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QUT Digital Repository: http://eprints.qut.edu.au/
This is the accepted version of this journal article. Published as:
Wu, Liping and Wei, Xi and Ling, Junqi and Liu, Lu and Liu, Shaojun and Li, Mintao and Xiao, Yin (2009) Early osteogenic differential protein profile detected by proteomic analysis in human periodontal ligament cells. Journal of Periodontal Research, 44(5). pp. 645‐654.
© Copyright 2008 Blackwell Publishing The definitive version is available at www.blackwell‐synergy.com
1
Early Osteogenic Differential Protein Profile Detected by Proteomic Analysis in
Human Periodontal Ligament Cells
Liping Wu1*, Xi Wei1*, Junqi Ling1†, Lu Liu1, Shaojun Liu2, Mintao Li2, and Yin Xiao3
1Guanghua School of Stomatology, Sun Yat-sen University, Guangzhou, Guangdong,
China
2Proteomics Laboratory, Zhongshan Medical College, Sun Yat-Sen University,
Guangzhou, China
3Institute of Health and Biomedical Innovation, Queensland University of Technology,
Brisbane, Queensland, Australia;
*Contributed equally to this study
†Corresponding author
A running title: Differential Protein Profile in PDLCs
Correspondance to:
Dr. Junqi Ling
Professor and Dean
Guanghua School of Stomatology
Sun Yat-sen University
Guangzhou 510055, P. R. China
2
Tel: +86-20-8386-2621
Fax: +86-20-8382-2807
E-mail: lingjq@ mail.sysu.edu.cn
Keywords: Human periodontal ligament cells; Osteogenic differentiation; Proteomics;
2D-DIGE
Number of words in the abstract: 200
Number of words in the abstract and the text (excluding tables, figure legends,
acknowledgments, and cited references): 3890
Number of figures: 6
Number of cited references: 31
There is no conflict of interest in this study and no author has financial affiliation or
involvement with any commercial organization with direct financial interest in the subject
or materials discussed in this manuscript.
3
Early Osteogenic Differential Protein Profile Detected by Proteomic Analysis in
Human Periodontal Ligament Cells
Abstract
Background and Objective: Human periodontal ligament cells (PDLCs) play a pivotal
role in maintaining periodontal ligament space, have the ability to differentiate into
cementoblasts/osteoblasts-like cells, and a tremendous potential to regenerate periodontal
tissue. The exact molecular mechanisms governing the differentiation status of PDLCs
remains largely unknown. This study was to investigate the differentially expressed
proteins involved in the osteogenic differentiation of PDLCs.
Material and Methods: Using two-dimensional gel electrophoresis (2D-DIGE), mass
spectrometry (MS), and peptide mass fingerprinting (PMF), we have analyzed the
differential protein profiles of PDLCs undergoing mineralization condition.
Results: Compared to undifferentiated PDLCs, 61 proteins with at least a 1.5-fold change
were detected, of which 29 differentially expressed proteins were successfully identified
by matrix assisted laser desorption ionization time-of-flight mass spectrometry
(MALDI-TOF MS). The expression of some of the identified proteins was further
confirmed by western blot and RT-PCR analysis. The identified proteins were found to
belong to cytoskeleton proteins and cytoskeleton-associated proteins, nuclear proteins
and cell membrane-bound molecules.
Conclusion: Our results suggest that these proteins may be associated with the unique
function of PDLCs in maintaining periodontal tissue homeostasis, providing a
comprehensive reference to understand and further study the molecular mechanisms of
4
PDLCs involved in periodontal regeneration.
Keywords: Human periodontal ligament cells; Osteogenic differentiation; Proteomics;
2D- DIGE.
Introduction
The periodontal ligament (PDL) is a narrow fibrous connective tissue that connects the
alveolar bone to teeth and plays an important role in providing anchorage and supporting
tooth function, maintaining homeostasis, and repairing damaged tissue in response to
periodontal disease or mechanical trauma. PDL contains a heterogeneous cell population
at various stages of differentiation and lineage commitment. Previous studies indicate that
periodontal ligament cells (PDLCs) can form mineralized nodules in vitro and express
bone-related proteins, such as alkaline phosphatase (ALP), bone sialoprotein (BSP) and
osteocalcin (OCN) (1-3). Recently Seo et al. reported that PDLCs contain stem cells with
high proliferative capacity, self-renewal propertie, multilineage differentiation potential,
and capable of forming cementum/PDL-like tissue in vivo (4). Thus, PDLCs play pivotal
role in maintaining periodontal ligament space with the ability to differentiate into
cementoblasts/osteoblasts-like cells, and have tremendous potential to regenerate
periodontal tissue. However, a comprehensive understanding of molecular mechanisms
controlling PDLCs differentiation into functional cells remains poor.
Proteomic techniques such as two-dimensional gel electrophoresis (2-DE), coupled with
protein identification by mass spectrometry (MS) and bioinformatics, has led to a
5
revolution in the ability of researchers to tease out the temporal and spatial changes of the
entire protein complement and their functions in a given cell type (5). The task of
detecting changes in protein expression has recently been made possible by the
introduction of difference in gel electrophoresis (DIGE) (6), This method increases
statistical confidence when combining experimental repetition with internal standards and
facilitates the identification of quantitative and qualitative protein alterations during cell
differentiation. Proteomics techniques are now widely accepted as an important tool for
finding potential biomarkers or studying the mechanisms of cell differentiation (7). In
order to identify early differential proteins in PDLCs osteogenic differentiation, DIGE
and MS based proteomics approaches were utilized to investigate PDLCs cultures for 7
days in osteogenic culture conditions. Twenty-nine proteins were identified by matrix
assisted laser desorption ionization time-of-flight mass spectrometry (MALDI-TOF MS),
of which 12 were up-regulated and 17 were down-regulation during early osteogenic
differentiation.
Material and Methods
PDLCs isolation and cell culture
Healthy periodontal ligament tissues were collected from the middle third part of the root
of premolars obtained from patients (12-18 years of age) undergoing orthodontic
treatment in the Department of Orthodontics, Sun Yat-sen University Dental Hospital.
Informed consent was obtained from each subject and the research protocols were
approved by the University Ethic Committee. PDL tissues were minced and digested in a
solution containing 3mg/mL type I collagenase (Worthington Biochem, Freehold, NJ,
6
USA) and 4mg/mL dispase (GIBCO-BRL Life Technologies, Breda, Netherlands) at
370C for 30 to 60 minutes as previously described (4). The digested solution was filtered
through a 70-μm strainer (Becton Dickinson, Sunnyvale, CA, USA) and the released cells
plated in 6-well plates containing alpha modified Eagle’s medium (α-MEM,
GIBCO-BRL) supplemented with 20% fetal bovine serum (FBS, GIBCO-BRL), 100
units/mL penicillin and 100µg/mL streptomycin (Sigma, St. Louis, MO, USA), and
incubated at 370C in 5% CO2. Cells from passages 2 to 4 were used in the following
experiments.
PDLCs surface characterization using flow cytometry analysis
1×105 PDLCs at passage 2 were harvested in phosphate buffered solution (PBS)
containing 1mM EDTA, washed in PBS, and then incubated with 0.5µg/100µL of mouse
antihuman STRO-1 antibodies (R&D systems, Minneapolis, MN, USA) and CD146
(Santa Cruz Biotechnology, Santa Cruz, CA) for 30 minutes at 4°C. Cells were washed
twice with cold PBS containing 2% FBS and incubated with 1µg/100µL of fluorescein
isothiocyanate (FITC onjugated goat antimouse IgM or IgG antibodies (Santa Cruz) for
30 minutes at 4°C. Mouse antihuman antibodies to CD29-FITC, CD44-FITC, CD106-PE,
CD34-FITC (BD Bioscience, Farmington, CT) were also used for phenotype
characterization. Mouse isotype antibodies (BD Bioscience) served as a control. Labeled
cells were analyzed by flow cytometer (Becton -Dickinson, Franklin Lakes, NJ, USA).
The experiments were repeated three times on all three patient samples.
Immunocytochemical staining and alizarin red staining
Comment [QSOE1]: 0.5ug per mL??
7
Cells at passage two were subcultured into 22×22mm slides (2×104cells/mL) for 24 hours
and fixed in 4% paraformaldehyde for 15 minutes, then blocked and incubated with
monoclonal antibody of anti-vimentin or anti-pancytokeratin (Boster Biotechnology, INC,
Wuhan, China) at 1:100 dilution, and rabbit anti-mouse antibody was as a secondary
antibody.
Osteogenic differentiation of PDLCs was verified by the bone nodule formation after
PDLCs had been cultured for 21 days in osteogenic media (α-MEM supplemented with
10mM β-glycerophosphate, 0.2mM ascorbic acid, 100nM dexamethasone [Sigma] with
15% FBS); controls were cultured in α-MEM with 15% FBS, Mineral deposits were
detected at day 21 by 2% alizarin red staining, and osteocalcin expression was monitored
at days 21 by immunocytochemical staining using polyclonal mouse antihuman
osteocalcin (Santa Cruz Biotechnology, Santa Cruz, CA, USA, 1:100 dilution).
Protein preparation
PDLCs were cultured in osteogenic and control medium for 7 days. Prior to the harvest
both the differentiated cells and controls were incubated with serum-free medium for 24
hours after which the medium was removed and the cells washed three times with
ice-cold Tris-buffered sucrose (10mM Tris-base, 250mM sucrose, pH 7.4). The cells were
lysed with sodium dodecyl sulfate (SDS) lysis buffer containing 7M urea, 2M thiourea,
4% CHAPS, and 30mM Tris (GE healthcare), the lysates sonicated on ice and then
centrifuged at 20000g for 30 minutes at 40C. The protein samples were purified using the
2-D Clean-Up Kit (GE healthcare) and protein content determined by 2D-Quant kit (GE
healthcare) according to the manufacturer’s instructions.
8
CyDye labeling of extracted proteins and two-dimensional electrophoresis (2-DE)
Prior to 2-DE the protein extracts were labeled with fluorescent cyanine dyes developed
for 2-D DIGE technology (GE Healthcare) following the manufacturer’s
recommendations. 50mg of differentiated and control proteins were labeled with Cy3 or
Cy5, and 50mg of the internal standard mixture was labeled with Cy2 (Table 1), followed
by incubation on ice for 30 minutes in the dark. The reactions were quenched by the
addition of 1μL of 10mM lysine for 10 minutes on ice in the dark. The quenched Cy3-
and Cy5-labeled samples and the Cy2-labeled internal standard were pooled prior to
analysis by 2-DE. Two preparative gels, each containing 500mg of unlabeled mixture
proteins, were analyzed, and four DIGE gels were run to analyze differentiated and
control samples.
2-DE was performed according to the manufacturer’s instructions (GE Healthcare).
Briefly, immobilized dry strips (pH4-7, 24 cm, GE Healthcare) were rehydrated for 12 h
in the 450μL rehydration buffer (7M urea, 2M thiourea, 4% w/v CHAPS, 1% v/v IPG
buffer (pH 4–7) ,40mM DTT and 0.002% (w/v) Bromophenol blue ) at 30 V for 12 hours
using an Ettan IPGphor II IEF system (GE Healthcare). After rehydration the samples
were focused at 500 V for 1 hour, 1000 V for 1 hour, and at 8000 V for a total of 80000
Vh at 200C. The strips were incubated in Equilibration Buffer I containing 6 M urea, 30%
glycerol, 2% SDS, 50 mM Tris-HCl (pH 8.8), 1% DTT for 15 minutes at room
temperature in the dark and then soaked in Equilibration Buffer II for an additional 15
minutes. Buffer II was identical to Buffer I with the exception of 2.5% iodoacetamide
instead of 40mM DTT. The equilibrated strips were embedded in 0.5 w/v agarose on top
9
of 12.5% acrylamide slab gels. Second dimension separations were performed on an
Ettan DALT six electrophoresis system (GE Healthcare). The proteins were separated
initially at 150C, 2 W/gel for 50 minutes, followed by 17 W/gel until the dye front
reached the bottom of the gel. The two preparative gels were stained with Deep purple
total protein stain (RPN6306, GE Healthcare) following the manufacturer’s instructions.
Gel scanning and image analysis
Both sample and preparative gels were imaged using a Typhoon Variable Mode Imager
9400 (GE Healthcare) using the excitation filters Blue 488nm (Cy2), Green 532nm (Cy3),
Red 633nm (Cy5), and 532nm (Deep Purple) with the resolution of 100μm. The 2-D
image of the gel from each treated sample was compared to that of the control sample via
the internal standard sample. Protein expression analysis was performed for each of the
four gels in parallel using the differential in-gel analysis (DIA) module of DeCyder
software 6.0 (GE Healthcare) using a value of 3000 as the initial estimation of the
number of protein spots present. The intensities of individual protein spots of the
proteomes of the differentiated samples were compared with the control. The DIA
analysis data was collated into a single analysis using the DeCyder biological variation
analysis (BVA) module, and final values for the expression ratio of specific protein spots
between differentiated samples and the control were determined. A total of 2787~3039
protein spots were analyzed across all cell samples and Student’s t-test and one-way
ANOVA were used to calculate significant differences in the relative abundance of
individual protein spot features between differentiated samples and the control. Protein
spots an abundance ratio greater than +1.5 or less than -1.5 were determined to be
10
differentially expressed.
In-gel digestion and MALDI-TOF MS
Selecting protein spots from the gels, in-gel digestion, peptides extraction, preparation of
the samples for MS and spotting on target slides were carried out automatically with an
Ettan spot handling workstation (GE Healthcare). Identification of proteins by peptide
mass fingerprinting (PMF) was carried out on an Ettan MALDI-TOF mass spectrometer
(GE Healthcare) operating in reflectron mode. Internal calibration was performed using
the trypsin autodigestion peaks at m/z 842.509 and 2211.104. Mass spectra were obtained
over the m/z range of 700–3000 Da. PMF data was used to search the human NCBI nr
protein database using the Profound search engine (http://www.
matrixscience.com/cgi/search_form.pl?FORMVER=2&SEARCH=PMF, GE Healthcare).
Search parameters were as follows: type of search, peptide mass fingerprint; enzyme,
trypsin; fixed modification, carbamidomethylation (Cys); variable modifications,
oxidation (Met); mass values, monoisotopic; peptide charge state, 1+; maximum missed
cleavages, 1; and peptide mass tolerance, 100ppm.
Western blot
PDLCs on days 0 (at 80% confluence, before the addition of osteogenic induction
medium) and 7 of osteogenic induction were harvested and lysed in SDS lysis buffer,
sonicated, and centrifuged at 12000g for 5 minutes. Equal amounts of protein (50μg)
were separated by electrophoresis on a 12.5% polyacrylamide gel and transferred to
nitrocellulose membranes by 100mA for 3 hours. The membranes were blocked in 5%
11
nonfat dry milk at room temperature for 1 hour, rinsed, and incubated with primary
antibodies (1:1000 dilution) of mouse anti-human heteronuclear ribonuclear proteins
C1/C2 (hnRNPC, Santa Cruz), mouse anti-human caldesmon (CaD), mouse anti-human
tropomyosin (Tm), rabbit anti-human polyclonal antibody AnnexinA4 (Cell Signaling,
LAB VISION Corporation NeoMarkers), or mouse anti-human β-actin (Santa Cruz) at
40C overnight. The membranes were washed, then incubated with HRP-conjugated
secondary antibodies (Santa Cruz, 1:5000 dilutions) at room temperature for 1 hour, and
the proteins visualized using enhanced chemiluminescence (Amersham Pharmacia
Biotech, Piscataway, NJ, USA).
Quantitative real-time reverse-transcription polymerase chain reaction
Prior to osteogenic induction and after 7 days of induction, cells were lysed to extract
total RNA by using RNeasy Mini Kit (Qiagen GmbH, Hilden, Germany). The primers
used for detection were listed in Table 2. Quantifications of mRNAs were performed with
an ABI Prism 7000 sequence detection system (Applied Biosystems, Foster City, CA).
cDNA was synthesized from 1�g of each RNA sample using the omniscript RT kit
(Qiagen) and RNase-free DNase Set (Qiagen) following the manufacturer’s instructions,
5µL of the reaction mixture was incubated with PCR master mix with double-stranded
DNA dye SYBR Green I (Qiagen) in a total volume of 50µL. All reactions were run with
a hot start preincubation step of 3 minutes at 93°C, followed by 40 cycles of 1 minute at
93°C, 1 minute at 55°C, and 1 minute at 72°C. The amount of template was quantified by
using the comparative cycle threshold method according to the manufacturer’s protocol.
Measured mRNA levels were normalized against β-actin mRNA expression. Experiments
12
were performed in triplicates on three different cell samples.
Statistical analysis
All experiments have been repeated three to four times, and the representative results are
presented. The quantitative data is presented as mean ± standard deviation. One-way
analysis of variance (ANOVA) and Bonferroni test was performed to analyze mRNA
expressions between induced samples and controls. Differences were considered
significant at p<0.05. The SPSS software package (version 13.0, SPSS Inc., Chicago, IL,
USA) was used for the statistical analysis.
Results
Cell characterization
PDLCs expressed cell surface epitopes associated with mesenchymal progenitors such as
STRO-1, CD-146, CD29, CD44, CD106, but did not express CD34, a hematopoietic
origin marker as shown by flow cytometry. The expression of STRO-1, CD-146, CD29,
CD44, CD106 was 15.3%, 47.6%, 99.9%, 99.8% and 76.8% respectively (Fig. 1A-F,
Table 3). The positive immunocytochemical staining for vimentin antibody, the most
widely distributed intermediate filament in fibroblasts, and negative staining for
pancytokeratin, a marker for tissue of epithelial origin, indicated that the PDLCs islolated
from PDL tissue in this study were of mesenchymal origin (Fig. 2A-B).
Alizarin red positive nodules were seen in PDLC cultures on day 21 of osteogenic
induction, however, no staining was detected in the controls (Fig. 2C). Furthermore,
PDLCs showed positive expression of OCN after 21 days of osteogenic induction (Fig.
13
2D). Quantitative real-time RT-PCR showed an upregulation of ALP, OCN and matrix
extracellular phosphoglycoprotein (MEPE) mRNA expressions in osteogenic culture
conditions (Fig 3). The difference between the induced cells versus controls at the same
time points was statistically significant (on days 14 and 21 for ALP and OCN, on day 21
for MEPE, ANOVA, p﹤0.05 or p﹤0.001) for each transcript. These results suggest that
PDLCs are able to differentiate into cementoblasts/osteoblasts in vitro.
Osteogenic differential protein expression in PDLCs identified by 2D-DIGE and
MALDI-TOF MS
Protein profiles were compared between the osteogenic induced cells and controls. The
DeCyder software detected more than 2,787 protein spots across all four gels. 61 protein
spots showed at least 1.5-fold changes in expression of which 14 proteins were
up-regulated and 47 proteins were down-regulated (p<0.05). The protein profile of
2D-DIGE is shown in Figure 4. MALDI-TOF MS identified 29 proteins in PDLCs by
their PMF using the Swiss-Prot database. These proteins were classified into seven
functional categories: cytoskeleton proteins, nuclear proteins, cell membrane-bound
molecules, proteins involved in matrix synthesis, protein synthesis, metabolic enzymes
and signal transduction (Table 4).
Western blot and RT-PCR analysis of up- or down-regulated proteins
To confirm the results obtained in 2D-DIGE gels, several proteins, such as the
cytoskeleton associated proteins caldesmon (CaD) and tropomyosin (Tm), heterogeneous
nuclear ribonucleoprotein C (hnRNPC) and calcium-binding protein annexin A4, were
14
selected for the further confirmation by western blot and quantitative PCR (qPCR). The
proteins and mRNA were extracted from PDLCs at days 0 and 7 of induction. Western
blot analysis confirmed the down-regulation of CaD, Tm, hnRNPC and up-regulation of
annexinA4 after osteogenic induction of PDLCs on days 7. Furthermore, qPCR analysis
showed similar changes in mRNA expressions of CaD, Tm, hnRNPC and annexin A4 in
osteogenic culture (Fig. 6).
Discussion
In this study, PDLCs isolated from periodontal ligament showed a similar profile of cell
surface epitopes compared with the studies reported by others (4, 8, 9). Seo et al. showed
that periodontal ligament stem cells (PDLSCs) are immunocytochemically positive for
STRO-1 and CD146, markers which have been used to isolate and purify human bone
marrow mesenchymal stem cells (MSCs) (4). By flow cytometry analysis, we found that
the percentage of STRO-1 positive cells at passage 2 was higher than previously reported
(8). Our findings that PDLCs expressed the mesenchymal stem cell-associated antigens
CD44 and CD106 and an absence of hematopoietic marker CD34 expression agreed with
that reported by Gronthos et al (9). These results indicate that PDLCs contain a
population of mesenchymal stem cell. We also demonstrated that PDLCs formed a
mineralized matrix and expressed the bone-related markers ALP, OCN and MEPE when
grown in osteogenic media. These data suggest that cultured PDLCs may represent a
heterogeneous stem-cell enriched population and have the potential to differentiate into
cementoblasts or osteoblasts in vitro.
15
Although some growth factors, genes and signaling molecular have been identified in the
process of cementogenesis/osteogenesis with conventional molecular biological
approaches (10-12), the differentiation mechanisms of stem/progenitor cells in
periodontal regeneration need to be further understood. Proteomic profiling analysis
provides a complementary and potentially more comprehensive approach to tease out
important protein candidates in the process of differentiation. In this study, PDLCs were
induced along cementoblasts/osteoblasts lineages. Changes in protein expression levels
during PDLCs differentiation on day 7 was determined by proteomics based on the
highly sensitive 2D-DIGE and MALDI-TOF MS technologies. 29 differentially
expressed proteins were identified in PDLCs during the cementoblast/osteoblast
differentiation. These proteins mainly effect the cytoskeleton, nuclear regulation, cell
membrane-bounding, matrix synthesis, metabolic enzymes and signal transduction.
We found that cytoskeleton proteins, including vimentin, CaD, Tm and Clathrin heavy
chain polypeptide (CHC), were down-regulated during cementoblastic/osteoblastic
differentiation of PDLCs. Significant down-regulation of vimentin has been demonstrated
in vitro in MSCs differentiating into cardiomyocytes (13), suggesting differentiation
stage-specific reorganization of the cytoskeleton. In addition, vimentin exhibits a
complex pattern of developmental and tissue-specific expression regulated by
transforming growth factor beta 1 (TGFβ-1), which plays an important role in cell
differentiation (14). CaD contains actin-, myosin-, tropomyosin-, and Ca2+-calmodulin
(CaM)-binding domains (15), and is often regarded as differentiation marker of smooth
muscle cells (16). CaD was down-regulated in MSCs during the process of neuron-like
16
differentiation (17), providing further evidence of its involvement in cell differentiation.
CaD can be phosphorylated by p21-activated kinases (PAKs), a dynamic process required
to regulate actin dynamics and membrane protrusions in wound-induced cell migration
(18). As a natural partner of CaD, tropomyosin regulate actomyosin-based contractility,
mediate the inhibitory effects of CaD on actomyosin and regulate cytokinesis speed and
membrane stability during cell division (19). CHC, another actin filament binding protein
identified in this study, has, together with Tm and annexin 4, been indentified to be
involved in the osteogenic differentiation of MSCs (20). An earlier proteomics study of
periodontal ligament fibroblasts found that the expression of actin, vimentin and Tms
were related to mechanical loading and remodeling of PDL (21). In our study, we found a
down-regulation of vimentin, CaD, beta Tm, skeletal muscle Tm, CHC and related kinase
PAK65 at day 7 of PDLCs osteogenic differentiation. Co-regulation of the functional
class of proteins during PDLCs differentiation suggests that these cytoskeleton proteins
are intimately involved in the differentiation process and that their regulation proceeds
via similar regulatory mechanisms. It is possible that these proteins may be involved in
regulating cell migration during the osteogenic differentiation of PDLCs, but this
hypothesis needs to be confirmed by further experiments.
The hnRNPC proteins (C1 and C2) belong to a class of proteins that bind to pre-mRNA
in the cell nucleus. Increased expression of hnRNPC induced the translation of p27
mRNA and triggered the inhibition of cell growth via p27 regulated cell cycle arrest (22).
Forster and colleagues, applying a proteomic approach, observed the co-regulation of five
members of hnRNPs family (hnRNP C1/C2, Q, U, K and G) during MSC osteogenic
17
differentiation; altered expression of hnRNPs was regarded to be related with cell
adhesion (20). The down-regulation of hnRNP C1/C2 found in our study further supports
this protein’s critical role in cell adhesion in PDLC osteogenic differentiation. In addition
to hnRNP C1/C2 proteins, the two nuclear proteins nucleophosmin 1 (NPM1) and lamins
A/C, were also down-regulated during PDLCs differentiation. NPM1 protein serves as a
shuttle protein for the nuclear transport of ribosomal components and presumably
collaborates with other nucleolar proteins in ribosome assembly (23). Nuclear lamins A/C
are intermediate filament proteins which form the nuclear lamina underlying the inner
nuclear membrane (24). The absence of lamin A/C has been identified as a novel marker
for undifferentiated embryoic stem (ES) cells and lamin A/C expression as an early
indicator of ES cell differentiation, indicating the functional role of lamin A/C in the
maintenance of the differentiated state (25). The concomitant down-regulation of hnRNP
C1/C2, NPM1 and lamin A/C in our study suggest that these nuclear proteins may work
together to allow osteogenic differentiation of PDLCs to be proceed.
Annexins belong to a family of structurally related of calcium-binding proteins (26),
several of which have already been found to play roles in osteogenesis and mineralization.
Ye et al found, by 2-DE and MS, that three isoforms of annexin A1 are down-regulated to
various degrees during rat MSC differentiation (13). Other proteomics studies have
demonstrated the differential expression of anexins A1, A2, A4 and V in hMSC
osteogenic differentiation (27, 28). Annexin A4 is reported to regulate a
calmodulin-dependent kinase II-activated (Ca2+/CaMKII) chloride conductance, and has
been proposed to play a role in exocytosis, vesicle aggregation and trafficking in a
18
Ca2+-dependent manner (29-31). In our study both the protein and mRNA expression of
annexins A4 were up-regulated in the mineralization process of PDLCs. Although some
possible biological functions of annexin A4 have been proposed, the exact role of this
molecule in osteogenic differentiation of PDLCs requires further investigation.
It is worth noting that typical bone-related markers, such as ALP, OCN and MEPE, were
not seen to be up-regulated in the proteomic map during early differentiation, although
these markers were significantly up-regulated during the late stages of osteogenic
differentiation of PDLCs, confirmed by qPCR. ALP is reported to be detectable in early
osteogenic differentiation, but in our study neither mRNA nor protein levels showed any
significant difference at day 7 of differentiation. One possible reason for this apparent
variation may be the source of cells and differentiation protocols utilized in the various
research laboratories. However, the early regulatory proteins identified in our study may
provide some insights into the potential molecular interactions between early and late
stage differential proteins.
Conclusion
In this study we present for the first time the differential protein expression profiles of
PDLCs at day 7 of osteogenic induction. 29 proteins were identified by MS analysis
showing differential expression during osteogenesis. These proteins mainly included
cytoskeleton proteins and cytoskeleton-associated proteins, nuclear proteins, cell
membrane-bound molecules, and may be associated with the unique function of PDLCs
in maintaining periodontal tissue homeostasis, especially in the mineralization nature of
PDL. Our results provide a comprehensive reference to understand and further study
19
molecular mechanisms of PDLCs in periodontal regeneration.
Acknowledgements
This investigation was supported by the National Nature Science Research Grant
(30672318) of China.
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