The Small GTPase RAC1/CED-10 Is Essential in Maintaining Dopaminergic Neuron Function and Survival Against α-Synuclein-Induced Toxicity
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Parkinson’s disease is associated with intracellular α-synuclein accumulation and ventral midbrain dopaminergic neuronal death in the Substantia Nigra of brain patients. The Rho GTPase pathway, mainly linking surface receptors to the organization of the actin and microtubule cytoskeletons, has been suggested to participate to Parkinson’s disease pathogenesis. Nevertheless, its exact contribution remains obscure. To unveil the participation of the Rho GTPase family to the molecular pathogenesis of Parkinson’s disease, we first used C elegans to demonstrate the role of the small GTPase RAC1 (ced-10 in the worm) in maintaining dopaminergic function and survival in the presence of alpha-synuclein. In addition, ced-10 mutant worms determined an increase of alpha-synuclein inclusions in comparison to control worms as well as an increase in autophagic vesicles. We then used a human neuroblastoma cells (M17) stably over-expressing alpha-synuclein and found that RAC1 function decreased the amount of amyloidogenic alpha-synuclein. Further, by using dopaminergic neurons derived from patients of familial LRRK2-Parkinson’s disease we report that human RAC1 activity is essential in the regulation of dopaminergic cell death, alpha-synuclein accumulation, participates in neurite arborization and modulates autophagy. Thus, we determined for the first time that RAC1/ced-10 participates in Parkinson’s disease associated pathogenesis and established RAC1/ced-10 as a new candidate for further investigation of Parkinson’s disease associated mechanisms, mainly focused on dopaminergic function and survival against α-synuclein-induced toxicity.
KeywordsParkinson’s disease Dopaminergic neurons Alpha-synuclein accumulation Autophagy impairment RAC1/ced-10
Parkinson’s disease (PD) is the second most frequent neurodegenerative disorder in the elderly. While most of cases are sporadic, monogenic PD caused by pathogenic point mutations in PD-associated genes occurs in less than 10% of cases (reviewed in ). The common neuropathological hallmarks of PD include a selective loss of the dopaminergic neurons (DAn) in the Substantia Nigra pars compacta and aggregation of the protein alpha-synuclein (α-SYN) in the surviving DAn and in the so called Lewy bodies (LB) and Lewy neurites (LN) which are found in the few surviving DAn (reviewed in ). α-SYN is intrinsically misfolded in pathological conditions such as PD  and forms multiple conformations, including amyloidogenic oligomers [4, 5] implicated in α-SYN toxicity .
There exist evidences of an essential role of actin cytoskeleton disruptions in both DAn cell death [7, 8] and α-SYN accumulation . In fact, the cytoskeleton is an important target of α-SYN  and neuronal microtubule-kinesin function could be impaired by α-SYN oligomers . Actin cytoskeletal organization is regulated by small GTPases of the Rho family encompassing Rho, Cdc42 and Rac subfamily members . These proteins act as molecular switches as they alternate between the active GTP-bound and the inactive GDP-bound forms [8, 16]. GTP binding increases the activity, and the hydrolysis of GTP to GDP renders the protein inactive. More specifically, RAC1 activity is mainly associated with cellular processes involving the regulation of actin polymerization such as cell migration, lamellipodia extension or the phagocytosis of dead cells or engulfment . In addition, RAC1 participates in the extension and retraction of neurites  and, together with other members of the Rho family, govern changes in neuronal morphology and the dynamics of neuronal processes (reviewed in ).
RAC1 function has been associated with two PD-related genes. We have previously shown in C elegans that RAC1 is ubiquitylated by PARKIN , mutated in the juvenile variant of PD. Likewise, Leucine-rich repeat kinase 2 (LRRK2), in which mutations cause the most common form of familial PD , strongly and selectively binds to RAC1 . Furthermore, neuronal apoptosis induced in DAn in vitro is correlated with decreased RAC1 activity . In contrast, in a monkey model of PD, it was suggested that aberrant activation of RAC1 in microglia may contribute to enhanced production of ROS underlying the death of neighboring DAn . Therefore understanding the cytoskeletal mechanisms associated with DA cell death and α-SYN degradation is important to elucidate other causative agents of the PD pathophysiology.
Autophagic flux is profoundly disrupted in PD patients (reviewed in  and α-SYN is normally degraded by autophagy . Indeed, autophagy has been associated with PD pathogenesis through several genes, such as LRRK2 , ATG9A  or ATG8/LC3 , and cellular processes such as lysosomal disruption [23, 24]. In addition, autophagy-related gene products are required for apoptotic clearance, either in dying cells or through a role in engulfment, in where RAC1 has a pivotal role [25, 26, 27].
In the present study we have systematically investigated RAC1 function in three disease models of PD including the following: (a) C elegans models of PD; (b) human-derived neuroblastoma BE(2) (M17) cells stably over-expressing α-SYN, wherein amyloidigenic accumulation of α-SYN is induced by sodium butyrate; and (c) iPSC-derived DAn generated by cell reprogramming of somatic skin cells from patients with monogenic LRRK2-associated PD . Using these models, we determine for the first time that RAC1/ced-10 participates specifically in PD-associated pathogenesis and establish RAC1/ced-10 as a new candidate to be considered for the investigation of PD-associated mechanisms, mainly focused on DA function and survival against α-SYN-induced toxicity.
RAC1/ced-10 Cell-Autonomous Depletion in DAn Hampers Dopamine- Associated Behavior in the Presence of α-SYN and Accelerates α-SYN Induced DAn Death in C elegans
We first investigated the role of RAC1/ced-10 in DAn function, by performing behavioral assays through analyzing the DA behavior in ced-10(n3246) mutant animals. The mutation ced-10(n3246) is a G-to-A transition resulting in a change of glycine 60 of CED-10 to arginine (G60R) which results in non-null altered function [28, 29]. The severity of this allele is stronger in contrast to other ced-10 alleles (11). To explore the role of ced-10 in PD pathogenesis, all the experiments included in this study involving the ced-10 gene were performed in a ced-10(n3246) mutant background. To simplify, ced-10(n3246) is named ced-10 from here on.
The basal slowing response is a DA dependent behavior widely used in C elegans for analyzing the functionality of the DA system [30, 31, 32]. Briefly, worms decrease locomotion speed when in physical contact with a food source whereas the turn frequency increases when worms leave the food source [31, 33]. The cat-2 gene encodes the enzyme tyrosine hydroxylase required for the synthesis of dopamine. Accordingly, cat-2(e1112) mutant worms have decreased levels of dopamine and altered DA behavior [30, 33] and were used as positive control.
Slow dose response quantifications
W/o food (body bends/20 s)
With food (body bends/20 s)
Significance (P value)
20.00 ± 0.423
9.55 ± 0.328
P < 0.001
19.05 ± 0.211
13.00 ± 0.145
P < 0.001
21.00 ± 0.191
20.00 ± 0.162
UA196 on EV
18.40 ± 0.255
9.20 ± 0.257
P < 0.001
UA196 on ced-10 RNAi
16.00 ± 0.254
13.15 ± 0.392
P < 0.001
UA196 on cat-2 RNAi
17.25 ± 0.502
16.40 ± 0.689
Ethanol avoidance quantifications
Avoidance (% of worms)
Significance (P value)
71.21 ± 2.120
57.80 ± 3.957
P < 0.05
26.67 ± 3.335
P < 0.001
UA196 on EV
70.35 ± 1.213
UA196 on ced-10 RNAi
12.95 ± 1.328
P < 0.001
UA196 on cat-2 RNAi
10.902 ± 1.524
P < 0.001
The absence of significant dopaminergic behavioral alterations observed in ced-10 mutants might be the consequence of compensating mechanisms existing in the worm that mask the effect of ced-10 function specifically in DAn. To discard any effect of ced-10 function onto DA responses, ced-10 was depleted conditionally in DAn by RNAi, in a C. elegans PD model in which DAn undergo age-dependent neurodegeneration following human α-SYN overexpression . In this model, animals express both α-SYN and GFP in DAn. Importantly, this is a neuronal-sensitive RNAi strain whereby the impact of RNAi knockdown targeting gene candidates can be selectively examined exclusively in the DAn  To simplify, this strain is called Pdat-1::α-SYN + Pdat-1::GFP herein. Animals exposed to ced-10 RNAi showed a mild but significant altered slow response assay (Fig. 1a and Table 1). In addition, selective depletion of ced-10 in DAn resulted in similar avoidance against ethanol as cat-2 depleted animals in the ethanol avoidance test (Fig. 1b and Table 2). Therefore, in the presence of α-SYN, ced-10 function is specifically necessary in C elegans DAn to execute a correct DA behavioral response.
CED-10 Expression Decreases α-SYN Inclusions Formation in C elegans
The number of body thrashes or thrashing have been used extensively to identify modifiers of protein aggregation [41, 43]. Thrashing in C elegans can be measured in liquid media by counting the number of body bends per unit of time . Using this method, we confirmed the observed damaged motility (Fig. 3c and Online Resources 2 – 4 ) of the PD worms in a ced-10 background. Whereas a decrease of 27% in the bending are observed in animals expressing YFP::α-SYN in comparison to the wild type N2 wild type strain (55.01 ± 7.5 vs. 75.96 ± 2.8 bends/min, respectively), the number of bends decreases almost 90% in animals harboring the ced-10 mutation in a YFP::SYN background in comparison with N2 wild type animals (7.93 ± 4.4 vs. 75.96 ± 2.8 bends/min, respectively) and 70% in comparison with worms expressing YFP::SYN, without the ced-10 mutation (7.93 ± 4.4 vs. 55.01 ± 7.5 bends/min, respectively). Thus, increased α-SYN in muscle with its concomitant locomotion decrease in ced-10 mutants, indicate the involvement of RAC1/ced-10 in the process of α-SYN accumulation in C. elegans.
α-SYN variants that form oligomers and protofibrils are associated to the most severe DAn nigral loss in PD models [1, 6]. To identify the biochemical nature of the apparent α-SYN aggregates increased by this ced-10 mutation, worm lysates from pkIs2386 worms without and with the ced-10 mutation at L4+ 5 days of development, were sequentially extracted by detergent-containing buffers  and the amount of α-SYN extracted in each fraction was assessed by immunoblotting (Fig. 3d). A faint band of 19 kDa was detected in the Tris-HCl fraction, most probably corresponding to the α-SYN monomer staining. The number of oligomeric species is increased in ced-10 mutant animals within all analyzed fractions.
Autophagy Is Impaired in ced-10(n3246) Mutant Animals
Human RAC1 Expression Reduces α-SYN Accumulation and Amyloidogenic Aggregation in a Neuroblastoma Cell Line
High RAC1 Activity Reduces α-SYN Levels and Increases Neurite Arborization in PD Patient-Specific Midbrain iPSC-Derived DAn
Lastly, to connect the nematode data with the human PD, we differentiated DAn upon cell reprogramming of skin fibroblasts into induced pluripotent stem cells (iPSC) from PD patients carrying the G2019S (G/S) mutation in the LRRK2 gene. While preserving the patient genetic background, this model exhibits some characteristic features and cellular phenotypes of PD including reduced axonal outgrowth, α-SYN accumulation, α-SYN-induced DAn cell death, and impaired autophagy . Therefore, it represents a suitable tool to contextualize and compare the nematode encountered data.
By transcriptome analysis we have previously reported that iPSC-derived DAn from PD patients exhibited a large number of gene expression changes. More specifically, we identified 437 differentially expressed genes (DEGs) in PD vs. controls of which 254 were up-regulated in PD patients and 183 were down-regulated . Here, to gain further insight into the canonical pathways affected by differential gene expression detected at early PD, we performed a biological enrichment analysis at 30 days of differentiation, by using the software and databases of Ingenuity Pathway Analysis (IPA). We found that the signaling by Rho family GTPases pathway was the top-1 statistically most significant canonical pathway in PD patients compared to controls (P = 2.56 × 10−4) (Online Resource 8). From the total of 245 members comprised in this pathway, 16 DEGs of which 9 genes were up-regulated and 7 down-regulated in PD DAn (Online Resource 9). Interestingly, the top 2 statistically most significant canonical pathway was the related Rho GDI pathway (P = 7.91 × 10−4). Overall, the results from this unbiased biological enrichment analysis identifies Rho family GTPases as top deregulated canonical pathway in iPSC-derived DAn from PD patients.
RAC1 Activity Increases the Long-Term Survival of PD-Patient-Derived DAn and Alleviates the Impairment of Autophagy
To assess whether the protective effect of RAC1 in reducing α-SYN levels correlated with increased survival rates over time, neurons were further cultured for 75 days (Online Resource 6b) by co-culturing them over a monolayer of mouse post-natal cortical astrocytes , which supported viable cultures of DAn for up to 75 days .
In conclusion, these results obtained in DAn derived from LRRK2-associated PD patients are in line with findings in the nematode models of PD, where RAC1 activity is directly involved with DAn survival in the presence of α-SYN, α-SYN inclusions formation and autophagic mechanisms.
Here, we demonstrate in C elegans and in human-derived PD cells that RAC1/ced-10 participates in the main pathogenic manifestations of PD such as DAn death, α-SYN accumulation and impaired autophagy. Besides, the results obtained in the nematode, suggest a role of ced-10 modulating DA behavior in the presence of α-SYN. Furthermore, RAC1 function is associated with the considered toxic α-SYN species. Overall, in this manuscript we propose RAC1/ced-10 as a potential therapeutic target for the treatment of PD-related disorders.
RAC1/ced-10 and DAn Death
Previous research has shown that Rac GTPases play an essential neuroprotective and pro-survival role in neuronal models and diseases [17, 56, 57, 58]. Indeed, our in depth analysis of the RAC1 signaling pathway arose from the transcriptomic data in human iPSC-derived DAn from PD patients, showing altered Rho signaling as top deregulated pathway, points to this same direction (Online Resources 8 – 9 ). However, Rac GTPases modulation in different cell types is much more complex. Loss of RAC GTPase activity may contribute to the death of DAn while increased Rac-GTP activity in microglia may contribute to the formation of toxic ROS . Hence, this complicated RAC1 modulation depending upon the tissue and the ROS state, might explain the behavioral differences observed between whole ced-10 mutant animals and RAC1/ced-10 specifically depleted in DAn in the presence of α-SYN (Fig. 1). Interestingly, a cell non-autonomous function for hypodermal RAC1/ced-10 in the maintenance of axonal survival has been recently proposed in C. elegans . Consequently, the influence of RAC1 activity in the neighboring tissues cannot be obviated.
There exist positive correlation between neuronal apoptosis and decreased RAC1 GTPase activity . Very different cellular models, such as human lymphoma cells or primary cerebellar granule neurons, suggest the inhibition of caspase-induced apoptosis by RAC1, whereby AKT-dependent pro-survival pathways and the consequent Bcl-2-associated death protein (BAD) phosphorylation were downstream and activated by RAC1 [59, 61].
The activation of the AKT by RAC1, also participates in the cytoskeleton reorganization and cellular growth [62, 63] and a failure to maintain the integrity of DAn after they are formed could cause DAn death . Accordingly, RAC1-modulated processes involved in the maintenance of cell integrity, might be crucial for cell survival.
LRRK2-PD-patient-derived DAn show increased neurite numbers after being transduced with RAC1 (Fig. 6), thus expanding the role of this GTPase in the maintenance and in the generation of new neurites , and thus contributing accordingly to DAn survival (Fig. 7). Therefore, our results are in accordance with LRRK2 inducing neurite retraction through diminished RAC1 GTPase activity . Surprisingly, neurite length was not rescued with any of the infected RAC1 constructs in the present manuscript. Differences between results can be explained based on the different cellular models used in both laboratories, since our results are provided directly from PD-derived cells, whereas the neuroblastoma cell line SHSY5Y is the model used by Chan et al. . In addition, the existing actin-microtubule cross talk in the process of neurite outgrowth and elongation has to be considered [65, 66]. Microtubules are the main cytoskeletal components of neurites  and decreased stability of microtubules is a common feature of neurodegenerative diseases . Interestingly, LRRK2-PD variants are characterized by defects in microtubule associated processes  and LRRK2 regulates microtubule stability .However, extension and navigation of neurites are normally driven by actin-rich growth cones and inhibition of microtubules dynamics does not stop neurite outgrowth . Thus, our results are consistent with cellular dysfunction in PD, with RAC1 modulating actin-associated mechanisms better than in microtubule linked processes.
RAC1/ced-10 and α-SYN Accumulation
One of the main factors linked with DAn death in PD progression is α-SYN accumulation. α-SYN overexpression in model systems, and its concomitant aggregation and deposition precede neuronal cell death. In the case of DAn, its degeneration is influenced by intracellular and extracellular α-SYN accumulation, mainly in its oligomeric form . Interestingly, extracellular oligomeric α-SYN impairs RAC1 activity in neuroblastoma cells . Considering the increased intracellular α-SYN aggregates together with increased oligomeric α-SYN species observed in ced-10 mutant animals, we hypothesize that altered RAC1/ced-10 function might accelerate α-SYN accumulation and the formation of α-SYN oligomers which might bind concurrently RAC1/ced-10  thus increasing the severity of RAC1/ced-10 altered function. Moreover, and considering the modulation of the actin cytoskeletal dynamics by α-SYN , a synergistic regulation between RAC1 and α-SYN cannot be excluded.
Additional experiments, where the amount of α-SYN could be tightly controlled, will provide some clues about the relevance of RAC1/α-SYN interaction in the progress of PD.
α-SYN accumulation in PD patients is associated with failure of the two major protein breakdown pathways, the ubiquitin proteasome system (UPS) and autophagy [72, 73, 74], which, in cooperation, reduce the misfolded protein burden . Stably increased levels of α-SYN can lead to impaired proteasome function  and ced-10 is proteasome regulated in the phagocytosis of dead cells . Hence, we hypothesize that increased α-SYN in a ced-10 mutant background might reinforce the severity of the ced-10 mutation in the degradation of α-SYN, due to the interaction of α-SYN with the proteasomal machinery.
Overexpression of α-SYN results in the inhibition of autophagy . Here we suggest RAC1/ced-10 being necessary for autophagy to occur (Figs. 3 and 7). Accordingly, α-SYN accumulation, due to ced-10 impairment, might increase the severity of ced-10 mutation. Therefore we add RAC1 to the already proposed feedback loop between proteasome activity and autophagy  and we propose that a tight regulation of RAC1 function is required to avoid excess of α-SYN accumulation and the concomitant cell death.
Impaired autophagy associated with LRRK2 mutations are already reported [78, 79], with the G2019S mutation showing less autophagic activity . In the context of LRRK-2 induced phenotypes, we propose RAC1-LRRK2 interaction as relevant factor favoring autophagy to occur, and helping in the clearance of α-SYN aggregates, thus warranting the proper neurite growth and maintenance.
Future scientific research is needed to unravel the mechanisms associated with PD-related disorders for finding efficient therapies. In light of our results the pharmacological modulation of RAC1 and RAC1-derived signaling pathways could be of therapeutic value.
C. elegans Strains
Nematodes were maintained using standard procedures . We obtained the strains CB1112 cat-2(e1112), NL5901, unc-119(ed3) III; [pkIs2386 (Punc-54::α-SYN::YFP; unc-119(+))]; DA2123 adIs2122 [Plgg-1::lgg-1::GFP; rol-6(su1006)] and HZ589, bpIs151 [Psqst-1::sqst-1::GFP; unc-76(+)] IV; him-5(e1490) V from the Caenorhabditis elegans Genetic Center (CGC). The strain BR3579, ced-10(n3246) was a generous gift from Dr. Ralf Baumeister (Albert-Ludwing University, Freiburg/Breisgau, Germany).
The strain BR3579 was crossed with NL5901 animals to generate the strain EDC101, unc-119(ed3) III; pkIs2386 [Punc-54::α-SYN::YFP; unc-119(+)]; ced-10(n3246).
The following strains is used to analyze the DAn degeneration as reported in Harrington et al., 2010 : Pdat-1::α-SYN +Pdat-1::GFP from the main text is named UA196, with the genotype: sid-1(pk3321); baIn33 [Pdat-1::sid-1; Pmyo-2::mCherry]; baIn11 [Pdat-1::α-SYN; Pdat-1::GFP].
For autophagy experiments, males from the DA2123 strain [Plgg-1::lgg-1::GFP; rol-6(su1006)] were crossed with ced-10(n3246) hermaphrodites. Males a from the HZ589 bpIs151 [Psqst-1::sqst-1::GFP; unc-76(+) IV]; him-5(e1490) V] strain, expressing SQST-1::GFP crossed with ced-10 (n3246) hermaphrodites.
N2 (Bristol) was used as the C. elegans wild-type (wt) strain. Hermaphrodites were used throughout of the study.
For feeding RNAi bacteria, egg lay from gravid adults were directly transferred to NGM plates containing 1 mM of isopropyl β-D-1-thiogalactopyranoside/ IPTG (referred to as RNAi plates) seeded with 20X concentrated bacteria containing 50 μg/ml ampicillin, carrying desired plasmid for RNAi of a specific gene (ced-10 or cat-1, depending upon the experiment) or bacteria carrying empty (EV) pL4440 as control and allowed to grow on plates for approximately 50 h to reach the L4 stage and then another 16 h for the conduction of actual experiment.
Note: Bacterial clones for RNAi feeding protocol were obtained from the Ahringer library (Source Bioscience, Nottingham, UK)  and were then streaked on LB-Tetracycline-Ampicillin plate which was then incubated at 37 °C. Individual colonies from this freshly streaked plate were grown for 10–12 h constantly shaking at 37 °C in LB medium containing 50 μg/ml ampicillin.
Blinding of Experiments and Replicates
All behavioral studies were completed such that the experimenter was blind to the genotype of the worms. Strains were given letter codes by another member of the laboratory and the code was not broken until all of the replicates for a particular assay were completed. For all assays, we completed a minimum of three biological replicates per strain.
Locomotor Rate Assay
Locomotor rate assay was performed as described in . Briefly, assay plates were prepared by spreading the E. coli strain OP50-1 in a ring on NGM agar  in 5-cm petri plates. Assay plates were always freshly spread with bacteria, incubated overnight at 37 °C, and allowed to cool to room temperature before use. Plates for measuring locomotor rate in the absence of bacteria were also incubated at 37 °C. Only synchronized young adult hermaphrodites (16 h after the late L4 larval stage) were tested. For well-fed animals, locomotor rate was measured by removing 5 animals from plates with ample bacteria, washing the animals twice in S basal buffer , and transferring them to an assay plate in a drop of buffer using a capillary pipette. The drop of buffer used to transfer the animals was absorbed with a Kimwipe. Five minutes after transfer, the number of body bends in 20 s intervals was sequentially counted for each of the five animals on the assay plate and then repeated the same thing for next set of animals in a different assay plate.
Ethanol Avoidance Assay
Ethanol avoidance assay was performed as described  (Cooper et al. 2015). Synchronized young adult hermaphrodites (16 h after the late L4 larval stage) were transferred to assay plates, which are divided into four quadrants: two quadrants seeded with 50 μl of 100% ethanol and the others without. Worms are placed in the center of the assay plate and allowed to move for 30 min at which point the entire plate is imaged and the worms are scored for their quadrant of preference. Ethanol avoidance is calculated as [(number of worms in control quadrants) − (number of worms in ethanol quadrants)]/total number of worms.
Generation of the Rescue Construct Pced-10:: CFP::ced-10
Pced-10::CFP::ced-10 plasmids were co-injected into worm strain EDC101 and UA196 to generate UA281, baEx167 [Pced-10::CFP::ced-10, rol-6(su1006)]; [Punc-54::α-SYN::YFP;ced-10(n3246)] and UA282, baEx167 [Pced-10::CFP::ced-10; rol-6(su1006)]; sid-1(pk3321); baIn33 [Pdat-1::sid-1, Pmyo-2::mCherry]; baIn11[Pdat-1::α-SYN; Pdat-1::GFP]). Hermaphrodites were used throughout of the study.
The construct Pced-10::GFP::ced-10 was provided by Erik Lundquist (University of Kansas, Lawrence, KS, USA) as a gift. TagMaster Site-directed mutagenesis (GM Biosciences, Rockville, USA) was used to create mutations (Y66W, Y145F, and M153T) in GFP sequence for changing fluorescence marker as CFP. The product plasmid Pced-10::CFP::ced-10 was sequenced (Eurofins Genomics, Huntsville, AL, USA) to confirm the presence of the desired mutations.
C. elegans Neurodegeneration Assays
Worms were analyzed for DA neurodegeneration as described previously . Briefly, 10 L1-stage worms (neuron-specific RNAi worm strain with α-Syn UA196 were transferred to the plates (empty vector (EV) and ced-10 RNAi) and grown at 20 °C until adulthood. Adult worms were then transferred to corresponding freshly made RNAi plates and allowed to lay eggs for 6 h to synchronize. α-SYN-induced DA neurodegeneration was scored at the indicated days after hatching (L4 + 7; L4 + 3; L4 + 1). To investigate the effect of CED-10 overexpression on α-SYN –induced DA degeneration, the strain UA282 was analyzed at L4 + 7 days of aging. Worms were considered normal when all six anterior DA neurons (four CEP (cephalic) and two ADE (anterior deirid)) were present without any visible signs of degeneration. If a worm displayed degeneration in at least one of the six neurons, it was scored as exhibiting degeneration. In total, at least 50 adult worms were analyzed for each independent transgenic line or RNAi treatment.
The quantification of aggregates was performed as previously described . Briefly, NL5901animals without and with ced-10(n3246) mutation, together with the EDC101, were age-synchronized by bleaching with NaOCl and left overnight to hatch. L1 animals were transferred onto individual NGM plates seeded with Escherichia coli. Aggregates were counted for each animal staged at L4 + 5 days. Images were captured using a Leica SP5 confocal microscope with a ×40 oil immersion lens (HCX PL APO CS). The number of α-syn aggregates was determined in the mid body of each animal, taking the vulva position (V) as a reference. Aggregates were defined as discrete, bright structures, with boundaries distinguishable from surrounding fluorescence. Measurements on inclusions were performed using ImageJ software taking into consideration the area dimensions.
At L4 + 5 days, animals from the strains N2 wild type, NL5901 [unc-119(ed3) III; pkIs2386 [Punc-54::α-SYN::YFP; unc-119(+)] and EDC01 unc-119(ed3) III; pkIs2386 [Punc-54::α-SYN::YFP; unc-119(+)]; ced-10 (n3246) were placed in a drop of M9 buffer and allowed to recover for 120 s (to avoid observing behavior associated with stress) after which the number of body bends was counted for 1 min. Movies of swimming worms were recorded using a Leica MZFFLIII stereomicroscope at nominal magnification of 30X and the Hamamatsu ORCA-Flash 4.0LT camera at 17 frames per second (17 fps) for 1 min. Bends per minute were obtained with the Worm Tracker pluggin (wrMTrck), from the ImageJ software . Thirty animals were counted in each experiment unless stated otherwise. Experiments were carried out in triplicate. Statistical analysis was performed using Graphpad Prism version 6.00 for Windows, GraphPad Software, La Jolla, CA, USA).
α-SYN oligomeric species were isolated by detergent fractionation as described (Kuwahara et al. 2012) with slight modifications. Briefly, worms were washed three times with M9 buffer, collected as a 100 μl pellet, and the pellet was snap-frozen in liquid nitrogen. The pellets were homogenized in 1 mL of 50 mM Tris-HCl buffer at pH 7.5 with complete protease inhibitor mixture (Roche Applied Science) by brief sonication. Sonicates were centrifuged two times at 1000×g for 5 min to remove debris of worm tissue. The supernatant was then ultracentrifuged at 350,000×g for 15 min, and the supernatant was collected as a Tris-HCl soluble fraction. The resulting pellet was subsequently extracted by sonication in 500 μl of Triton X-100 (Tris-HCl buffer with 1% TritonX-100), 200 μl of Sarkosyl (Tris-HCl with 1% Sarkosyl), and 100 μl of SDS (TrisHCl with SDS sample buffer containing 2% SDS) followed by centrifugation at 350,000×g for 15 min. The Tris-HCl fraction containing 20 μg of total proteins, along with equal volumes of Triton X-100, Sarkosyl, and SDS fractions to the Tris-HCl fraction, were loaded onto the acrylamide gel and separated by SDS-PAGE.
Twenty microliters of protein per strain were loaded from each sample and fraction on Novex NuPAGE 4–12% Bis-Tris Gels (Thermo Fisher) an run in MES SDS buffer at 200 V for 40 min. Resolved proteins were transferred onto 0.45 μm nitrocellulose membranes (Amersham) at 200 mA for 1 h. Blocking was done in 5% milk powder in PBS for 1 h, followed by overnight incubation at 4 °C with a mouse monoclonal antibody against α-synuclein (1:1000, BD Biosciences, #610787) diluted in 2% bovine serum albumin (BSA)/PBS. Incubation with a donkey anti-mouse (1:5000, Amersham) secondary antibody diluted in 1% milk powder/PBS was performed for 1 h at room temperature.
Membranes were developed using Supersignal West Femto (Thermo Scientific) in a ImageQuant RT ECL Imager (GE Healthcare).
For measuring the involvement of ced-10(n3246) mutation in autophagy, we followed specific C. elegans protocols [48, 85]. LGG-1::GFP foci were analyzed in the hypodermal seam cells at L3 stage of development. Images were not considered for quantification where the hypodermis was not clear. In total, at least 40 total regions were quantified from 30 different worm samples per genotype.
To confirm the involvement of ced-10 in impairing autophagy, we followed the protocol described in . Pictures of L1 animals (whole animal) and L4 animals (whole intestine), were analyzed by using a 63× objective. The GFP internal intensity (FI), corresponding to SQST-GFP foci, was quantified at L4 stage of development. The presence of the ced-10 mutation was checked by PCR as described . The presence of the GFP reporter was double checked by PCR using the gfp primers, and under the fluorescence microscope.
Microscopy and Imaging
For neurodegeneration assays and aggregates quantification animals were mounted with a coverslip on a 4% agarose pad in M9, containing 10 mM of sodium azide. Confocal microscopy was performed using a Leica TCS-SP5 confocal spectral microscope (Leica, Barcelona, Spain) and analyzed using ImageJ software (NIH, ver. 1.43, Schindelin, 2015). Animals were examined at 100× magnification to examine α-SYN induced DA cell death and at 40X to examine α-SYN apparent aggregates.
For autophagy measurements, animals were placed in a 5 μL drop of 10 mM solution of levamisole (Sigma-Aldrich, Madrid, Spain). For each independent experiment, between 20 and 30 7-day-old worms of each treatment were examined under a Nikon EclipseTE2000-E epifluorescence microscope equipped with a monochrome camera (Hamamatsu ORCA-ER) coupled to the Metamorph software (Molecular Devices Corp., Sunnyvale, CA). The system acquires a series of frames at specific Z-axis position (focal plane) using a Z-axis motor device.
Cell Culture Experiments in BE(2)-M17 Neuroblastoma Cell Line
Human neuroblastoma cell line BE(2)-M17 over-expressing wild type α-SYN were maintained at 37 °C and 5% CO2 in Optimem medium (Gibco) (Thermo-Fisher Scientific, Madrid, Spain) supplemented with 10% fetal bovine serum (Gibco) (Thermo-Fisher Scientific, Madrid, Spain), 500 μg/ml G418 (Geneticin) (Sigma-Aldrich, Madrid, Spain) and Penicillin/Streptomycin (Sigma-Aldrich, Madrid, Spain). For immunofluorescence, 2 × 104 cells/well were seeded in 24-well plates on coverslips coated with poly-D-lysine. α-SYN aggregation was induced as previously reported ( by differentiation with 10 μM retinoic acid (Sigma-Aldrich, Madrid, Spain) for 10 days, followed by treatment with the histone deacetylases inhibitor sodium butyrate (SB) (Sigma-Aldrich, Madrid, Spain) at a concentration of 10 mM for 36 h. To analyze the effect of RAC1 on α-SYN aggregation, cells were transduced 24 h before SB treatment with either the lentiviral empty vector or with the wild type or the constitutively active isoforms of RAC1 at an estimated multiplicity of infection (MOI) of 5.
BE(2)-M17 cells were fixed in 4% paraformaldehyde (PFA) (Sigma-Aldrich, Madrid, Spain) in phosphate saline buffer (PBS) for 30 min at 4 °C and permeabilized with Tris-buffered saline (TBS) containing 0.5% Triton X-100 (Sigma-Aldrich, Madrid, Spain) for 5 min. Cells were then blocked with 3% normal goat serum (NGS) (Vector Laboratories, Palex Medical, Sant Cugat del Vallès, Spain) in TBS for 1 h and subsequently incubated with the corresponding primary antibody in 1%NGS/TBS overnight at 4 °C. The following primary antibodies were used: mouse anti-α-SYN (610,787; 1:500) (BD Biosciences, Madrid, Spain), rabbit anti-α-SYN (2642; 1:500) (Cell Signaling, Leiden, The Netherlands). Incubation with goat secondary antibodies conjugated with Alexa488 (anti-mouse, A11001; or Alexa594 (anti-mouse, A11005; anti-rabbit, A11012) (Thermo-Fisher Scientific, Madrid, Spain) was done in 1% NGS/TBS for 1 h at RT. Between each incubation period cells were rinsed three times in TBS.
Thioflavin S Staining
After incubation with the antibodies, coverslips were immersed in 0.005% thioflavin S (Sigma-Aldrich, Madrid, Spain) in PBS for 8 min and then rinsed twice in ethanol 70% and once in PBS. Only after thioflavin S staining, nuclei were counterstained with Hoechst 33342 (Thermo Fisher Scientific, Madrid, Spain, 1:10,000 in PBS) for 10 min.
Microscopy and IF Quantification
Cells were cover slipped using Dako Cytomation Fluorescent Mounting Medium (Dako, Sant Just Desvern, Spain). Immunofluorescence images were acquired using standard filter sets using an Olympus FluoView TM FV1000 confocal microscope and the FV10_ASW 4.2 visualization software.
α-SYN fluorescence intensity for each condition was analyzed in an average of 150 cells from 6 different random fields at an objective magnification of 40×. Quantification of Thioflavin S positive aggregates in each condition was analyzed in an average of 20 cells from 3 different random fields by measuring the fluorescent area per cell. All quantification analyses were done using ImageJ software (NIH, USA).
Cell Culture Experiments with iPSC Cell Lines Derived from Human Patients
Previously generated iPSC lines SP-11.1 (from control) and SP-12.3 (from patients with familial PD with the LRRK2 G2019S mutation) were used and culture and differentiation were carried out as described, (34), following a protocol approved by the Spanish competent authorities (Commission on Guarantees concerning the Donation and Use of Human Tissues and Cells of the Carlos III Health Institute). Briefly, hiPSC were cultured on matrigel (Corning Limited, Life Sciences, UK) and maintained in hESC medium, consisting on KO-DMEM (Invitrogen, Thermo Fisher Scientific, Madrid, Spain) supplemented with 20% KO-Serum Replacement (Invitrogen, Thermo Fisher Scientific, Madrid, Spain), 2 mM Glutamax (Invitrogen, Thermo Fisher Scientific, Madrid, Spain), 50 μM 2-mercaptoethanol (Invitrogen, Thermo Fisher Scientific, Madrid, Spain), non-essential aminoacids (Cambrex, Nottingham, UK) and 10 ng/ml bFGF (Peprotech, London, UK). Medium was preconditioned overnight by irradiated mouse embryonic fibroblast and hiPSC were maintained on Matrigel (Corning Limited, Life Sciences, UK) at 37 °C, 5% CO2.
For DAn differentiation, iPSC were transduced with LV.NES.LMX1A.GFP and processed as previously described (79). Briefly, confluent iPSC 10 cm dishes were disaggregated with accutase and embryoid bodies (EB) were generated using forced aggregation method in V-shaped 96 well plates. Two days later, EBs were patterned as ventral midbrain by culturing them in suspension for 10 days in N2B27 supplemented with 100 ng/ml SHH (Peprotech, London, UK), 100 ng/ml FGF8 (Peprotech, London, UK) and 10 ng/ml FGF2 (Peprotech, London, UK). Then, for α-SYN and neurite analysis, differentiation to midbrain DAn was performed on the top of PA6 murine stromal cells for 3 weeks (79). To analyze α-SYN levels, neuronal cultures were gently trypsinized and re-plated in matrigel-coated slides for 3 days, then transduced with the two different RAC1 isoforms or the control LV, at an estimated MOI of 10. Cells were fixed and analyzed 7 days after transduction. For long-term culture studies, EBs were mechanically dissociated by repeated pipetting after the induction step. Salient EB fragments were transduced with the two different RAC1 isoforms or the control LV at an estimated MOI of 3. Three days post-transduction, the aggregates were seeded on primary murine astrocytes and cultured for 9 weeks.
RAC1 wild type (WT) and constitutively active (V12) (CA) forms were amplified by means of PCR from expression plasmids kindly provided by (Dr Francisco Sánchez-Madrid; Spanish National Center for Cardiovascular Research (CNIC), Madrid, Spain). Subsequently, RAC1-(WT) and RAC1-(CA) cDNA were cloned under the human phosphoglycerate kinase (PGK) promoter of pCCL.cPPT-hPGK-IRES.eGFP-WPRE lentiviral transfer vector. High-titer vesicular stomatitis virus (VSV)–pseudotyped LV stocks were produced in 293T cells by calcium phosphate–mediated transient transfection of the transfer vector, the late generation packaging construct pMDL, and the VSV envelope–expressing construct pMD2.G, and purified by ultracentrifugation as previously described . Expression titers, determined on HeLa cells by fluorescence-activated cell sorter (FACS) analysis (FACSCalibur, Becton Dickinson), were as follows: LV-RAC1 (WT): 2.60 · 10^8 TU/mL; LV-RAC1 (CA): 2.24 · 10^8 TU/mL; LV-PGK-GFP: 5.08 · 10^9 TU/mL.
Immunofluorescence for iPSC-Derived Cells
iPSC-derived cells were fixed with 4% paraformaldehyde (PFA) in Tris-buffered saline (TBS) buffer for 20 min and blocked in 0.3% Triton X-100 (Sigma-Aldrich, Madrid, Spain) with 3% donkey serum for 2 h. In the case of α-SYN and LC3 staining, Triton X-100 was kept at 0.01% for the blocking and antibody incubation steps. The following primary antibodies were used: mouse anti-α-SYN (610787; 1:500) (BD Biosciences, Madrid, Spain), rabbit anti-TH (sc-14007; 1:500) (Santa Cruz Biotechnology, Madrid, Spain), chicken anti-GFP (1020; 1:250) from Aves Labs (Cosmo Bio, AbBcn S.L., Bellaterra, Spain), rabbit anti-cleaved Caspase3 (9664; 1:400) (Cell Signaling) and LC3B (2775; 1:100) (Cell Signaling). Images were acquired using a Leica SP5 confocal microscope.
α-SYN and Neurite Analysis
α-SYN and neurite analysis were performed after a total of 4 weeks of differentiation plus 1 week after LV transduction on iPSC-derived DA neurons. DA neurons were randomly selected, using a Leica SP5 confocal microscope, and analyzed with ImageJ for α-SYN intensity levels and with the ImageJ plugin NeuronJ to determine the number of neurites per cell, number of terminals and branch points.
Cleaved Caspase-3, Apoptotic Cell Number and Autophagosome Accumulation and Analysis
Cleaved caspase-3, apoptotic cell number and autophagosome accumulation analysis were performed after a total of 9 weeks of differentiation on iPSC-derived DAn grown on murine astrocytes. DA neurons were randomly selected, using a Leica SP5 confocal microscope, and analyzed with ImageJ to determine the fraction of the neuronal soma area stained by cleaved caspase-3 or covered by LC3-positive particles.
All experiments were performed at least three independent times. All data are presented as mean ± SEM. Group means were compared with either the Student’s t test or ANOVA. All P values were two tailed, and a P value of less than 0.05 was considered statistically significant. All statistical analyses were analyzed using GraphPad Prism (San Diego, CA, USA) software.
Outlier values were identified with the Grubbs’ tests and excluded from the analysis.
Differences among means were analyzed either by 1- or 2-way analysis of variance (ANOVA), as appropriate, using the post hoc Tukey’s multiple comparison test. In all cases, the null hypothesis was rejected at the 0.05 level.
Biological Enrichment Analysis
Transcriptomic analysis of iPSC-derived DAn from PD patients (n = 10) and healthy controls (n = 4) was done as previously described . Identified differentially expressed genes (DEGs) after multiple testing adjustment of P values (n = 437) were subjected to biological enrichment analysis. To this end, we used the Core Analysis module of the Ingenuity® Pathway Analysis (IPA) software (Qiagen, Redwood City, www.qiagen.com/ingenuity) to identify biological enrichment of canonical pathways deregulated in iPSC-derived DAn from PD patients. More specifically, we used the Ingenuity Knowledge Base of Genes, and considered only direct molecules and/or relationships for humans. Statistical significance of canonical pathways was computed by using the Fischer’s exact test and significance levels were set at P below 0.05. Using IPA we also calculated Z-score values which consider the directional effect of one molecule on another molecule or on a process, and also the direction of change of molecules in the dataset and provide predictions about whether the pathway is predicted to be activated or inhibited, or if the pathway is ineligible for such an assessment.
The genetic strain BR3579 was kindly provided by Dr. Ralf Baumeister (Albert-Ludwing University, Freiburg/Brisgau, Germany). Plasmids Rac1-GFP WT and Rac1-GFP (CA) HYM772 were kindly provided by Dr. Francisco Sánchez-Madrid (Spanish National Center for Cardiovascular Research (CNIC), Madrid, Spain). The construct Pced-10::CFP::CED-10 was a generous gift provided by Erik Lundquist (University of Kansas, Lawrence, KS, USA). Human neuroblastoma cell line BE(2)-M17 over-expressing wild type α-SYN was provided by Dr. B. Wolozin (Boston University School of Medicine).
This work was supported by the following grants: Instituto de Salud Carlos III (PI15/01255), co-funded by European Union (ERDF/ESF, "investing in your future"; Spanish Ministry of Economy and Competitiveness (MINECO) (BFU2015-64408-P) and the Instituto de Salud Carlos III (PI11/00072, co-financed by the Fondo Social Europeo) to AMV; Spanish Ministry of Economy and Competitiveness (MINECO) (SAF2016-77541-R) to MV; (SAF2015-69706-R) and Instituto de Salud Carlos III (ISCIII)/FEDER (Red de Terapia Celular-TerCel RD16/0011/0024) to AR; and (BFU2016-80870-P) to AC. This work was also supported by the European Research Council (ERC) 2012-StG (311736-PD-HUMMODEL) to AC. The authors also thank the CERCA Program from the Generalitat de Catalunya and AGAUR (2014-SGR-1460). ED and AV are members of the GENIE and EU-ROS Cost Action of the European Union. CC was partially supported by pre-doctoral fellowships from the Spanish Ministry of Education–MEC (FPU12/03332).
ED and AV are members of the GENIE and EU-ROS Cost Action of the European Union.
Compliance with Ethical Standards
All experiments were performed under the guidelines and protocols of the Ethical Committee for Animal Experimentation (CEEA) of the University of Barcelona. All procedures adhered to internal and EU guidelines for research involving derivation of pluripotent cell lines. All subjects gave informed consent for the study using forms approved by the Ethical Committee on the Use of Human Subjects in Research at Hospital Clinic in Barcelona, Spain. Generation of iPSC lines was approved by the Advisory Committee for Human Tissue and Cell Donation and Use, by the Commission on Guarantees concerning the Donation and Use of Human Tissues and Cells of the Carlos III Health Institute, Madrid, Spain. All procedures were done in accordance with institutional guidelines following the Spanish legislation.
Conflict of Interest
The authors declare that they have no conflict of interest.
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