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Alleviating toxic α-Synuclein accumulation by membrane depolarization: evidence from an in vitro model of Parkinson’s disease
Molecular Brain volume 13, Article number: 108 (2020)
Parkinson’s disease (PD) is characterized by the formation of toxic, fibrillar form alpha-synuclein (α-Syn) protein aggregates in dopaminergic neurons. Accumulating evidence has shown a multifactorial interplay between the intracellular calcium elevation and α-Syn dynamics. However, whether membrane depolarization regulates toxic α-Syn aggregates remains unclear. To understand this better, we used an in vitro α-Syn preformed fibrils (PFF) model of PD in human neural cells. We demonstrated functional membrane depolarization in differentiated SH-SY5Y cells induced by two independent treatments: high extracellular K+ and the GABAA receptor blocker picrotoxin. We then observed that these treatments significantly alleviated toxic α-Syn aggregation in PFF-treated SH-SY5Y cells. Moreover, clinically relevant direct current stimulation (DCS) also remarkably decreased toxic α-Syn aggregation in PFF-treated SH-SY5Y cells. Taken together, our findings suggest that membrane depolarization plays an important role in alleviating PFF-induced toxic α-Syn aggregates, and that it may represent a novel therapeutic mechanism for PD.
Parkinson’s disease (PD) is characterized by the formation of insoluble toxic alpha-synuclein (α-Syn) protein aggregates called amyloid fibrils in dopaminergic neurons [18, 19, 21, 38, 54]. α-Syn is a small soluble protein that concentrates at presynaptic terminals throughout the brain [8, 51]. Under physiological conditions, α-Syn monomers facilitate neurotransmitter release through modulating synaptic vesicle maturation and release [6, 19, 44]. However, these soluble α-Syn monomers are prone to undergoing posttranslational modifications under pathological conditions and consequently, form insoluble toxic α-Syn oligomers and fibrils . Toxic α-Syn fibrils aggregate into Lewy bodies and Lewy neurites which represent the key trigger for the onset of synapse deconstruction and subsequent neurodegeneration [5, 18, 43]. Understandably, targeting the mechanisms regulating and clearing toxic α-Syn aggregation has represented a promising disease-modifying strategy for PD treatment [23, 38, 51].
Previous studies using in vivo animal models and in vitro cell culture systems suggest an important role of depolarization-induced disruption of calcium homeostasis in α-Syn monomer secretion and aggregation . In fact, even transient elevation of intracellular calcium by increasing neuronal activities in vivo  and in vitro [17, 35] can stimulate the secretion of physiological α-Syn monomers in neurons. On the other hand, in the context of cells overexpressing α-Syn, membrane depolarization leads to an increase in α-Syn aggregation [15, 34]. Thus, it seems that a multifactorial interplay occurs between the intracellular calcium levels and α-Syn dynamics. However, how intracellular toxic α-Syn fibril accumulation is affected by membrane depolarization or the disruption of calcium homeostasis under pathological conditions is completely unknown.
With aggregation, α-Syn fibrils can have toxic consequences, leading to neuronal loss and characteristic PD pathology [9, 26, 30, 51]. To better understand the relationship between membrane depolarization and pathological α-Syn accumulation, we have used an in vitro α-Syn Preformed fibrils (PFF) model of PD in human neural cells. We first assessed whether functional membrane depolarization, induced by treatment of high extracellular K+ or GABAA receptor blocker, would alleviate aggregation and promote clearance of toxic α-Syn in PFF-treated SH-SY5Y cells. Secondly, we determined whether clinically relevant direct current stimulation (DCS) could decrease α-Syn aggregation in PFF-treated SH-SY5Y cells. Our findings indicate that these depolarizing treatments did indeed prevent α-Syn pathological aggregation through promoting α-Syn secretion into extracellular medium. This points to the fundamental importance of neuronal activity state in the processing of α-Syn and hence, could lead to the development of novel clinical strategies for PD.
SH-SY5Y cells, a human neuroblastoma cell line, were maintained in Dulbecco’s Modified Eagle Media (DMEM) supplemented with 10% fetal bovine serum (FBS) and 1% penicillin/streptomycin (pen-strep) at 37o in a humidified 90% air and 5% CO2 incubator. Cells were plated at a density of 1 × 105 cells/well in cell media, in either flat-bottomed 96 well plates (100 μL/well) for immunohistochemistry, or 24-well plates with coverslips (500 μL/well) for electrophysiology and live-cell imaging. 24-well plates were coverslipped and coated with Poly-D-Lysine (PDL) and Laminin (LM) at 1:1000 in DMEM for 2 h in incubator before plating. Cells were cultured for 2 weeks in complete media (DMEM supplemented with 10% FBS and 1% pen-strep) (week 1) or reduced media (DMEM supplemented with 1% FBS and 1% pen-strep) (week 2) supplemented with 0.1% retinoic acid (RA). Half-media changes were performed every 2 days.
Whole-cell patch clamp recordings
Differentiated SH-SY5Y cells were collected from 24-well culture plates at 2–3 weeks in culture. Before cells were transferred to the recording chamber under an upright Nikon Eclipse FN1 microscope, culture medium was gradually changed to oxygenated artificial cerebral spinal fluid (ACSF) containing (mM): 124 NaCl, 5 KCl, 1.25 NaH2PO4, 1.2 MgSO4, 26 NaHCO3, 2 CaCl2, and 10 glucose, in 30 mins at room temperature. Whole-cell patch clamp recordings were obtained from differentiated neurons at 2–3 weeks following the initiation of the differentiation procedure . Patch electrodes with a resistance of 5–10 MΩ were prepared from borosilicate glass capillaries with a Narishige micropipette puller (Model PC-100, Tokyo, Japan). Pipette intracellular solution contains (mM): 130 K-Gluconate, 2 MgCl2, 0.6 EGTA, 10 HEPES, 5 KCl, 2 ATP-Mg(Na2), pH 7.3. Data were collected using MultiClamp 700B amplifier. To evoke action potentials in these differentiated SH-SY5Y cells, depolarizing rectangular pulses of 500 ms duration (10pA/step) were applied. Signals were filtered at 2 kHz, digitized at 20 kHz by a Digidata 1500 interface, acquired by the pClamp 10.7 software, and analyzed with the Clampfit 10.7 program (Molecular Devices).
Live cell voltage sensitive dye imaging
As mentioned above, culture medium was gradually changed to oxygenated ACSF containing (mM): 124 NaCl, 5 KCl, 1.25 NaH2PO4, 1.2 MgSO4, 26 NaHCO3, 2 CaCl2, and 10 glucose, in 30 mins before the start of the fast voltage-sensitive dye (Di-4-ANEPPS, Biotium, CA) staining procedure. Cells were stained with 0.2 mM Di-4-ANEPPS for 30 min in the incubation chamber and then transferred into the recording chamber. Imaging was performed at room temperature. Excitation light emitted by a shuttered green LED (LEX2, Brainvision, Tokyo, Japan) was reflected toward the cells through an excitation filter (531 nm wavelength). Emitted fluorescence signals passed through an absorption filter (580 nm wavelength) was imaged (0.5 ms frame rate; 6–8 min time lapse period) by a MiCam05 CMOS-based camera (SciMedia) with a Leica Plan APO 5x objective (NA: 0.5, Leica Microsystems, Wetzlar, Germany). The imaging data were acquired and analyzed using Brainvision Analysis Software (Brainvision). Fluorescence intensity changes (∆F/F) were normalized to baseline fluorescence recorded during the initial 10 ms of each recording and represented by pseudo-colors. Red color indicated a membrane depolarization, while blue color indicated a membrane hyperpolarization.
Preparation of fibrils
Human α-Syn monomer protein for making pre-formed fibrils (PFFs) (1 mg aliquots, Proteos, cat. RP003) were generated over a seven-day period. Aliquots were thawed on ice for approximately 3 h. Once thawed, aliquots were centrifuged at 4 °C and 14.8 RPM. The supernatant was obtained and transferred into an autoclaved 1.5 mL microcentrifuge tube. Protein concentration of each aliquot was determined by a NanoDrop 2000 Spectrophotometer using the A280 protein method. 2 μL of 10x DPBS was used as a blank, followed by 2 μL of sample. Beer’s law was used to measure concentration (ε = 5960; kDa = 14.6). PFFs were diluted into 10x DPBS for a final concentration of 5 mg/mL. Tubes were vortexed for 3 s and lids were locked to prevent opening during the shaking process. Tubes were placed in an Eppendorf Thermomixer R at 37 °C. PFFs were shaken for 7 days (168 h) at 1000 RPM. Following shaking period, PFFs were aliquoted into 25 μL samples using gel loading pipet tips. Aliquots were frozen on dry ice and stored at − 80 °C until use in experiments.
Cells were exposed to PFFs (25 μg/ml), TTX (1 μM)), Picrotoxin (100 μM) or KCL (10 mM) alone or in combination in order to modulate cell activity. α-Syn PFFs were sonicated in pulses at approximately 1 pulse/second for 60 s before use. In some experiments, cultures we pre-treated with TTX, Picrotoxin or KCL for one hour at 37 °C and 5% CO2, then PFFs for 3 days. Cells were also co-incubated with TTX, Picrotoxin, KCL and/or PFFs for 3 days. Each experiment was performed in triplicate.
In vitro direct current stimulation (DCS)
DCS was delivered to cells in each well of a custom-built 24-well culture plate (see Fig. 4a-c) through two L-shaped Ag/AgCl electrodes (0.5 mm diameter, Sigma, Oakville, ON) that were submerged in culture medium and connected to a Grass s8800 stimulator with a constant-current stimulus isolation unit (Grass Instrument Co., USA). Before each use, electrodes were sterilized using 70% ethanol for 15–20 min and washed with sterile culture medium. The stimulation intensity was set to achieve 50 mV/mm electric field for 40 mins and was applied following the 3-day incubation with PFFs. Immunohistochemistry, cell viability, and ELISA evaluation were performed 24 h after the DCS.
To measure the amount of α-Syn found extracellularly in cell culture medium, a sandwich ELISA kit (AnaSpec, Fremont, CA) was used. Following treatments, 300 μL per well of whole cell media was collected in duplicates from SH-SY5Y cells and stored at -80 °C until use. Samples were thawed, vortexed, and 100 μL of each diluted sample and standard was applied to microtiter plates pre-coated with anti-α-Synuclein monoclonal antibodies. Then, a detection antibody (Rabbit Polyclonal anti-α-Synuclein IgG-HRP, 10 μg/50 μl) was applied. After a four-hour incubation, wells were aspirated and washed with 350 μl/well of 1x wash buffer 6 times. Each wash included a 10 s lag time and was dried by inverting the plate and hitting it until no moisture appeared. The substrate was added and incubated at room temperature until a blue gradient was clearly observed (approximately 10 min). The colour reaction was measured using a Molecular Devices SpectraMax microplate reader at 450 nm within 20 min of adding the stop solution. The software (Soft-Max Pro) was used to create a standard curve and calculate the concentration of α-Syn in the samples.
Evaluation of cell viability
To ensure the toxins and DCS were modulating cell activity without causing substantial cell death, a cytotoxicity assay was used. Cells that were incubated with fibrils alone or in combination with TTX, Picrotoxin or KCL for 3 days as well as DCS treated cells were analyzed. After incubation, cells had all media removed and replaced with complete media containing 2 drops/mL Hoeschst33342 (NucBlue™ live cell stain) and SYTOX (NucGreen™ dead cell indicator) (Invitrogen, Carlsbad, CA, USA). The plate was incubated at 37 °C with 5% CO2 for 15 min then imaged using the EVOS FL Imaging System (Invitrogen, Carlsbad, CA, USA). The counted nuclei of both dead (green) and live (blue) cells were averaged for six replicates and presented as a percentage of dead/live cells.
Cells were fixed with 4% PFA in PBS for 15 min, then washed 3 × 5 minutes in PBS. Next, the cells were blocked with 2% BSA + 0.1% Triton-X in PBS for 30 min. The cells were subsequently incubated with anti-alpha synuclein filament antibody (1:1000, Abcam, Cambridge, MA, USA) which is a conformation specific antibody and specifically detects alpha-synuclein filaments or an anti-GABAA receptor alpha 1 (Abcam, Cambridge, MA, USA) primary antibody at 1:250 in 0.1% BSA in PBS. Cells were washed 3 × 5 minutes in PBS, after which they were labelled with Alexa 488 anti-rabbit antibodies (Invitrogen, Carlsbad, CA, USA) at 1:1000 for 30 min at room temperature in 0.1% BSA in PBS. Cells were washed 3 × 5 minutes in PBS then imaged using the EVOS FL Imaging System (Invitrogen, Carlsbad, CA, USA).
Fibril formation was analyzed as total intensity using Image J (NIH). 30 cells were randomly selected per experimental condition, and total intensity was measured based on cell area and background. All evaluation and analysis were performed blindly.
Data analysis and statistics
All experimental data are presented as mean ± standard error (S.E.M). Data were first analyzed for normality using the Shapiro-Wilk test and for equal variance using Levene’s method. The two-tailed unpaired or paired t test was performed for two-group comparisons. A one-way ANOVA followed by Tukey’s HSD post hoc tests was used for multi-group comparisons. Statistical significance was considered at p < 0.05.
Preformed fibrils (PFF) treatment induced α-Syn inclusion accumulation in differentiated SH-SY5Y cells
In order to test the effects of membrane depolarization on α-Syn accumulation, we first added 0.1% RA to the culture medium for two weeks to differentiate the SH-SY5Y neuroblastoma cells. Consistent with previous studies [16, 22, 47], differentiated SH-SY5Y cells showed a variety of neuron-like phenotypes including long neurites and complex network connections (Fig. 1a1). Furthermore, whole-cell current clamp recordings demonstrated that while no spontaneous action potentials were detected, appropriate depolarizing current injections could evoke overshooting action potentials in differentiated SH-SY5Y cells (Fig. 1a2). We next proceeded to treat the differentiated SH-SY5Y cells with different concentrations (5, 10, and 25 μg/ml) of PFFs or vehicle for 3 days, and subsequently, evaluated α-Syn accumulation (Fig. 1e and f). The PFF treatments induced significant increases in α-Syn accumulation (5 μg/ml: 13.36 ± 5.89, n = 19, p < 0.001; 10 μg/ml: 27.58 ± 6.15, n = 19, p < 0.001; 25 μg/ml: 34.70 ± 6.47, n = 20, p < 0.001) compared to control cells (6.92 ± 2.44, n = 20). α-Syn accumulation appeared to increase with PFF concentrations and peaked in 25 μg/ml PFF-treated SH-SY5Y cells (25 μg/ml vs 5 μg/ml: p < 0.001; 25 μg/ml vs 10 μg/ml, p < 0.001). In addition, PFFs (25 μg/ml) did not cause a significant change in resting membrane potentials (RMPs), but there was a trend towards hyperpolarization (− 46.7 ± 3.2 mV, n = 10, p = 0.18) compared to control SH-SY5Y cells (− 42.3 ± 1.3 mV, n = 13, Fig. 1c. This was associated with an increase in the action potential threshold in PFF-treated SH-SY5Y cells (PFF: 18.0 ± 2.2 mV, n = 6 vs Control: − 23.9 ± 1.6 mV, n = 10, p = 0.049, Fig. 1d). These results suggest that 3-day PFF treatment induced significant pathological α-Syn accumulation in differentiated SH-SY5Y cells.
Membrane depolarization significantly reduces α-Synuclein fibril accumulation in differentiated SH-SY5Y cells
We next sought to assess the effects of membrane depolarization on α-Syn fibril accumulation in differentiated SH-SY5Y cells. To achieve membrane depolarization, we employed two independent strategies rather than simply one in order to avoid possible stimulation-specific effects. 1) By increasing extracellular K+ concentration in the culture medium through addition of 10 mM KCL. Fast voltage-sensitive dye imaging of Di-4-ANEPPS-loaded SH-SY5Y cells confirmed high extracellular K+-induced membrane depolarization (Fig. 2a, n = 5). 2) Blockade of the inhibitory GABAA receptors by specific inhibitor Picrotoxin (100 μM) was applied to depolarize the cell membrane. Immunohistochemistry with an antibody against GABAA receptor α1subunit confirmed the expression levels of GABAA receptors in differentiated SH-SY5Y cells (Fig. 2b, n = 4). Consistent with the expression of GABAA receptors, fast voltage-sensitive dye imaging showed GABAA receptor inhibitor Picrotoxin evoked membrane depolarization in differentiated SH-SY5Y cells (Fig. 2c, n = 4). These results provide functional evidence of KCL and Picrotoxin induced membrane depolarization in differentiated SH-SY5Y cells.
We then examined whether these treatments affect α-Syn fibril accumulation in differentiated SH-SY5Y cells. The effects were evaluated by quantifying the integrated density of α-Syn fibril immunostaining. After 72 h of treatment with 100 μM Picrotoxin or 10 mM KCL in combination with 25 μg/ml PFFs, the accumulation of α-Syn fibrils in differentiated SH-SY5Y cells significantly decreased by 30.98% (PFF + Picro: Integrated Intensity 26.77 ± 1.03, n = 30, p < 0.0001) and 34.96% (PFF + KCL: Integrated Intensity 28.03 ± 1.21, n = 30, p < 0.0001), compared to the PFF-only group (Integrated Intensity 36.92 ± 1.58, n = 30, Fig. 3a-c). Furthermore, after 1 h pre-treatment with 100 μM Picrotoxin or 10 mM KCL followed by 72 h treatment with 25 μg/ml PFFs, the accumulation of α-Syn fibrils in differentiated SH-SY5Y cells also significantly decreased by 43.61% (Picro then PFF: Integrated Intensity 20.82 ± 1.14, n = 30, p < 0.0001) and 36.85% (KCL then PFF: Integrated Intensity 22.74 ± 1.35, n = 30, p < 0.0001), respectively, compared to the PFF-only group (Fig. 3a-c). In addition, there was a significant difference in the integrated density of α-Syn fibril immunostaining between the group that received combined PFF + Picro, compared to those that first received Picrotoxin followed by PFFs (p = 0.0208); however, no difference was evident between the combined PFF + KCL, compared to those administered KCl and then PFFs (p = 0.9878). Interestingly, consistent with the fact that no spontaneous action potentials were detected in differentiated SH-SY5Y cells, the sodium channel blocker TTX (1 μM) in combination with 25 μg/ml PFFs or 1 h pre-treatment with TTX did not induce significant changes in α-Syn fibril accumulation (PFF + TTX: Integrated Intensity 30.85 ± 1.42, n = 30, p = 0.0692; TTX then PFF: Integrated Intensity 33.02 ± 1.81, n = 30, p = 0.4521), compared to compared to the PFF-only group (Fig. 3a-c). Collectively, these data strongly suggest that membrane depolarization is crucial for eliminating α-Syn fibril accumulation in PFF-treated differentiated SH-SY5Y cells.
Direct current stimulation (DCS) significantly alleviates α-Synuclein fibril accumulation in differentiated SH-SY5Y cells
Given the promising protective effects of KCL/Picrotoxin-induced membrane depolarization in clearing α-Syn fibril accumulation, we further evaluated whether the clinically relevant DCS treatment would induce a similar outcome. To this end, PFF-treated differentiated SH-SY5Y cells were exposed to 0 or 50 mV/mm DCS with constant frequency of 50-100 Hz for 40 mins through L-shape Ag/AgCl electrodes in a custom-built 24-well culture plate (Fig. 4a-c). Using optical fast voltage-sensitive dye imaging, we confirmed that 50 mV/mm DCS evoked robust membrane depolarization in differentiated SH-SY5Y cells as evidenced by robust red fluorescent signals (Fig. 4d-f, n = 4). After 40mins DCS treatment in combination with 25 μg/ml PFFs, the accumulation of α-Syn fibrils in differentiated SH-SY5Y cells significantly reduced by 23.26% (Integrated Intensity 27.28 ± 1.16, n = 106, p < 0.0001, compared to the PFF-only group (Integrated Intensity 35.55 ± 1.28, n = 106, Fig. 4g-h and j). Importantly however, the stimulation intensity of 50 mV/mm did not cause detectable changes in cell morphology or significant long-lasting membrane depolarization after DCS treatment (RMP: before DCS -45.8 ± 2.8 mV, n = 8 vs after DCS -40.5 ± 2.5 mV, n = 8, p = 0.17, Fig. 4i). These results demonstrated a protective effect of DCS on the clearance of α-Syn fibril accumulation in differentiated SH-SY5Y cells.
Membrane depolarization causes the secretion of α-Synuclein fibrils into the extracellular medium in differentiated SH-SY5Y cells
To investigate the mechanism of membrane depolarization induced α-Syn fibril clearance, an ELISA was used determine the total amount of α-Syn in the extracellular medium following membrane depolarization. To this end, the concentration of extracellular total α-Syn in the culture medium was significantly elevated following membrane depolarization evoked by KCL (1547 ± 25.72 pg/ml, n = 4, p < 0.0001), PTX (1618 ± 10.38 pg/ml, n = 4, p < 0.0001) or DCS (1603 ± 9.341 pg/ml, n = 5, p < 0.0001) compared to PFF alone (1316 ± 29.27 pg/ml, n = 4, Fig. 5). Importantly, this coincides with the decreases in intracellular α-Syn fibril accumulation following membrane depolarization (as demonstrated by immunohistochemistry). These results strongly support the notion that membrane depolarization alleviates intracellular α-Syn aggregation, at least in part through promoting α-Syn secretion.
Membrane depolarization does not cause cell death in PFF-treated differentiated SH-SY5Y cells
We next examined whether membrane depolarization-induced elimination of α-Syn accumulation resulted from any changes in cell death. Cytotoxicity was determined by the live/dead ratio calculated through NucGreen™ staining. In PFF only treated (25 μg/ml) differentiated SH-SY5Y cells, the distribution of NucGreen positive cells was very sparse (0.55 ± 0.11%, n = 12). Further, membrane depolarization induced by administration of additional treatment of 10 mM KCL (0.58 ± 0.43%, n = 12, p = 0.99), 100 μM Picrotoxin (0.56 ± 0.51%, n = 12; p = 0.99), 1 μM TTX (0.42 ± 0.41%, n = 12; p = 0.95), or DCS (0.84 ± 0.46%, n = 12, p = 0.50) did not cause significant changes in cytotoxicity compared to the background level seen with PFF only treatment (Fig. 6a and b). Collectively, these results suggest that membrane depolarization-induced changes in α-Syn accumulation were not mediated by treatment induced increases in cytotoxicity in differentiated SH-SY5Y cells.
Widespread toxic α-Syn inclusions are a hallmark of PD pathology [18, 19, 21, 38] and novel methods of inducing clearance of α-Syn aggregation may be a promising potential therapeutic approach [23, 38, 51]. In the present study, using an in vitro α-Syn PFF model of PD in human neural cells, we demonstrated for the first time that membrane depolarization plays an important role in alleviating PFF-induced toxic α-Syn aggregates. We showed that PFF treatment for 3 days reliably induced a robust dose-dependent α-Syn accumulation in differentiated human neural cells. Importantly, functional membrane depolarization induced by either high extracellular K+ or the GABAA receptor blocker significantly alleviated the toxic α-Syn aggregation. We further demonstrated that clinically relevant DCS also remarkably decreased toxic α-Syn aggregation in PFF-treated human neural cells. Furthermore, this membrane depolarization-induced decrease in intracellular α-Syn observed with KCL, PTX and DCS was coupled with an increase in extracellular α-Syn. Importantly, the treatments used in the present study did not induce confounding cell cytotoxicity. Our results provide direct evidence of an important interplay between membrane depolarization and clearance of intracellular α-Syn aggregation.
α-Syn PFFs have been repeatedly shown to initiate Lewy body pathological changes through templating and recruiting endogenous α-Syn to accumulate and form insoluble inclusions in neurons in a variety of PD models [9, 14, 24, 26, 36, 47]. Here, we used an α-Syn PFF model in the differentiated SH-SY5Y cells which have already been extensively used in PD research due to their human-specific proteins , dopaminergic phenotypes [1, 3, 41], and neuronal electrophysiological properties, i.e., overshooting action potentials  (Fig. 1b). Consistent with previous studies [9, 47], our results showed that α-Syn PFF treatment effectively induced endogenous α-Syn inclusions and modulated membrane properties in the differentiated SH-SY5Y cells. Prolonged exogenous PFF treatment for two weeks has previously been reported to lead to neurotoxicity in primary hippocampal neurons . In the present study, to avoid the sustained PFF treatment-induced cell death, a higher concentration (25 μg/ml) of α-Syn PFF was applied for a relatively short period of time (3 days). Under these conditions, toxic α-Syn inclusions were induced with no detectable cell toxicity in either PFF only or PFF in combination with KCL/TTX/Picrotoxin/DCS treated SH-SY5Y cells (Fig. 6), supporting that changes in the levels of α-Syn inclusions were not due to treatment-induced cell death.
An important finding of our study is that functional membrane depolarization has a crucial role in clearing PFF-induced toxic α-Syn aggregation. Previous in vivo and in vitro studies have shown that depolarization or increased neuronal activity can increase the mobility of physiological α-Syn monomers and promote their disassociation from presynaptic membranes and release to extracellular spaces through a Ca2+ dependent mechanism [12, 13, 17, 52]. In undifferentiated human cell lines overexpressing physiological α-Syn monomers, however, a transit (about an hour) elevation of intracellular Ca2+ through the addition of high extracellular KCL or Ca2+ levels can induce an increase in intracellular α-Syn aggregation [15, 34, 40], while this same treatment also promoted the extracellular secretion of α-Syn monomers after longer elevations (6 h) of intracellular Ca2+ in differentiated human neuroblastoma cells . These studies support a potential multifactorial interplay between the intracellular calcium levels and α-Syn dynamics. It is important to note that the high level of α-Syn monomers used in these studies can increase the potential mitochondrial oxidative stress  and the vulnerability of α-Syn aggregation [18, 27] and thus may introduce confounds while evaluating the α-Syn toxicity. Currently, it is still not entirely clear whether membrane depolarization can affect endogenous α-Syn fibrilization during pathological conditions.
In the present study, we used human wild-type PFF-treated human neural cells to seed endogenous α-Syn inclusions without the additional complications of α-Syn overexpression. Two independent pharmacological strategies were used to evoke functional membrane depolarization to avoid the possibility of stimulation-specific effects. We revealed that membrane depolarization evoked by either KCL or PTX for 3 days alleviated the PFF-induced toxic α-Syn aggregates in human neural cells by significantly increasing the secretion of α-Syn into the extracellular media (Figs. 3 and 5). Whether or not the secreted α-Syn has undergone conformational changes will require further investigation. Furthermore, while we found that chronic membrane depolarization for 3 days did not induce detectable cytotoxicity, we cannot exclude the potential possibility of excitotoxicity due to prolonged Ca2+ influx. The time course of depolarization treatment may need to be further optimized to balance any potential excitotoxicity with alterations in the clearance of α-Syn aggregates. Membrane depolarization might enhance the clearance of the toxic α-Syn aggregates by upregulating the expression of heat shock protein 70 (HSP70) and the activation of autophagy, both of which have been shown to promote the clearance of α-Syn inclusions [18, 20, 29, 53]. Interestingly, TTX did not cause a significant change in the amount of α-Syn accumulation regardless of when it was administered. The lack of response seen with TTX is in line with the perspective that SH-SY5Y cells do not show spontaneous action potentials during the resting condition. It is of interest that PFFs have been shown to impair the initiation of synaptogenesis and synaptic function in cultured excitatory hippocampal neurons . This might, in turn, induce further α-Syn fibrilization and synaptic dysfunction resulting in a vicious cycle to promoting toxic α-Syn aggregates in synucleinopathies. Further research is needed to explore the molecular mechanisms mediating the membrane depolarization-induced disaggregation. Although we can not exclude the possibility that our alpha Synuclein filament antibody may label PFFs in addition to endogenous alpha-Syn fibrils, our results clearly demonstrate that membrane depolarization does significantly decrease the levels of intracellular alpha-Syn fibrils (PFF or endogenous alpha-syn fibrils), and importantly, also increased the extracellular secretion of a-Syn. Therefore, membrane depolorization might represent an effective strategy to interfere with the intitiation of synaptic dysfunction-α-Syn fibrilization in PD pathophysiology.
Finally, we induced membrane depolarization by applying an external electrical field using a clinically relevant DCS procedure. Physiological α-Syn contains two structural domains, the N-terminal lipid-binding domain including a hydrophobic NAC (non-amyloid-β component) and the C-terminal domain [4, 28, 31]. Toxic α-Syn fibril formation requires significant α-Syn conformational changes from α-helix to β-sheet to expose hydrophobic NAC, leading to the formation of α-Syn protofibrils and fibrils in neurons [7, 45]. Interestingly, the α-Syn N-terminal is positively charged, while the C-terminal is negatively charged [11, 31, 49]. Therefore, theoretically, an external electrical field could disrupt α-Syn aggregation by aligning α-Syn with induced dipoles following the axis of the electric field or directly interacting with the α-Syn dipoles to induce a β-sheet to α-helix conformational switch [2, 42]. Indeed, using a novel, custom-built 24-well culture plate, we obtained direct evidence for the first time to demonstrate that clinically relevant DCS effectively alleviated the accumulation of PFF-induced toxic α-Syn aggregates in differentiated human neural cells, very much the same as we observed with high extracellular K+ and the GABAA receptor blocker picrotoxin. Interestingly, Electroconvulsive therapy (ECT) has been shown to cause antiparkinsonian effects in patients with advanced PD [32, 33]. Furthermore, we have recently shown that epilepsy was associated with significant improvement in clinical motor symptoms and cognitive decline in PD patients . While the mechanism behind these positive effects remains elusive, our findings suggest this effect may be due in part to the clearing of toxic α-Syn aggregates from dopaminergic neurons and offers beneficial information that could provide therapeutic benefits in controlling PD pathology. Future in vivo studies may wish to investigate the mechanism responsible for the interplay between membrane depolarization and α-Syn fibril clearance and the relationship to clinical improvement.
Overall, employing several novel approaches that utilize a new in vitro α-Syn PFF model of PD, we have shown that membrane depolarization, through provocation of α-Syn fibril secretion, can protect against intracellular accumulation of toxic PFF-induced α-Syn aggregates and importantly, that this occurs in the absence of any cell death. The present data could have important clinical implications for synucleinopathies, specifically PD, and may also help determine a mechanism of action for the accumulation of α-Syn aggregates.
Availability of data and materials
The datasets used and/or analyzed during the current study available from the corresponding author on reasonable request.
Direct current stimulation
Dulbecco’s Modified Eagle Media
Fetal bovine serum
Artificial cerebral spinal fluid
Bovine serum albumin
- GABAA :
γ-Aminobutyric acid type A
Heat shock protein 70
Arun P, Madhavarao CN, Moffett JR, Namboodiri AM. Antipsychotic drugs increase N-acetylaspartate and N-acetylaspartylglutamate in SH-SY5Y human neuroblastoma cells. J Neurochem. 2008;106(4):1669–80.
Baumketner A. Electric field as a disaggregating agent for amyloid fibrils. J Phys Chem B. 2014;118:14578–89.
Biedler JL, Roffler-Tarlov S, Schachner M, Freedman LS. Multiple neurotransmitter synthesis by human neuroblastoma cell lines and clones. Cancer Res. 1978;38(11 Pt 1):3751–7.
Breydo L, Wu JW, Uversky VN. Alpha-synuclein misfolding and Parkinson's disease. Biochim Biophys Acta. 2012;1822:261–85.
Bridi JC, Hirth F. Mechanisms of alpha-Synuclein induced Synaptopathy in Parkinson’s disease. Front Neurosci. 2018;12:80.
Burre J, Sharma M, Sudhof TC. Alpha-Synuclein assembles into higher-order multimers upon membrane binding to promote SNARE complex formation. Proc Natl Acad Sci U S A. 2014;111:E4274–83.
Chandra S, Chen X, Rizo J, Jahn R, Sudhof TC. A broken alpha -helix in folded alpha -Synuclein. J Biol Chem. 2003;278:15313–8.
Chandra S, Gallardo G, Fernandez-Chacon R, Schluter OM, Sudhof TC. Alpha-synuclein cooperates with CSPalpha in preventing neurodegeneration. Cell. 2005;123:383–96.
Chu Y, Muller S, Tavares A, Barret O, Alagille D, Seibyl J, Tamagnan G, Marek K, Luk KC, Trojanowski JQ, et al. Intrastriatal alpha-synuclein fibrils in monkeys: spreading, imaging and neuropathological changes. Brain. 2019;142:3565–79.
Dryanovski DI, Guzman JN, Xie Z, Galteri DJ, Volpicelli-Daley LA, Lee VM, Miller RJ, Schumacker PT, Surmeier DJ. Calcium entry and alpha-synuclein inclusions elevate dendritic mitochondrial oxidant stress in dopaminergic neurons. J Neurosci. 2013;33:10154–64.
Emamzadeh FN. Alpha-synuclein structure, functions, and interactions. J Res Med Sci. 2016;21:29.
Emmanouilidou E, Melachroinou K, Roumeliotis T, Garbis SD, Ntzouni M, Margaritis LH, Stefanis L, Vekrellis K. Cell-produced alpha-synuclein is secreted in a calcium-dependent manner by exosomes and impacts neuronal survival. J Neurosci. 2010;30:6838–51.
Emmanouilidou E, Minakaki G, Keramioti MV, Xylaki M, Balafas E, Chrysanthou-Piterou M, Kloukina I, Vekrellis K. GABA transmission via ATP-dependent K+ channels regulates alpha-synuclein secretion in mouse striatum. Brain. 2016;139:871–90.
Fares MB, Maco B, Oueslati A, Rockenstein E, Ninkina N, Buchman VL, Masliah E, Lashuel HA. Induction of de novo alpha-synuclein fibrillization in a neuronal model for Parkinson’s disease. Proc Natl Acad Sci U S A. 2016;113:E912–21.
Follett J, Darlow B, Wong MB, Goodwin J, Pountney DL. Potassium depolarization and raised calcium induces alpha-synuclein aggregates. Neurotox Res. 2013;23:378–92.
Forster JI, Koglsberger S, Trefois C, Boyd O, Baumuratov AS, Buck L, Balling R, Antony PM. Characterization of differentiated SH-SY5Y as neuronal screening model reveals increased oxidative vulnerability. J Biomol Screen. 2016;21:496–509.
Fortin DL, Nemani VM, Voglmaier SM, Anthony MD, Ryan TA, Edwards RH. Neural activity controls the synaptic accumulation of alpha-synuclein. J Neurosci. 2005;25:10913–21.
Gao J, Perera G, Bhadbhade M, Halliday GM, Dzamko N. Autophagy activation promotes clearance of alpha-synuclein inclusions in fibril-seeded human neural cells. J Biol Chem. 2019;294:14241–56.
Ghiglieri V, Calabrese V, Calabresi P. Alpha-Synuclein: from early synaptic dysfunction to Neurodegeneration. Front Neurol. 2018;9:295.
Hu F, Zhou J, Lu Y, Guan L, Wei NN, Tang YQ, Wang K. Inhibition of Hsp70 suppresses neuronal Hyperexcitability and attenuates epilepsy by enhancing A-type potassium current. Cell Rep. 2019;26:168–81 e164.
Iarkov A, Barreto GE, Grizzell JA, Echeverria V. Strategies for the treatment of Parkinson’s disease: beyond dopamine. Front Aging Neurosci. 2020;12:4.
Ito K, Eguchi Y, Imagawa Y, Akai S, Mochizuki H, Tsujimoto Y. MPP+ induces necrostatin-1- and ferrostatin-1-sensitive necrotic death of neuronal SH-SY5Y cells. Cell Death Discov. 2017;3:17013.
Kalia LV, Lang AE. Parkinson’s disease. Lancet. 2015;386:896–912.
Karampetsou M, Ardah MT, Semitekolou M, Polissidis A, Samiotaki M, Kalomoiri M, Majbour N, Xanthou G, El-Agnaf OMA, Vekrellis K. Phosphorylated exogenous alpha-synuclein fibrils exacerbate pathology and induce neuronal dysfunction in mice. Sci Rep. 2017;7:16533.
Leandrou E, Emmanouilidou E, Vekrellis K. Voltage-gated calcium channels and alpha-Synuclein: implications in Parkinson's disease. Front Mol Neurosci. 2019;12:237.
Luk KC, Kehm V, Carroll J, Zhang B, O'Brien P, Trojanowski JQ, Lee VM. Pathological alpha-synuclein transmission initiates Parkinson-like neurodegeneration in nontransgenic mice. Science. 2012;338:949–53.
Luna E, Decker SC, Riddle DM, Caputo A, Zhang B, Cole T, Caswell C, Xie SX, Lee VMY, Luk KC. Differential alpha-synuclein expression contributes to selective vulnerability of hippocampal neuron subpopulations to fibril-induced toxicity. Acta Neuropathol. 2018;135:855–75.
Luna E, Luk KC. Bent out of shape: alpha-Synuclein misfolding and the convergence of pathogenic pathways in Parkinson’s disease. FEBS Lett. 2015;589:3749–59.
Lyamzaev KG, Tokarchuk AV, Panteleeva AA, Mulkidjanian AY, Skulachev VP, Chernyak BV. Induction of autophagy by depolarization of mitochondria. Autophagy. 2018;14:921–4.
Masuda-Suzukake M, Nonaka T, Hosokawa M, Oikawa T, Arai T, Akiyama H, Mann DM, Hasegawa M. Prion-like spreading of pathological alpha-synuclein in brain. Brain. 2013;136:1128–38.
McClendon S, Rospigliosi CC, Eliezer D. Charge neutralization and collapse of the C-terminal tail of alpha-synuclein at low pH. Protein Sci. 2009;18:1531–40.
Moellentine C, Rummans T, Ahlskog JE, Harmsen WS, Suman VJ, O'Connor MK, Black JL, Pileggi T. Effectiveness of ECT in patients with parkinsonism. J Neuropsychiatry Clin Neurosci. 1998;10:187–93.
Narang P, Glowacki A, Lippmann S. Electroconvulsive therapy intervention for Parkinson's disease. Innov Clin Neurosci. 2015;12:25–8.
Nath S, Goodwin J, Engelborghs Y, Pountney DL. Raised calcium promotes alpha-synuclein aggregate formation. Mol Cell Neurosci. 2011;46:516–26.
Paillusson S, Clairembault T, Biraud M, Neunlist M, Derkinderen P. Activity-dependent secretion of alpha-synuclein by enteric neurons. J Neurochem. 2013;125:512–7.
Panattoni G, Rota L, Colla E. Exogenous Administration of Microsomes-associated Alpha-synuclein Aggregates to primary neurons as a powerful cell model of fibrils formation. J Vis Exp. 2018;136:57884.
Peng C, Gathagan RJ, Covell DJ, Medellin C, Stieber A, Robinson JL, Zhang B, Pitkin RM, Olufemi MF, Luk KC, et al. Cellular milieu imparts distinct pathological alpha-synuclein strains in alpha-synucleinopathies. Nature. 2018;557:558–63.
Pujols J, Pena-Diaz S, Lazaro DF, Peccati F, Pinheiro F, Gonzalez D, Carija A, Navarro S, Conde-Gimenez M, Garcia J, et al. Small molecule inhibits alpha-synuclein aggregation, disrupts amyloid fibrils, and prevents degeneration of dopaminergic neurons. Proc Natl Acad Sci U S A. 2018;115:10481–6.
Rawjani S, Ross A, Zhang H, Hayley S, Sun H. An unrecognized “excitement” of epilepsy in Parkinson disease: evidence of systemic biomarkers and cognitive function. J Psychiatry Neurosci. 2019;44:S14.
Rcom-H'cheo-Gauthier AN, Davis A, Meedeniya ACB, Pountney DL. Alpha-synuclein aggregates are excluded from calbindin-D28k-positive neurons in dementia with Lewy bodies and a unilateral rotenone mouse model. Mol Cell Neurosci. 2016;77:65–75.
Ross RA, Biedler JL. Presence and regulation of tyrosinase activity in human neuroblastoma cell variants in vitro. Cancer Res. 1985;45(4):1628–32.
Saikia J, Pandey G, Sasidharan S, Antony F, Nemade HB, Kumar S, Chaudhary N, Ramakrishnan V. Electric field disruption of amyloid aggregation: potential noninvasive therapy for Alzheimer's disease. ACS Chem Neurosci. 2019;10:2250–62.
Schirinzi T, Madeo G, Martella G, Maltese M, Picconi B, Calabresi P, Pisani A. Early synaptic dysfunction in Parkinson's disease: insights from animal models. Mov Disord. 2016;31:802–13.
Scott D, Roy S. Alpha-Synuclein inhibits intersynaptic vesicle mobility and maintains recycling-pool homeostasis. J Neurosci. 2012;32:10129–35.
Snead D, Eliezer D. Alpha-synuclein function and dysfunction on cellular membranes. Exp Neurobiol. 2014;23:292–313.
Sun H, Takesian AE, Wang TT, Lippman-Bell JJ, Hensch TK, Jensen FE. Early seizures prematurely Unsilence auditory synapses to disrupt Thalamocortical critical period plasticity. Cell Rep. 2018;23:2533–40.
Taylor-Whiteley TR, Le Maitre CL, Duce JA, Dalton CF, Smith DP. Recapitulating Parkinson’s disease pathology in a three-dimensional human neural cell culture model. Dis Model Mech. 2019;12:dmm038042.
Tosetti P, Taglietti V, Toselli M. Functional changes in potassium conductances of the human neuroblastoma cell line SH-SY5Y during in vitro differentiation. J Neurophysiol. 1998;79:648–58.
Vamvaca K, Volles MJ, Lansbury PT Jr. The first N-terminal amino acids of alpha-synuclein are essential for alpha-helical structure formation in vitro and membrane binding in yeast. J Mol Biol. 2009;389:413–24.
Volpicelli-Daley LA, Luk KC, Patel TP, Tanik SA, Riddle DM, Stieber A, Meaney DF, Trojanowski JQ, Lee VM. Exogenous alpha-synuclein fibrils induce Lewy body pathology leading to synaptic dysfunction and neuron death. Neuron. 2011;72:57–71.
Wu Q, Takano H, Riddle DM, Trojanowski JQ, Coulter DA, Lee VM. Alpha-Synuclein (alphaSyn) preformed fibrils induce endogenous alphaSyn aggregation, compromise synaptic activity and enhance synapse loss in cultured excitatory hippocampal neurons. J Neurosci. 2019;39:5080–94.
Yamada K, Iwatsubo T. Extracellular alpha-synuclein levels are regulated by neuronal activity. Mol Neurodegener. 2018;13:9.
Yang T, Hsu C, Liao W, Chuang JS. Heat shock protein 70 expression in epilepsy suggests stress rather than protection. Acta Neuropathol. 2008;115:219–30.
Zhang W, Zhang L, Zhou N, Huang E, Li Q, Wang T, Ma C, Li B, Li C, Du Y, et al. Dysregulation of respiratory center drive (P0.1) and muscle strength in patients with early stage idiopathic Parkinson’s disease. Front Neurol. 2019;10:724.
We thank all members of the Hayley lab and the Sun lab for valuable comments.
This work was supported by an NSERC Discovery Grant (to H.S.), and CIHR grants (to H.S. and S.H.). H.S. holds a Canada Research Chair in Developmental Neuroscience. A.R. holds a Queen Elizabeth II Scholarship in Science and Technology.
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Ross, A., Xing, V., Wang, T.T. et al. Alleviating toxic α-Synuclein accumulation by membrane depolarization: evidence from an in vitro model of Parkinson’s disease. Mol Brain 13, 108 (2020). https://doi.org/10.1186/s13041-020-00648-8
- Parkinson’s disease
- Membrane depolarization
- Preformed fibrils
- GABAA receptor
- Calcium channel
- Direct current stimulation