They were cultured on structured and flat quartz for 4 days and each value represents the mean of 6 samples.
6.4.3. Cell morphology
Differences in morphology were observed between the immortalized and primary fibroblasts and
on the different quartz surfaces. F-actin staining (phalloidin) and scanning electron microscopy
were used to compare cell morphologies.
3T3 cells grown on flat quartz had a spread morphology with a mean diameter of 50 µm (Fig.
6.6). In contrast, a spherical morphology was observed on both pillar structures with a mean
diameter of 30 µm. The fixing and dehydration of the cells considerably limited the extent to
which the images may be interpreted, particularly the position of the cell membrane on the pillar
structures.
The primary cells had a highly spread and flattened morphology on flat quartz and were
significantly larger at around 150 µm in diameter (Fig. 6.7). The 520 nm pillars dramatically
modified their morphology resulting in a spindle-shaped, flattened morphology with a
considerable reduction in spreading.
Chapter 6 Effect of sub-micron topography on cell adhesion
106
Fig. 6.6. Comparison of 3T3 cells by confocal microscopy (ACE) showing the actin fibres (labeled with AlexaFluor
488 Phalloidin) and scanning electron microscopy (BDF) on different quartz surfaces: flat (AB), 270 nm pillars
(CD) and 520 nm pillars (EF).
Fig. 6.7. Comparison of PMEF cells by confocal microcopy (AC) showing the actin fibres (labeled with AlexaFluor
488 Phalloidin) and scanning electron microscopy (BD) on two quartz surfaces: flat (AB) and 520 nm pillars (CD).
Chapter 6 Effect of sub-micron topography on cell adhesion
107
6.5. Discussion
6.5.1. Detachment of adherent cells
The force distance curves obtained during cell detachment were analyzed to obtain three
characteristic mechanical parameters: the maximum force applied during the detachment; the
work necessary for cell detachment; the distance of retraction at which the cell detached from the
surface. Of the three, the maximum force was the most intuitively accessible and seemed most
characteristic of the different experimental conditions used in this study. The rest of the
discussion is focussed on this parameter.
The maximum forces applied in the detachment experiments on 3T3 cells on quartz (Fig. 6.2)
reveal, firstly, that the adhesion between cell and substrate varies widely. In order to investigate
the sensitivity of this technique to changes in cell/surface adhesion, two important experimental
parameters were altered: the topography of the quartz surface and the cell type. Changing the
quartz substrate from a flat surface to one covered with sub-micron pillars resulted in a
significant reduction in cell adhesion. The fraction of cells detached from the substrate went from
70% to 95-100% while the mean maximum force applied to the cell during detachment was
reduced by a factor of approximately two. These results are in accordance with most literature
reports on the effect of topography on fibroblast adhesion252,253,251,254,258,259,260.
6.5.2. Cell adhesion to quartz and glass
Adhesion strength for 3T3 cells detaching from quartz surfaces coated with poly-L-lysine or from
glass surfaces were different. While the percentages of cell detachment were similar on both
surfaces (70%-75%), the maximum forces of detachment were different. The mean maximum
forces of detachment were 420 nN from flat quartz surfaces coated with poly-L-lysine and 230
nN from plain glass surfaces. The difference of the maximum forces of detachment is probably
due to the presence of poly-L-lysine on quartz. In contrast, the explanation of the similar
percentages of detachment remains unclear. The fibronectin-based functionalization of the AFM
cantilevers is capable of supporting at least a mean maximum force of detachment of 420 nN.
The cantilever functionalization was also capable of detaching all the cells from the quartz
surfaces with sub-micron pillars. Therefore, there is an explanation that is independent of the
efficiency of the cantilever functionalization. The cells might have exhibited a different
Chapter 6 Effect of sub-micron topography on cell adhesion
108
morphology modifying their area of contact with the AFM cantilever but in this case, the
percentages of cell detachment should have been different. Alternatively, poly-L-lysine may
active cell adhesion not only on the surface but also on the cantilever, resulting in higher
maximum forces of detachment and similar percentages of cell detachment than from glass.
6.6. Limitation of the cell type When the 3T3 cells were replaced by PEMF cells, only 10% of the cells detached from flat
quartz, while 30% detached from the sub-micron pillars on quartz. The absolute numbers of cells
detached from the surfaces are so low that no meaningful quantitative analysis of cell/substrate
adhesion is possible. The force distance curves obtained with PEMF cells do, however, give
information about the cell/cantilever interactions. The mean maximum forces obtained on PEMF
cells were approximately 200 nN on both flat and structured quartz. In contrast the mean
maximum forces obtained for the detachment of the 3T3 cells from the cantilever were around
300 nN. A statistical analysis finds the probability that these distributions are the same to be 5%
(p=0.05), the limit of statistical significance chosen for this study. It is likely, that a reduction in
adhesion to the cantilever contributes to the failure to detach PEMF from the quartz surface.
The differences in cell/cantilever adhesion may be linked to inherent differences in the adhesive
properties of 3T3 and PEMF cell surfaces, or to the speed of reaction of the different cell types. It
is likely, however, that the very different morphologies of 3T3 and PEMF cells also play a role.
3T3 cells on quartz are relatively thick – at least at the cell nucleus – when compared to the
extremely flat, spread form of the PEMFs. The raised cell nucleus allows a relatively large area
of contact between cell and AFM cantilever (which is tilted at 10° to the horizontal). In contrast,
it is very difficult to obtain a large contact area between PEMF and cantilever.
Despite the failure to detach the PEMF, it is possible to draw some qualitative conclusions about
their adhesion to the quartz surfaces. Firstly, the PEMF adhere more strongly to the flat quartz
surfaces than the structured quartz surfaces. Secondly, a comparison between the detachment of
3T3s from the 520 nm pillars (100% detachment with a mean maximum force of 180 nN) and
PEMF from the same structure (30% detachment with a mean maximum force of 210 nN) shows
clearly that the PEMF adhere more strongly to the structured quartz surfaces than the 3T3s.
Chapter 6 Effect of sub-micron topography on cell adhesion
109
The failure to detach a significant number of PEMF cells highlights a key issue with this
approach: if the number of cells detached from the substrate is close to 100% then the values
obtained for the detachment parameters (force, work and distance) may be considered
representative of the cell’s adhesion, irrespective of the forces between cell and cantilever.
However, as the percentage of cells detached from the substrate decreases, the accuracy of the
values obtained also decreases: a bias is introduced into the distribution because only the least
adherent cells can be measured.
6.7. Conclusion Force spectroscopy can be used to detach single adherent fibroblasts from flat and structured
quartz surfaces by traction normal to the surface. Measurements of the percentage of cells
detached from the substrate surface and the maximum force necessary for detachment were used
to investigate different factors influencing the adhesion of fibroblasts to surfaces. 3T3 mouse
fibroblast adhesion was shown to be higher on flat quartz surfaces and lower on quartz surfaces
with a structure of sub-micron pillars. The rugophobia of fibroblasts on sub-micron topography
has been reported by other authors252,253,251,254,258,259,260 but in this work the adhesion forces were
quantified. No differences in adhesion were observed when the height of the sub-micron pillars
was changed from 270nm to 520nm.
Primary embryonic mouse fibroblasts were also studied and were found to be rugophobic.
However, only very few PEMFs could be detached from the surface using the experimental
parameters optimized for 3T3s. For this reason it was not possible to quantify the PEMF adhesion
to the surface. Qualitatively, it is clear that PEMF adhesion is lower on structured quartz than on
flat quartz. The PEMF also adhere more strongly at least one of the quartz surfaces than the 3T3s.
Cell/cantilever adhesion seems lower for PEMF than for 3T3. A less favourable cell morphology
resulting in smaller contact area between cell and cantilever may contribute to this effect. This
reduced cell/cantilever adhesion for the PEMFs seems to be a major factor in the different
percentages of cell detachment. The different cell/cantilever adhesions obtained for different cell
types is a significant limitation of the technique because it renders comparisons between cell
types difficult. The experimental parameters of cell detachment have to be similar and optimized
for both cell types when adhesion forces have to be compared.
Chapter 6 Effect of sub-micron topography on cell adhesion
110
Chapter 7 Conclusions & Outlook
111
Chapter 7
Conclusions & Outlook
The main objective of this work was to use force spectroscopy to quantify the long-term global
adhesion between cells and surfaces and their response to modified surfaces. This objective was
achieved. Force spectroscopy was used to quantify the global adhesion forces of individual
adherent cells. Adherent cells were detached from glass surfaces modified with polyelectrolytes
and a thermo-responsive polymer, as well as from quartz surfaces with a structure of sub-micron
pillars. The cells were detached after twenty-four hours in culture using fibronectin-decorated
AFM cantilevers that were pressed onto the adherent cells for thirty minutes. The mechanical
parameters acquired during detachment were used to quantify the cell adhesion forces.
The first step was to verify if cell adhesion has to be studied independently of cell cycle or not.
Short-term adhesion was used to demonstrate that binding proteins at the cell membrane remain
similar both in number and in their binding properties during interphase and mitosis. The
rounding up and greatly reduced adhesion of cells during mitosis was associated with an
increased stiffness of the cell caused by a cytoskeletal reorganization. Mitosis was not paired with
large differences in the binding proteins at the cell membrane but with cytoskeletal changes. In
this way, it was demonstrated that cell adhesion can be studied independently of cell cycle as
Chapter 7 Conclusions & Outlook
112
long as mitotic cells are not chosen due to their different morphology. However, the
demonstration was performed using short-term adhesion with osteoblasts captured on the AFM
cantilever. It is hoped that results are similar for the adherent fibroblasts studied in the rest of the
thesis. A more powerful demonstration, verifying this, would use adherent fibroblasts,
synchronized in the different phases of the cell cycle, and detached from their culture substrate.
Long-term cell adhesion was quantified on glass surfaces coated with polyelectrolyte bilayers.
Large differences in cellular adhesion were observed depending on the number of polyelectrolyte
bilayers. The reduced level of cell adhesion associated with an increased number of bilayers was,
however, sufficient to allow good initial cell attachment and proliferation. Wide dispersions in
the force values were observed within the same condition reflecting the heterogeneity of the cell
population. However, the statistical analysis of the values indicated highly significant differences
between the conditions.
The measurements of cell adhesion on glass showed that a reduction of the temperature from 37
°C to 27 °C did not induce significant changes in cell adhesion due to physiological changes in
the cell. This result allows global cell adhesion measurements, not exceeding one hour, to be
performed without an accurate control of the temperature (between 27 °C and 37 °C).
Long-term cell adhesion was quantified on thermally-responsive PNIPAM brushes. Cell adhesion
was dramatically reduced by lowering the temperature to below the LCST. The observation of
cells between the adhesive and non-adhesive states indicates only if cells are detached or not. In
contrast, the quantification of the adhesion forces details the PNIPAM’s effect on cell adhesion in
both states. Glass surfaces patterned with periodic PNIPAM micro-domains were used to reduce
cell surface adhesion while keeping cell morphology unchanged. This approach to reduce cell
adhesion and to keep cell morphology could be interesting in the stimulation of single adherent
cells that are detachable. The stimulation could be performed at 37 °C and the detachment at 27
°C for further single cell analysis.
Long-term cell adhesion was shown to be higher on flat quartz surfaces than on quartz surfaces
with a structure of sub-micron pillars. This was already reported by other authors but here the
adhesion forces were quantified. In contrast to cell adhesion, cell proliferation was not affected
by the sub-micrometer pillars. No differences in adhesion were observed when the height of the
sub-micrometer pillars was changed. Three-dimensional positioning of cells was not clearly
Chapter 7 Conclusions & Outlook
113
determined by microscopic analysis due to artifacts coming from the cell fixation. The micro-
fabrication of higher quartz pillars in order to eliminate any contact of the cells with the surface
between the pillars was not possible.
Finally, an immortalized cell line was compared with primary cells in long-term adhesion
experiments. The failure to detach the primary cells revealed the importance of the cell type. This
allowed the potential and limitations of the technique in measuring cell/surface interactions to be
discussed in more detail. The differences of detachment between the two cell types may be linked
to several independent reasons including the contact area with the AFM cantilever and how
quickly the cells adhere to the cantilever. The cell surface-to-volume ratio is important because in
cases where the cell adhesion forces are greater than the cell cohesion forces, detachment of such
cells is not possible. Primary cells may break in case of strong connection with the AFM
cantilever.
As with most new techniques, single cell force spectroscopy needs to mature. The modification
of experimental parameters during this study highlighted some biological and physical
limitations. A key issue with the technique is the adhesion of the cells to the AFM cantilever used
to detach them. The cantilever functionalization is crucial to promote cell attachment. The contact
time cell/cantilever has to be minimized to limit the inevitable reorganization of the adhesion
cell/substrate. The connection could be addressed by a mechanical approach instead of
functionalizing the cantilever. A mechanical connection would suppress the reorganization of the
adhesion of the cell to the substrate and would reduce the time of the measurements. Hollow
force-controlled AFM cantilevers were used for local dispensing of a solution into individual
cells261. The adaptation of these micro-channeled cantilevers for aspiration instead of injection
could be used to capture single cells. The concept should be first validated for cell capture of
non-adherent cells.
Another significant limitation was the acquisition of a sufficiently large data set for a statistically
significant analysis of cell behavior. Adhesion measurements that use single cells are time
consuming because only one cell can be characterized at a time. Therefore, it would be useful to
adjust the size of the representative sample depending on the magnitude of the effect which is
sought. The detection of the influence of one polyelectrolyte bilayer on cell adhesion may require
fifty or hundred measurements whereas ten measurements could have been sufficient for one and
Chapter 7 Conclusions & Outlook
114
nine bilayers. Since the cell dynamics limits the speed of individual experiments, the throughput
has to be increased by parallelizing the AFM experiments. Performing experiments in parallel
also offers the possibility of testing various parameters under the same experimental conditions.
Parallelizing the AFM experiments requires the use of a cantilever array. One of the major
challenges is the development of a readout system for cantilever arrays.
A large proportion of cells were detached from glass and quartz surfaces. Surface modifications
with polyelectrolytes, PNIPAM and sub-micron topography allowed the detachment of all the
adherent cells. In this work, cell adhesion measurements were focused on surfaces dedicated for
cell sheet engineering and bone implant applications. Many effects on cell adhesion were already
reported but this was the first time that global cell adhesion was measured quantitatively.
Single cell force spectroscopy is a powerful tool for the study of long-term adhesion. Under
suitable experimental conditions, force spectroscopy allows quantification of adhesion forces
between adherent cells and their culture substrates. Quantitative data of this nature should open
the way for more rigorous investigation and a comparison of the influence of different parameters
on cell/substrate adhesion. Force spectroscopy is highly complementary to molecular biology
approaches and to existing qualitative techniques already used in cell adhesion studies.
Acknowledgements
115
Acknowledgements
It is my great pleasure to thank all the people who supported me during my project, scientifically
as well as personally (2006-2010). I would like to thank them either in English or in French.
I would like to thank Janos Vörös for giving me the opportunity to perform my PhD thesis in his
group and for being my official supervisor as I carried out my PhD thesis outside the ETH
domain. - Janos, you always considered me as a full member of your group and you gave me so
many incredible and great ideas.
I would like also to thank Mathis Riehle who agreed to come from Glasgow to be part of my
board of co-referees. - Mathis, I thank you very much for coming in Switzerland and for the time
you spent for me.
Je tiens à remercier sincèrement Martha Liley d’avoir été ma superviseure principale. - Martha,
ces quelques mots seront insuffisants pour t’adresser toute ma reconnaissance. Je te remercie
pour m’avoir engagé dans ton groupe, pour m’avoir guidé techniquement et pour m’avoir
supervisé durant ce projet de quatre ans. Ces éléments font partis du cahier des charges d’un bon
superviseur et tu les as accomplis avec brio. Par contre, ton côté humain est unique. J’ai apprécié
quotidiennement ta porte toujours ouverte, ton écoute attentive, ta compréhension des problèmes
personnels, ta tolérance et ta bonne humeur. Ces valeurs ne s’apprennent pas dans les livres
scientifiques. Tu m’as démontré qu’elles étaient compatibles avec un travail appliqué et je m’en
souviendrai toute ma vie, merci infiniment.
Acknowledgements
116
Je remercie Marta Giazzon et Nadège Matthey qui sont mes 2 amours du boulot ! - Marta,
Nadège, je vous remercie du fond du cœur pour votre soutien continu et pour votre contribution
dans ce travail. Votre bonne humeur légendaire reste inoubliable.
Je remercie chaleureusement Harry Heinzelmann d’avoir été mon co-superviseur. Harry, je te
remercie pour m’avoir engagé dans ta division et pour ta disponibilité en toutes circonstances. Je
pense que ce n’est pas un hasard si tu es à la tête d’une division regroupant tant de personnes
intéressantes.
Un grand merci à tous les collègues de mon groupe : Nadège Matthey, Joanna Bitterli, Mélanie
Favre, Marta Giazzon, Silvia Angeloni, Martha Liley, Sher Ahmed, Jérôme Maris-Polesel,
Fabrizio Spano et André Meister.
Première ligne : Martha Liley, Marta Giazzon, Nadège Matthey, Harry Heinzelmann, Janos Vörös et Jérôme Maris-
Polesel. Deuxième ligne : André Meister, Silvia Angeloni, Fabrizio Spano, Joanna Bitterli, Mélanie Favre et Sher
Ahmed.
Un grand merci à tous les autres collègues qui ont contribué de près ou de loin à ce travail,
notamment à Orane Guillaume-Gentil, Mona Klein, Patricia Fernandes, Marta Bally, Jérôme
Maris-Polesel, Nicolas Blondiaux, Franck Montagne et Raphaël Pugin.
Les mots ne sont pas assez forts pour remercier Delphine Hügli, la femme de ma vie, et mes
parents, Sylvia Weder et Michel Miserez, qui ont été là inconditionnellement pour moi.
Finalement, je remercie les amis qui ont eu une oreille particulièrement attentive à mes aventures
professionnelles, notamment Cédric Jecker, Nicolas Forster, Thibaud Rossel, Grégory Franc et
les autres.
Curriculum Vitae
117
Curriculum Vitae
Gilles WEDER
Vivier 20 Ι 2016 Cortaillod Ι Switzerland
13th June 1983 Ι Swiss
Education
2006 – 2010 Doctoral student at the Swiss Center for Electronics and Microtechnique (CSEM
SA), Division Nanotechnology & Life Sciences, Neuchâtel, Switzerland. PhD
performed in collaboration with the Laboratory of Biosensors and Bioelectronics,
Institute for Biomedical Engineering, Department of Information Technology and
Electrical Engineering, ETH Zürich, Switzerland.
2005 – 2006 Master of Science part 2, University of Neuchâtel, Switzerland - Cum Laude
2004 – 2005 Master of Science part 1, University of Lausanne, Switzerland
2001 – 2004 Bachelor of Science, University of Neuchâtel, Switzerland - Cum Laude
1998 – 2001 Baccalaureate of Science, Lycée Denis-de-Rougemont, Neuchâtel, Switzerland
Curriculum Vitae
118
Publications
2010 G. Weder, N. Matthey, H. Heinzelmann, J. Vörös, and M. Liley. Cantilever
Functionalization for Cell Detachment. In Preparation.
2010 G. Weder, O. Guillaume-Gentil, N. Matthey, F. Montagne, H. Heinzelmann, J.
Vörös, and M. Liley. Quantification and Characterization of Single Cell Adhesion
on Functionalized Surfaces for Cell Sheet Engineering. Submitted to Biomaterials.
2010 G. Weder, N. Blondiaux, M. Giazzon, N. Matthey, M. Klein, R. Pugin, H.
Heinzelmann, J. Vörös, and M. Liley. Use of Force Spectroscopy to Investigate the
Adhesion of Living Adherent Cells. Langmuir. Article ASAP DOI:
10.1021/la904526u.
2009 G. Weder, J. Vörös, M. Giazzon, N. Matthey, H. Heinzelmann and M. Liley.
Measuring Cell Adhesion Forces during the Cell Cycle by Force Spectroscopy.
Biointerphases. Vol. 4(2): 27 – 34.
2009 G. Guibert, T. Rossel, G. Weder, B. Betschart, C. Meunier and S. Mikhailov.
Surface Treatment of Polymers by Ion Beam Irradiation to Control the Human
Osteoblast Adhesion: Fluence and Current Density. AIP Proceedings. Vol. 1099:
511 – 515.
2008 R. Pugin, N. Blondiaux, A. M. Popa, E. Scolan, Hoogerwerf A., T. Overstolz, M.
Giazzon, G. Weder and H. Heinzelmann. Surface Nanostructuration: From
Coatings to MEMS Fabrication. NSTI Proceedings. Vol. 1: 431 – 434.
2006 M. Vukicevik, G. Weder, A. Boillat, A. Boesch and S. Kellenberger. Trypsin
Cleaves Acid-Sensing Ion Channel 1a in a Domain that is Critical for Channel
Gating. The Journal of Biological Chemistry. Vol. 281: 714 – 722.
Curriculum Vitae
119
Oral presentations
2009 G. Weder et al. Measuring Cell Adhesion Forces during the Cell Cycle by Force
Spectroscopy. European Society of Biomaterials, Lausanne, Switzerland.
2008 G. Weder et al. Measuring Cell Adhesion Forces during the Cell Cycle by Force
Spectroscopy. European Society of Biomechanics, Luzern, Switzerland.
2007 G. Weder et al. Atomic Force Microscopy: Applications in Biology and Materials
Sciences. EU Project Newbone, Public Conference, Lugano, Switzerland.
Poster presentations
2009 G. Weder et al. Microstructured Non-Metallic Bone Implants: In Vitro & In Vivo
Evaluation. Bioforum, Neuchâtel, Switzerland.
2008 G. Weder et al. Measuring Cell Adhesion Forces during the Cell Cycle by Force
Spectroscopy. Bioforum, Neuchâtel, Switzerland.
2008 G. Weder et al. Measuring Cell Adhesion Forces during the Cell Cycle by Force
Spectroscopy. Single Cell Analysis Workshop, Zürich, Switzerland.
2008 G. Weder et al. Measuring Cell Adhesion Forces during the Cell Cycle by Force
Spectroscopy. World Biomaterials Congress, Amsterdam, Netherlands.
2007 G. Weder et al. Measuring Cell Adhesion Forces of the Cell Cycle by Force
Spectroscopy. Swiss Society for biomedical Engineering, Neuchâtel, Switzerland.
2007 G. Weder et al. Measuring Cell Adhesion Forces of the Cell Cycle by Force
Spectroscopy. European Cell and Materials VIII: bone tissue engineering, Davos,
Switzerland.
2007 G. Weder et al. Measuring Cell Adhesion Forces on Nanostructured Surfaces by
Force Spectroscopy. Gorden Research Conference Cell Contact & Adhesion, Il
Ciocco, Italy.
2007 G. Weder et al. Measuring Cell Adhesion Forces of the Cell Cycle by Force
Spectroscopy. Swiss Society for Biomaterials, Neuchâtel, Switzerland.
Curriculum Vitae
120
2007 G. Weder et al. Measuring Cell Adhesion Forces on Nanostructured Surfaces by
Force Spectroscopy. Swiss User Group Surfaces and Interfaces, Fribourg,
Switzerland.
2006 G. Weder et al. Topographical and Chemical Modifications of Polymer Surfaces
and their Influence on Human Cell Behaviour. Swiss User Group Surfaces and
Interfaces, Fribourg, Switzerland.
Prize
2009 First Baxter Prize for the Interuniversity Doctoral Program in Organismal
Biology. Microstructured Non-Metallic Bone Implants: In Vitro & In Vivo
Evaluation . Bioforum, Neuchâtel, Switzerland.
References
121
References
1. Albelda S. M.andBuck C. A. Integrins and other cell adhesion molecules. The FASEB
Journal, 1990, 4, 2868-2880.
2. Hynes R. O. Integrins: Versatility, modulation, and signaling in cell adhesion. Cell, 1992, 69, 11-25.
3. Takeichi M. The Cadherins - Cell Cell-Adhesion Molecules Controlling Animal Morphogenesis. Development, 1988, 102, 639-655.
4. Kansas G. S. Selectins and their ligands: Current concepts and controversies. Blood, 1996, 88, 3259-3287.
5. Lodish H. F. Molecular cell biology. 2003, 1-973.
6. Takada Y., Ye X. J. and Simon S. The integrins. Genome Biology, 2007, 8, 639-655.
7. Pierschbacher M. D.andRuoslahti E. Cell attachment activity of fibronectin can be duplicated by small synthetic fragments of the molecule. Nature, 1984, 309, 30-33.
8. Humphries J. D., Byron A. and Humphries M. J. Integrin ligands at a glance. Journal of Cell Science, 2006, 119, 3901-3903.
9. Ingber D. Integrins as mechanochemical transducers. Current Opinion in Cell Biology, 1991, 3, 841-848.
10. Berman A. E., Kozova N. I. and Morozevich G. E. Integrins: Structure and signaling. Biochemistry-Moscow, 2003, 68, 1284-1299.
References
122
11. Kreidberg J. A., Donovan M. J., Goldstein S. L., Rennke H., Shepherd K., Jones R. C. and Jaenisch R. Alpha 3 beta 1 integrin has a crucial role in kidney and lung organogenesis. Development, 1996, 122, 3537-3547.
12. Yang J. T., Rayburn H. and Hynes R. O. Cell-Adhesion Events Mediated by Alpha 4 Integrins Are Essential in Placental and Cardiac Development. Development, 1995, 121, 549-560.
13. Yang J. T., Rayburn H. and Hynes R. O. Embryonic Mesodermal Defects in Alpha 5 Integrin-Deficient Mice. Development, 1993, 119, 1093-1105.
14. GeorgesLabouesse E., Messaddeq N., Yehia G., Cadalbert L., Dierich A. and LeMeur M. Absence of integrin alpha 6 leads to epidermolysis bullosa and neonatal death in mice. Nature Genetics, 1996, 13, 370-373.
15. Mayer U., Saher G., Fassler R., Bornemann A., Echtermeyer F., vonderMark H., Miosge N., Poschl E. and vonderMark K. Absence of integrin alpha 7 causes a novel form of muscular dystrophy. Nature Genetics, 1997, 17, 318-323.
16. Muller U., Wang D. N., Denda S., Meneses J. J., Pedersen R. A. and Reichardt L. F. Integrin alpha 8 beta 1 is critically important for epithelial-mesenchymal interactions during kidney morphogenesis. Cell, 1997, 88, 603-613.
17. Schon M. P., Schon M., Warren H. B., Donohue J. P. and Parker C. M. Cutaneous inflammatory disorder in integrin alpha E (CD103)-deficient mice. Journal of Immunology, 2000, 165, 6583-6589.
18. Stephens L. E., Sutherland A. E., Klimanskaya I. V., Andrieux A., Meneses J., Pedersen R. A. and Damsky C. H. Deletion of Beta-1 Integrins in Mice Results in Inner Cell Mass Failure and Periimplantation Lethality. Genes & Development, 1995, 9, 1883-1895.
19. Hodivala-Dilke K. M., McHugh K. P., Tsakiris D. A., Rayburn H., Crowley D., Ullman-Cullere M., Ross F. P., Coller B. S., Teitelbaum S. and Hynes R. O. Beta 3-integrin-deficient mice are a model for Glanzmann thrombasthenia showing placental defects and reduced survival. Journal of Clinical Investigation, 1999, 103, 229-238.
20. vanderNeut R., Krimpenfort P., Calafat J., Niessen C. M. and Sonnenberg A. Epithelial detachment due to absence of hemidesmosomes in integrin beta 4 null mice. Nature Genetics, 1996, 13, 366-369.
21. Huang X. Z., Wu J. F., Cass D., Erle D. J., Corry D., Young S. G., Farese R. V. and Sheppard D. Inactivation of the integrin beta 6 subunit gene reveals a role of epithelial integrins in regulating inflammation in the lungs and skin. Journal of Cell Biology, 1996, 133, 921-928.
22. Wagner N., Lohler J., Kunkel E. J., Ley K., Leung E., Krissansen G., Rajewsky K. and Muller W. Critical role for beta 7 integrins in formation of the gut-associated lymphoid tissue. Nature, 1996, 382, 366-370.
References
123
23. Vogel V.andSheetz M. Local force and geometry sensing regulate cell functions. Nat Rev Mol Cell Biol, 2006, 7, 265-275.
24. Burridge K., Fath K., Kelly T., Nuckolls G. and Turner C. Focal adhesions: transmembrane junctions between the extracellular matrix and the cytoskeleton. Annual review of cell biology, 1988, 4, 487-525.
25. Burridge K.andChrzanowskaWodnicka M. Focal adhesions, contractility, and signaling. Annual Review of Cell and Developmental Biology, 1996, 12, 463-518.
26. Bono P., Rubin K., Higgins J. M. G. and Hynes R. O. Layilin, a novel integral membrane protein, is a hyaluronan receptor. Molecular Biology of the Cell, 2001, 12, 891-900.
27. Borowsky M. L.andHynes R. O. Layilin, a novel talin-binding transmembrane protein homologous with C-type lectins, is localized in membrane ruffles. Journal of Cell Biology, 1998, 143, 429-442.
28. Zamir E.andGeiger B. Components of cell-matrix adhesions. Journal of Cell Science, 2001, 114, 3577-3579.
29. Leslie M. Focal adhesions come unstuck. Journal of Cell Biology, 2009, 187, 585-585.
30. Palecek S. P., Schmidt C. E., Lauffenburger D. A. and Horwitz A. F. Integrin dynamics on the tail region of migrating fibroblasts. Journal of Cell Science, 1996, 109, 941-952.
31. Ezratty E. J., Bertaux C., Marcantonio E. E. and Gundersen G. G. Clathrin mediates integrin endocytosis for focal adhesion disassembly in migrating cells. Journal of Cell Biology, 2009, 187, 733-747.
32. Ruoslahti E.andÍbrink B. r. Common Principles in Cell Adhesion. Experimental cell research, 1996, 227, 1-11.
33. Makrilia N., Kollias A., Manolopoulos L. and Syrigos K. Cell Adhesion Molecules: Role and Clinical Significance in Cancer. Cancer Investigation, 2009, 27, 1023-1037.
34. Puleo D. A.andNanci A. Understanding and controlling the bone-implant interface. Biomaterials, 1999, 20, 2311-2321.
35. Langer R.andVacanti J. P. Tissue Engineering. Science, 1993, 260, 920-926.
36. Roy P., Rajfur Z., Pomorski P. and Jacobson K. Microscope-based techniques to study cell adhesion and migration. Nature Cell Biology, 2002, 4, E91-E96.
37. Stephens D. J.andAllan V. J. Light Microscopy Techniques for Live Cell Imaging. Science, 2003, 300, 82-86.
38. Curtis A. S. G. The mechanism of adhesion of cells to glass: a study by interference reflection microscopy. Journal of Cell Biology, 1964, 20, 199-215.
References
124
39. Verschueren H. Interference reflection microscopy in cell biology: methodology and applications. Journal of Cell Science, 1985, 75, 279-301.
40. Tsien R. Y. The green fluorescent protein. Annual review of biochemistry, 1998, 67, 509-544.
41. Kam Z., Zamir E. and Geiger B. Probing molecular processes in live cells by quantitative multidimensional microscopy. TRENDS in Cell Biology, 2001, 11, 329-334.
42. Ha T., Enderle T., Ogletree D. F., Chemla D. S., Selvin P. R. and Weiss S. Probing the interaction between two single molecules: Fluorescence resonance energy transfer between a single donor and a single acceptor. Proceedings of the National Academy of Sciences of the United States of America, 1996, 93, 6264-6268.
43. Baneyx G., Baugh L. and Vogel V. Coexisting conformations of fibronectin in cell culture imaged using fluorescence resonance energy transfer. Proceedings of the National Academy of Sciences of the United States of America, 2001, 98, 14464-14468.
44. Kam Z., Volberg T. and Geiger B. Mapping of adherens junction components using microscopic resonance energy transfer imaging. Journal of Cell Science, 1995, 108, 1051-
45. Lippincott-Schwartz J., Cole N. and Presley J. Unravelling Golgi membrane traffic with green fluorescent protein chimeras. TRENDS in Cell Biology, 1998, 8, 16-20.
46. Wolf D. E. Designing, Building, and Using A Fluorescence Recovery After Photobleaching Instrument. Methods in Cell Biology, 1989, 30, 271-306.
47. Edlund M., Lotano M. A. and Otey C. A. Dynamics of a-actinin in focal adhesions and stress fibers visualized with a-actinin green fluorescent protein. Cell Motil.Cytoskeleton, 2001, 48, 190-200.
48. Van Vliet K. J., Bao G. and Suresh S. The biomechanics toolbox: experimental approaches for living cells and biomolecules. Acta Materialia, 2003, 51, 5881-5905.
49. Harris A. K., Wild P. and Stopak D. Silicone rubber substrata: a new wrinkle in the study of cell locomotion. Science (New York, NY), 1980, 208, 177-179.
50. Brown T. D. Techniques for mechanical stimulation of cells in vitro: a review. Journal of Biomechanics, 2000, 33, 3-14.
51. Pelham R. J.andWang Y. Cell locomotion and focal adhesions are regulated by substrate flexibility. Proceedings of the National Academy of Sciences of the United States of America, 1997, 94, 13661-13665.
52. Lotz M. M., Burdsal C. A., Erickson H. P. and McClay D. R. Cell adhesion to fibronectin and tenascin: quantitative measurements of initial binding and subsequent strengthening response. The Journal of Cell Biology, 1989, 109, 1795-1805.
References
125
53. Beningo K. A.andWang Y. L. Flexible substrata for the detection of cellular traction forces. TRENDS in Cell Biology, 2002, 12, 79-84.
54. Oliver T., Dembo M. and Jacobson K. Traction forces in locomoting cells. Cell motility and the cytoskeleton, 1995, 31, 225-240.
55. Munevar S., Wang Y. and Dembo M. Traction force microscopy of migrating normal and H-ras transformed 3T3 fibroblasts. Biophysical Journal, 2001, 80, 1744-1757.
56. Wang Y. L.andPelham R. J. Preparation of a flexible, porous polyacrylamide substrate for mechanical studies of cultured cells. Methods in enzymology, 1998, 298, 489-496.
57. Dike L. E., Chen C. S., Mrksich M., Tien J., Whitesides G. M. and Ingber D. E. Geometric control of switching between growth, apoptosis, and differentiation during angiogenesis using micropatterned substrates. In Vitro Cellular & Developmental Biology-Animal, 1999, 35, 441-448.
58. Singhvi R., Kumar A., Lopez G. P., Stephanopoulos G. N., Wang D. I., Whitesides G. M. and Ingber D. E. Engineering cell shape and function. Science, 1994, 264, 696-698.
59. Galbraith C. G.andSheetz M. P. Keratocytes pull with similar forces on their dorsal and ventral surfaces. Journal of Cell Biology, 1999, 147, 1313-1324.
60. Galbraith C. G.andSheetz M. P. A micromachined device provides a new bend on fibroblast tractionΓÇëforces. Proceedings of the National Academy of Sciences of the United States of America, 1997, 94, 9114-9118.
61. Petronis S., Gold J. and Kasemo B. Microfabricated force-sensitive elastic substrates for investigation of mechanical cell–substrate interactions. Journal of Micromechanics and Microengineering, 2003, 13, 900-913.
62. Balaban N. Q., Schwarz U. S., Riveline D., Goichberg P., Tzur G., Sabanay I., Mahalu D., Safran S., Bershadsky A. and Addadi L. Force and focal adhesion assembly: a close relationship studied using elastic micropatterned substrates. Nature Cell Biology, 2001, 3, 466-472.
63. Wang J. H. C.andLin J. S. Cell traction force and measurement methods. Biomechanics and Modeling in Mechanobiology, 2007, 6, 361-371.
64. Thoumine O., Cardoso O. and Meister J. J. Changes in the mechanical properties of fibroblasts during spreading: a micromanipulation study. European Biophysics Journal, 1999, 28, 222-234.
65. Evans E.andYeung A. Apparent viscosity and cortical tension of blood granulocytes determined by micropipet aspiration. Biophysical Journal, 1989, 56, 151-160.
66. Hochmuth R. M. Micropipette aspiration of living cells. Journal of Biomechanics, 2000, 33, 15-22.
References
126
67. Chu Y. S., Thomas W. A., Eder O., Pincet F., Perez E., Thiery J. P. and Dufour S. Force measurements in E-cadherin-mediated cell doublets reveal rapid adhesion strengthened by actin cytoskeleton remodeling through Rac and Cdc42. Journal of Cell Biology, 2004, 167, 1183-1194.
68. Evans E., Ritchie K. and Merkel R. Sensitive force technique to probe molecular adhesion and structural linkages at biological interfaces. Biophysical Journal, 1995, 68, 2580-2587.
69. King M. R. Principles of cellular engineering: understanding the biomolecular interface. 2005, 1-314.
70. Forero M., Thomas W. E., Bland C., Nilsson L. M., Sokurenko E. V. and Vogel V. A catch-bond based nanoadhesive sensitive to shear stress. Nano Letters, 2004, 4, 1593-1597.
71. Lu H., Koo L. Y., Wang W. C. M., Lauffenburger D. A., Griffith L. G. and Jensen K. F. Microfluidic shear devices for quantitative analysis of cell adhesion. Analytical Chemistry, 2004, 76, 5257-5264.
72. Alon R., Hammer D. A. and Springer T. A. Lifetime of the P-selectin-carbohydrate bond and its response to tensile force in hydrodynamic flow. Nature, 1995, 374, 539-542.
73. Dwir O., Solomon A., Mangan S., Kansas G. S., Schwarz U. S. and Alon R. Avidity enhancement of L-selectin bonds by flow: shear-promoted rotation of leukocytes turn labile bonds into functional tethers. Journal of Cell Biology, 2003, 649-659.
74. Hammer D. A.andApte S. M. Simulation of Cell Rolling and Adhesion on Surfaces in Shear-Flow - General Results and Analysis of Selectin-Mediated Neutrophil Adhesion. Biophysical Journal, 1992, 63, 35-57.
75. JPK instruments Nanotracker: force-sensing optical tweezers and 3D particle tracking platform. 2009, 1-8.
76. Choquet D., Felsenfeld D. P. and Sheetz M. P. Extracellular matrix rigidity causes strengthening of integrin-cytoskeleton linkages. Cell, 1997, 88, 39-48.
77. Thoumine O., Kocian P., Kottelat A. and Meister J. J. Short-term binding of fibroblasts to fibronectin: optical tweezers experiments and probabilistic analysis. European Biophysics Journal, 2000, 29, 398-408.
78. Dai J.andSheetz M. P. Mechanical properties of neuronal growth cone membranes studied by tether formation with laser optical tweezers. Biophysical Journal, 1995, 68, 988-996.
79. Feneberg W., Westphal M. and Sackmann E. Dictyostelium cells' cytoplasm as an active viscoplastic body. European Biophysics Journal, 2001, 30, 284-294.
80. Bausch A. R., Muller W. and Sackmann E. Measurement of local viscoelasticity and forces in living cells by magnetic tweezers. Biophysical Journal, 1999, 76, 573-579.
References
127
81. Walter N., Selhuber C., Kessler H. and Spatz J. P. Cellular unbinding forces of initial adhesion processes on nanopatterned surfaces probed with magnetic tweezers. Nano lett, 2006, 6, 398-402.
82. Athanasiou K. A., Thoma B. S., Lanctot D. R., Shin D., Agrawal C. M. and LeBaron R. G. Development of the cytodetachment technique to quantify mechanical adhesiveness of the single cell. Biomaterials, 1999, 20, 2405-2415.
83. Balaban N. Q., Schwarz U. S., Riveline D., Goichberg P., Tzur G., Sabanay I., Mahalu D., Safran S., Bershadsky A., Addadi L. and Geiger B. Force and focal adhesion assembly: a close relationship studied using elastic micropatterned substrates. Nat Cell Biol, 2001, 3, 466-472.
84. Burton K., Park J. H. and Taylor D. Keratocytes generate traction forces in two phases. Molecular Biology of the Cell, 1999, 10, 3745-
85. Binnig G., Quate C. F. and Gerber C. Atomic Force Microscope. Physical Review Letters, 1986, 56, 930-933.
86. Kelsall R. W., Hamley I. W. and Geoghegan M. Nanoscale science and technology. 2005, 1-456.
87. JPK instruments The nanowizard AFM handbook. 2005, 1-40.
88. Morris V. J., Kirby A. R. and Gunning A. P. Atomic force microscopy for biologists. 1999, 1-364.
89. Shao Z., Mou J., Czajkowsky D. M., Yang J. and Yuan J. Y. Biological atomic force microscopy: what is achieved and what is needed. Advances in Physics, 1996, 45, 1-86.
90. Heinz W. F.andHoh J. H. Spatially resolved force spectroscopy of biological surfaces using the atomic force microscope. Trends in Biotechnology, 1999, 17, 143-150.
91. Muller D. J. AFM: A Nanotool in Membrane Biology. Biochemistry, 2008, 47, 7986-7998.
92. Fisher T. E., Carrion-Vazquez M., Oberhauser A. F., Li H., Marszalek P. E. and Fernandez J. M. Single Molecule Force Spectroscopy of Modular Proteins in the Nervous System. Neuron, 2000, 27, 435-446.
93. Janshoff A., Neitzert M., Oberdurfer Y. and Fuchs H. Force Spectroscopy of Molecular Systems Single Molecule Spectroscopy of Polymers and Biomolecules. Angew.Chem.Int.Ed, 2000, 39, 3212-3237.
94. Muller D. J.andDufrene Y. F. Atomic force microscopy as a multifunctional molecular toolbox in nanobiotechnology. Nature Nanotechnology, 2008, 3, 261-269.
References
128
95. Zlatanova J., Lindsay S. M. and Leuba S. H. Single molecule force spectroscopy in biology using the atomic force microscope. Progress in Biophysics and Molecular Biology, 2007, 74, 37-61.
96. Florin E. L., Moy V. T. and Gaub H. E. Adhesion forces between individual ligand-receptor pairs. Science, 1994, 264, 415-417.
97. Merkel R., Nassoy P., Leung A., Ritchie K. and Evans E. Energy landscapes of receptorûligand bonds explored with dynamic force spectroscopy. Nature, 1999, 397, 50-53.
98. Simson D. A., Strigl M., Hohenadl M. and Merkel R. Statistical breakage of single protein A-IgG bonds reveals crossover from spontaneous to force-induced bond dissociation. Physical Review Letters, 1999, 83, 652-655.
99. Strigl M., Simson D. A., Kacher C. M. and Merkel R. Force-induced dissociation of single protein A-IgG bonds. Langmuir, 1999, 15, 7316-7324.
100. Evans E. A.andCalderwood D. A. Forces and bond dynamics in cell adhesion. Science, 2007, 316, 1148-1153.
101. Evans E.andRitchie K. Dynamic strength of molecular adhesion bonds. Biophysical Journal, 1997, 72, 1541-1555.
102. Hemmerle J., Altmann S. M., Maaloum M., Horber J. K. H., Heinrich L., Voegel J. C. and Schaaf P. Direct observation of the anchoring process during the adsorption of fibrinogen on a solid surface by force-spectroscopy mode atomic force microscopy. Proceedings of the National Academy of Sciences of the United States of America, 1999, 96, 6705-6710.
103. Rudolf R.andHorst V. Single molecules & nanotechnology. Springer, 2008, 1-318.
104. Rief M., Gautel M., Oesterhelt F., Fernandez J. M. and Gaub H. E. Reversible unfolding of individual titin immunoglobulin domains by AFM. Science, 1997, 276, 1109-1112.
105. Tskhovrebova L., Trinick J., Sleep J. A. and Simmons R. M. Elasticity and unfolding of single molecules of the giant muscle protein titin. Science, 1994, 266, 1709-1713.
106. Janovjak H., Kessler M., Oesterhelt D., Gaub H. and Muller D. J. Unfolding pathways of native bacteriorhodopsin depend on temperature. The EMBO Journal, 2003, 22, 5220-5229.
107. Muller D. J., Kessler M., Oesterhelt F., Muller C., Oesterhelt D. and Gaub H. Stability of Bacteriorhodopsin alpha-Helices and Loops Analyzed by Single-Molecule Force Spectroscopy. Biophysical Journal, 2002, 83, 3578-3588.
108. Oesterhelt F., Oesterhelt D., Pfeiffer M., Engel A., Gaub H. E. and Muller D. J. Unfolding pathways of individual bacteriorhodopsins. Science, 2000, 288, 143-146.
References
129
109. Clausen-Schaumann H., Seitz M., Krautbauer R. and Gaub H. E. Force spectroscopy with single bio-molecules. Current Opinion in Chemical Biology, 2000, 4, 524-530.
110. Rief M., Pascual J., Saraste M. and Gaub H. E. Single molecule force spectroscopy of spectrin repeats: low unfolding forces in helix bundles. Journal of Molecular Biology, 1999, 286, 553-561.
111. Klimov D. K.andThirumalai D. Stretching single-domain proteins: phase diagram and kinetics of force-induced unfolding. Proceedings of the National Academy of Sciences, 1999, 96, 6166-6170.
112. Rief M., Clausen-Schaumann H. and Gaub H. E. Sequence-dependent mechanics of single DNA molecules. nature structural biology, 1999, 6, 346-350.
113. Krautbauer R., Rief M. and Gaub H. E. Unzipping DNA oligomers. Nano Letters, 2003, 3, 493-496.
114. Leger J. F., Robert J., Bourdieu L., Chatenay D. and Marko J. F. RecA binding to a single double-stranded DNA molecule: a possible role of DNA conformational fluctuations. Proceedings of the National Academy of Sciences, 1998, 95, 12295-12299.
115. Bartels F. W., Baumgarth B., Anselmetti D., Ros R. and Becker A. Specific binding of the regulatory protein ExpG to promoter regions of the galactoglucan biosynthesis gene cluster of Sinorhizobium meliloti-a combined molecular biology and force spectroscopy investigation. Journal of Structural Biology, 2003, 143, 145-152.
116. Ros R., Eckel R., Bartels F., Sischka A., Baumgarth B., Wilking S. D., Puhler A., Sewald N., Becker A. and Anselmetti D. Single molecule force spectroscopy on ligand-DNA complexes: from molecular binding mechanisms to biosensor applications. Journal of Biotechnology, 2004, 112, 5-12.
117. Marszalek P. E., Oberhauser A. F., Pang Y. P. and Fernandez J. M. Polysaccharide elasticity governed by chairûboat transitions of the glucopyranose ring. Nature, 1998, 396, 661-664.
118. Marszalek P. E., Pang Y. P., Li H., Yazal J. E., Oberhauser A. F. and Fernandez J. M. Atomic levers control pyranose ring conformations. Proceedings of the National Academy of Sciences, 1999, 96, 7894-7898.
119. Rief M., Oesterhelt F., Heymann B. and Gaub H. E. Single Molecule Force Spectroscopy on Polysaccharides by Atomic Force Microscopy. Science, 1997, 275, 1295-1297.
120. Muller D. J., Sapra K. T., Scheuring S., Kedrov A., Frederix P. L., Fotiadis D. and Engel A. Single-molecule studies of membrane proteins. Current opinion in structural biology, 2006, 16, 489-495.
121. Muller D. J., Helenius J., Alsteens D. and Dufrene Y. F. Force probing surfaces of living cells to molecular resolution. Nature Chemical Biology, 2009, 5, 383-390.
References
130
122. Helenius J., Heisenberg C. P., Gaub H. E. and Muller D. J. Single-cell force spectroscopy. Journal of Cell Science, 2008, 121, 1785-1791.
123. Benoit M., Gabriel D., Gerisch G. and Gaub H. E. Discrete interactions in cell adhesion measured by single-molecule force spectroscopy. Nature Cell Biology, 2000, 2, 313-317.
124. Matzke R., Jacobson K. and Radmacher M. Direct, high-resolution measurement of furrow stiffening during division of adherent cells. Nature Cell Biology, 2001, 3, 607-610.
125. Radmacher M., Fritz M., Kacher C. M., Cleveland J. P. and Hansma P. K. Measuring the viscoelastic properties of human platelets with the atomic force microscope. Biophysical Journal, 1996, 70, 556-567.
126. Sun Z., Martinez-Lemus L. A., Trache A., Trzeciakowski J. P., Davis G. E., Pohl U. and Meininger G. A. Mechanical properties of the interaction between fibronectin and alpha5-beta1-integrin on vascular smooth muscle cells studied using atomic force microscopy. American Journal of Physiology- Heart and Circulatory Physiology, 2005, 289, 2526-2535.
127. Trache A., Trzeciakowski J. P., Gardiner L., Sun Z., Muthuchamy M., Guo M., Yuan S. Y. and Meininger G. A. Histamine effects on endothelial cell fibronectin interaction studied by atomic force microscopy. Biophysical Journal, 2005, 89, 2888-2898.
128. Taubenberger A., Cisneros D. A., Friedrichs J., Puech P. H., Muller D. J. and Franz C. M. Revealing Early Steps of alpha 2 beta1 Integrin-mediated Adhesion to Collagen Type I by Using Single-Cell Force Spectroscopy. Molecular Biology of the Cell, 2007, 18, 1634-1644.
129. Alon R., Feigelson S. W., Manevich E., Rose D. M., Schmitz J., Overby D. R., Winter E., Grabovsky V., Shinder V. and Matthews B. D. alpha4beta1-dependent adhesion strengthening under mechanical strain is regulated by paxillin association with the alpha4-cytoplasmic domain. Journal of Cell Biology, 2005, 171, 1073-1084.
130. Zhang X., Craig S. E., Kirby H., Humphries M. J. and Moy V. T. Molecular Basis for the Dynamic Strength of the Integrin a 41/VCAM-1 Interaction. Biophysical Journal, 2004, 87, 3470-3478.
131. Thie M., Rospel R., Dettmann W., Benoit M., Ludwig M., Gaub H. E. and Denker H. W. Interactions between trophoblast and uterine epithelium: monitoring of adhesive forces. Human Reproduction, 1998, 13, 3211-3219.
132. Zhang X., Wojcikiewicz E. and Moy V. T. Force spectroscopy of the leukocyte function-associated antigen-1/intercellular adhesion molecule-1 interaction. Biophysical Journal, 2002, 83, 2270-2279.
133. Zhang X., Wojcikiewicz E. P. and Moy V. T. Dynamic adhesion of T lymphocytes to endothelial cells revealed by atomic force microscopy. Experimental Biology and Medicine, 2006, 231, 1306-1312.
References
131
134. Wojcikiewicz E. P., Abdulreda M. H., Zhang X. and Moy V. T. Force spectroscopy of LFA-1 and its ligands, ICAM-1 and ICAM-2. Biomacromolecules, 2006, 7, 3188-3195.
135. Li F., Redick S. D., Erickson H. P. and Moy V. T. Force measurements of integrin fibronectin interaction. Biophysical Journal, 2003, 84, 1252-1262.
136. Puech P. H., Poole K., Knebel D. and Muller D. J. A new technical approach to quantify cell cell adhesion forces by AFM. Ultramicroscopy, 2006, 106, 637-644.
137. Panorchan P., Thompson M. S., Davis K. J., Tseng Y., Konstantopoulos K. and Wirtz D. Single-molecule analysis of cadherin-mediated cell-cell adhesion. Journal of Cell Science, 2006, 119, 66-74.
138. Panorchan P., George J. P. and Wirtz D. Probing intercellular interactions between vascular endothelial cadherin pairs at single-molecule resolution and in living cells. Journal of Molecular Biology, 2006, 358, 665-674.
139. Hanley W. D., Wirtz D. and Konstantopoulos K. Distinct kinetic and mechanical properties govern selectin-leukocyte interactions. Journal of Cell Science, 2004, 117, 2503-2511.
140. Dobrowsky T. M., Panorchan P., Konstantopoulos K. and Wirtz D. Live-Cell Single-Molecule Force Spectroscopy. 2008, 411-418.
141. Puech P. H., Taubenberger A., Ulrich F., Krieg M., Muller D. J. and Heisenberg C. P. Measuring cell adhesion forces of primary gastrulating cells from zebrafish using atomic force microscopy. Journal of Cell Science, 2005, 118, 4199-4206.
142. Ulrich F., Krieg M., Schutz E. M., Link V., Castanon I., Schnabel V., Taubenberger A., Mueller D., Puech P. H. and Heisenberg C. P. Wnt11 functions in gastrulation by controlling cell cohesion through Rab5c and E-cadherin. Developmental cell, 2005, 9, 555-564.
143. Selhuber C. Biological adhesion on nanopatterned substrates studied with force spectroscopy and microinterferometry. PhD thesis, Heidelberg University, 2006, 1-150.
144. Lamontagne C. A., Cuerrier C. M. and Grandbois M. AFM as a tool to probe and manipulate cellular processes. European Journal of Physiology, 2008, 456, 61-70.
145. Ludwig T., Kirmse R., Poole K. and Schwarz U. S. Probing cellular microenvironments and tissue remodeling by atomic force microscopy. European Journal of Physiology, 2008, 456, 29-49.
146. Blondiaux N., Scolan E., Popa A. M., Gavillet J. and Pugin R. Fabrication of superhydrophobic surfaces with controlled topography and chemistry. Applied Surface Science, 2009, 256, S46-S53.
147. Krek W.andDeCaprio J. A. Cell synchronization. Methods Enzymol, 1995, 254, 114-124.
References
132
148. Terasima T.andTolmach L. J. Changes in X-ray sensitivity of HeLa cells during the division cycle. Nature, 1961, 190, 1210-1211.
149. Wojcikiewicz E. P., Zhang X. and Moy V. T. Force and compliance measurements on living cells using atomic force microscopy (AFM). Biol.Proced.Online, 2004, 6, 1-9.
150. Hutter J. L.andBechhoefer J. Calibration of atomic force microscope tips. Review of Scientific Instruments, 1993, 64, 1868-1873.
151. Mahaffy R. E., Park S., Gerde E., Kas J. and Shih C. K. Quantitative Analysis of the Viscoelastic Properties of Thin Regions of Fibroblasts Using Atomic Force Microscopy. Biophysical Journal, 2004, 86, 1777-1793.
152. Franz C. M., Taubenberger A., Puech P. H. and Muller D. J. Studying integrin-mediated cell adhesion at the single-molecule level using AFM force spectroscopy. Science's STKE, 2007, 2007, 1-16.
153. JPK instruments Determining the elastic modulus of biological samples using atomic force microscopy. 2008, 1-9.
154. Li Q. S., Lee G. Y. H., Ong C. N. and Lim C. T. AFM indentation study of breast cancer cells. Biochemical and Biophysical Research Communications, 2008, 374, 609-613.
155. Rosenbluth M. J., Lam W. A. and Fletcher D. A. Force microscopy of nonadherent cells: a comparison of leukemia cell deformability. Biophysical Journal, 2006, 90, 2994-3003.
156. Stolz M., Raiteri R., Daniels A. U., VanLandingham M. R., Baschong W. and Aebi U. Dynamic elastic modulus of porcine articular cartilage determined at two different levels of tissue organization by indentation-type atomic force microscopy. Biophysical Journal, 2004, 86, 3269-3283.
157. Alberts B. Essential cell biology. 2003, Garland, 1-630.
158. Porter K., Prescott D. and Frye J. Changes in surface morphology of chinese hamster ovary cells during the cell cycle. The Journal of Cell Biology, 1973, 57, 815-836.
159. Théry M.andBornens M. Get round and stiff for mitosis. HFSP Journal, 2008, 2, 65-71.
160. Otey C. A. An interaction between alpha-actinin and the beta 1 integrin subunit in vitro. The Journal of Cell Biology, 1990, 111, 721-729.
161. Schwartz M. A., Schaller M. D. and Ginsberg M. H. Integrins: Emerging Paradigms of Signal Transduction. Annual Review of Cell and Developmental Biology, 1995, 11, 549-599.
162. Pugacheva E. N., Roegiers F. and Golemis E. A. Interdependence of cell attachment and cell cycle signaling. Current Opinion in Cell Biology, 2006, 18, 507-515.
References
133
163. Fowler V. M.andAdam E. J. Spectrin redistributes to the cytosol and is phosphorylated during mitosis in cultured cells. The Journal of Cell Biology, 1992, 119, 1559-1572.
164. Curtis M., Nikolopoulos S. N. and Turner C. E. Actopaxin is phosphorylated during mitosis and is a substrate for cyclin B1/cdc2 kinase. Biochem J, 2002, 363, 233-242.
165. Hildebrand J. D., Schaller M. D. and Parsons J. T. Paxillin, a tyrosine phosphorylated focal adhesion-associated protein binds to the carboxyl terminal domain of focal adhesion kinase. Molecular Biology of the Cell, 1995, 6, 637-647.
166. Ma A., Richardson A., Schaefer E. M. and Parsons J. T. Serine Phosphorylation of Focal Adhesion Kinase in Interphase and Mitosis: A Possible Role in Modulating Binding to p130Cas. Molecular Biology of the Cell, 2001, 12, 1-12.
167. Suzuki T.andTakahashi K Reduced cell adhesion during mitosis by threonine phosphorylation of integrin. J.Cell.Physiol, 2003, 197, 297-305.
168. Yamaguchi R., Mazaki Y., Hirota K., Hashimoto S. and Sabe H. Mitosis specific serine phosphorylation and downregulation of one of the focal adhesion protein, paxillin. Oncogene, 1997, 15, 1753-1761.
169. Yamakita Y., Totsukawa G., Yamashiro S., Fry D., Zhang X., Hanks S. K. and Matsumura F. Dissociation of FAK/p130CAS/c-Src Complex during Mitosis: Role of Mitosis-specific Serine Phosphorylation of FAK. The Journal of Cell Biology, 1999, 144, 315-324.
170. Clarke D. M., Brown M. C., LaLonde D. P. and Turner C. E. Phosphorylation of actopaxin regulates cell spreading and migration. The Journal of Cell Biology, 2004, 166, 901-912.
171. Tong X.andHowley P. M. The bovine papillomavirus E6 oncoprotein interacts with paxillin and disrupts the actin cytoskeleton. Proceedings of the National Academy of Sciences, 1997, 94, 4412-4417.
172. Bellissent-Waydelich A., Vanier M. T., Albiges-Rizo C. and Simon-Assmann P. Talin Concentrates to the Midbody Region During Mammalian Cell Cytokinesis. Journal of Histochemistry and Cytochemistry, 1999, 47, 1357-1368.
173. Théry M.andBornens M. Cell shape and cell division. Current Opinion in Cell Biology, 2006, 18, 648-657.
174. Kunda P., Pelling A. E., Liu T. and Baum B. Moesin Controls Cortical Rigidity, Cell Rounding, and Spindle Morphogenesis during Mitosis. Current Biology, 2008, 18, 91-101.
175. Benoit M.andGaub H. E. Measuring Cell Adhesion Forces with the Atomic Force Microscope at the Molecular Level. Cells Tissues Organs, 2002, 172, 174-189.
References
134
176. Wojcikiewicz E. P., Zhang X., Chen A. and Moy V. T. Contributions of molecular binding events and cellular compliance to the modulation of leukocyte adhesion. Journal of Cell Science, 2003, 116, 2531-2539.
177. Maddox A. S.andBurridge K. RhoA is required for cortical retraction and rigidity during mitotic cell rounding. The Journal of Cell Biology, 2003, 160, 255-265.
178. Docheva D., Popov C., Mutschler W. and Schieker M. Human mesenchymal stem cells in contact with their environment: surface characteristics and the integrin system. Journal of Cellular and Molecular Medicine, 2007, 11, 21-38.
179. Docheva D., Padula D., Popov C., Mutschler W., Clausen-Schaumann H. and Schieker M. Researching into the cellular shape, volume and elasticity of mesenchymal stem cells, osteoblasts and osteosarcoma cells by atomic force microscopy. Journal of Cellular and Molecular Medicine, 2008, 12, 537-552.
180. Shin D.andAthanasiou K. Cytoindentation for obtaining cell biomechanical properties. Journal of Orthopaedic Research, 1999, 17, 880-890.
181. Domke J., Dannohl S., Parak W. J., Muller O., Aicher W. K. and Radmacher M. Substrate dependent differences in morphology and elasticity of living osteoblasts investigated by atomic force microscopy. Colloids and Surfaces B: Biointerfaces, 2000, 19, 367-379.
182. Friedrichs J., Torkko J. M., Helenius J., Teravainen T. P., Fullekrug J., Muller D. J., Simons K. and Manninen A. Contributions of galectin-3 and-9 to epithelial cell adhesion analyzed by single cell force spectroscopy. Journal of Biological Chemistry, 2007, 282, 29375-29381.
183. Selhuber-Unkel C., Lopez-Garcia M., Kessler H. and Spatz J. P. Cooperativity in adhesion cluster formation during initial cell adhesion. Biophysical Journal, 2008, 95, 5424-5431.
184. Micoulet A. Uniaxial mechanical assays on adherent living single cells: animal embryonic fibroblats and human pancreas cancer cells. PhD thesis, Heidelberg University, 2004, 1-95.
185. Park K., Jang J., Irimia D., Sturgis J., Lee J., Robinson J. P., Toner M. and Bashir R. Living cantilever arrays: for characterization of mass of single live cells in fluids. Lab on a Chip, 2008, 8, 1034-1041.
186. Bally M. Smart Sensing with Beads and Vesicles: a Bioassay Toolbox for High-Performance Fluorescent Microarrays. PhD thesis, ETH Zurich, 2009, 1-170.
187. Feng S., Ye M., Zhou H., Jiang X., Jiang X., Zou H. and Gong B. Immobilized zirconium ion affinity chromatography for specific enrichment of phosphopeptides in phosphoproteome analysis. Molecular & Cellular Proteomics, 2007, 6, 1656-1665.
References
135
188. Xue Y., Wei J., Han H., Zhao L., Cao D., Wang J., Yang X., Zhang Y. and Qian X. Application of open tubular capillary columns coated with zirconium phosphonate for enrichment of phosphopeptides. Journal of Chromatography B, 2009, 877, 757-764.
189. Zhou H., Xu S., Ye M., Feng S., Pan C., Jiang X., Li X., Han G., Fu Y. and Zou H. Zirconium phosphonate-modified porous silicon for highly specific capture of phosphopeptides and MALDI-TOF MS analysis. Journal of proteome research, 2006, 5, 2431-2437.
190. Michl J., Baudysovβ M., Sochorovβ L. and Deyl Z. Fibronectin is not a serum spreading factor for HeLa cells. Cell Biochemistry and Function, 1983, 1,
191. Morgan J.andGarrod D. HeLa cells form focal contacts that are not fibronectin dependent. Journal of Cell Science, 1984, 66, 133-
192. Nerem R. M.andSambanis A. Tissue engineering: from biology to biological substitutes. Tissue Engineering, 1995, 1, 3-13.
193. Hubbell J. A. Biomaterials in tissue engineering. Nature Biotechnology, 1995, 13, 565-576.
194. Chen G., Ushida T. and Tateishi T. Scaffold design for tissue engineering. Macromolecular Bioscience, 2002, 2, 67-77.
195. Dahlberg L.andKreicbergs A. Demineralized allogeneic bone matrix for cartilage repair. Journal of Orthopaedic Research, 1991, 9, 11-19.
196. Watt F. M.andDudhia J. Prolonged expression of differentiated phenotype by chondrocytes cultured at low density on a composite substrate of collagen and agarose that restricts cell spreading. Differentiation, 1988, 38, 140-147.
197. Ponticiello M. S., Schinagl R. M., Kadiyala S. and Barry F. P. Gelatin-based resorbable sponge as a carrier matrix for human mesenchymal stem cells in cartilage regeneration therapy. Journal of biomedical materials research, 2000, 52, 246-255.
198. Allemann F., Mizuno S., Eid K., Yates K. E., Zaleske D. and Glowacki J. Effects of hyaluronan on engineered articular cartilage extracellular matrix gene expression in 3-dimensional collagen scaffolds. Journal of biomedical materials research, 2001, 55, 13-19.
199. Bonaventure J., Kadhom N., Cohen-Solal L., Ng K. H., Bourguignon J., Lasselin C. and Freisinger P. Reexpression of cartilage-specific genes by dedifferentiated human articular chondrocytes cultured in alginate beads. Experimental cell research, 1994, 212, 97-104.
200. Freed L. E., Vunjak-Novakovic G., Biron R. J., Eagles D. B., Lesnoy D. C., Barlow S. K. and Langer R. Biodegradable polymer scaffolds for tissue engineering. Nature Biotechnology, 1994, 12, 689-693.
References
136
201. Thomson R. C., Wake M. C., Yaszemski M. J. and Mikos A. G. Biodegradable polymer scaffolds to regenerate organs. Advances in polymer science, 1995, 122, 245-274.
202. Wong W. H.andMooney D. J. Synthesis and properties of biodegradable polymers used as synthetic matrices for tissue engineering. Synthetic Biodegradable Polymer Scaffolds, 1997, 51-82.
203. Drury J. L.andMooney D. J. Hydrogels for tissue engineering: scaffold design variables and applications. Biomaterials, 2003, 24, 4337-4351.
204. Lee K. Y.andMooney D. J. Hydrogels for tissue engineering. Chemical reviews, 2001, 101, 1869-1879.
205. Athanasiou K. A., Niederauer G. G. and Agrawal C. M. Sterilization, toxicity, biocompatibility and clinical applications of polylactic acid/ polyglycolic acid copolymers. Biomaterials, 1996, 17, 93-102.
206. Bostman O., Hirensalo E., Vainionpaa S., Makela A., Vihtonen K., Tormala P. and Rokkanen P. Ankle fractures treated using biodegradable internal fixation. Clinical orthopaedics and related research, 1989, 238, 195-207.
207. Hirvensalo E. Fracture fixation with biodegradable rods Forty-one cases of severe ankle fractures. Acta Orthopaedica, 1989, 60, 601-606.
208. Babensee J. E., Anderson J. M., McIntire L. V. and Mikos A. G. Host response to tissue engineered devices. Advanced Drug Delivery Reviews, 1998, 33, 111-139.
209. Hutmacher D. W. Scaffolds in tissue engineering bone and cartilage. Biomaterials, 2000, 21, 2529-2543.
210. Sung H. J., Meredith C., Johnson C. and Galis Z. S. The effect of scaffold degradation rate on three-dimensional cell growth and angiogenesis. Biomaterials, 2004, 25, 5735-5742.
211. Yamato M.andOkano T. Cell sheet engineering. Materials Today, 2004, 7, 42-47.
212. Nishida K., Yamato M., Hayashida Y., Watanabe K., Yamamoto K., Adachi E., Nagai S., Kikuchi A., Maeda N. and Watanabe H. Corneal reconstruction with tissue-engineered cell sheets composed of autologous oral mucosal epithelium. New England Journal of Medicine, 2004, 351, 1187-1196.
213. Nishida K., Yamato M., Hayashida Y., Watanabe K., Maeda N., Watanabe H., Yamamoto K., Nagai S., Kikuchi A. and Tano Y. Functional bioengineered corneal epithelial sheet grafts from corneal stem cells expanded ex vivo on a temperature-responsive cell culture surface. Transplantation, 2004, 77, 379-385.
214. Shimizu T., Yamato M., Kikuchi A. and Okano T. Cell sheet engineering for myocardial tissue reconstruction. Biomaterials, 2003, 24, 2309-2316.
References
137
215. Okano T., Yamada N., Sakai H. and Sakurai Y. A novel recovery system for cultured cells using plasma-treated polystyrene dishes grafted with poly (N-isopropylacrylamide). Journal of biomedical materials research, 1993, 27, 1243-1251.
216. Okano T., Yamada N., Okuhara M., Sakai H. and Sakurai Y. Mechanism of cell detachment from temperature-modulated, hydrophilic-hydrophobic polymer surfaces. Biomaterials, 1995, 16, 297-303.
217. Yamada N., Okano T., Sakai H., Karikusa F., Sawasaki Y. and Sakurai Y. Thermo-responsive polymeric surfaces; control of attachment and detachment of cultured cells. Die Makromolekulare Chemie, Rapid Communications, 1990, 11, 571-576.
218. Yang J., Yamato M., Kohno C., Nishimoto A., Sekine H., Fukai F. and Okano T. Cell sheet engineering: Recreating tissues without biodegradable scaffolds. Biomaterials, 2005, 26, 6415-6422.
219. Harimoto M., Yamato M., Hirose M., Takahashi C., Isoi Y., Kikuchi A. and Okano T. Novel approach for achieving double-layered cell sheets co-culture: overlaying endothelial cell sheets onto monolayer hepatocytes utilizing temperature-responsive culture dishes. Journal of biomedical materials research, 2002, 62, 464-470.
220. Shiroyanagi Y., Yamato M., Yamazaki Y., Toma H. and Okano T. Urothelium regeneration using viable cultured urothelial cell sheets grafted on demucosalized gastric flaps. BJU international, 2004, 93, 1069-1075.
221. Hasegawa M., Yamato M., Kikuchi A., Okano T. and Ishikawa I. Human periodontal ligament cell sheets can regenerate periodontal ligament tissue in an athymic rat model. Tissue Engineering, 2005, 11, 469-478.
222. Shimizu T., Yamato M., Isoi Y., Akutsu T., Setomaru T., Abe K., Kikuchi A., Umezu M. and Okano T. Fabrication of pulsatile cardiac tissue grafts using a novel 3-dimensional cell sheet manipulation technique and temperature-responsive cell culture surfaces. Circulation research, 2002, 90, 1-9.
223. Yamato M., Utsumi M., Kushida A. I., Konno C., Kikuchi A. and Okano T. Thermo-responsive culture dishes allow the intact harvest of multilayered keratinocyte sheets without dispase by reducing temperature. Tissue Engineering, 2001, 7, 473-480.
224. Ai H., Jones S. A. and Lvov Y. M. Biomedical applications of electrostatic layer-by-layer nano-assembly of polymers, enzymes, and nanoparticles. Cell biochemistry and biophysics, 2003, 39, 23-43.
225. Richert L., Arntz Y., Schaaf P., Voegel J. C. and Picart C. pH dependent growth of poly (L-lysine)/poly (L-glutamic) acid multilayer films and their cell adhesion properties. Surface Science, 2004, 570, 13-29.
References
138
226. Schuler M., Owen G. R., Hamilton D. W., de Wild M., Textor M., Brunette D. M. and Tosatti S. G. P. Biomimetic modification of titanium dental implant model surfaces using the RGDSP-peptide sequence: A cell morphology study. Biomaterials, 2006, 27, 4003-4015.
227. VandeVondele S., Vörös J. and Hubbell J. A. RGD-grafted poly-L-lysine-graft-(polyethylene glycol) copolymers block non-specific protein adsorption while promoting cell adhesion. Biotechnology and bioengineering, 2003, 82, 784-790.
228. Semenov O. V., Malek A., Bittermann A. G., Vörös J. and Zisch A. H. Engineered Polyelectrolyte Multilayer Substrates for Adhesion, Proliferation, and Differentiation of Human Mesenchymal Stem Cells. Tissue Engineering Part A, 2009, 15, 2977-2990.
229. Decher G., Hong J. D. and Schmitt J. Buildup of ultrathin multilayer films by a self-assembly process. III: Consecutively alternating adsorption of anionic and cationic polyelectrolytes on charged surfaces. Thin solid films, 1992, 210, 831-835.
230. Tang Z., Wang Y., Podsiadlo P. and Kotov N. A. Biomedical Applications of Layer-by-Layer Assembly: From Biomimetics to Tissue Engineering. Advanced Materials, 2006, 18, 3203-3224.
231. Boulmedais F., Tang C. S., Keller B. and Vörös J. Controlled Electrodissolution of Polyelectrolyte Multilayers: A Platform Technology Towards the Surface-Initiated Delivery of Drugs. Advanced Functional Materials, 2006, 16, 63-70.
232. Tang C. S., Schmutz P., Petronis S., Textor M., Keller B. and Vörös J. Controlled Electrodissolution of Polyelectrolyte Multilayers: A Platform Technology Towards the Surface-Initiated Delivery of Drugs. Biotechnology and bioengineering, 2005, 91, 285-295.
233. Guillaume-Gentil O., Akiyama Y., Schuler M., Tang C., Textor M., Yamato M., Okano T. and Vörös J. Polyelectrolyte coatings with a potential for electronic control and cell sheet engineering. Advanced Materials, 2008, 20, 560-565.
234. Picart C., Lavalle P., Hubert P., Cuisinier F. J. G., Decher G., Schaaf P. and Voegel J. C. Buildup mechanism for poly (L-lysine)/hyaluronic acid films onto a solid surface. Langmuir, 2001, 17, 7414-7424.
235. Richert L., Boulmedais F., Lavalle P., Mutterer J., Ferreux E., Decher G., Schaaf P., Voegel J. C. and Picart C. Improvement of Stability and Cell Adhesion Properties of Polyelectrolyte Multilayer Films by Chemical Cross-Linking. Biomacromolecules, 2003, 5, 284-294.
236. Mendelsohn J. D., Yang S. Y., Hiller J. A., Hochbaum A. I. and RUBNER M. F. Rational design of cytophilic and cytophobic polyelectrolyte multilayer thin films. Biomacromolecules, 2003, 4, 96-106.
References
139
237. Richert L., Lavalle P., Vautier D., Senger B., Stoltz J. F., Schaaf P., Voegel J. C. and Picart C. Cell interactions with polyelectrolyte multilayer films. Biomacromolecules, 2002, 3, 1170-1178.
238. Charest J. L., Garcia A. J. and King W. P. Myoblast alignment and differentiation on cell culture substrates with microscale topography and model chemistries. Biomaterials, 2007, 28, 2202-2210.
239. Dalby M. J., Riehle M. O., Yarwood S. J., Wilkinson C. D. W. and Curtis A. S. G. Nucleus alignment and cell signaling in fibroblasts: response to a micro-grooved topography. Experimental cell research, 2003, 284, 272-280.
240. Fitton J. H., Dalton B. A., Beumer G., Johnson G., Griesser H. J. and Steele J. G. Surface topography can interfere with epithelial tissue migration. Journal of biomedical materials research, 1998, 42, 245-257.
241. Rajnicek A.andMcCaig C. Guidance of CNS growth cones by substratum grooves and ridges: effects of inhibitors of the cytoskeleton, calcium channels and signal transduction pathways. Journal of Cell Science, 1997, 110, 2915-2924.
242. Wan Y., Wang Y., Liu Z., Qu X., Han B., Bei J. and Wang S. Adhesion and proliferation of OCT-1 osteoblast-like cells on micro- and nano-scale topography structured poly(l-lactide). Biomaterials, 2005, 26, 4453-4459.
243. Zinger O., Anselme K., Denzer A., Habersetzer P., Wieland M., Jeanfils J., Hardouin P. and Landolt D. Time-dependent morphology and adhesion of osteoblastic cells on titanium model surfaces featuring scale-resolved topography. Biomaterials, 2004, 25, 2695-2711.
244. Dalby M. J., Riehle M. O., Johnstone H. J. H., Affrossman S. and Curtis A. S. G. Polymer-demixed nanotopography: control of fibroblast spreading and proliferation. Tissue Engineering, 2002, 8, 1099-1108.
245. Brunette D. M. The effects of implant surface topography on the behavior of cells. The International journal of oral & maxillofacial implants, 1988, 3, 231-246.
246. Brunette D. M. Effects of surface topography of implant materials on cell behavior in vitro and in vivo. Nanofabrication and biosystems: integrating materials science, engineering, and biology, 1996, 335-355.
247. Dalby M. J., Yarwood S. J., Riehle M. O., Johnstone H. J. H., Affrossman S. and Curtis A. S. G. Increasing fibroblast response to materials using nanotopography: morphological and genetic measurements of cell response to 13-nm-high polymer demixed islands. Experimental cell research, 2002, 276, 1-9.
248. Smith L. L., Niziolek P. J., Haberstroh K. M., Nauman E. A. and Webster T. J. Decreased fibroblast and increased osteoblast adhesion on nanostructured NaOH-etched PLGA scaffolds. International Journal of Nanomedicine, 2007, 2, 383-388.
References
140
249. Dalby M. J., Giannaras D., Riehle M. O., Gadegaard N., Affrossman S. and Curtis A. S. G. Rapid fibroblast adhesion to 27 nm high polymer demixed nano-topography. Biomaterials, 2004, 25, 77-83.
250. Dalby M. J., Riehle M. O., Johnstone H. J. H., Affrossman S. and Curtis A. S. G. Nonadhesive nanotopography: Fibroblast response to poly(n-butyl methacrylate)-poly(styrene) demixed surface features. Journal of Biomedical Materials Research Part A, 2003, 67A, 1025-1032.
251. Dalby M. J., Gadegaard N. and Wilkinson C. D. W. The response of fibroblasts to hexagonal nanotopography fabricated by electron beam lithography. Journal of Biomedical Materials Research Part A, 2008, 84A, 973-979.
252. Dalby M. J., Childs S., Riehle M. O., Johnstone H. J. H., Affrossman S. and Curtis A. S. G. Fibroblast reaction to island topography: changes in cytoskeleton and morphology with time. Biomaterials, 2003, 24, 927-935.
253. Dalby M. J., Riehle M. O., Sutherland D. S., Agheli H. and Curtis A. S. G. Fibroblast response to a controlled nanoenvironment produced by colloidal lithography. Journal of Biomedical Materials Research Part A, 2004, 69A, 314-322.
254. Gallagher J. O., McGhee K. F., Wilkinson C. D. W. and Riehle M. O. Interaction of animal cells with ordered nanotopography. IEEE transactions on nanobioscience, 2002, 1, 24-28.
255. Schulte V. A., Diez M., Moller M. and Lensen M. C. Surface Topography Induces Fibroblast Adhesion on Intrinsically Nonadhesive Poly(ethylene glycol) Substrates. Biomacromolecules, 2009, 10, 2795-2801.
256. Dalby M. J., Marshall G. E., Johnstone H. J. H., Affrossman S. and Riehle M. O. Interactions of human blood and tissue cell types with 95-nm-high nanotopography. IEEE transactions on nanobioscience, 2002, 1, 18-23.
257. Perez A. L., Spears R., Gutmann J. L. and Opperman L. A. Osteoblasts and MG-63 osteosarcoma cells behave differently when in contact with ProRootÖ MTA and white MTA. International Endodontic Journal, 2003, 36, 564-570.
258. Choi C. H., Hagvall S. H., Wu B. M., Dunn J. C. Y., Beygui R. E. and "CJ" Kim C. J. Cell interaction with three-dimensional sharp-tip nanotopography. Biomaterials, 2007, 28, 1672-1679.
259. Choi C. H., Heydarkhan-Hagvall S., Wu B. M., Dunn J. C. Y., Beygui R. E., Kim C. J. and Foundation F. Cell growth as a sheet on three-dimensional sharp-tip nanostructures. Journal of biomedical materials research.Part A, 2008, 89A, 804-817.
References
141
260. Heydarkhan-Hagvall S., Choi C. H., Dunn J., Heydarkhan S., Schenke-Layland K., MacLellan W. R. and Beygui R. E. Influence of systematically varied nano-scale topography on cell morphology and adhesion. Cell Communication and Adhesion, 2007, 14, 181-194.
261. Meister A., Gabi M., Behr P., Studer P., Vo r., Niedermann P., Bitterli J., Polesel-Maris J., Liley M. and Heinzelmann H. FluidFM: Combining Atomic Force Microscopy and Nanofluidics in a Universal Liquid Delivery System for Single Cell Applications and Beyond. Nano lett, 2009, 9, 2501-2507.