Progressive striatonigral degeneration in a transgenic mouse model of multiple system atrophy: translational implications for interventional therapies
© The Author(s). 2018
Received: 8 November 2017
Accepted: 16 December 2017
Published: 3 January 2018
Multiple system atrophy (MSA) is a rapidly progressive neurodegenerative disorder characterized by widespread oligodendroglial cytoplasmic inclusions of filamentous α-synuclein, and neuronal loss in autonomic centres, basal ganglia and cerebellar circuits. It has been suggested that primary oligodendroglial α-synucleinopathy may represent a trigger in the pathogenesis of MSA, but the mechanisms underlying selective vulnerability and disease progression are unclear. The post-mortem analysis of MSA brains provides a static final picture of the disease neuropathology, but gives no clear indication on the sequence of pathogenic events in MSA. Therefore, alternative methods are needed to address these issues. We investigated selective vulnerability and disease progression in the transgenic PLP-α-syn mouse model of MSA characterized by targeted oligodendroglial α-synuclein overexpression aiming to provide a neuropathological correlate of motor deterioration. We show progressive motor deficits that emerge at 6 months of age and deteriorate up to 18 months of follow-up. The motor phenotype was associated with dopaminergic cell loss in the substantia nigra pars compacta at 6 months, followed by loss of striatal dopaminergic terminals and DARPP32-positive medium sized projection neurons at 12 months. Olivopontocerebellar motor loops remained spared in the PLP-α-syn model of MSA. These findings replicate progressive striatonigral degeneration underlying Parkinson-variant MSA. The initiation of the degenerative process was linked to an increase of soluble oligomeric α-synuclein species between 2 and 6 months. Early region-specific α-synuclein-associated activation profile of microglia was found in MSA substantia nigra. The role of abnormal neuroinflammatory signalling in disease progression was further supported by increased levels of CD68, CCL3, CCL5 and M-CSF with a peak in aged PLP-α-syn mice. In summary, transgenic PLP-α-syn mice show a distinctive oligodendroglial α-synucleinopathy that is associated with progressive striatonigral degeneration linked to abnormal neuroinflammatory response. The model provides a relevant tool for preclinical therapeutic target discovery for human Parkinson-variant MSA.
Multiple system atrophy (MSA) is a fatal rapidly progressive neurodegenerative disorder without effective therapy . In the Western hemisphere the Parkinson variant predominates over the cerebellar subtype of MSA in up to 4:1 of the cases . The clinical diagnosis of MSA relies on the coexistence of autonomic failure and parkinsonian or cerebellar motor impairment, however, a definite diagnosis still requires autopsy . Autonomic or other non-motor features such as urogenital disturbances, neurogenic orthostatic hypotension or REM sleep behaviour disorder may precede the onset of the motor syndrome .
The pathological hallmark feature of MSA is the presence of glial cytoplasmic inclusions (GCIs) in oligodendrocytes . The major component of the GCIs is filamentous α-synuclein (α-syn) [31, 53, 63, 67]. In addition, neuronal α-syn aggregates have also been reported in MSA . Analysis of SNCA mRNA identifies increased levels of SNCA140 (full-length α-syn) and SNCA112 isoform in substantia nigra, striatum, cerebellar cortex and nucleus dentatus of MSA patients as compared to healthy controls and PD patients, while SNCA126 mRNA is significantly lower in MSA cases . Epitope-specific antibodies confirm the over-expression of full-length α-syn and α-syn 112 isoform (detectable by 5G4 antibody, which is considered to bind predominantly to aggregate α-syn [8, 33]. The end-stage neuropathological features of MSA include striatonigral degeneration (SND) and olivopontocerebellar atrophy (OPCA), as well as neuronal loss in brainstem and spinal cord autonomic centres [5, 45, 69, 70]. Despite the fact that the major focus of α-syn accumulation are the oligodendrocytes in MSA, only minor changes of oligodendroglial numbers (mostly non-significant) are detectable by stereological analysis of MSA brains [41, 45, 46]. In mildly or moderately affected MSA brains no significant demyelination is detected . A region-specific increase in astrocyte numbers (astrogliosis) is found in basal ganglia and cortex, but not in white matter of end-stage MSA [41, 45, 46]. Finally, widespread microgliosis has been reported in MSA brains in parallel to the α-syn pathology [28, 29, 41, 45, 46].
It has been suggested that primary oligodendroglial α-synucleinopathy may represent a trigger in the pathogenesis of MSA . However, the mechanisms underlying selective vulnerability and disease progression are unclear. The post-mortem analysis of MSA brains provides a static final picture of the disease neuropathology, but gives no clear indication on the sequence of pathogenic events in MSA. Therefore, alternative methods are needed to address selective vulnerability and disease progression in MSA.
Several rodent models have been developed over the last two decades to serve as pre-clinical testbeds of MSA [59, 60, 64]. Each of these models shows advantages and limitations as previously discussed . The transgenic mouse overexpressing α-syn in oligodendroglia under the proteolipid protein (PLP) promoter  is especially interesting because this transgenic murine model of MSA develops a progressive phenotype, including non-motor and motor symptoms similar to the human disease [7, 18, 19, 26, 34, 35, 57, 58, 61]. However, studies on the progressive evolution of the MSA-like phenotype from the very early stages are limited in the PLP-α-syn mouse. We here investigate motor dysfunction and neurodegeneration in aging PLP-α-syn mice in order to identify patterns of selective vulnerability downstream of GCI pathology. Our data provide new insights into MSA pathogenesis and they are therefore important for future preclinical studies investigating candidate neuroprotective agents for the human disease.
Materials and methods
Homozygous transgenic PLP-α-syn mice (MGI:3,604,008) overexpressing human α-syn under the PLP-promoter  and background-, age- and sex-matched non-transgenic C57Bl/6 mice were used in this study. They were bred and housed in a temperature-controlled room under a 12/12 h dark/light cycle, with free access to food and water, in the animal facility of the Medical University of Innsbruck, under special pathogen free conditions. During the study, all efforts were made to minimize the number of animals used and their suffering. All experiments were performed in accordance with the Austrian law and after permission for animal experiments by the authorities (BMWF-66.011/0034-II/10b/2010 and BMWFW-66.011/0041-WF/II/3b/2014).
Motor behaviour in PLP-α-syn mice and non-transgenic controls was tested at 2, 6, 12 and 18 months of age by applying the beam walking test, the pole test, gait analysis, and grip strength analysis.
Motor coordination and balance was assessed with the method adapted from Fernagut et al.  by measuring the ability of the mice to traverse a narrow beam to reach a dark goal box. The beams consist of two different strips of wood (each 50 cm long; one was 1.6 cm and the other 0.9 cm square cross-section) placed horizontally 20 and 50 cm above the floor, respectively. During training, three daily sessions of three trials (nine crossings) were performed using the 1.6 cm square large beam. Mice were then tested using the 0.9 cm square beam. Mice were allowed to perform three consecutive trials. The time to cross the beam and the number of sideslips (errors) were recorded on each trial, and the mean number of sideslips during a three-trial session, as well as the best time, was kept as the variable.
The pole test was performed according to established protocols . Each mouse was habituated to the test the day before. A wooden vertical pole with rough surface, 1 cm wide and 50 cm high was used. Each mouse was placed with the head up at the top of the pole and the time for turning downwards (Tturn) as well as the total time for climbing down the pole until the mouse reached the floor with the four paws (Ttotal) was taken in 5 trials. The best performance of all the five trials was kept for the statistical analysis.
Gait analysis was quantified with the DigiGait™ Imaging system (Mouse Specifics Inc., Boston, MA). Briefly, a video camera mounted below a transparent treadmill belt captured ventral images of each mouse. The images were automatically digitized and software algorithms analysed the digital images to define the area of each paw, and generate a set of periodic waveforms that describe the advance and retreat of the four limbs relative to the treadmill belt through consecutive strides. The software identified the portions of the paw that were in contact with the treadmill belt in the stance and swing phase of the stride, and measured several postural and kinematic metrics of gait dynamics. A treadmill physiological speed of 25 cm/s was applied and a maximum of 3 min was videotaped at constant light and camera settings.
Grip strength was measured by testing the ability of each mouse to remain clinging to an inverted cage lid at a height of 70 cm above the surface for a period of up to 1 min.
Mice received an overdose of thiopental. The head and neck were fixed and the muscles over cisterna magna were carefully removed. Blood was completely removed before puncture of the cisterna magna. A pulled capillary was used to puncture cisterna magna and collect CSF (up to 5 μl per mouse). CSF was stored at −80 °C before further analysis.
Western blot analysis
Sequential α-syn extraction and quantification
Hemibrain tissue was collected after PBS perfusion and stored at −80 °C until analysis. We followed a previously published protocol with minor modifications . Shortly, tissue was homogenized in Triton-X (TX) extraction buffer (50 mM Tris-base pH 7.6, 150 mM NaCl, 1% Triton-X-100, 2 mM EDTA) containing protease and phosphatase inhibitors. The lysate was sonicated and then centrifuged (120,000×g for 60 min at 4 °C) and the supernatant was collected (TX soluble fraction). The pellet was then washed 3 times with 1 M PBS/1% TX, centrifuged (13,000 x g for 15 min) and re-suspended in SDS extraction buffer (50 mM Tris pH 7.6, 150 mM NaCl, 1% Triton-X-100, 0.5% Na-deoxycholate, 1% SDS), sonicated, and centrifuged (120,000×g for 60 min at 4 °C) and the supernatant was collected (TX insoluble fraction). The samples were run on 12% SDS-PAGE gels. Primary antibodies included antibodies against α-syn [rabbit monoclonal anti-phospho-α-syn (pS-129), (1:500; Abcam, EP1536Y), human-specific monoclonal 4B12, (1:1000; Genetex, GTX21904), monoclonal syn-1, (1:1000; BD Biosciences, 619,787), polyclonal C20, (1:1000; Santa Cruz, sc-7011-R)] and β-actin (1:2000; Cell Signalling Technology, 8H10D10) as a loading control. The intensity of the immunoreactive bands was estimated by densitometric quantification using ImageJ (relative density, RD) and then normalized to the corresponding β-actin levels.
Subregion-specific α-syn analysis
Tissue homogenates from all selected brain regions were prepared in RIPA-lysis buffer containing 65 mM Tris-base, 150 mM NaCl, 1% Triton-X, 0.25% sodium deoxycholate, 1 mM EDTA, and a mix of phosphatase and protease inhibitors (“phosSTOP” and “Complete, mini, EDTA-free,” Roche Applied Science). BCA Protein Assay Kit (Pierce #23225, ThermoScientific) was used for determining the protein concentration. Equal amounts of protein (typically 20 μg) per sample were loaded on a 10% SDS-polyacrylamide gel for separation and then transferred on a polyvinyldifluoride membrane. Membranes were incubated in blocking buffer (20 mM Tris, 136 mM NaCl, pH 7.6, 0,1% Tween 20, 5% non-fat dry milk) and thereafter incubated overnight at 4 °C using one of the following primary antibodies: rabbit polyclonal anti GDNF (1:1000; Santa Cruz Biotechnologies, CA); rabbit polyclonal anti-BDNF (1:1000; Santa Cruz Biotechnologies, CA), mouse anti-mouse and human SNCA monoclonal antibody clone 42 (1:500; BD Transduction Laboratories, CA, USA), mouse anti-myelin basic protein (MBP, Abcam, ab62631), rabbit anti-p25α (, generously provided by Prof. Paul Henning Jensen, Aarhus University, Denmark), and mouse anti-myelin oligodendrocyte glycoprotein (MOG, clone 8-18C5 , generously provided by Prof. Markus Reindl, Medical University of Innsbruck, Austria).
After appropriate washing steps, membranes were incubated with HRP-linked secondary antibodies: anti-biotin, HRP-linked antibody (1:2500; Cell Signaling Technology, #7075); anti-rabbit IgG, HRP-linked (1:5000; Cell Signaling Technology, #7074); anti-mouse IgG, HRP-linked (1:4000; Cell Signaling Technology, #7076). Signals were visualized using a chemiluminescence ECL kit (Pierce, #32106, Thermo Scientific) and images were acquired using a CCD camera (LAS1000 system, Fuji Films). Optical density was measured on specific immunoreactive bands using ImageJ Software. Membranes were then stripped and re-probed with β-actin (1:120,000; Sigma-Aldrich) or mouse anti-alpha-tubulin (ab7750, Abcam). The optical density of specific bands was then normalized to the corresponding β-actin or alpha-tubulin levels.
Selected brain areas were mixed 1:5 with RIPA buffer as described above, homogenized with IKA Ultra Turrax T8 and centrifuge for 15 min at 16000 g at 4 °C, the supernatant was collected and stored at −80 °C for further analysis. A commercially available ELISA kit for detection of α-syn (Invitrogen, CA, US) was applied to measure the concentration of α-syn in selected brain regions according to the manufacturer’s protocol.
The total level of α-syn in cerebrospinal fluid (CSF) was measured with an in-house ultra-sensitive sandwich ELISA for total α-syn as previously described (Emmanouilidou et al. 2011) adapted for measurement of mouse CSF. 3–5 μl samples of CSF were pooled from 3 to 6 animals of each group (control or MSA at 2, 6 or 18 months of age) or recombinant α-syn (as standard). The samples were controlled for haemoglobin content by absorbance at 414 nm, thereafter diluted in TBST/BSA (10 mM Tris-Cl, pH 7.6, 100 mM NaCl, 0.1% Tween-20 and 1% BSA), and measured in duplicate for α-syn levels. The limit of detection of this assay is 0.024 ng/ml. The total number of pooled samples per group that were detectable was 7/13 control and 6/11 MSA samples.
Mice underwent transcardial perfusion with PBS followed by 4% paraformaldehyde for 15 min under deep thiopental anaesthesia. The brains were removed and post-fixed in the same fixative overnight at 4 °C. After 30% sucrose cryoprotection the brains were frozen and stored at −80 °C until further processing. Six series of 40 μm were cut on a cryotome (Leica, Nussloch, Germany). One series was directly mounted on slides and stained with cresyl violet. Immunohistochemistry on free-floating sections was performed using standard protocols and the following antibodies: anti-tyrosine hydroxylase (TH, 1:750, AB152, Millipore, Germany), anti-dopamine and cyclic AMP-regulated phosphoprotein (DARPP32, 1:15,000, 611,520, BD Transduction Laboratories), anti-Iba1 (1:800, ab108539, Abcam, UK), anti-CD68 (1:1000, MCA1957GA, Serotec (Bio-Rad), UK), anti-mouse MHCII (1:100, 14–5321, eBiosciences), anti-GFAP (1:1000, MAB3402, Millipore, Germany), rat anti-human α-synuclein (1:200, 15G7, Enzo Life Sciences, Switzerland), anti-phosphorylated α-synuclein (1:1000, phospho-S129, ab51253, Abcam, UK), anti-aggregated α-synuclein (1:1000, 5G4, Linaris, Germany), biotinylated anti-mouse, anti-rat and anti-rabbit IgG (1:500, respectively, BA-1000, BA-9400 and BA-2001, Vector Laboratories, US). The reaction was enhanced with ABC Elite kit (PK-6100, Vector Laboratories, US) and visualized with 3, 3′-diaminobenzidine. Cresyl violet was used for counterstaining of sections immunostained with anti-Iba1 antibody.
Stereology and image analysis
Stereological estimate of number of neurons and microglia in striatonigral and olivopontocerebellar regions was performed by the use of the optical fractionator method with the StereoInvestigator Software (MicroBrightField) provided to a Nikon Eclipse 80i microscope with motorized stage and high resolution digital camera. A low power objective lens (2×, SPlan) was used to delineate the borders of the areas of interest at all levels in the rostro-caudal axis, according to anatomical points following the mouse brain atlas, between levels AP: +1.7 - -2.0 mm for striatum, −2.5 - -3.9 mm for SN, −3.8 - -4.6 mm for pontine nuclei and −6.7 - -7.5 mm for the inferior olives . The described above cutting protocol and collection of section series yielded the following average number of sections per area: 15 for Striatum, 5 for SN, 4 for pontine nuclei and 4 for the inferior olives. The following design of the optical fractionator was used for the analyses. The cutting thickness of the sections was 40 μm, the final mounted thickness of the sections was 25 μm. Guard zones were 2.5 μm on each surface of the section, therefore resulting in a dissector height of 20 μm. The sampling frequency was chosen by adjusting the X-Y grid size between 80 μm and 250 μm (depending on the region), so that about 100–200 cells were counted in each structure. Counting frames of 50x50μm2 were systemically and randomly positioned throughout the region of interest led by the sampling grid as provided by the StereoInvestigator system. Actual counting was done using a 100× objective (NA 0.75). The coefficient of error (CE) did not exceed 0.07 and ratio CE2/CV2 was less than 0.5 as previously recommended .
Astrogliosis was assessed by measuring the optical density (OD) of GFAP immunostaining as previously reported .
Three-dimensional stacks were acquired with an SP8 confocal microscope (Leica Microsystems, Wetzlar, Germany) using a HC PL APO CS2 63×, 1.3 NA glycerol immersion objective. Imaging was performed using WLL laser with excitation lines for Alexa 488 at 498 nm and for Alexa 594 at 590 nm. Fluorescence emission was detected in sequence 1 from 503 to 576 nm (Alexa 488) and in sequence 2 from 594 to 742 nm (Alexa 594). Images were acquired using the Leica LAS X 3.1.1 acquisition software (Leica Microsystems). Image deconvolution was performed using Huygens Professional software (Scientific Volume Imaging, Hilversum, Netherlands). The Ortho Slicer function was used to define spatial co-localization of signals in 3D.
Characterization of microglia activation
Microglia cells were identified as a nucleus covered and surrounded by Iba1 immunostaining. During the stereological quantification, each microglial cell underwent morphological characterization, and was classified to one of four activation stages (namely A, B, C and D) based on their morphology (detailed description is provided in the results section). The quantification and morphological characterization was performed by a researcher blinded to the genotype and age of the animals.
Hemibrain tissue (n = 4 per group) was snap-frozen after PBS perfusion and stored at −80 °C until analysis. Tissue homogenates from hemibrains were prepared in RIPA-lysis buffer containing 65 mM Tris-base, 150 mM NaCl, 1% Triton-X, 0.25% sodium deoxycholate, 1 mM EDTA, and a mix of phosphatase and protease inhibitors (“phosSTOP” and “Complete, mini, EDTA-free,” Roche Applied Science). BCA Protein Assay Kit (Pierce #23225, ThermoScientific, Waltham, MA USA) was used for determining the total protein concentration. To measure the concentration of cytokines we used the ProcartaPlex® Multiplex Immunoassay (eBioscience, Waltham, MA USA) that uses the Luminex technology (multi-analyte profiling beads) to enable the simultaneous detection and quantitation of multiple cytokines and chemokines per sample, including IFN gamma; IL-12p70; IL-13; IL-1 beta; IL-2; IL-4; IL-5; IL-6; TNF alpha; GM-CSF; IL-18; IL-10; IL-17A; IL-22; IL-23; IL-27; IL-9; GRO alpha; IP-10; MCP-1; MCP-3; MIP-1 alpha; MIP-1 beta; MIP-2; RANTES; Eotaxin; IFN alpha; IL-15/IL-15R; IL-28; IL-31; IL-1 alpha; IL-3; G-CSF; LIF; ENA-78/CXCL5; and M-CSF. All samples were measured in duplicate and the mean values of the two reads were calculated and used in subsequent statistical analysis. Data are presented as pg cytokine/chemokine per mg total protein for the brain lysates.
All data are presented as mean ± SEM. Two-way ANOVA (two-tailed) was used to compare groups with variables “genotype” and “age” or “genotype” and “brain region”, if not indicated otherwise. Bonferroni test was used to correct for multiple comparisons. Statistical significance was set at p < 0.05. Precise statistical data are reported in the Figure legends.
α-Synuclein pathology and aging of PLP-α-syn mice
Analysis of α-syn protein levels in subregions of the MSA mouse brain revealed significantly lower levels of α-syn in the forebrain as compared to midbrain, cerebellum and lower brainstem at all ages (Fig. 2c). Between 2 and 12 months of age, the lower brainstem showed significantly higher levels of α-syn protein expression as compared to all other regions, but this difference to midbrain and cerebellum was lost at 18 months of age (Fig. 2c). The midbrain was the only region that showed a significant age-related increase in the level of α-syn protein expression with aging between 12 and 18 months (p < 0.05), while the other regions showed no significant age-related changes (Fig. 2c). We also examined by Western blotting relative α-syn expression in the striatum, SN, hippocampus, lower brainstem and cerebellum in MSA and control mice, at 2 and 12 months of age. MSA mice showed at all ages significantly higher levels of α-syn than the controls, with the highest levels of α-syn expression in lower brainstem, as observed also in the ELISA. However, we found no indication of age-related dynamics in any of the studied regions using this technique (Fig. 2d).
Progression of motor deficits in PLP-α-syn mice
In order to identify any behavioural phenotypes induced by the oligodendroglial overexpression of α-syn, we used a battery of tests, which revealed progressive motor defects in the PLP-α-syn mice.
Age-linked motor deterioration in the PLP-α-syn mice was detected between 2 and 6 months of age with the beam test (increased beam crossing time at 6 months, p < 0.01, Fig. 3c). At 12 months of age, the PLP-α-syn mice showed significant age-related deterioration in both beam crossing and pole test (Fig. 3a-d). In comparison, up to 12 months of age the control mice showed no aging changes in their motor performance with any of the applied tests (Fig. 3). Finally, at 18 months of age, both control and transgenic mice had significant motor deterioration; however, it was much more prominent in the PLP-α-syn mice. In the control group, age-related change was identified only by the beam walking test (Fig. 3d) and by the analysis of the grip strength (Fig. 3h). In comparison, PLP-α-syn mice at 18 months of age showed aging deterioration in all the applied tests (pole test, Fig. 3a,b; beam walking, Fig. 3c, d; gait analysis, Fig. 3f, g, and grip strength, Fig. 3h). The only parameter that remained stable over time in both control and PLP-α-syn mice appeared to be the stride length (Fig. 3e).
Progression of neuronal loss in PLP-α-syn mice
Next, we assessed the number of DARPP-32-positive neurons in the striatum and identified significant loss in PLP-α-syn mice as compared to controls at 12 months and 18 months of age (p < 0.001, Fig. 4c). While mild age-related loss of DARPP-32-positive striatal neurons was seen in controls (2 vs 12 months, p < 0.05), striatal neuronal loss in PLP-α-syn mice occurred earlier (2 vs 6 months of age, p < 0.05) and persisted later on (2 vs 12 months of age, p < 0.001 and 2 vs 18 months of age, p < 0.001).
We identified age-related Purkinje cell loss in PLP-α-syn mice after 6 months of age (6 vs 12 months, p < 0.05 and 6 vs 18 months, p < 0.05, Fig. 4d). Control mice showed a similar trend without reaching significance. No significant differences between PLP-α-syn mice and controls were detected at any of the studied ages in Purkinje cells’ numbers (Fig. 4d).
We did not observe significant differences in the number of neurons in the PN between PLP-α-syn mice and controls at any of the studied ages (Fig. 4e). We identified similar degree of age-related neuronal loss at the age of 18 months in the PN in both PLP-α-syn mice and controls (6 vs 18 months, respectively p < 0.001 and p < 0.01).
Finally, in the IO, age-related neuronal loss was evident in both controls (2 vs 12 months, p < 0.05, 2 vs 18 months, p < 0.001, and 6 vs 18 months, p < 0.01) and PLP-α-syn mice (2 vs 12 months, p < 0.001, 2 vs 18 months, p < 0.001, 6 vs 12 months, p < 0.001, and 6 vs 18 months, p < 0.001, Fig. 4f). Interestingly, a transient significant difference in the neuronal number in IO between PLP-α-syn mice and controls was detected at 12 months of age (p < 0.05), suggesting an accelerated aging in the presence of oligodendroglial α-syn (Fig. 4f).
Region-specific progression of microglia activation in PLP-α-syn mice
Since microglia may respond to a neurodegenerative process without modifying their number, but instead undergoing a significant change in profile, counting and morphological profiling of Iba1-positive cells were performed simultaneously. To classify the activation profile we adapted a scale previously described for rats and monkeys [3, 48]. Microglia cells were rated to type A, “resting” (homeostatic), B hyper-ramified, C hyper-trophic, or D ameboid, according to the appearance of their processes, nucleus and cell body (Fig. 5b). Thereafter we analysed the percentage of each type in the total Iba1-positive population in each group and area.
In the SN of control mice, the Iba1-positive population was mostly represented by type A and B microglia, with virtually no C or D type microglia detected in this area. We observed no major redistribution in the activation subtypes of microglia with age, except for a mild reduction of Type A (p < 0.003) with a shift towards the Type B phenotype at 15 months of age (Fig. 5c). In contrast, in SN of PLP-α-syn mice, the presence of the type C and D became apparent at 5 months of age and the percentage of the activated subtypes (B, C and D) showed a significant increase (p < 0.003 at 15 vs 2 months of age) in parallel to the significant reduction of homeostatic microglia (type A) at the age of 5 and 15 months (for both p < 0.003 as compared to 2 months of age; Fig. 5c). Respectively, there was a significant increase of the activated microglia subtypes (B, C and D) in SN of PLP-α-syn as compared to control mice at 5 and 15 months of age (Additional file 1: Table S1 and Table S3).
In PN there was a clear shift from homeostatic (type A) to activated (Type B, C, D) microglia at the age of 15 months (Fig. 5e), with no significant differences between control and MSA mice (Additional file 1: Table S1 and Table S3). A similar picture was identified in the IO. A clear shift towards activated phenotypes of microglia was seen at 15 months of age, which was more prominent in control than in PLP-α-syn mice (Fig. 5f).
In order to characterize the phenotypic response of the microglia, we analysed the expression of MHCII and CD68 by immunohistochemistry in the selected brain regions. While Iba-1 is constitutively expressed in all microglia, MHCII and CD68 expression is upregulated during α-syn induced neurodegeneration . MHCII is related to antigen processing, and it therefore confers antigen presenting cell identity to the microglia. Our analysis showed that only very few, single MHCII-positive cells are present in the brains of 5- and 15-months-old PLP-α-syn mice (data not shown). On the other hand, CD68 expression is considered an indicator of phagocytic activity of microglia [68, 76]. This microglial lysosomal protein showed typical distribution in an intracytoplasmic dot-like pattern, consistent with the labelling of lysosomes within microglia (Fig. 6a). Furthermore, CD68 immunostaining revealed increased levels of microglial phagocytic activity in the SN of PLP-α-syn mice at 5 months of age, which further extended in all the studied regions at 15 months of age in the PLP-α-syn brain. In contrast, in healthy age-matched mice, only few or none CD68-positive cells were identified (Fig. 6a).
To further characterize the immune response in the PLP-α-syn mice, we used a multi-panel to analyse levels of 36 cytokines and chemokines in whole brain extracts. A heatmap depicting the overall age-related changes of cytokines/chemokines in control and PLP-α-syn mice showed different aging profiles between the genotypes (Fig. 6b). The analysis revealed age-related increase in the levels of CCL3 (MIP-1alpha), CCL5 (RANTES) and the macrophage colony stimulating factor (M-CSF) in PLP-α-syn mouse brains, reaching significant difference from age-matched controls at 15 months of age (Fig. 6c-e). The brain concentration of the remaining analytes showed no significant effect of either genotype or age (Additional file 1: Table S2).
Since the neuroinflammatory response may be related to astrogliosis in the advanced stages of the disease we wanted to address this feature in the neuropathology of the PLP-α-syn mouse too. We found age-related increase of GFAP OD in both control and transgenic mice, however no significant increase of astroglial activation was evident in the presence of oligodendroglial α-syn pathology up to 18 months of age in the MSA mice (Additional file 1: Figure S1).
Region-specific changes of neurotrophic support in PLP-α-syn mice
No evidence of myelin dysfunction in symptomatic PLP-α-syn mice
As robust indications of neurodegeneration and motor dysfunction were detected in PLP-α-syn mice at the age of 12 months, we performed histological and biochemical analysis of myelination at this age. No demyelinated lesions were seen with classical luxol fast blue staining (data not shown). There was no significant difference in MBP, MOG and p25α protein expression levels between hemibrains of PLP-α-syn mice and healthy controls as measured by western blotting (Additional file 1: Figure S2), suggesting that the overexpression of α-syn in oligodendrocytes under the PLP promoter did not have any significant early impact on the production of myelin proteins in this model, and could hardly be causative for the early neurodegeneration occurring in the PLP-α-syn brain long before the age of 12 months.
Relevance of the PLP-α-syn mouse phenotype to human MSA clinical presentation and neuropathology: Insights into disease progression
Previous studies in the PLP-α-syn transgenic mouse model of MSA have identified prominent GCI-like pathology , loss of dopaminergic neurons in SNc [18, 54, 57, 58], early microglial activation , and motor deficits [18, 57]. Furthermore, MSA-like non-motor features including neurogenic bladder dysfunction , cardiovascular autonomic failure [35, 61], breathing variability , and REM sleep behaviour disorder  have been reported in the PLP-α-syn mouse in relation to neurodegeneration affecting selected brainstem nuclei including the laterodorsal tegmental nucleus, pedunculopontine tegmental nucleus, nucleus ambiguus, the pontine micturition centre, raphe nuclei, as well as centres in the spinal cord including the parasympathetic outflow in the intermediolateral columns and the Onuf’s nucleus. The objective of the current study was to characterize the motor phenotype and its underlying neuropathology in aging PLP-α-syn mice. Here we report progression of motor deficits with first mild signs at 6 months of age and further deterioration and robust detection of decline versus control mice at 12 and 18 months of age. Therefore, the functional phenotype of the PLP-α-syn transgenic mouse replicates the natural history of MSA with early non-motor symptoms like neurogenic bladder dysfunction and REM sleep behaviour disorder followed by a progressive motor syndrome . The PLP-α-syn mouse model gave us the unique opportunity to follow the onset and progression of neuropathological events that underlie the MSA-like phenotype with aging.
Insights into the mechanisms of region-specific MSA-P-like neurodegeneration
In search of the mechanisms that may underlie selective SND in the PLP-α-syn mouse, we addressed several possible candidates, including α-syn protein species and levels, oligodendroglial dysfunction, trophic support and neuroinflammation.
Oligomeric α-syn and selective microglial activation as triggers of SND
We identified, by both histological and biochemical analyses, region-specific differences in the level of human α-syn expression in the PLP-α-syn brain, with highest protein levels in the brainstem. These region-specific differences can be explained with the typical caudal-to-rostral spatial distribution of PLP, with highest expression in the adult brain in the hindbrain, midbrain and the white matter tracts . However, the region-specific levels of α-syn in the PLP-α-syn transgenic mouse cannot account for the selective neuronal loss observed in the striatonigral region, but the relative sparing of the olivopontocerebellar pathways. Age-related changes in the solubility and oligomerization of α-syn were further detected in the brains of PLP-α-syn mice. For the first time we report here an increase in the TX-soluble oligomeric α-syn species between 2 and 6 months that remains stable over the further lifespan of the animals. Interestingly, the time of oligomeric α-syn increase and dopaminergic nigral loss coincides. Therefore, the greater toxicity of oligomeric forms may contribute to the initiation rather than the progression of the neurodegenerative process in the PLP-α-syn mouse, as previously suggested in PD models [44, 73]. Despite the cell-to-cell transfer, only oligodendroglial aggregates, but no actual accumulation of α-syn in neurons was identified in the PLP-α-syn brain, suggesting that the MSA-P-like selective neuronal loss is not dependent on specific intra-neuronal accumulation of α-syn, and other mechanisms might be responsible for the progressive disease phenotype.
The PLP-α-syn mouse presents with significant microglial activation that accompanies the α-syn accumulation in oligodendrocytes [57, 58], similar to human MSA [29, 45]. The heterogeneous nature of microglia within the brain has been recently shown using single cell and population genetic analysis [12, 38]. Our current results demonstrate that SN microglia shows the strongest and earliest response to the α-syn overexpression in the PLP-α-syn mouse. Both Iba1 morphological profiling and CD68 immunohistochemistry point towards SN-specific responses of microglia that may mediate early neuronal loss in the region. Indeed, the selective vulnerability of SN dopaminergic cells to inflammatory events has been long proposed [25, 62] and corroborated in this study. The causative role of the α-syn-triggered microglial activation for the nigral neuronal loss in the PLP-α-syn mouse is supported by previous data demonstrating that early suppression of microglial activation between 2 and 4 months of age can rescue nigral dopaminergic neurons in these mice . Furthermore, we observed increased levels in M1-associated chemokines: CCL3/MIP-1a and CCL5/RANTES and the latter has been recently shown to have a key role in dopaminergic toxicity . However, we also found increased M-CSF, a cytokine associated to M2 signalling in macrophages , which suggests a complex ongoing inflammatory process and disrupted balance of immune signals being essential for neuronal survival. These data seem to further support the dual role of microglial activation which we and others have previously discussed [15, 16, 54, 66]. The fine balance between the beneficial (clearance of α-syn) and detrimental effects (pro-inflammatory toxic signalling) of microglial activation may interfere with the degenerative process and may present an important target to selectively modulate disease progression in MSA and other synucleinopathies. On a side note, astrogliosis was not found to be a major contributor to the genotype-specific neuroinflammatory profile of the PLP-α-syn mouse (Additional file 1: Figure S1) suggesting that astrogliosis may only represent a late event of the disease progression, but not a strong contributor of early disease progression.
We also observed progressive age-related changes of microglia, irrespective of the genetic background of the animal indicative of microglia senescence . However, in the PN and IO of PLP-α-syn mice, the additional ongoing disease process seems to interfere with the proliferative activity and possibly the normal function of microglia. The increased exposure to α-syn oligomers and/or the decrease of GDNF and BDNF in the area may contribute to this specific change in the senescent chronically activated microglia of PLP-α-syn mice. Intriguingly, a recent study showed phagocytic defects of macrophages towards oligomeric α-syn in parallel to stronger pro-inflammatory response related to aging . The relevance of disrupted senescence of microglia has not been addressed to date in human α-synucleinopathies, whereas all experimental data summarized here point towards the importance of this pathogenic factor. Furthermore, knowledge on the changes in microglia senescence in α-synucleinopathies may give an explanation of the failure of clinical trials which target microglial activation in these disorders [11, 39, 40].
Disrupted trophic support or dysmyelination cannot explain SND in the PLP-α-syn mouse
Ubhi et al. suggested decreased neurotrophic factors as a candidate mechanism of neurodegeneration in MSA . In the PLP-α-syn mouse we observed significant reductions of BDNF in the lower brainstem (including pons and medulla oblongata - the region with highest α-syn protein expression in this model), but not in the midbrain and the degenerating SN of these mice. Therefore, neurotrophic changes do not seem to be accountable for the early nigral dopaminergic loss in this model. It is plausible that the observed early neurotrophic deficits in the lower brainstem (pons and medulla) of PLP-α-syn mice are responsible for the neuronal loss in central autonomic nuclei linked to the non-motor phenotype, including loss of cholinergic neurons in the nucleus ambiguus, the laterodorsal tegmental nucleus, and the pedunculopontine nucleus, and glutamatergic neurons of the Barrington’s nucleus (the pontine micturition centre) [7, 35, 61]. However, the trophic factor deficit in the lower brainstem of the PLP-α-syn mice does not trigger neuronal loss in the PN (griseum pontis) projecting predominantly to the cerebellum and involved in the control of motor activity .
Finally, demyelination is not typically found in the PLP-α-syn model featuring SND in contrast to the MBP-α-syn mouse model characterized by neuronal loss in the neocortex . Although principally based on a similar approach –the targeted overexpression of human full-length α-syn in oligodendrocytes-, the two MSA models differ in phenotype and selectivity of the neurodegenerative process. The PLP-α-syn mouse represents a model of typical MSA-P with SND and neuronal loss in non-motor brainstem centres of cardiovascular, micturition, respiration and sleep control, linked to changed microglial responses in the basal ganglia and deficient neurotrophic support in the lower brainstem. In contrast, the MBP-α-syn mouse presents with axonal degeneration in the basal ganglia, brainstem and cerebellum linked to widespread demyelination and neuronal loss in the cortex, associated with neurotrophic deficits. In summary, the two models represent the heterogeneous pathology of MSA and suggest that dependent on the α-syn-triggered secondary pathology (microglial activation, demyelination), variable disease phenotypes may arise.
The authors are grateful to Ms. Monika Hainzer for the excellent technical assistance in performing part of the immunohistochemical stainings and the ELISA measurements of α-syn, to Ms. Julia Kuen for supporting the performance of the motor phenotyping, and to Ms. Carlijn Borm for supporting the performance of the neuronal counts. The confocal microscopy was performed at the Biooptics Core Facility of the Medical University of Innsbruck.
The study was supported by grants of the Austrian Science Fund (FWF) W01206–08, F4404, F4414, and P25161, by a grant of the European Community’s Seventh Framework Programme (FP7/2007–2013) under agreement n 603,646 (Multisyn), and by a grant of the Swedish Parkinson Foundation (to MAC). VR received a fellowship from the Network of European Neuroscience School to perform the experiments included here.
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