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Universitätsklinikum Ulm
Institut für Pathologie
Ärztlicher Direktor: Prof. Dr. med. Peter Möller
Mitochondrial alterations in different Alzheimers d isease
mouse models
Dissertation
zur Erlangung des Doktorgrades der Medizin
der Medizinischen Fakultät
der Universität Ulm
vorgelegt von
Frederik Scheibe
Aachen
2014
Amtierender Dekan: Prof. Dr. Thomas Wirth
1. Berichterstatter: Prof. Dr. Dietmar Thal
2. Berichterstatter: Prof. Dr. Christine von Arnim
Tag der Promotion: 24.04.2015
Contents
I
Contents
Contents........................................... ...................................................................... I
Abbreviations ...................................... ................................................................ III
1 Introduction ....................................... ..................................................... 1
1.1 Alzheimers disease ....................................................................... 1
1.2 Neuropathology ............................................................................. 1
1.2.1 APP and Aβ ........................................................................... 2
1.2.2 The amyloid hypothesis ......................................................... 3
1.2.3 Intraneuronal Abeta ............................................................... 4
1.3 Mitochondria.................................................................................. 5
1.3.1 Mitochondrial function in AD .................................................. 6
1.4 Mouse models ............................................................................... 7
1.5 Aims of the study......................................................................... 10
2 Material and Methods ............................... ........................................... 12
2.1 Material and Equipments used.................................................... 12
2.2 Mouse models ............................................................................. 15
2.3 Tissue praparation and DiI tracing............................................... 15
2.4 Microscopic and quantitative analysis ......................................... 16
2.5 Immunohistochemistry ................................................................ 17
2.6 Protein extraction from brain tissue ............................................. 18
2.7 SDS-PAGE and Western blot analysis........................................ 18
2.8 Aβ Enzyme Linked Immunosorbent Assay (ELISA) .................... 19
2.9 Stereology ................................................................................... 19
2.10 Electron microscopy, immuno electron microscopy..................... 19
2.10.1 Semiquantitative analysis of synapse densities ................. 20
2.10.2 Semiquantitative analysis of dystrophic dendrites ............. 20
2.10.3 Analysis of mitochondria .................................................... 21
2.11 Statistical analysis ....................................................................... 23
3 Results ............................................ ...................................................... 25
3.1 Different patterns of Aβ-pathology in APP23 and APP48 mice ... 25
3.2 Degeneration of neurites and asymetric synapses in APP23 but
not in APP48 mice.................................................................................. 28
II
3.3 Neuron loss in the CA1 subfield but not in the frontocentral cortex
of APP48 and APP23 mice .................................................................... 34
3.4 Increased mitochondrial alterations in APP48 in neuronal somata
of APP48 but not in APP23 .................................................................... 34
4 Discussion......................................... ................................................... 39
4.1 Aβ effects on mitochondrial integrity............................................ 40
4.2 Neurite and synapse degeneration in APP23 and APP48 mice .. 42
4.3 Two types of Aβ-induced neurodegeneration in the frontocentral
cortex: somatic type and neuritic type.................................................... 43
4.4 Conclusions................................................................................. 45
5 Summary............................................ ................................................... 47
6 References......................................... ................................................... 49
Supplementary Material ............................. ........................................................ 64
Supplementary Tab. 1............................................................................ 64
Acknowledgements................................... ......................................................... 77
Curriculum vitae ................................... .............................................................. 78
Abbreviations
III
Abbreviations
ABAD Aβ-binding alcohol dehydrogenase
ABC complex avidin-biotin-peroxidase complex
Acetyl-CoA acetyl coenzyme A
AD Alzheimers disease
ADP Adenosine diphosphate
AICD Amyloid precursor protein intracellular domain
ANOVA Analysis of variance
APH-1 anterior pharynx defective protein 1
APOE Apolipoprotein E
APP Amyloid precursor protein
ATP Adenosine triphosphate
Aβ Amyloid beta protein
CA1 Cornu ammonis
CAA Cerebral amyloid angiopathy
CTF C-terminal fragment
CypD Cyclophilin D
DAB 3,3'-Diaminobenzidine
DNA Deoxyribonucleic acid
ELISA Enzyme Linked Immunosorbent Assay
ETC electron transfer chain
FADH flavin adenine dinucleotide
IgG Immunoglobulin G
IHC Immunohistochemistry
kDa kilo Dalton
LDS lithium dodecyl sulfate
M Mol
M1 primary motor cortex
M2 secondary motor cortex
MW molecular weight
NADH Nicotinamide adenine dinucleotide
NFTs Neurofibrillary tangles
Abbreviations
IV
P1 pellet containing the membrane-associated and the
insoluble, plaque-associated fraction after
homogenization
P2 dispersible fraction after ultracentrifugation
P3 pellet after SDS-resuspension and centrifugation
pAβ phosphorylated Amyloid beta protein
PBS Phosphate buffer saline
PEN2 Presenilin enhancer 2
PFA Phosphate buffer saline
PSEN1 Presenilin 1
PSEN2 Presenilin 2
RNA Ribonucleic acid
ROS reactive oxygen species
S1 supernatant with the soluble and dispersible fraction in
homogenization
S2 supernatant after ultracentrifugation
S3 supernatant after SDS-resuspension and centrifugation
sAPPα soluble amyloid precursor protein N-terminal fragment α
sAPPβ soluble amyloid precursor protein N-terminal fragment β
SC1 primary somatosensory cortex
SDS sodium dodecyl sulfate
SDS-PAGE sodium dodecyl sulfate polyacrylamide gel
electrophoresis
TBS Tris-Buffer Saline
TIM Translocase of the inner mitochondrial membrane
TOM Translocase of the outer mitochondrial membrane
τ protein Tau protein
Introduction
1
1 Introduction
1.1 Alzheimers disease
Alzheimers disease (AD) is the most common form of dementia in the elderly. It
was first described by Alois Alzheimer in 1907. He reported the case of a 51 year
old woman with progressive mental disorders and histologic brain pathology, i.e.
senile plaques and neurofibrillary tangles (Alzheimer, 1907). Accordingly, the
typical clinical symptoms of AD are difficulties in learning, memory loss,
disorientation in time and/or place, changes in mood and personality. In 2000 the
prevalence of AD in the U.S. population was estimated to be as high as 4.5 million
persons with an expected increase up to 13.2 million by 2050 (Hebert et al., 2003).
The prevalence of AD in the age group of people ≥ 65 years is 13 % while it
increases in the group of people ≥ 85 years up to 43% (Thies and Bleiler, 2011).
Most AD cases are sporadic. Most sporadic AD cases are late-onset AD cases,
i.e. dementia manifests at the age of 65 years or older. Here, age and the
prevalence of the Apolipoprotein E (APOE) ε4 allele are the most important risk
factors. When AD manifests at age < 65 years, the cases are referred to as “early-
onset” AD cases. Early onset cases frequently have a familial history and carry
mutations in the APP, PS1 or PS2 gene. Other established risk factors are mild
cognitive impairment, cardiovascular disease risk factors, traumatic brain injury
and female gender (Corder et al., 2004).
1.2 Neuropathology
In patients with typical AD symptoms there are degenerative changes in various
brain regions. Macroscopic examination of the brain shows cortical atrophy
especially in frontal, temporal and parietal lobes. Accompanied with a widening of
the cerebral sulci and with enlargement of the central ventricel. Microscopically,
the hallmarks of the AD neuropathology are:
1) Extracellular senile plaques, consisting of Amyloid-β (Aβ) which is generated
from the amyloid precursor protein (APP) and that forms aggregates in a
hierarchical manner in the brain (Masters et al., 1985; Thal et al., 2002). The major
component of these amyloid plaques consist of the 40-42 amino acid amyloid beta
protein which can also be shown in different Alzheimers disease mouse models.
Introduction
2
2) Intracellular neurofibrillary tangles (NFTs), consisting of the protein tau (τ) which
is physiologically involved in stabilization and assembly of microtubules in nerve
cells (Goedert and Spillantini, 2006). Its pathologic hyperphosphorylated
appearance leads to the aggregation and formation of NFTs. Tau is a major
hallmark of different kinds of dementia including AD in the class of tauopathies
(Duyckaerts et al., 2009).
3) Cerebral amyloid angiopathy (CAA), showing vascular Aβ deposits in brain
vessels similar to senile plaques and being capable of causing hemorrhage and
infarction (Ghiso et al., 2010). In almost all persons with dementia CAA was found
(Arvanitakis et al., 2011).
Although these changes follow a typical regional progression in AD brain they are
not specific (Montine et al., 2012) and can also be seen in non-demented elderly.
Additionaly neuron loss, dendritic and synaptic degeneration are seen in AD
brains.
1.2.1 APP and A β
Aβ protein was identified as the major component in cerebrovascular amyloid
deposits (Glenner and Wong, 1984a) and as the main core protein in AD typical
extracellular plaques (Masters et al., 1985). It is a 36-43 amino acid peptide of 4
kDa molecular weight with its most common monomeric forms Aβ1-40 and Aβ1-42.
Aβ is derived from a larger protein, the APP, by proteolytic cleavage. APP is a
highly conserved single-pass transmembrane protein with a large extracellular
domain (O'Brien and Wong, 2011) and its 695 amino acids form is the most
common isoform in the central nervous system (Bayer et al., 1999). It is cleaved
by proteases, forming different proteolytic fragments.
Two different pathways for APP cleavage exist, the non-amyloidogenic pathway by
the α-secretase without pathological consequences and the amyloidogenic
pathway driven by the β-secretase leading to the formation of toxic Aβ.
The α-secretase cleaves APP within the Aβ region, leading to generation of the
secreted N-terminal APP processing product, (sAPPα) and retending a C-terminal
membrane-bound fragment (CTF) which can be cleaved by the γ-secretase
releasing the p3 fragment (Selkoe, 2001) and the APP intracellular domain (AICD).
It was shown that sAPPα is an actor in many physiological processes, i.e.
neuroprotection (Mattson et al., 1993; Furukawa et al., 1996; Kogel et al., 2005),
Introduction
3
modulation of neuronal excitability (Mattson et al., 1993; Mattson and Furukawa,
1998), synaptic plasticity (Turner et al., 2003; Ring et al., 2007), axonal growth and
branching (Moya et al., 1994; Ikin et al., 2007), dendritic outgrowth (Mattson,
1997) and in synaptogenesis (Mattson and Furukawa, 1998; Wang et al., 2011).
Also the α-secretase derived C-terminal fragment p3 and AICD are discussed to
have neuroprotective and neurotrophic properties. This non-amyloidogenic
pathway precludes the formation of toxic Aβ by cutting APP within the Aβ region
(Esch et al., 1990; Sinha and Lieberburg, 1999).
Alternatively to the non-amyloidic pathway, APP can be cleaved by β-and γ-
secretase, releasing a smaller fragment, sAPPβ, Aβ and AICD. This
amyloidogenic pathway leads to Aβ-formation when γ-secretase processes the β-
secretase derived C-terminal fragment (APP-CTFβ) fragment and leads to the
formation of different Aβ species, especially Aβ1-40 and Aβ1-42 (Seubert et al.,
1993) and the C-terminal fragment.
The γ-secretase is a protein complex consisting of Presenilin 1 (PSEN1) or
Presenilin 2 (PSEN2) and Nicastrin, Presenilin enhancer 2 (PEN2) and the
anterior pharynx defective protein (APH-1) (De Strooper, 2003). The presenilins
form the active center of the γ-secretase. Presenilin 1 and 2 knockout mice and
cells did not produce Aβ (De Strooper et al., 1998; Herreman et al., 2000).
Mutations causing familial Alzheimer disease occur in the PSEN1, PSEN2 and
APP genes (Goate et al., 1991; Levy-Lahad et al., 1995; Sherrington et al., 1995).
A pathological role of APP and Aβ in AD was considered because mutations on
the APP gene locus were shown to cause familial early-onset AD (Goate et al.,
1991; Mullan et al., 1992) by an elevated production of Aβ (Citron et al., 1992; Cai
et al., 1993). Interestingely nearly all patients with trisomy 21 beyond 45 years of
age develop an AD and plaque pathology (Glenner and Wong, 1984b) while the
APP encoding gene resides on chromosome 21 (Robakis et al., 1987). Recently, a
protective APP mutation was found in an icelandic cohort that decreases formation
of amyloid peptides, protects against cognitive decline in the elderly and is
discussed to reduce β–cleavage of APP (Jonsson et al., 2012).
1.2.2 The amyloid hypothesis
Because neuritic plaques contain Aβ, the so called “amyloid hypothesis” was
instandly suggested (Hardy and Higgins, 1992) and later on modified in
Introduction
4
accordance to new findings (Hardy and Selkoe, 2002). It proposes that altered
APP processing drives Aβ production, Aβ results in plaque formation, plaques or
soluble Aβ aggregates induce neurodegeneration, and the resultant neuronal loss
results in the clinical dementia syndrome typical of AD (Hardy and Allsop, 1991;
Hardy, 1997; Swerdlow, 2007b). The presenilin mutations lead to an increased
production and aggregation of Aβ42 in total but also in relation to Aβ40 (Scheuner et
al., 1996). The Aβ42 protein is more prone to aggregate than Aβ40, is predominant
in senile plaques (Roher et al., 1993) and is toxic to cells in culture (Younkin,
1995; Swerdlow, 2007b).
The amyloid hypothesis has evolved since it was first postulated. Two major
modifications are 1) Neuritic plaques are no longer considered as the toxic
aggregates but as sinks for Aβ. Soluble Aβ aggregates such as oligomers not
sequestered in plaques are today suggested to represent toxic agents in AD
(Hardy and Selkoe, 2002; Lesne and Kotilinek, 2005; Walsh et al., 2005). 2) Aβ42
has a major importance for toxicity instead of total Aβ (Younkin, 1995).
Extracellular deposits of Aβ are typical for AD brains but nevertheless are also
found in cognitively normal elderly people. The number of Aβ deposits found do
not allow a conclusion to the degree of cognitive impairment (Hardy and Selkoe,
2002). However, amyloid plaque deposition in the AD brain follows a hierarchichal
sequence in which many brain areas are subsequently affected (Thal et al., 2002).
1.2.3 Intraneuronal Abeta
In addition to extracellular Aβ-deposition in plaques, intracellular Aβ occurs in
nerve cells in the AD brain (Gouras et al., 2000; D'Andrea et al., 2002) and in
mouse models for AD (Tomiyama et al, 2010; Wirths et al., 2001; Takahashi et al.,
2002; Abramowski et al., 2012b). The role of intracellular Aβ for
neurodegeneration and the development of AD has been discussed
controversially. Mutant intracellular Aβ has been shown to induce hippocampal cell
loss associated with endoplasmatic reticulum stress and mitochondrial alterations
in AD mouse models (Umeda et al., 2011), suggesting that intracellular Aβ might
be an early event in AD pathology (LaFerla et al., 2007). In young patients with
trisomy 21 it has been shown that high intracellular Aβ levels declined when
extracellular plaques accumulated (Mori et al., 2002). Within the neuron Aβ
accumulates in multivesicular bodies in pre- and postsynaptic compartments while
Introduction
5
abnormal synaptic morpholgy is present in AD mouse models Tg2576 with the
human APP Swedish mutation 670/671 (Takahashi et al., 2002). In this mouse
model mitochondria were found to be a site of Aβ accumulation, also showing a
decrease of cytochrome c activity suggesting that Aβ could affect mitochondrial
function. Here, an increase of hydrogen peroxide was directly correlated to levels
of soluble Aβ suggesting that soluble Aβ may be responsible for hydrogen
peroxide production leading to oxidative stress (Manczak et al., 2006).
In the following paragraph I will give a short introduction to general mitochondrial
function and its role in AD pathology.
1.3 Mitochondria
Mitochondria are essential parts of the eucaryotic cell and are often localized close
to structures with a high metabolic rate of ATP, e.g. in muscles near the actin and
myosin filaments. The average diameter of mitochondria is about 0,5 – 1 μm but
studies have shown that size and plasticity of mitochondria are in a state of
permanent change and that they have the ability to fuse with other mitochondria
(fusion) and to seperate again (fission) (Dimmer and Scorrano, 2006). Whithin the
cell mitochondria are transported along microtubules which determine direction of
internal transport and distribution in distant cell types.
Mitochondria are enclosed by two membranes, the inner and the outer
mitochondrial membrane. These membranes divide the inner mitochondrial space
in two seperate compartments; the inner matrix and the intermembranal space.
There are more than 1000 mitochondrial proteins which are encoded in the
nucleus and imported to the different mitochondrial compartments by translocases
of the outer and inner membrane (TOM/TIM). The outer membrane also contains
transport proteins like voltage-dependant anion channels making it permeable to
molecules and proteins of the size of 5000 daltons or less (Wohlrab, 2009). The
inner membrane is highly specialised and is characterised by cristae which
increase the inner membrane surface. In contrast to the outer membrane it is
impermeable to ions by its lipid bilayer membrane but different transport proteins
make it selectively permeable to metabolized molecules or those which are
requiered by enzymes in the matrix for Krebs cycle and the electron transport
chain. In the Krebs cycle pyruvate and fatty acids are converted to acetyl CoA.
Great amounts of NADH (and FADH2) are created by this oxidative reaction. This
Introduction
6
energy carrier looses its electrons on its way through the respiratory chain in the
inner mitochondrial membrane converting O2 to H20. In so doing, its energy is
stored as an electrochemical proton gradient which enables the membranebound
enzyme ATP synthase to convert ADP to ATP via oxidative phosphorylation. 15
times more ATP can be produced this way than by glycolysis alone. This
demonstrates the importance of mitochondria to the cell for its energy generation.
The inner matrix contains the mitochondrial genome, ribosomes, transfer RNA and
a variety of enzymes necessary for expression of mitochondrial genes. The
mitochondrial genome is present as a double stranded, circular DNA molecule
which provides the mitochondrion with only a part of the requiered proteins. Some
of the catalytically most important subunits of the cytochrome c oxidase complex
are encoded in the mitochondrial genome (Swerdlow et al., 2010). However, most
proteins of the mitochondrial matrix are encoded in the cellular DNA and are
imported from the cytosol. The mitochondrial DNA, which is especially important to
the electron chain and ATP generation is highly susceptible to reactive oxygen
species (ROS). When mitochondrial DNA is damaged by accumulation of ROS a
threshold can be reached leading to a point of no return that results in the
induction of apoptosis. This intrinsic pathway of apoptosis can also be induced by
other mechanisms of cell injury, for example DNA damage, oxidative stress,
accumulation of misfolded proteins and the lack of oxygen or nutrients. It is started
by the release of cytochrome c, a part of the electron transport chain, to the
cytosol what is followed by the activation of the caspase cascade, ultimately
leading to nuclear fragmentation and cell death.
1.3.1 Mitochondrial function in AD
An alternative hypothesis for the development of AD is that oxidative stress leads
to mitochondrial dysfunction as one of the primary events in AD related
neurodegeneration. This mitochondrial cascade hypohesis was proposed in order
to understand the correlation of advancing age and AD and the cause of Aβ
amyloidosis in late-onset AD (Swerdlow and Khan, 2004). The main assertions of
the hypothesis are that
1. mitochondrial function and durability is determined by inheritance,
2. the structural and functional changes of mitochondria going along with age are
determined by mitochondrial durability and
Introduction
7
3. mitochondrial changes with age pass a threshold causing AD pathology and
symptoms e.g. via apoptosis of nerve cells (Swerdlow et al., 2010).
Mitochondrial dysfunction has been described in several studies of AD brains, in
APP mouse models and cell lines (Gibson et al., 1998; Keil et al., 2004; Lustbader
et al., 2004; Manczak et al., 2004; Reddy et al., 2004; Caspersen et al., 2005; Devi
et al., 2006; Manczak et al., 2006; Eckert et al., 2008; Hauptmann et al., 2009).
Structural changes and a reduction of neuronal mitochondria were shown in
morphological studies (Hirai et al., 2001). Also early defects in glucose metabolism
of AD patients suggest alterations in mitochondrial functions (Hoyer, 2000).
Important findings were also the deficiency of enzymes of the Krebs cycle, such as
pyruvate dehydrogenase complex, ketoglutarate dehydrogenase complex, and the
reduction of cytochrome c oxidase activity. Here, it was shown that Aβ directly
disrupts mitochondrial function by inhibiting key enzymes and may thereby
contribute to the deficiency of energy metabolism seen in AD (Casley et al., 2002).
The reduction of cytochrome c oxidase activity was also shown in so called cybrid
cell lines with AD mitochondria compared to cell lines with control subject
mitochondria. Other findings in these cybrid cells were altered homeostasis,
reduction of mitochondrial membrane potential, activation of apoptosis pathways
and increased Aβ42 production (Swerdlow, 2007a). Some of these studies suggest
that mitochondrial changes preceed AD pathology like Aβ accumulation, others do
not. It is tempting to hypothesize that there are several events of mitochondrial
damage affecting each other leading to a vicious cycle of neurodegeneration.
1.4 Mouse models
Transgenic mouse models for AD pathology have been created to understand
disease mechanisms. They are also important for drug tests and clinical trials. A
great number of mouse models has been developed, most of them overexpressing
wildtype or mutant APP, PSEN 1, PSEN 2 or tau protein or expressing two or
more of the gene combination in multiple transgenic mice (Sturchler-Pierrat et al.,
1997; Mineur et al., 2005). However, it is difficult to create a mouse model
imitating human AD pathology. Even the coexpression of Aβ and tau phenotype
does not allow to answer the questions why this pathology develops in the human
brain without overproduction of Aβ and tau as it is necessary in the mouse model
to create the pathology.
Introduction
8
The APP23 mouse overexpresses mutant APP with the Swedish double mutation
(Sturchler-Pierrat et al., 1997). This mutation results in an increased production
and secretion of Aβ due to increased β-secretase activity in the secretory pathway
in patients developing early onset AD (Haass et al., 1995). In APP23 mice this
double mutation is driven by a murine Thy-1 promoter which leads to an
increased, selective expression of APP in neuronal cells. Neuropathologically, Aβ
is highly overexpressed and mice present Aβ deposits from the age of 6 month in
neocortex and hippocampus. Aβ-deposits increase with age in size and number,
affecting following brain regions such as thalamus, olfactory nucleus and caudate
putamen. Other findings were neuron loss especially found in hippocampal region
CA1 (Calhoun et al., 1998), what is also seen in AD patients (West et al., 1994),
furthermore dystrophic neurites, hyperphosphorylated tau-protein, inflammatory
response and synapse loss. Also cerebral amyloid angiopathy was shown (Winkler
et al., 2001). In 2006 a retrograde DiI tracing study demonstrated that especially
layer III commissural neurons with highly ramified dendritic trees, i.e. type I
commissural neurons of the frontocentral neocortex (Tab. 1) were reduced in
number, these neurons also presented alterations in the dendritic tree (Capetillo-
Zarate et al., 2006).
Introduction
9
Table 1 : Types of commissural neurons in layer III of the frontocentral cortex
identified by DiI-tracing (Capetillo-Zarate et al., 2006)
Type I commissural
neurons
Pyramidal neurons with a highly ramified dendritic
tree showing multiple secondary and tertiary
branches
Type II commissural
neurons
Pyramidal neurons with a dendritic tree that
branches distant from the cell soma, secondary and
tertiary branches are usually not observed in 100µm
thick sections
Type III commissural
neurons
Non-pyramidal commissural neurons
Not only neuropathologically but also in behavioral tests APP23 mice showed
cognitive decline compared to wildtype littermates from the age of 3 months
onwards, preceeding amyloid plaque depositioning (Van Dam et al., 2003).
Because of these findings APP23 mice were considered to be a useful model to
analyze the contribution of APP and Aβ for the pathogenesis of AD (Sturchler-
Pierrat and Staufenbiel, 2000; Kuo et al., 2001). However, other authors presume
that this mouse model is a limited model of AD because only low tau
phosphorylation without NFT formation and low complement and microglial
response was seen compared to AD patients (Schwab et al., 2004). Therefore,
other transgenic mouse models some of which combine two or more mutations
were created in order to mimic AD pathology more exactly. Accordingly, PSEN1/2
and/or tau-protein mutations were combined with APP mutation. Here amyloid
pathology was combined with neuron loss described earlier and the generation of
NFTs (Lewis et al., 2001; Perez et al., 2005). In another 3x transgenic mouse
models (APP, PSEN1 and Tau transgenes) the mutations also led to these
pathologies but showed also intracellular τ accumulation (Oddo et al., 2003; Oddo
et al., 2006). Combining these features in a single mouse model made it an
interesting model in AD research. A problem in investigating AD pathology with
these multi-mutant mouse models is the interaction of the different proteins.
However, to clarify which protein leads to a specific pathology these models are
Introduction
10
suboptimal in comparison to single trangenic ones. Here, the APP23 mouse model
combines a single mutation and some of the typical AD pathology features.
The APP48 transgenic mouse model expresses intracellular Aβ42 and shows
intracellular Aβ lesions. Neurodegeneration is represented by the reduction of
hippocampal CA1 neurons and white matter reduction going along with an
impaired motor function in the Rotarod test (Abramowski et al., 2012b) In
comparison to the APP23 mice, APP48 mice do not show extracellular amyloid
plaques. In so doing, they can serve as an artificial model for intraneuronal Aβ
toxicity.
In so doing, the APP23 and APP48 mouse models are ideally suited to study the
influence of APP, intra- and extracellular Aβ on mitochondrial structure in vivo.
APP23 mice show intra- and extracellular Aβ pathology and an overexpression of
APP whereas intracellular Aβ is studied in APP48 mice. In contrast to other
transgenic mouse models these mouse models permit the analysis of Aβ effects
under distinct conditions without interference of a second transgenic manipulation
that could explain pathologies as well:
APP23 mice are used for the analysis of extra- and intraneuronal Aβ production by
APP cleavage.
APP48 mice are used for the analysis of APP independent intraneuronal Aβ
toxicity.
1.5 Aims of the study
To address the question whether 1. intra- or 2. extracellular Aβ leads to
mitochondrial and/or dendritic alterations and to identify the role of APP-derived
Aβ production for Aβ-induced mitochondrial and/or dendritic changes I studied the
mitochondrial morphology and distribution in neurons of the frontocentral cortex of
APP23 and APP48 transgenic mice in comparison to that of wildtype mice.
In detail my specific aim was to answer the following question:
1. does intracellular overexpression of Aβ independent from APP cleavage in
APP48 mice affect mitochondrial integrity and/or distribution in the cell and
dendritic morphology?
Introduction
11
2. does extracellular Aβ accumulation in APP23 mice affect intracellular
mitochondrial structure and/or distribution and/or dendritic morphology?
By addressing these questions I will be able to elucidate whether beta- and
gamma-secretase directed APP processing including Aβ formation or APP
independent Aβ formation leads to intra- and extracellular AD pathology. Although
the mouse models are artificial and can not be considered as good models for
human AD pathology, this study will lead to a better understanding of the cellular
and subcellular effects induced by Aβ in the brain under different conditions.
Material and Methods
12
2 Material and Methods
2.1 Material and Equipments used
Table 2: Buffer and Reagents
A. Tris-Buffer Saline (TBS), pH 7.4
Components Concentration/Amount Company Tris-HCl 20 mM Merck, Darmstadt, Germany NaCl 150 mM Merck, Darmstadt, Germany
ddH2O To 1 liter Millipore GmbH, Schwalbach, Germany
B. Phosphate buffer saline (PBS), pH 7.6
KCl 2.7 Mm Merck, Darmstadt, Germany KH2PO4 1.46 Mm Merck, Darmstadt, Germany NaCl 137 mM Merck, Darmstadt, Germany Na2HPO4.2H2O 8.1 mM Merck, Darmstadt, Germany
ddH2O To 1 liter Millipore GmbH, Schwalbach, Germany
Tween 0.05 % Bio-Rad, Hercules, CA, USA C. 2.6% Phosphate buffer paraformaldehyde solution (PFA), pH 7.6
PFA 2.6% Sigma, Taufkirchen, Germany PBS 0.2M, pH 7.6 500 ml See PBS solution
ddH2O 500 ml Millipore GmbH, Schwalbach, Germany
D. Reducing Solution (IHC)
Methanol 10% Merck, Darmstadt, Germany H2O2 30% Sigma, Taufkirchen, Germany in TBS, pH 7.6 0.05 M See TBS solution E. Blocking Solution (IHC)
DL-Lysine 0.1 M Sigma, Taufkirchen, Germany Triton-X 0.25% Sigma, Taufkirchen, Germany in BSA 10% Sigma, Taufkirchen, Germany F. Perfusion solution
Heparin 0,5% Roche, Mannheim, Germany In TBS 0,05 M pH 7,3
To 1 liter See TBS solution
Material and Methods
13
G. Tracing solution in PFA Iodocetic acid 0,8% Sigma, Taufkirchen, Germany Sodium periodate 0.8% Sigma, Taufkirchen, Germany DL-Lysine 0.1 M Sigma, Taufkirchen, Germany In PFA To 1 liter See PFA solution H. Other Reagents
3,3'-Diaminobenzidine (DAB) Merck, Darmstadt, Germany
Alcohol Sigma-Aldrich, Steinheim, Germany
Avidin-Biotin Complex Kit (ABC-Kit) Vectastain, Vector laboratories, Burlingame, CA. USA
Aβ42 ELISA plates ELISA from Innogenetics, Ghent, Belgium
BCA Protein Assay Bio-Rad, Hercules, CA, USA BSA (10%) Sigma, Taufkirchen, Germany BSAc Aurion, Wageningen, Netherlands
Carbocyanine DiI Molecular Probes, Eugene, OR, USA
cold washed fish gelatine (CWFG) BBInternational, Cardiff, UK
ECL detection system
Supersignal Pico Western system, ThermoScientific-Pierce, Waltham, MA, USA
ECL Hyperfilm GE Healthcare, Buckinghamshire, UK
Epon Sigma-Aldrich, Steinheim, Germany
Eukitt© Kindler, Freiburg, Germany Formic acid Applichem, Darmstadt, Germany Glutaraldehyd Plano, Wetzlar, Germany
Ketamin 25% Bela-Pharma GmbH, Vechta, Germany
lithium dodecyl sulfate (LDS) sample buffer Invitrogen, Carlsbad, CA, USA
LR-white London Resins Co. Ltd, Birkshire, England
Micropestle Eppendorf, Hamburg, Germany Na-Borhydrit Merck, Darmstadt, Germany NGS (normal goat serum) Aurion, Wageningen, Netherlands NuPAGE 4-12% Bis-Tris gel system Invitrogen, Carlsbad, CA, USA Osmium tetroxide Chempur, Karlsruhe, Germany
Ponceau S staining or β-actin Santa Cruz Biotechnology, CA, USA
Propanol Sigma-Aldrich, Steinheim, Germany
Propylenoxid Merck, Darmstadt, Germany protease and phosphatase inhibitor-cocktail (Complete and PhosphoSTOP)
Roche, Mannheim, Germany
synthetic Aβ1-42 Bachem, Bubendorf, Switzerland Uranyl acetate Merck, Darmstadt, Germany
Material and Methods
14
Xylazin 2% Riemser Arzneimttel AG, Greifswald, Germany
Table 3: List of Antibodies used for Immunoelectron microscopy
Primary antibody Antigen Source of primary antibody
4G8 Aβ17-24 Covance, Dedham, USA
MBC42 Aβ37-42 Gift of H. Yamaguchi, Gunma, Japan
GAM IgG Aurion, Wageningen, Netherlands IgG polyclonal goat,
MSIgG Biomeda, Foster City, CA, USA
6E10 anti-Aβ1-17 Covance, Dedham, USA
anti-AβN3pE AβN3pE IBL International GmbH, Hamburg, Germany
Phosphorylated Aβ (pAβ) Phosphorylated Aβ
Girft of J. Walter, Department of Neurology, University of Bonn, Bonn, Germany
Table 4: List of Equipments used
Table centrifuge
Mikro 200 Hettich Zentrifugen, Tuttlingen, Germany
vacuum centrifuge
Vacufuge Eppendorf, Hamburg, Germany
Magnetic Stirrer
MR Hei Standard Heidolph Instruments, Solingen, Germany
Microscopes Fluorescence Microscope Leica DMLB
Leica, Bensheim, Germany
Scanning Confocal Microscope Leica TSC NT
Leica, Bensheim, Germany
Electron microscope
JEM 1400 Jeol, Tokyo, Japan
EM400T 120KV Philips, Eindhoven, The Netherlands
EM 10 Zeiss, Oberkochen, Germany
pH Meter pH-meter 210 Hanna Intruments, Kehl am Rhein, Germany
Vortex VM 3000 Mini vortexer Henry Troemner LLC, NJ, USA Vibratome Leica VT 1000S Leica, Bensheim, Germany Grids for EM Plano, Wetzlar, Germany Diamont knive Diatomeknives Hatfield, PA, USA Embedding film
TED Pella Inc., Redding, CA, USA
Microtome Ultracut Reichert Jung, Depew, NY, USA
Material and Methods
15
Table 5: List of Softwares used
CorelDRAW Graphics Suite 12 CorelDRAW, Unterschleissheim, Germany
EndNote 8.0 Thomson ISI ResearchSoft, Philadelphia, PA, USA
ImageJ, Imaging Processing and Analysis Software
NIH, Bethesda, MD, USA
Leica FireCam Software Leica, Bersheim, Germany Leica TCS Software Leica, Bersheim, Germany
Open Office Apache Software Foundation, DE, USA
SPSS software Chicago, IL, USA Microsoft Office Microsoft, CA, USA
2.2 Mouse models
Table 6: Mouse models used
Model 3 month 15 - 18 month APP23 n = 12 n = 17 APP48 n = 12 n = 17 Wildtype n = 14 n = 20
APP23 and APP48 mice were generated as described previously (Sturchler-
Pierrat et al., 1997; Herzig et al., 2004; Abramowski et al., 2012b) and
continuously back-crossed to C57BL/6. An expression construct containing a
murine Thy-1 promoter was used to drive neuron-specific expression of human
mutant APP751 with the Swedish mutation 670/671 KM→NL in APP23 mice. In
APP48 mice an expression construct encoding a rat proenkephalin signal
sequence followed by Aβ1-42 driven by the neuron specific Thy-1 promoter was
used to drive neuron-specific expression of human wildtype Aβ1-42.
For this study female APP23 mice (3 months, n = 12; 15 months, n = 17) and
female and male APP48 mice (3 months, n = 12; 18 months, n = 17) were
analyzed. As control, respective female and male wildtype littermates of 3 (n = 14),
15 (n = 10), and 18 months (n = 10) were used (Rijal Upadhaya et al., 2013).
2.3 Tissue praparation and DiI tracing
The commissural neurons in the frontocentral cortex were stained using DiI as a
tracer. The dye is a lipophilic tracer and is absorbed through the cell membranes
being in contact to the dye and diffuses along the cell membrane labelling the cell
with all of its processes. In neurons this results in an antero- and retrograde
Material and Methods
16
tracing which leads to the staining of the complete cell including synapses and
dendrites. This dye allows precise Golgi-like tracing of neurons in postmortem
fixed tissue in a quality similar to in vivo tracing methods using rhodamine tracers
even in only weakly traced neurons (Galuske and Singer, 1996; Capetillo-Zarate et
al., 2006).
For DiI tracing the brains of 3 and 15-18-months-old APP23, APP48 and wildtype
mice were studied. Animals were treated in agreement with the German laws on
the use of laboratory animals. Mice were anesthetized. Perfusion was performed
transcardially with Tris-buffered saline (TBS) with heparin (pH 7.4) followed by the
injection of 0.1 M PBS (pH 7.4) containing 2.6% paraformaldehyde (PFA), 0.8%
iodoacetic acid, 0.8% sodium periodate and 0.1 M D-L lysine. The brains were
removed in total and post-fixed in 2.6% phosphate-buffered PFA (pH 7.4)
containing 0.8% iodoacetic acid, 0.8% sodium periodate and 0.1 M D-L lysine
(Galuske et al., 2000). Three days later a single crystal (~0.3 mm3) of the
carbocyanine dye DiI was implanted into the left frontocentral cortex, 1 mm
rostrally from the central sulcus, 2 mm laterally from the middle line and 1 mm
deep in the cortex as reported earlier (Capetillo-Zarate et al., 2006). After
incubation in 2.6% phosphate-buffered PFA for at least 3 months at 37°C, 100-µm
thick coronal vibratome sections were cut. All sections of a given mouse brain
were separately stored and continuously numbered. Sections were temporarily
mounted in TBS for microscopic analysis (Rijal Upadhaya et al., 2013).
2.4 Microscopic and quantitative analysis
In layer III of the frontocentral cortex of the right hemisphere, contralateral to the
implantation site of the tracer, the morphology of traced commissural neurons was
examined. The traced neurons were assigned to different types according to their
morphology (Capetillo-Zarate et al., 2006) (Tab. 1). Then the number of traced
commissural neurons of each type in wildtype mice was counted and compared
with that in APP23 and APP48 mice. For qualitative and quantitative analysis 10
consecutive sections (100-mm thickness each) representing a tissue block of 1
mm thickness were studied for each mouse. Analysis started at the anterior
commissure setting the caudal limit of the investigated tissue block. For each
coronal section, the medial boundary of the region investigated was set as the
vertical line at the cingulum that separated the cingulate cortex from secondary
Material and Methods
17
motor cortex (M2). The horizontal boundary was set as the horizontal line
separating the primary somatosensory cortex (SC1) from the insular cortex.
For the qualitative analysis a laser scanning confocal microscope was used.
Stacks of 2D images were superimposed digitally using the Image J Image
Processing and Analysis software, and 3D data sets were generated for the
visualization of neurons with their entire dendritic tree. For quantification, traced
neurons in layer III were counted in the region of interest in 10 consecutive
sections of the tissue block taken for qualitative and quantitative analysis using a
fluorescence microscope. In so doing, we analyzed a cortex volume of 5–6 mm³ in
each mouse. Mean and median values of the number of traced neurons were
calculated and compared between wildtype, APP23 and APP48 mice (Rijal
Upadhaya et al., 2013).
2.5 Immunohistochemistry
Immunohistochemistry was performed for the visualization of Aβ pathology as well
as dendritic morphology in APP48 and APP23 mice. After formic acid pretreatment
free-floating sections were incubated in goat anti-mouse immunoglobulin (IgG) to
block cross-reactions with intrinsic mouse IgG as previously described (Thal et al.,
2007). To detect Aβ-positive material the sections were stained with monoclonal
antibodies specifically detecting the C-terminus of Aβ42 (MBC42) (Yamaguchi et
al., 1998). In APP23 mice anti-Aβ17-24 (4G8) was used to stain Aβ-deposits
regardless of Aβ40 or Aβ42. C-terminus-specific MBC40 (Yamaguchi et al., 1998),
antibodies detecting exclusively the C-terminus of Aβ40 were used in APP23 mice
as well. N-terminal-truncated and pyroglutamate modified AβN3pE was detected
with anti-AβN3pE (Saido et al., 1995). Phosphorylation of serine 8 of Aβ was
detected with antibodies against phosphorylated Aβ (pAβ) (Kumar et al., 2011;
Kumar et al., 2013).
The primary antibodies were detected with a biotinylated secondary antibody and
the avidin-biotin-peroxidase complex (ABC complex), and visualized with
Diaminobenzidine (DAB) (Hsu et al., 1981). Sections were mounted in Eukitt©.
The immunostained sections were analyzed with a Leica DMLB fluorescence
microscope. Positive and negative controls were performed (Rijal Upadhaya et al.,
2013).
Material and Methods
18
2.6 Protein extraction from brain tissue
Protein extraction was carried out from female APP23 (n = 4), APP48 (n = 4), and
wildtype littermates (n = 4) mouse brains, aged 9–11 months. Mice of this age
were taken to demonstrate the differences in the biochemical distribution of Aβ in
APP23 and APP48 mice.
Fresh frozen forebrain (0.4 g) was homogenized in 2 ml of 0.32 M sucrose
dissolved in TBS containing a protease and phosphatase inhibitor-cocktail with
Micropestle followed by sonication. The homogenate was centrifuged for 30 min at
14.000 × g at 4°C. The supernatant (S1) with the soluble and dispersible fraction
not separated from one another was kept. The pellet (P1) containing the
membrane-associated and the insoluble, plaque-associated fraction was
resuspended in 2% sodium dodecyl sulfate (SDS).
Ultracentrifugation of the supernatant S1 at 175.000 × g was used to separate the
soluble, i.e. the supernatant after ultracentrifugation (S2), from the dispersible
fraction, i.e. the resulting pellet (P2). The pellet P2 with the dispersible fraction was
resuspended in TBS.
The SDS-resuspended pellet P1 was centrifuged at 14.000 × g. The supernatant
(S3) was kept as membrane-associated SDS-soluble fraction. The pellet (P3) that
remained was dissolved in 70% formic acid and dried in a vacuum centrifuge and
reconstituted in 100 µl of 2X lithium dodecyl sulfate (LDS) sample buffer followed
by heating at 70°C for 5 min. The resultant sample was considered as insoluble,
plaque-associated fraction (Mc Donald et al., 2010). The total protein amounts of
soluble, dispersible, and membrane-associated fractions were determined using
BCA Protein Assay (Rijal Upadhaya et al., 2013).
2.7 SDS-PAGE and Western blot analysis
For sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE,)
soluble (S2), dispersible (P2), membrane-associated (SDS-sobluble, S3), and
insoluble, plaque-associated (formic acid soluble, P3) fractions (50 µg total
protein) were electrophoretically resolved in a precast NuPAGE 4-12% Bis-Tris gel
system. The protein load was controlled either by Ponceau S staining or β-actin
immunoblotting. Aβ was detected by western blotting with anti-Aβ1-17. Blots were
developed with an ECL detection system and illuminated in ECL Hyperfilm (Rijal
Upadhaya et al., 2013).
Material and Methods
19
2.8 Aβ Enzyme Linked Immunosorbent Assay (ELISA)
For analysis of Aβ by ELISA, forebrain homogenates from APP23 and APP48
mice of each age group (2-3 months: n = 6 (APP23), 6 (APP48); 15-18 months: n
= 7 (APP23), (8 APP48)) were homogenized, centrifuged and loaded on sandwich
ELISA plates for quantification of Aβ peptides as previously described (Capetillo-
Zarate et al., 2006). Standard curves were prepared with synthetic Aβ1-42 and
diluted in extracts of non-transgenic mouse forebrain prepared in parallel as
described above. Each sample was analyzed in duplicate (Rijal Upadhaya et al.,
2013).
2.9 Stereology
Six APP23, six APP48, and six wildtype mice at the age of 3 and 15-18-months,
respectively, were chosen randomly for stereology. One brain section of the
frontocentral cortex already quantified for the number of DiI-traced neurons was
selected by chance and stained with aldehyde fuchsin-Darrow red. Quantification
of neurons was performed according to the principles of unbiased stereology
(Schmitz and Hof, 2000). The frontocentral cortex volume was defined as the
volume of the subfields M2, primary motor cortex (M1), SC1 starting at the level of
the anterior commissure as described previously (Capetillo-Zarate et al., 2006).
The CA1 volume was measured in serial 100µm thick sections of the entire mouse
brain at 5x magnification. Neurons were counted in three different, randomly
chosen microscopic fields (40 x magnification) of an aldehyde fuchsin-Darrow red
stained section of the frontocentral cortex and CA1, respectively. For optical
dissection, stacks of 10 images in 2 µm focus distance were generated for each
microscopic field. Only those neurons having nuclei with dark and round nucleoli
visible in the center of soma in one of the stack-images were considered for
quantification using the ImageJ software. The number of neurons in the
frontocentral cortex and CA1 was calculated on the basis of the respective
reference volumes and neuron densities (Rijal Upadhaya et al., 2013).
2.10 Electron microscopy, immuno electron microsco py
100 µm thick vibratome sections of the frontocentral cortex and of the
hippocampus from six wildtype, six APP23 and six APP48 mice, aged 3 and 15-18
month respectively, were flat-embedded in Epon. A second vibratom section from
Material and Methods
20
each animal and region was flat embedded in LR-White-Resin. A part of the
frontocentral cortex covering all six cortical layers was dissected under
microscopic control and pasted on Epon blocks with a drop of Epon. Likewise, a
part of CA1 subfield of the hippocampus with adjacent stratum oriens and
radiatum was cut and pasted on a second Epon block. Ultrathin sections were cut
at 70 nm. Epon sections were block stained with uranyl acetate and lead citrate,
and viewed with a Philips EM400T 120KV, a Zeiss EM10, or a JEM-1400 electron
microscope. LR-White sections were immunostained with anti-Aβ42 (MBC42) and
anti-Aβ1-17 (6E10) antibodies and visualized with anti-mouse secondary antibodies
labeled with 10 nm nanogold particles. Digital pictures were taken (Rijal Upadhaya
et al., 2013).
2.10.1 Semiquantitative analysis of synapse densiti es
Digital pictures from Epon embedded sections were taken from 20 soma- and
plaque-free neuropil areas located in layers II-VI at 4600-times magnification. The
numbers of the symmetric and asymmetric synapses were counted and the length
of the synapses was determined with the ImageJ software. The synaptic density
was determined separately for symmetric and asymmetric synapses according to
DeFelipe et al. (DeFelipe et al., 1999) (synaptic density = Number of synapse-
profiles in a given area/length of synaptic profiles). These semiquantitative data
were used to compare the synaptic densities between the different mouse lines.
Asymmetric and symmetric synapses were distinguished according to published
criteria (Colonnier, 1968; Miranda et al., 2009).
Synaptic densities in the CA1 regions were measured in 10 randomly taken
pictures of the stratum oriens and in 10 randomly taken pictures of the stratum
radiatum at 4600-times magnification (Rijal Upadhaya et al., 2013).
2.10.2 Semiquantitative analysis of dystrophic dend rites
The frequency of dystrophic dendrites was observed by counting the number of
dystrophic neurites in the 20 pictures taken for the determination of the synapse
densities. The criteria for the identification of dystrophic dendrites at the
ultrastructural level were: neurite profiles with a disorganized cytoplasm,
occurrence of multilamellar, whirl-like structures in the absence of ultrastructurally
intact cell organelles in the area of the lesion, and an enlarged size compared with
neighboring neuritic profiles (Fig. 1) (Rijal Upadhaya et al., 2012). This number
Material and Methods
21
was determined in six APP23, six APP48 and six wildtype mice and used as a
semiquantitative score for structural dendritic alterations (Rijal Upadhaya et al.,
2013).
Fig. 1 Identification of dystrophic neurites. Electron microscopy was used to identify dystrophic neurites (arrows ) as previously described (Rijal Upadhaya et al., 2012) and shown here in the frontocentral cortex of 15-month-old APP23 mice. Such neurites are characterized by neuritic swelling and contain vesicles with electron dense bodies (black arrowheads ) probably representing autophagic vacuoles. Mitochondria (M) in these neurites appear morphologically intact. Few multivesicular bodies are seen in these neurites as well (white arrowhead ). The calibration bar corresponds to: 250 nm (Rijal Upadhaya et al., 2013).
2.10.3 Analysis of mitochondria
To clarify whether APP-independant production of intraneuronal Aβ or APP-
derived intra- and extracellular Aβ accumulation are critical for mitochondrial
changes in neurons, mitochondrial alterations in frontocentral and CA1 neurons of
six APP23, six APP48 and six wildtype mice were compared at the electron-
microscopic level. For this purpose I compared the area profiles from neuritic and
somatic neuronal mitochondria as well as from the respective somata and
Material and Methods
22
peripheral neurites in plaque-free areas. Mitochondria in peripheral dendrites and
axons were analyzed in the 20 pictures taken from soma- and plaque-free areas of
the frontocentral cortex and in 20 pictures of the stratum oriens and radiatum of
the CA1 hippocampal subfield also used for the assessment of synapse densities.
The mitochondria in neuronal somata were studied in 40 pictures from 10 different
randomly taken of layer II – layer VI neurons of the frontocentral cortex and in 40
pictures from 10 randomly taken CA1 neurons with a Philips EM400T 120 KV
electron microscope at 6000-times magnification (4 pictures per neuron) in each
individual mouse. The area profiles from morphologically intact mitochondria and
from those with an altered ultrastructure, i.e. degeneration of christae as
previously described in prion disease (Siskova et al., 2010), were separately
obtained for somatic and peripheral neuritic mitochondria. Volume densities in
percent of soma and neurite profiles were calculated according to the criteria for
unbiased stereology (Weibel, 1969) following the determinations provided in (Tab.
7).
Those mitochondria which exhibited th typical ultrastructural pattern with outer and
inner membranes as well as christa membranes and altered mitochondria with
clear structural changes of the christa membranes like rarefication, loss, abnormal
structures were considered for quantification (Fig. 2). Assessments were
performed without previous knowledge of the genotypes of the animals.
Two APP23, two APP48, and two wildtype mice at the age of 15-18-months were
chosen randomly for immunoelectron microscopy analysis of Aβ deposition in
nerve cell somata and soma-free neuropil. LR-White sections were immunostained
with anti-Aβ42 (MBC42) antibodies and visualized with anti-mouse secondary
antibodies labelled with 15 nm nanogold particels. Digital pictures were taken with
a JEM 1400 electron microscope and a Zeiss EM 10 from 20 soma-free neuropil
areas located in layers II-VI and of 10 neuron somata at various magnification
levels. The different Aβ-deposition characteristics seen as the 15 nm gold particels
in the neurite, soma or mitochondria were compared to relate them with
stereological findings (Rijal Upadhaya et al., 2013).
Material and Methods
23
Fig. 2: Electromicroscopical images for several steps of the assesment of stereological data of neuronal mitochondria in the frontocentral cortex of an APP48 mouse. A, various cell compartements are shown, nucleus (N), mitochondria (M), rough endoplasmic reticulum (RER), axon (Ax ). B, mitochondria measured and labelled black. C, alterated mnitochondria labelled red, normal mitochondria labelled black. D, intracellular, perinuclear area labelled in black. Pictures were taken with a Philips EM400T 120KV at 6000 times magnification.
2.11 Statistical analysis
SPSS 19.0 (SPSS, Chicago, IL, USA) software was used to calculate statistical
tests. Non-parametric tests were used to compare wild type, APP23, and APP48
mice. p-values were corrected for multiple testing using the Bonferroni method.
Parametric data were analyzed by ANOVA with subsequent Games-Howell post-
hoc test to correct for multiple testing or using the Welch test. The results of the
statistical analysis are summarized in Supplementary Tab. 1 (Rijal Upadhaya et
al., 2013).
Material and Methods
24
Table 7 : Determinations of the parameters employed for quantification of mitochondrial alterations
in neurites and nerve cell somata (Rijal Upadhaya et al., 2013)
Percentage of altered mitochondria in nerve cell somata =
∑ altered mitochondrial area within nerve cell somata
∑ complete mitochondrial area within nerve cell somatax100
Percentage of altered mitochondria in neurites (axons and dendrites) =
∑ altered mitochondrial area within neurites
∑ complete mitochondrial area within neuritesx 100
Mitochondrial volume density in the nerve cell somata =
∑ complete mitochondrial area within nerve cell somata
∑ area of nerve cell somatax100
Mitochondrial volume density in neurites =
∑ complete area of mitochondria within neurites
∑ area of neuritesx100
Volume density of altered mitochondria in the nerve cell somata =
∑ altered mitochondrial area within nerve cell somata
∑ area of nerve cell somatax100
Volume density of altered mitochondria in neurites =
∑ altered mitochondrial area within neurites
∑ area of neuritesx 100
Results
25
3 Results
3.1 Different patterns of A β-pathology in APP23 and APP48 mice
As previously published, 15 month-old APP23 mice exhibited a high number of
extracellular Aβ-plaques in the cerebral cortex (Fig. 3a – indicated by arrows) as
well as cerebral amyloid angiopathy as previously described in male and female
animals (Sturchler-Pierrat and Staufenbiel, 2000). Intracellular Aβ42 detectable
with MBC42 was not abundant at the light microscopic level in this region neither
in neurons nor in glial cells. MBC40-positive Aβ40 was observed in the perikarya of
pyramidal neurons. At 3 month of age APP23 mice did not exhibit Aβ plaques or
vascular Aβ deposits as previously described in male and female animals
(Abramowski et al., 2012a; Rijal Upadhaya et al., 2013). APP48 mice, on the other
hand, did not show Aβ plaques but intracellular accumulation of Aβ in dendritic
threads, somatic granules in neurons and in microglial Aβ-grains at 3 and 18
months of age (Fig. 3b). This pathology was seen in male and female animals
(Abramowski et al., 2012a).
Modified Aβ such as AβN3pE was detected in a large number of plaques in 15-
month-old APP23 mice (Figure 3c). In APP48 mice only few dendritic threads
exhibited AβN3pE at 3 months of age (Figure 3d) whereas at 18 months of age a
significant number of AβN3pE-positive inclusions was observed as shown previously
(Abramowski et al., 2012a). pAβ in APP23 mice was detected in plaques of 15
months old APP23 mice (Figure 3e). Intraneuronal pAβ in APP23 mice was
apparent as previously reported in APP-PS1 transgenic animals (Kumar et al.,
2013). Only single pAβ-positive threads were stained in 3-month-old APP48 mice
(Figure 3f) whereas a few more pAβ-positive threads, grains and somatic granules
were observed at 18 months of age (Rijal Upadhaya et al., 2013).
Results
26
Fig. 3 Amyloid beta protein (Aβ) -pathology in 15-month-old APP23 (a, c, e) and 3-month-old-APP48 mice (b, d, f). a: The APP23 mouse showed a high number of extracellular Aβ plaques detectable with an antibody raised against Aβ17-24 (arrows ). Intracellular Aβ was negligible. b: In the 3-month-old APP48 mouse no extracellular Aβ -pathology was apparent. These animals showed intraneuronal dendritic threads (arrowheads) and somatic granules (lucent arrow ) as well as intramicroglial Aβ–grains (arrows ) detectable with anti-Aβ17-24 as previously published (Abramowski et al., 2012a). c: Amyloid plaques in APP23 mice did also contain N-terminal truncated and pyroglutamate modified AβN3pE (arrows ). d: AβN3pE was also found in even 3-month-old APP48 mice in some neuritic threads (arrowheads ). e: phosphorylated Aβ (pAβ) was detected in amyloid plaques in 15-month-old APP23 mice. f: In 3-month-old APP48 mice only single threads showed labeling with anti-pAβ . Calibration bar in b corresponds to: a, b = 30 μm; c = 80 μm; e = 60 μm; d, f = 20 μm (Rijal Upadhaya et al., 2013).
Biochemical analysis revealed that 3-month-old APP48 mice contained ~70 times
more total Aβ42 detected by ELISA than APP23 mice whereas at 15–18 months of
Results
27
age APP23 mice contained Aβ42 in a concentration ~17 fold higher than in APP48
mice (Figure 4a, Supplementary Tab. 1a) (Rijal Upadhaya et al., 2013).
Fig. 4 Biochemical analysis of Amyloid beta protein (Aβ) in APP23 and APP48 mice. a: Total Aβ42 levels detected by ELISA in forebrain hemispheres of 2–3 and 15-18-month-old APP23 and APP48 mice. At 2–3 months APP23 mice exhibited low amounts of Aβ42 whereas APP48 mice displayed significantly more Aβ42 in the brain. At 15–18 months APP48 mice showed more Aβ than at 2–3 months of age but APP23 mice exhibited several times more Aβ in the forebrain. b: For demonstration of the types of Aβ aggregates in APP23 and APP48 mice brain homogenates of 9-11-month-old animals were analyzed by SDS-PAGE and western blotting after preparation of the soluble, dispersible, membrane-associated and insoluble (plaque-associated) fraction. Soluble Aβ as detected with antibodies raised against Aβ1-17 (6E10) was restricted to APP23 mice. Dispersible, membrane-associated, and insoluble (plaque-associated, formic acid soluble) Aβ aggregates were found in both transgenic mouse lines. The Aβ detected in the insoluble fraction of the forebrain homogenates of APP48 mice represents Aβ aggregates that require formic acid pretreatment before analysis similar to plaque-associated Aβ in APP23 mice. Since APP48 mice did not develop Aβ plaques this insoluble Aβ presumably represented intracellular fibrillar aggregates, such as dendritic threads. Wildtype controls did not exhibit detectable amounts of Aβ in all four fractions. The original western blots are depicted in Supplementary Fig. 1 (ELISA data from APP23 mice were previously published in a different context (Abramowski et al., 2012a). ***p < 0.001 Welch-test (Rijal Upadhaya et al., 2013).
Results
28
To document the distribution of Aβ aggregates brain homogenates of 9-11-month-
old APP23 and APP48 mice for Aβ in the soluble (S2), dispersible (P2),
membrane-associated (S3) and insoluble fraction (P3) were analyzed. APP23
mice exhibited soluble, dispersible, membrane-associated and insoluble, plaque-
associated Aβ (Figure 4b) as reported previously in detail (Rijal Upadhaya et al.,
2012). In contrast, APP48 mice only exhibited dispersible, membrane-associated
and insoluble, aggregated Aβ whereas soluble Aβ was not detectable (Figure 4b)
(Rijal Upadhaya et al., 2013).
3.2 Degeneration of neurites and asymetric synapses in APP23
but not in APP48 mice
Using retrograde tracing with DiI three types of commissural neurons were
subclassified as previously published (Capetillo-Zarate et al., 2006) in APP23,
APP48, and wildtype mice (Tab. 1). Type I and type II commissural neurons
exhibited alterations in the dendritic tree as well as a decrease in number in
APP23 mice compared to wildtype littermates as previously reported (Capetillo-
Zarate et al., 2006) (Fig. 5). Type III commissural neurons did not exhibit
differences in their morphological appearance among APP48, APP23, and
wildtype littermates. There were no significant differences in the numbers of type I,
II, and III commissural neurons in APP48 mice compared to the respective
wildtype littermates (Fig. 5 c-i, Supplementary Tab. 1). Thus, 15 month-old APP23
mice exhibited dendritic degeneration of commissural neurons whereas APP48
mice did not (Rijal Upadhaya et al., 2013).
Results
29
Fig. 5 Dendritic degeneration in frontocentral commissural neurons of APP23 and APP48 mice. a: A type I neuron in an 18 month-old wildtype animal exhibits a symmetric dendritic tree with prominent secondary and tertiary branches. b: In contrast, the dendritic tree of a representative type I commissural neuron (I) in a 15-month-old APP23 mouse is degenerated. Most basal dendrites were shrunken and had a reduced caliber (arrows ). The degenerated dendrites showed some branches (arrows ) that distinguished the degenerated type I neuron (I) from type II neurons without ramifications near the soma (II). c: Such a degeneration of the dendritic tree was not seen in APP48 mice. d-f : Numbers of DiI-traced type I, type II and type III commissural neurons in 15-18-month-old mice. d: APP23 mice at 15 months of age showed a decrease by more than 50% of the type I commissural neurons compared with 18-month-old wild type and APP48 mice. e: There was a significant reduction of type II commissural neurons in APP23 mice at 15 months of age compared with wild type littermates and APP48 mice at 18 months of age. f: Although APP23 mice had higher numbers of type III commissural neurons there was no significant difference from wild type littermates. g-h : No significant differences among the frequencies of DiI-traced type I, type II, and type III commissural neurons were observed at 3 months of age. ** p < 0.01 (Further statistical analysis: Supplementary Tab. 1). Means and standard errors are depicted in d-i. (Quantitative data from APP23 mice and their respective wild type littermates were previously published in a different context (Abramowski et al., 2012a; Rijal Upadhaya et al., 2013). Calibration bar in c corresponds to: a-c = 30 μ m. To confirm neuritic degeneration transmission electron microscopy was used to
compare the presence of dystrophic neurites among APP23, APP48 and wildtype
mice. The frequency of dystrophic neurites was higher in the frontocentral cortex
of 15 month-old APP23 mice when compared to 15-18 month-old APP48 and
Results
30
wildtype mice (Fig. 6, Supplementary Tab. 1c). There were no differences in the
frequency of dystrophic neurites between APP48 and wildtype mice or between 3
month-old animals of each genotype (Fig. 6) (Rijal Upadhaya et al., 2013).
Fig. 6 Frequencies of dystrophic neurites in wild type, APP23, and APP48 mice. The semiquantitatively assessed frequency of dystrophic neurites in the soma- and plaque-free frontocentral neuropil at the electron microscopic level was higher in 15-month-old APP23 mice than in wild type and APP48 mice of the same age group. In APP48 mice there was no increase in the frequency of dystrophic neurites in comparison to wild type mice. 3-month-old mice did not exhibit significant differences in the frequency of dystrophic neurites among the 3 genotypes nor were differences found in neuropil of the stratum radiatum and oriens of the CA1 region. (Data from APP23 mice and their respective wild type littermates were previously published in a different context (Rijal Upadhaya et al., 2012). *p < 0.05 (Further statistical analysis: Supplementary Tab. 1). Means and standard errors are depicted (Rijal Upadhaya et al., 2013). Qualitative changes in synapse morphology other than the generation of
dystrophic neurites as in 15 month-old APP23 mice were not observed.
Semiquantitative analysis of the densities of symmetric and asymmetric synapses
showed a reduction of the density of asymmetric synapses in the frontocentral
cortex of 3 and 15 month-oldAPP23 mice in comparison to wildtype mice. In the
stratum radiatum and oriens of CA1 a similar trend was observed but did not reach
significance. Such a reduction of asymmetric synapses was not observed in
APP48 mice in comparison to wildtype littermates (Fig. 7a). There were no
significant differences in the numbers of symmetric synapses among APP23,
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31
APP48, and WT mice (Fig. 7b, Supplementary Tab. 1d) (Rijal Upadhaya et al.,
2013).
Figure 7 Synapse densities in wild type, APP23 and APP48 mic e. a: Loss of asymmetric synapses in the frontocentral cortex of 3- and 15-month-old APP23 mice in comparison to wild type mice. 18-month-old APP48 and wild type mice did not differ significantly in the density of asymmetric synapses. At 3 months of age APP48 mice had even more asymmetric synapses than wild type animals. In CA1 there were also slightly less asymmetric synapses in APP23 mice than in wild type controls and APP48 mice. However, these differences were not significant. b: There were no significant differences in the number of symmetric synapses in the frontocentral cortex and in CA1 in 3- and 15-18-month-old animals. c: APP23 and APP48 mice of both age groups exhibited reduced numbers of CA1 neurons compared to wild type mice whereby CA1 neuron loss was most pronounced in APP23 mice. d: The number of neurons in the frontocentral cortex did not vary significantly among 15-18-month-old wild type, APP23, and APP48 mice. Therefore, younger animals were not studied for the number of neurons in the frontocentral cortex. *p < 0.05, **p < 0.01, ***p < 0.001 (Further statistical analysis: Supplementary Tab. 1). Means and standard errors are depicted. (Some data were previously published in a different context (Abramowski et al., 2012a; Rijal Upadhaya et al., 2012; Rijal Upadhaya et al., 2013). The number of asymmetric synapses increased with age in the frontocentral
neocortex of wild type, APP23, and APP48 mice (Figure 7a, Supplementary Tab.
1d). Such an increase in the number of asymmetric synapses with age was not
seen in the stratum radiatum and oriens of CA1 (Figure 7a, Supplementary Tab.
1d). The number of symmetric synapses did not differ between 3 and 15-18-
month-old mice of each genotype (Figure 7b, Supplementary Tab. 1d)(Rijal
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32
Upadhaya et al., 2013).
Immunoelectron microscopy showed Aβ within dendrites of 15-18 month-old
APP23 and APP48 mice. In 15 month-old APP23 mice extracellular Aβ plaques
contained fibrillar Aβ that could easily be labelled with Anti-Aβ1-17 (Fig.8a, b).
Plaque-associated dystrophic neurites were seen in the middle of bundles of
extracellular Aβ fibrils. No fibrillar Aβ was found within neurites of APP23 mice.
However, intracellular Aβ was detected in a few of these dystrophic neurites near
the membrane in electron dense spherical particles, which may represent non-
fibrillar Aβ oligomers or protofibrils (Figure 8c-e). In APP48 mice fibrillar Aβ
aggregates presumably representing the ultrastructural correlate of dendritic
threads were found in the dendrites as seen morphologically in Epon-embedded
tissue. These dendrites were not enlarged (Figure 8f). Immunoelectron microscopy
with anti-Aβ1-17 indicated that the fibrillar structures identified in the Epon-
embedded sections contain Aβ (Figure 8g) (Abramowski et al., 2012a). Organelles
near dendritic threads in APP48 mice, thereby, did not differ from that elsewhere in
APP48 mouse neurons as demonstrated for a mitochondrium in Figure 8g (m)
(Rijal Upadhaya et al., 2013).
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33
Fig. 8 Electron microscopy and immunogold labeling of Amyloid beta protein (Aβ) in APP23 and APP48 mice. a, b: Immunogold particles specifically labeled fibrillar Aβ (arrowheads ) of a plaque in a 15-month-old APP23 mouse. At high magnification small amyloid fibrils were identified (arrowheads in b ). They were located in the extracellular space. c, d: Dystrophic neurites (outlined structures ) were associated with extracellular bundles of plaque-associated Aβ fibrils (arrowheads ) in an 15-month-old APP23 mouse. Within the neurite, Aβ was localized in electron
Results
34
dense material near the surface as well as in the center of the neurite (arrows in c ). d: A second dendrite without signs of dystrophy such as multilamellar bodies was also located near extracellular Aβ fibrils (outlined structure labeled with e ). e: Higher magnification of this dendrite showed a dendrite cross section with an intact mitochondrium (m) and with condensed Aβ–positive material in the cytoplasm (arrows ). Similar Aβ -positive material was found in the neighboring extracellular space (arrowhead ). Both, intra- and extracellular Aβ aggregates did not exhibit fibrillar morphology. As such it is quite likely that these Aβ aggregates represent non-fibrillar oligomers and/or protofibrils occurring in the neighborhood of extracellular, plaque-associated Aβ fibrils. f: Fibrillar material (arrows ) was observed in some dendrites of a 3-month-old APP48 mouse in an Epon-embedded, not immunostained section presumably representing the ultrastructural correlative for dendritic threads. g: Immunoelectron microscopy confirmed Aβ –positive material in fibrillar aggregates within dendritic threads labeled by gold particles (arrows ) in APP48 mice. No Aβ was observed in the neighboring, non-altered mitochondrium (m). Calibration bar in g is valid for: a = 570 nm, b = 200 nm, c = 750 nm, d = 1000 nm, e = 275 nm, f, g = 350 nm (Rijal Upadhaya et al., 2013).
3.3 Neuron loss in the CA1 subfield but not in the frontocentral
cortex of APP48 and APP23 mice
The number of CA1 neurons was lower in 3 and 18 month-old APP48 mice
compared to wildtype animals indicating CA1 neuron loss in APP48 mice
(Abramowski et al., 2012a). A decrease in the number of CA1 neurons was also
observed in 3 and 15-18 month-old APP23 mice in comparison to wildtype animals
(Fig. 7c, Supplementary Tab. 1e) (Rijal Upadhaya et al., 2012).
In contrast, the number of neurons in the frontocentral cortex of 15-18 month-old
APP23 and APP48 mice was not significantly different from that in wildtype mice
(Fig. 7d, Supplementary Tab. 1e) (Abramowski et al., 2012a). Therefore, 3 month-
old animals were not analyzed for the numbers of frontocentral neurons (Rijal
Upadhaya et al., 2013).
3.4 Increased mitochondrial alterations in APP48 in neuronal
somata of APP48 but not in APP23
The analysis of mitochondrial alterations in neurites and the somata of
frontocentral neurons showed differences between 15-18 month-old wildtype,
APP23, and APP48 mice (Fig. 9 a-f). Increased percentages and volume densities
of altered mitochondria with destruction and rarefaction of the christa membranes
as depicted in Figure 9c were observed in somata of neurons from APP48 mice in
contrast to predominantly ultrastructually intact mitochondria in wildtype and
APP23 mice (Figure 9 a, b, d, e, Supplementary Tab. 1 f, g). However, few altered
mitochondria were also observed in wildtype and APP23 mice. Such an increase
in the percentage and volume density of altered mitochondria in APP48 mice was
Results
35
not observed in the hippocampal subfield CA1 and in the frontocentral neocortex
of 3-month-old animals (Figure 9 d, e, g, h, Supplementary Tab. 1 f, g). Neurites
studied distant from nerve cell somata exhibited a small number of altered
mitochondria in all mice but did not show differences in the percentage and
volume densities of altered mitochondria among the three mouse lines at both
ages and locations Supplementary Tab. 1i, j, Supplementary Tab. 1a-c). The
volume densities of somatic and neuritic mitochondria in general, i.e. unaltered
and altered mitochondria together, did not significantly differ in APP23, APP48 and
wild type mice (Figure 9 f, i, Supplementary Tab. 1h, k, Supplementary Tab. 1c, f).
In the neuronal somata, the percentages and volume densities of altered
mitochondria in frontocentral and CA1 neurons increased with age (Figure 9 d, e,
g, h, Supplementary Tab. 1 f, g). The volume densities of all, altered and healthy-
looking mitochondria increased in APP23 and APP48 mice with age whereas in
wildtype animals such an increase was not observed (Figure 9 f, i, Supplementary
Tab. 1h).
In neuritic processes, an increase or at least an increasing trend with age in the
percentages and volume densities of altered mitochondria was observed in the
frontocentral cortex of APP23, APP48 and wildtype mice (Supplementary Tab. 1 k,
Supplementary Tab. 1 a, b). In the stratum radiatum and oriens neurites of CA1,
the percentages and volume densities of altered mitochondria in 15-month-old
APP23 mice were lower than in wildtype mice whereas no differences were
observed between 3-month-old APP23 and wildtype mice as well as between
APP48 mice of any age and wildtype mice (Supplementary Tab. 1 k,
Supplementary Tab. 1 d, e). In neurites, the volume densities of all, healthy-
looking and altered mitochondria did not increase with age (Supplementary Tab. 1
c, f, k) (Rijal Upadhaya et al., 2013).
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36
Figure 9 Electron microscopy of mitochondria in wil d type, APP23, and APP48 mice. a-b: Electron microscopy showed predominantly non-altered mitochondria in nerve cell somata of wildtype (WT) (a) and APP23 mice (b). c: More altered mitochondria in the nerve cell somata were observed in frontocentral neurons of 18-month-old APP48 mice. Mitochondrial alteration was characterized by a loss of mitochondrial christae although the double membrane architecture and at least single christa structures (arrow ) were preserved. d-f : The percentage of altered mitochondria in the nerve cell somata of 18-month-old APP48 mice was higher than in 15-18-month-old wild type and APP23 mice (d). The volume density of altered mitochondria in the frontocentral nerve cell somata of 18-month-old APP48 mice was increased in comparison to 15-18-month-old wild type and APP23 mice (e). At 3 months of age such differences in the presence of altered mitochondria were not observed. The total mitochondrial volume density, i.e. altered and non-altered mitochondria together, did not differ among the investigated mouse lines in both age groups (f). g-i : In CA1 there were no obvious changes in the percentage and volume density of altered mitochondria in the nerve cell somata. *p < 0.05, **p < 0.01 (Further statistical analysis: Supplementary Tab. 1). Means and standard errors are depicted in d-f. Calibration bar in c is valid for: a-c = 150 nm (Rijal Upadhaya et al., 2013).
At the immuno electron microscopic level Aβ was detected in lipofuscin granules
or in association with other cytoplasmic material in neurons of APP23 (Figure 8 c-
e, Figure 10 a, b) and APP48 mice as previously reported (Huang et al., 2006;
Results
37
Abramowski et al., 2012a; Rijal Upadhaya et al., 2012) with or without
mitochondrial alterations. Even neurons of wildtype mice without detectable Aβ
contained single altered mitochondria. In 15-month-old APP23 mice Aβ was seen
only in few mitochondria (Figure 10 c) whereas most somatic and neuritic
mitochondria did not contain Aβ-positive material (Figure 10 b). In contrast, altered
and non-altered mitochondria labeled for Aβ showing goldparticles in association
with mitochondrial membranes were often found in the nerve cell somata of 18-
month-old APP48 mice (Figure 10d, e) (Rijal Upadhaya et al., 2013).
Results
38
Figure 10 Immunoelectron microscopy of mitochondria in wild type, APP23, and APP48 mice. a : Immunoelectron microscopy revealed gold-labeled Amyloid beta protein (Aβ) (arrows ) within lipofuscin-like granules in the cytoplasm of frontocentral pyramidal neurons in 15-month-old APP23 mice. b. Most mitochondria in the somata of frontocentral pyramidal neurons in 15-month-old APP23 mice did not contain immunogold labeled Aβ–positive material (arrowheads ). c: Only few neuronal mitochondria exhibited single gold particles in a 15-month-old APP23 mouse indicating anti-Aβ-positive material within these mitochondria (arrow ). d: In a few mitochondria within frontocentral pyramidal nerve cell somata of 18-month-old APP48 mice we found immunogold labeled Aβ -positive material associated with the membranes of healthy-looking mitochondria (arrow ). Neighboring non-altered mitochondria often did not contain Aβ (arrowheads ). Aβ fibrils were not seen inside the mitochondria. e: Altered mitochondria within pyramidal neurons in the frontocentral cortex of a 18-month-old APP48 mouse also exhibited single gold particles in association with their membranes indicating the presence of Aβ (arrows ) although Aβ fibrils were not observed inside the mitochondria. Due to the use of LR-white embedded tissue required for post-embedding immunoelectron microscopy (a,b) the tissue preservation was less good than in the Epon embedded sections used for the morphological analysis of the mitochondria (Figure 8a-c). Calibration bar in e is valid for: a, b = 540 nm, c = 325 nm, d = 288 nm, e = 180 nm (Rijal Upadhaya et al., 2013).
Discussion
39
4 Discussion Here we employed two different mouse models for Aβ pathology to clarify
mechanisms of Aβ-related neurodegeneration. In APP48 mice, where exclusively
intracellular Aβ is exhibited, increased numbers of mitochondria exhibiting
alterations in frontocentral pyramidal cells and neuron loss in CA1 neurons were
found. Synaptic and dendritic degeneration was not seen in APP48 in contrast to
APP23 mice. The latter mouse model overexpresses human mutant APP and
shows extra- and intracellular Aβ pathology and neurodegeneration. Here
mitochondrial alterations did not exceed the levels seen in wildtype animals. These
results lead to the suggestion that different mechanisms are causative for neuron
loss in the two AD mouse models. The following paragraphs will discuss causes
and consequences of Aβ accumulation in the brain of the described mouse models
as well as its significance for the AD pathology.
APP23 and APP48 mice differ considerably with respect to the mechanism of
transgenic, human Aβ generation. Cleavage of Aβ from APP with the Swedish
mutation as in APP23 mice occurs after APP internalization from the membrane in
the early endosomal compartment (Rajendran et al., 2006; Rajendran and
Annaert, 2012). Once generated Aβ is rapidly secreted to a large extent. In APP48
mice, on the other hand, expression of Aβ42 with a cleaved signal sequence
targets the released Aβ to the endoplasmic reticulum. Intracellular accumulation
occurs in neurites and lysosomes whereas only very little Aβ42 is secreted into the
extracellular space (Abramowski et al., 2012a). APP48 mice lack human APP and
its metabolites except for Aβ42 whereas APP23 mice produce more Aβ40 than Aβ42
and, in addition to Aβ, N- and C-terminal fragments of APP. A transgenic mouse
expressing only Aβ40 with a similar construct as used in APP48 mice for Aβ42 did
not show Aβ aggregation and neuronal degeneration (Abramowski et al., 2012a).
In double transgenic animals expressing both Aβ42 and Aβ40 constructs a similar
pattern of pathological lesions was observed as in APP48 mice (Abramowski et
al., 2012a) indicating that Aβ40 has only a marginal effect in these animals.
Both, APP23 and APP48 mice exhibited intracellular Aβ in the lysosomal
compartment and in mitochondria whereas early endosomal Aβ was not seen in
APP48 mice. The distribution of the transgene mRNA in the neocortex and the
hippocampus as well as the expression levels were quite similar in APP23 and
APP48 mice (Sturchler-Pierrat et al., 1997; Abramowski et al., 2012a).
Discussion
40
Accordingly, neocortical and hippocampal neurons did not vary much in the
transgene expression levels in APP23 and APP48 mice. Both mouse models were
used to determine the effects of Aβ under given artificial conditions. None of these
two mouse models reflects human AD pathology because none showed significant
neurofibrillary tangle pathology and both overexpressed a transgenic construct
made to produce large amounts of Aβ (Sturchler-Pierrat et al., 1997; Abramowski
et al., 2012a; Rijal Upadhaya et al., 2013).
4.1 Aβ effects on mitochondrial integrity
The results obtained in this study show that APP-independant intraneuronal
production and accumulation of Aβ in 18 month-old APP48 mice is associated with
increased numbers of mitochondria exhibiting alterations in frontocentral nerve
cells compared to APP23 and wildtype mice. The questions which need to be
discussed are a) how does Aβ affect mitochondrial structure and b) how does
mitochondrial damage affect the neuron?
Structural changes were found, i.e. increased levels of mitochondria with distorted
christae in APP48 mice similar to those recently reported in prion disease (Siskova
et al., 2010). The increase of mitochondrial alterations in APP48 mice was accom-
panied by the detection of Aβ in a moderate number of altered and non-altered
neuronal somatic mitochondria whereas only few somatic mitochondria in APP23
mice exhibited Aβ and none in wild type animals. Several arguments suggest that
the increase of mitochondrial alterations in APP48 mice was related to the
presence of Aβ and may have functional consequences:
1) Aβ is capable to induce apoptosis through the mitochondria-caspase-3 pathway
(Costa et al., 2010; Wang et al., 2010), and
2) mitochondrial Aβ levels are associated with the extent of mitochondrial
dysfunction, cognitive impairment and oxidative stress in AD mouse models and
AD (Dragicevic et al., 2010),
3) histologically altered mitochondria showed a reduced number of christa
membranes presumably providing the morphological correlative for an impairment
of mitochondrial function, they were found most frequently in APP48 mice which
also contained more mitochondrial Aβ than APP23 mice.
Oxidative stress with consecutive mitochondrial dysfunction and cell death may
result from Aβ interaction with Aβ-binding alcohol-dehydrogenase (ABAD) as a Aβ
Discussion
41
binding site in the mitochondrion, (Lustbader et al., 2004; Takuma et al., 2005), Aβ
interaction with Cyclophillin D (CypD) (Du et al., 2008) or Aβ induced inhibition of
complex IV of the ETC (Canevari et al., 1999; Crouch et al., 2005; Manczak et al.,
2006; Wang et al., 2008).
As shown, there are a number of mechanisms by which intracellular Aβ in
mitochondria could lead to mitochondrial damage. It is proposed that Aβ-related
mitochondrial pathology is compensated by various mechanisms until
mitochondria reach a functional threshold which leads to neurodegeneration
(Swerdlow et al., 2010).
For APP23 mice, however, we cannot rule out that trophic effects reported for APP
expression (Mattson, 1997) compensate the Aβ toxicity to mitochondria.
It is noteworthy that only mitochondria in the nerve cell somata showed increased
alterations in APP48 mice whereas mitochondria in distal dendrites and axons did
not exhibit differences in volume density as well as in the percentage of alterations
among APP23, APP48 and wildtype mice. Thus, intraneuronal Aβ42 exhibited its
major toxic effects on mitochondria close to its production site in APP48 mice, i.e.
close to the endoplasmic reticulum. Biochemical assessment of respiratory chain
complex I and complex IV, α-ketoglutarate dehydrogenase, and tricarboxylic acid
cycle enzyme activity did not show significant differences in forebrain
homogenates (data not shown, received from Staufenbiel M). However, the local
effect in the soma is probably not sufficient to reduce the overall activities in a
brain homogenate.
In the AD brain and in in-vitro studies, APP was found to accumulate in
mitochondria in neurons of AD brains (Anandatheerthavarada et al., 2003; Keil et
al., 2004; Park et al., 2006), leading to mitochondrial dysfunction. APP was found
to be imported into mitochondria via mitochondrial import channels and formed
complexes with them. These complexes were suggested to lead to to the blockade
of further import of nuclear encoded proteins with the result of decreased
cytochrome c oxidase activity and increased reactive oxygen species
(Anandatheerthavarada et al., 2003; Devi et al., 2006; Rijal Upadhaya et al.,
2013).
Discussion
42
4.2 Neurite and synapse degeneration in APP23 and A PP48 mice
APP23 mice showed dendritic degeneration in DiI-traced commissural neurons,
loss of asymmetric synapses and dystrophic neurites whereas none of these
pathologies was observed in APP48 mice. In this context, it is important to note
that fibrillar Aβ was present in dendrites of APP48 mice indicating that the mere
presence of intracellular Aβ was not sufficient to induce this pathology.
Accordingly, neuritic degeneration and loss of asymmetric synapses may either
require high concentrations of extracellular Aβ40/42 and/or the presence of APP and
its metabolites including APP-derived Aβ as in APP23 mice. The amount of total
Aβ42 determined by ELISA did not explain neuritic degeneration because APP48
mice contained more Aβ42 in the brain than 3–5 months old APP23 mice (see also
(Capetillo-Zarate et al., 2006)) although 5-month-old APP23 mice did already
exhibit dendrite pathology as previously reported (Capetillo-Zarate et al., 2006).
Consistent with our observations, the prevalence of high levels of extracellular Aβ
aggregates, e.g. soluble Aβ oligomers and protofibrils and Aβ plaques have been
shown to be associated with altered synapse function (Wang et al., 2002; Lacor et
al., 2004; Shankar et al., 2008). Neuritic alterations were frequently seen near
amyloid plaques (Tsai et al., 2004; Spires et al., 2005). The electron microscopic
detection of extracellular non-fibrillar and fibrillar Aβ-positive aggregates in
association with dystrophic neurites in APP23 but not in APP48 mice further
argues in favor of a critical role of extracellular Aβ in neuritic degeneration.
Electrophysiological changes in response to extracellularly administered Aβ–
aggregates were mainly reported for excitatory synapses (Wang et al., 2002;
Shankar et al., 2008). Since asymmetric synapses represent mainly excitatory
(glutamatergic) synapses (Miranda et al., 2009) the loss of these synapses likely
represented the result of toxic interactions with Aβ aggregates. We have detected
Aβ within few dystrophic neurites in APP23 mice indicating that we cannot exclude
a contribution of intraneuronal Aβ to neuritic degeneration.
The Bri-Aβ42 mouse, that produces only extracellular Aβ42 derived from an ABri-
Aβ42 construct did not show behavioral changes but Aβ plaques (McGowan et al.,
2005). Bri-Aβ40 mice expressing an ABri-Aβ40 construct did not even develop
plaques. These findings may argue against a contribution of extracellular Aβ to Aβ
toxicity. However, it is not yet clear whether the ABri-derived Aβ42 aggregates
contain similar amounts of AβN3pE and pAβ as Aβ aggregates in APP23 or APP48
Discussion
43
mice, whether APP expression or the presence of both, Aβ42 and Aβ40 , is required
for extracellular Aβ toxicity, or whether this mouse model did not produce enough
Aβ42 to cause symptoms.
APPE693Δ transgenic mice produce Aβ lacking glutamate-22 (E22Δ). This mouse
model does not develop amyloid plaques but APP-derived intracellular Aβ
aggregates and synapse loss (Tomiyama et al., 2010). Exogenous synthetic
AβE22Δ also lead to synaptic alterations in hippocampal slice culture experiments or
after intraventricular injection (Takuma et al., 2008; Tomiyama et al., 2008)
[46,47]. As such, neuritic changes and/or synapse pathology can be explained by
APP-derived Aβ production regardless of the presence of Aβ plaques whereas
such changes were not reported in APP48, Bri-Aβ42 and Bri-Aβ40 mice, which
produce non-APP derived Aβ. A further argument for a role of APP in Aβ toxicity in
APP23 mice is the recent finding of a coaggregation of Aβ with C-terminal APP
fragments in dispersible Aβ aggregates (Rijal Upadhaya et al., 2012) supporting
the hypothesis that APP is a molecular target of Aβ toxicity (Bignante et al., 2013;
Rijal Upadhaya et al., 2013).
4.3 Two types of A β-induced neurodegeneration in the
frontocentral cortex: somatic type and neuritic typ e
In the frontocentral cortex of APP23 mice neuritic degeneration and asymmetric
synapse loss was found in the absence of neuron loss suggesting that both events
indicate a neuritic type of nerve cell degeneration with neuritic degeneration
preceding nerve cell death. APP48 mice, on the other hand, showed a different
type of nerve cell damage characterized by morphologically altered mitochondria
in the cell soma and thread-like Aβ aggregates in dendrites. Although the
appearance of the dendrites and axons was, except for the Aβ threads,
morphologically normal and no synapse loss was observed, mitochondrial
changes in nerve cell somata represented early signs of a somatic type of
neurodegeneration. Since mitochondrial alterations caused by Aβ have been
demonstrated to induce apoptosis (Costa et al., 2010; Wang et al., 2010) it is
tempting to speculate that this type of somatic neurodegeneration with increased
amounts of morphologically altered mitochondria finally results in apoptosis
without the development of dystrophic neurites and dendrite degeneration before
cell death. Hence, APP23 mice and APP48 mice develop two different types of
Discussion
44
nerve cell degeneration in the frontocentral cortex (Figure 11):
1) APP23 mice showed a neuritic type of neurodegeneration with early neuritic
and synaptic degeneration but without increased numbers of altered mitochondria;
2) APP48 mice exhibited a somatic type of neurodegeneration with increased
somatic mitochondrial degeneration but morphologically intact dendrites and
axons. APP48 and APP23 mice both showed neuron loss in the CA1 region as
previously described (Calhoun et al., 1998; Abramowski et al., 2012a; Rijal
Upadhaya et al., 2012).
It was not accompanied by a reduction in synaptic density suggesting replacement
of lost synapses by surviving neurons. Except for Aβ plaques in APP23 mice and
intracellular Aβ in both transgenic animals, significant reduction of synapse
densities and mitochondrial alterations could not be identified in this brain region
possibly because the more vulnerable CA1 neurons die faster than altered
neurons in the frontocentral cortex and do not accumulate at early stages of nerve
cell degeneration. Since 3-month-old animals have more CA1 neurons than 15-18-
month-old mice (Figure 7c) and the decrease in number was higher than the age-
related loss of CA1 neurons in wild type mice it appears likely that the age-related
loss of CA1 neurons is enhanced by Aβ toxicity in APP23 and APP48 mice.
Although both types of Aβ-related neurodegeneration were observed in artificial
mouse models that were made to produce large amounts of Aβ there are
arguments for the hypothesis that both mechanisms of Aβ-related
neurodegeneration are relevant in AD: 1) synapse loss and dystrophic neurites
especially around neuritic plaques are well known features of AD pathology
(DeKosky and Scheff, 1990; Wang and Munoz, 1995; Dickson, 1997) that might
be explained in part by the neuritic type of Aβ-related neurodegeneration and 2)
mitochondrial alterations are well known in AD cases as well (Lustbader et al.,
2004) presumably indicative for somatic type neurodegeneration in the presence
of intracellular Aβ (Gouras et al., 2000; Rijal Upadhaya et al., 2013).
Discussion
45
Figure 11 Schematic representation of the somatic a nd neuritic type of Amyloid beta protein (Aβ) -related neurodegeneration in frontocentral neuro ns of APP23 and APP48 mice. In APP48 mice Aβ accumulates within neurons and in microglial cells as previously reported (Abramowski et al., 2012a). Extracellular Aβ is not detectable suggesting that Amyloid precursor protein (APP) independently produced intracellular Aβ leads to functional impairment of neurons as indicated by motor deficits (Abramowski et al., 2012a). Mitochondrial alterations occur more frequently in the nerve cell somata of APP48 mice than in wildtype and APP23 mice and are proposed to lead to apoptotic cell death as suggested previously (Umeda et al., 2011) without preceding neuritic alteration. This type of somatic neurodegeneration in APP48 mice is different from that seen in APP23 mice, which contains less intracellular Aβ but significant amounts of extracellular Aβ aggregates including plaques. We propose that extra- and intracellular APP-derived Aβ causes synapse loss, dendrite degeneration and often plaque-associated, dystrophic neurites in APP23 mice indicative for a second neuritic type of neurodegeneration. Intracellular Aβ in APP23 mice may be produced within the nerve cell or may be taken up from the extracellular space (Wirths et al., 2001; Tampellini et al., 2007; Ovsepian et al., 2013; Ovsepian and Herms, 2013; Rijal Upadhaya et al., 2013).
4.4 Conclusions
The data suggest two independent mechanisms by which Aβ causes
neurodegeneration (Fig. 11): a somatic type and a neuritic type. The neuritic type
of neurodegeneration is characterized by a loss of asymmetric synapses,
degeneration of dendrites, occurrence of dystrophic neurites and is associated
with the occurrence of extracellular Aβ aggregates in APP23 mice. The somatic
type of neurodegeneration shows mitochondrial alterations in the neuronal somata
but no changes in neurite morphology. It is linked to intraneuronal accumulation of
Aβ and functional changes in APP48 mice (Abramowski et al., 2012a). Both
Discussion
46
mechanisms may finally lead to neuron loss as observed in the hippocampal
sector CA1 in APP23 and APP48 mice (Abramowski et al., 2012a) (Calhoun et al.,
1998) and both mechanisms may account for neurodegeneration in AD. As such,
for the development of therapeutic strategies aimed at protecting neurons from
AD-related degeneration it appears important to consider both types of Aβ-related
neurodegeneration (Rijal Upadhaya et al., 2013).
Summary
47
5 Summary
The deposition of the amyloid beta protein (Aβ) peptide in the brain is one of the
hallmarks of Alzheimer’s disease. It is not yet clear whether Aβ always leads to
similar changes or whether it induces different features of neurodegeneration in
relation to its intra- and/or extracellular localization. Two transgenic mouse models
APP48 and APP23 mice were analyzed. The APP48 mouse expresses Aβ1-42 with
a signal sequence in neurons. These animals produce intracellular Aβ42
independent of amyloid precursor protein (APP) but do not develop extracellular
Aβ plaques. The APP23 mouse overexpresses human APP with the Swedish
mutation (KM670/671NL) in neurons and produces APP-derived extracellular Aβ
plaques and intracellular Aβ aggregates. Tracing of commissural neurons in layer
III of the frontocentral cortex with the DiI tracer showed no morphological signs of
dendritic degeneration in APP48 mice compared to littermate controls. In contrast,
the dendritic tree of highly ramified commissural frontocentral neurons was altered
in 15-month-old APP23 mice. The density of asymmetric synapses in the
frontocentral cortex was reduced in 3- and 15-month-old APP23 but not in 3- and
18-month-old APP48 mice. Frontocentral neurons of 18-month-old APP48 mice
showed an increased percentage of altered mitochondria in the soma compared to
wildtype and APP23 mice. Aβ was often seen in the membrane of neuronal
mitochondria in APP48 mice at the electron microscopic level. These results
indicate that APP-independent intracellular Aβ accumulation in APP48 mice is not
associated with neuritic degeneration but with mitochondrial alterations whereas
APP-derived intra- and extracellular Aβ pathology in APP23 mice is linked to
dendrite degeneration and synapse loss independent of obvious mitochondrial
alterations. Thus, Aβ aggregates in APP23 and APP48 mice induce
neurodegeneration presumably by a somatic and a neuritic mechanism. The
neuritic type of neurodegeneration is characterized by a loss of asymmetric
synapses, degeneration of dendrites, occurrence of dystrophic neurites and is
associated with the occurrence of extracellular Aβ aggregates in APP23 mice. The
somatic type of neurodegeneration shows mitochondrial alterations in the neuronal
somata but no changes in neurite morphology. It is linked to intraneuronal
accumulation of Aβ and functional changes in APP48 mice. Both mechanisms may
Summary
48
finally lead to neuron loss as observed in the hippocampal sector CA1 in APP23
and APP48 mice and both mechanisms may account for neurodegeneration in AD.
References
49
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Supplementary Material
64
Supplementary Material
Supplementary Tab. 1
a. Aβ1-42 levels detected by ELISA: Mean, standard devia tion, Welch-test
Mean Aβ1-42 (pmol/g) p-value
APP23 – 2-3 months (n=4) 2.25 +/- 0.36
APP48 – 2-3 months (n=6) 165.00 +/- 6.48 } <0.001
APP23 – 15 months (n=7) 6019.74 +/- 1146.88
APP48 – 18 months (n=8) 352.38 +/- 34.47 } <0.001
(Rijal Upadhaya et al., 2013)
b. DiI tracing of commissural neurons in the fronto central cortex
DiI-tracing of commissural neurons: Mann-Whitney U-test (exact test – two sided)
Comparison between transgenic and wildtype mice
3 months of age Type I neurons Type II
neurons
Type III
neurons
APP23 mice vs wildtype
littermates
p = 0.589 p = 1.000 p = 0.394
APP48 mice vs wildtype
littermates
p = 0.573 p = 0.573 p = 0.228
n = 6 (APP23, APP48); n = 5 (wildtype (APP23-littermates)); n = 8 (wildtype
(APP48-littermates))
(Rijal Upadhaya et al., 2013)
Supplementary Material
65
DiI-tracing of commissural neurons: Mann-Whitney U-test (exact test – two sided)
Comparison between transgenic and wildtype mice
15-18 months of age Type I neurons Type II
neurons
Type III
neurons
APP23 mice vs wildtype
littermates
p = 0.001 p = 0.004 p = 0.093
APP48 mice vs wildtype
littermates
p = 0.422 p = 0.235 p = 0.134
n = 8 (APP23); n = 9 (wildtype (APP23-littermates)); n = 11 (wildtype (APP48-
littermates)); n = 12 (APP48)
(Rijal Upadhaya et al., 2013)
DiI-tracing of commissural neurons: Mann-Whitney U-test (exact test – two sided)
Comparison between age groups
3 months vs.
15-18 months
Type I
neurons
Type II
neurons
Type III
neurons
n (3m;
15/18m)
Wildtype
littermates
APP23
p = 0.012 p = 0.689 p < 0.001 * 5; 9
Wildtype
littermates
APP48
p = 0.009 p = 0.152 p = 0.442 8; 11
APP23 p = 0.001 p = 0.001 p = 0.142 6; 8
APP48 p = 0.018 p = 0.018 p = 0.553 6; 12
*not considered different because not confirmed in APP48 wildtype littermates
(Rijal Upadhaya et al., 2013)
Supplementary Material
66
c. Frequency of dystropic neurites at the electron microscopic level
Comparison by genotype: ANOVA with Games-Howell post-hoc test
frontocentral cortex CA1
3 months 15-18
months
3 months 15-18
months
Wildtype vs. APP23 0.445 0.032 0.300 0.970
Wildtype vs. APP48 0.198 0.939 0.829 0.228
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age: Welch-test
frontocentral cortex CA1
Wildtype 0.093 0.485
APP23 0.004 0.015
APP48 0.818 0.394
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
67
d. Number of synapses: Mann-Whitney-U-test (exact t est-two sided)
Comparison by genotype
frontocentral cortex CA1
Asymmetric synapses 3 months 15-18
months
3 months 15-18
months
Wildtype vs. APP23 0.026 0.041 0.240 0.065
Wildtype vs. APP48 0.041 1.000 0.818 0.240
Symmetric synapses
Wildtype vs. APP23 0.240 0.589 0.093 0.394
Wildtype vs. APP48 0.310 0.310 0.310 0.589
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age
Asymmetric synapses frontocentral cortex CA1
Wildtype 0.002 0.699
APP23 0.002 0.180
APP48 0.009 0.937
Symmetric synapses
wildtype 1.000 0.093
APP23 0.093 0.240
APP48 0.937 0.699
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
68
e. Number of hippocampal CA1 and of frontocentral n eurons
Comparison by genotype: ANOVA with Games-Howell post-hoc test
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 n.a. 0.812
Wildtype vs. APP48 n.a. 0.999
CA1
Wildtype vs. APP23 0.004 <0.001
Wildtype vs. APP48 0.004 <0.001
n = 6 (15-18 months wildtype, APP23, APP48 and 3-month-old APP23, APP48); n
= 7 (3-month-old wildtype)
(Rijal Upadhaya et al., 2013)
Comparison by age: Welch test
Frontocentral cortex CA1
Wildtype n.a. 0.005
APP23 n.a. <0.001
APP48 n.a. 0.002
n = 6 (15-18 months wildtype, APP23, APP48 and 3-month-old APP23, APP48); n
= 7 (3-month-old wildtype)
(Rijal Upadhaya et al., 2013)
Supplementary Material
69
f. Percentage of altered somatic mitochondria: Mann -Whitney-U-Test (exact
test-two sided)
Comparison by genotype
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 0.065 0.937
Wildtype vs. APP48 0.132 0.009
CA1
Wildtype vs. APP23 0.394 0.394
Wildtype vs. APP48 0.240 0.937
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
comparison by age
Frontocentral cortex CA1
Wildtype 0.015 0.026
APP23 0.002 0.015
APP48 0.002 0.004
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
70
g. Volume density of altered somatic mitochondria: Mann-Whitney U-test
(exact test – two sided)
Comparison by genotype
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 0.026 0.818
Wildtype vs. APP48 0.132 0.015
CA1
Wildtype vs. APP23 0.240 0.310
Wildtype vs. APP48 0.132 0.818
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age
Frontocentral cortex CA1
Wildtype 0.009 0.041
APP23 0.002 0.002
APP48 0.002 0.065
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
71
h. Volume density of somatic mitochondria: Mann-Whi tney U-test (exact test
– two sided)
Comparison by genotype
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 0.394 0.240
Wildtype vs. APP48 0.699 0.180
CA1
Wildtype vs. APP23 0.093 0.818
Wildtype vs. APP48 0.394 0.589
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age
Frontocentral cortex CA1
Wildtype 0.394 0.818
APP23 0.002 0.065
APP48 0.026 0.485
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
72
i. Percentage of altered neuritic mitochondria: Man n-Whitney U-test (exact
test – two sided)
Comparison by genotype
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 0.180 0.699
Wildtype vs. APP48 0.132 0.132
CA1
Wildtype vs. APP23 0.394 0.026
Wildtype vs. APP48 0.310 0.394
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age
Frontocentral cortex CA1
Wildtype 0.041 0.394
APP23 0.002 0.699
APP48 0.180 0.485
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
73
j. Volume density of altered neuritic mitochondria: Mann-Whitney U-test
(exact test – two sided)
Comparison by genotype
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 0.180 0.485
Wildtype vs. APP48 0.394 0.132
CA1
Wildtype vs. APP23 0.394 0.026
Wildtype vs. APP48 0.394 0.394
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age
Frontocentral cortex CA1
Wildtype 0.065 0.394
APP23 0.002 0.699
APP48 0.065 0.065
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
74
k. Volume density of neuritic mitochondria: Mann-Wh itney U-test (exact test
– two sided)
Comparison by genotype
Frontocentral cortex 3 months 15-18 months
Wildtype vs. APP23 0.394 0.589
Wildtype vs. APP48 0.699 0.818
CA1
Wildtype vs. APP23 0.310 0.699
Wildtype vs. APP48 0.394 0.093
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Comparison by age
Frontocentral cortex CA1
Wildtype 0.394 0.310
APP23 0.394 0.937
APP48 0.240 0.065
n = 6 (each group)
(Rijal Upadhaya et al., 2013)
Supplementary Material
75
Supplementary Fig. 1: Western blot analysis of solu ble, dispersible, membrane-associated, and insoluble (plaque-associated) A β in wildtype, APP48 and APP23 mice. Original blots related to Fig. 4b(Rijal Upadhaya et al., 2013).
Supplementary Material
76
Supplementary Fig 2: Mitochondrial alterations in peripheral neurites. a-c: Percentage of altered mitochondria (a), volume densities of altered mitochondria (b), and volume densities of all mitochondria (c) in peripheral neurites did not show significant changes among frontocentral neurons in wild type (WT), APP23 and APP48 mice. d-f: No significant differences in the percentage of altered mitochondria (d), volume densities of altered mitochondria (e), and volume densities of all mitochondria (f) in peripheral neurites of the CA1 sector of the Ammon’s horn were found between APP48 mice and wild type controls. 3-month-old APP23 mice had less morphologically altered mitochondria (d, e) than wild type controls. In 15-month-old animals the trend was still visible but did not reach significance (d, e). *p < 0.05 (Further statistical analysis: Supplementary Tab. 1)(Rijal Upadhaya et al., 2013).
Acknowledgements
77
Acknowledgements
I would like to express my gratitude to my supervisor Prof. Dr. med. Dietmar Thal,
for providing me with such an interesting topic, for the excellent supervision and
support during this work as well as for providing immunohistochemical data,
synapse density data and dystrophic neurites frequency data.
I wish to thank all colleagues of the Section of Neuropathology, especially to Dr.
rer. nat. Ajeet Rijal Upadhaya for analysis of DiI tracing data from APP48 and
wildtype mice, for altered mitochondria data of 3 month old mice, stereological
data of hippocampal and frontocentral cortex neuron numbers as well as SDS-
PAGE and Western Blot data and to Irina Kosterin for the help with electron
microscope. I am very grateful to M. Staufenbiel and D. Abramowski at the
Novartis Institute for Biomedical Research (Basel, Switzerland) for providing the
animal models and ELISA data, to Estibaliz Capetillo-Zarate for providing DiI
tracing data for APP23 and wildtype mice (Cornell University, NY, USA), to H.
Yamaguchi at the Gunma University School of Health Sciences (Maebashi,
Gunma, Japan) for the kind gift of antibodies and Stefan Liebau for providing
Laser-Scan Microscopy figures of traced neurons. Thanks to Jochen Walter,
Satish Kumar, Janina Gerth for providing phosphorylated Aβ antibodies and
immunohistochemical data. Thanks to Stephan Harf for technical help on Fig. 1.
This work has been published in Acta Neuropathologica Communications and
contains, in addition to my work, experimental data carried out by coworkers as
described above. The text of this dissertation contains text blocks of its published
version in Acta Neuropathologica Communications.
Special thanks to my parents Helga and Dirk Scheibe for all the love and support
during my studies and this work. I am so thankful for everything you gave me and
all I have learned from you! I know it means a lot to you as it means to me to finish
this work.
Special thanks also to Heike Luise Schwarz for the love and motivation to finish
this work.
Thanks also to my sister and brothers and their families as well as to my friends
and colleagues for the distraction and nice time we had together.
Curriculum vitae
78
Curriculum vitae
Der Lebenslauf ist in der Online-Version aus Gründen des Datenschutzes nicht
enthalten.
Curriculum vitae
79
Parts of this dissertation have already been published in
Ajeet Rijal Upadhaya*, Frederik Scheibe*, Irina Kosterin, Dorothee Abramowski,
Janina Gerth, Sathish Kumar, Stefan Liebau, Haruyasu Yamaguchi, Jochen
Walter, Matthias Staufenbiel and Dietmar Rudolf Thal (2013) The type of
Abeta related neuronal degeneration differs between amyloid precursor
protein (APP23) and amyloid beta-peptide (APP48) transgenic mice. Acta
Neuropathologica Communications 2013, 1:77
* Equal contributors
© 2013 Rijal Upadhaya, Scheibe et al.; licensee BioMed Central Ltd. This is an
Open Access article distributed under the terms of the Creative Commons
Attribution License (http://creativecommons.org/licenses/by/2.0), which permits
unrestricted use, distribution, and reproduction in any medium, provided the
original work is properly cited. The Creative Commons Public Domain Dedication
waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data
made available in this article, unless otherwise stated.