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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
J Neurosci. Author manuscript; available in PMC 2010 September 29.
Published in final edited form as:
PMCID: PMC2947449
NIHMSID: NIHMS183868

Phosphorylation at S87 is enhanced in synucleinopathies, inhibits α-synuclein oligomerization and influences synuclein-membrane interactions

Summary

Increasing evidence suggests that phosphorylation may play an important role in the oligomerization, fibrillogenesis, Lewy body (LB) formation and neurotoxicity of α-synuclein (α-syn) in Parkinson’s disease. Herein we demonstrate that α-syn is phosphorylated at S87 in vivo and within Lewy bodies. The levels of S87-P are increased in brains of transgenic (TG) models of synucleinopathies and human brains from Alzheimer’s disease (AD), Lewy body disease (LBD), and multiple system atrophy (MSA) patients. Using antibodies against phosphorylated α-syn (S129-P and S87-P), significant amount of immunoreactivity was detected in the membrane in the LBD, MSA and AD cases but not in normal controls. In brain homogenates from diseased human brains and TG animals, the majority of S87-P α-syn was detected in the membrane fractions. A battery of biophysical methods were used to dissect the effect of S87 phosphorylation on the structure, aggregation and membrane binding properties of monomeric α-syn. These studies demonstrated that phosphorylation at S87 expands the structure of α-syn, increases its conformational flexibility and blocks its fibrillization in vitro. Furthermore, phosphorylation at S87, but not S129, results in significant reduction of α-syn binding to membranes. Together, our findings provide novel mechanistic insight into the role of phosphorylation at S87 and S129 in the pathogenesis of synucleinopathies and potential roles of phosphorylation in α-syn normal biology.

Keywords: Parkinson’s disease, α-synuclein, phosphorylation, synucleinopathies, phosphomimics, serine 87

Introduction

Increasing evidence suggests that phosphorylation may play an important role in the fibrillogenesis, Lewy body (LB) formation and neurotoxicity of α-synuclein (α-syn) in vivo (Fujiwara et al., 2002; Anderson et al., 2006). Immunohistochemical and biochemical studies revealed that the majority of α-syn within inclusions isolated from patients with Parkinson’s Disease (PD) and other synucleinopathies (Kahle et al., 2000; Okochi et al., 2000; Fujiwara et al., 2002; Takahashi et al., 2003a; Anderson et al., 2006) is phosphorylated at S129 (S129-P). Proteinaceous inclusions formed in cellular and animal models overexpressing WT or mutant α-syn (Lo Bianco et al., 2002; Takahashi et al., 2003a; Yamada et al., 2004; Chen and Feany, 2005) can also be stained with an antibody against S129-P. Although the kinases and phosphatases responsible for regulating α-syn phosphorylation at S129 in vivo are still not known, a series of in vitro and cell culture-based studies have identified a number of kinases, which phosphorylate α-syn at S129 and/or S87, including CKI (S87 & S129) and CKII (S129) (Okochi et al., 2000) and the G-protein coupled receptor kinases (GRKs 1, 2, 5, and 6, S129) (Pronin et al., 2000), LRRK2 (S129) (Qing et al., 2009) and PLKs (S129) (Inglis et al., 2009; Mbefo et al., 2009)

A close comparison of the amino acid sequences of all synucleins from humans and other species shows that the majority of potential α-syn phosphorylation sites, including (Y125, S129, Y133 and Y136) are highly conserved in all species (supplemental Fig. 1A). Considering all the α-syn phosphorylation sites identified in vivo (S129 (Fujiwara et al., 2002; Chen and Feany, 2005)) and in vitro (S87 (Okochi et al., 2000; Kim et al., 2006), S129 (Okochi et al., 2000; Pronin et al., 2000; Fujiwara et al., 2002; Takahashi et al., 2003a; Chen and Feany, 2005; Kim et al., 2006), Y125, Y133 and Y136 (Ellis et al., 2001; Nakamura et al., 2001; Ahn et al., 2002; Negro et al., 2002; Takahashi et al., 2003b)), it is striking that only S87 lies in the hydrophobic non-amyloid component (NAC) region of α-syn, which is essential for α-syn aggregation and fibrillogenesis (El-Agnaf et al., 1998). S87 is one of the few residues and phosphorylation sites that distinguish the human α-syn sequence from that of mouse and rat α-syn (supplemental Fig. 1B). It is noteworthy that the sequences of mouse and rat α-syn contains the PD associated mutation A53T, but do not develop PD pathology and symptoms. Therefore, we hypothesized that S87 might be an important contributor to PD-like pathology and symptoms induced in human, but not mouse and rat α-syn, where this residue is absent.

These observations prompted us to investigate the physiological relevance of S87 phosphorylation in vivo and its consequences on the structural and aggregation properties of α-syn in vitro. Towards these goals, we generated an antibody against phosphor-S87 and used it to investigate the presence of S87-P in Lewy bodies and compare the levels of S87-P α-syn in the brains of transgenic (TG) models of α-synucleinopathies as well as in human Alzheimer’s disease (AD), Lewy Body Disease (LBD) and MSA brains. To examine further the role of S87 phosphorylation in modulating the structural, aggregation and membrane-binding properties of α-syn, we carried out a thorough comparative characterization of the phosphomimic S87E and the in vitro phosphorylated S87-P α-syn, as well as the S87A and WT α-syn using an array of biochemical and biophysical methods. Our findings and their implications for the understanding of the normal biology of α-syn and its role in the pathogenesis of PD are discussed.

Materials and Methods

Validation of the anti-S87P antibody in vivo

Plasmid construction and production of recombinant AAV2/6 viral vectors

A single-nucleotide mutation coding for S87D was introduced into the cDNA of human α-syn already containing the A30P pathogenic mutation using the QuickChange Site-Directed Mutagenesis kit (Stratagene, La Jolla, CA, USA). Beforehand, the A30P α-syn cDNA had been cloned into the AAV-CMV-MCS backbone (Stratagene, La Jolla, CA, USA). The S129A mutation had been generated previously (Azeredo da Silveira et al. 2009). For the S87D variant, the mutagenesis primers were: sense 5’-GGAGGGAGCAGGGGACATTGCAGCAGCCAC-3’ and antisense 5’-GTGGCTGCTGCAATGTCCCCTGCTCCCTCC-3’. Production and titration of the recombinant pseudotyped AAV2/6 vectors (serotype 2 genome/serotype 6 capsid) were performed as previously described in Azeredo da Silveira et al. 2009.

Stereotaxic injections

Male Wistar rats (Charles river Laboratories, France), weighing 180–200 g at the time of surgery were maintained under 12h light/dark cycle, with ad libitum access to food and water, in accordance with the Swiss legislation and the European Community council directive (86/609/EEC) for the care and use of laboratory animals. Stereotaxic injections were performed under xylazine/ketamine anesthesia. Animals were placed in the stereotaxic frame (David Kopf Instruments, Tujunga, CA, USA) and received a unilateral intranigral injection of 2 µl of viral suspension, corresponding to a viral load of 2.5×107 transducing units. Injections were performed in the right brain hemisphere at a speed of 0.2 µl/min controlled by an automatic pump (CMA Microdialysis, Solna, Sweden), using a 10 µl Hamilton syringe connected to a 34-gauge blunt-tip needle. The needle was left in place for an additional 5 min before being slowly withdrawn. Stereotaxic coordinates for virus injections above the substantia nigra pars compacta were as follows: anteroposterior (AP): −5.2 mm, lateral (L): −2.0 mm; dorso-ventral (DV): −7.8 from the skull surface; with the incisor bar at 0.0 mm, according to the rat stereotaxic atlas by Paxinos & Watson (1986). To examine the in vivo specificity of our antibody against S87-P, animals injected with AAV2/6- α-syn A30P S129A viruses were sacrificed 13 weeks post-injection and transcardially perfused with 4% paraformaldehyde (PFA, Fluka-Sigma, Buchs SG, Switzerland). Brains were removed, post-fixed overnight in PFA 4% and then transferred into 30% sucrose. Twenty-five µm-thick coronal sections were cut at −20°C with a microtome (SM2400; Leica, Nussloch, Germany) and slices were stored at −20°C in antifreeze medium.

Samples and Tissue Processing

Analysis of α-syn phosphorylation was performed with postmortem human temporal cortex samples and with the brains of α-syn TG mice. The human samples were obtained from the Alzheimer’s disease research center (ADRC) at the University of San Diego (UCSD). A total of 21 cases were included, of which 6 were non-demented controls, 6 were diagnosed as AD, 6 as LBD and 3 as MSA. In all cases the brains were processed within 8 h after death. Brains were divided sagitally, the right hemibrain was serially sectioned and preserved at −70 C, and the left hemibrain was fixed in formaldehyde. For neuropathological diagnosis, paraffin sections from cortical and subcortical brain regions were stained with H&E, and thiofavine-S, and immunostained with antibodies against ubiquitin and α-syn.

Three different α-syn TG mouse lines were used for this study: PDGF α-syn WT (Rockenstein et al., 2002), mThy1 α-syn WT (van der Putten et al., 2000) and MBP α-syn WT (Shults et al., 2005). Control experiments were performed with age-matched non-TG littermates. The PDGF α-syn WT TG mice display abundant α-syn accumulation in the neocortex and limbic system and mimicks some aspects of diffuse LBD, the mThy1-syn WT shows more abundant accumulation of α-syn in subcortical regions with motor defects and mimics some aspects of PD. The MBP α-syn TG line accumulates syn in oligodendrocytes in cortical and subcortical regions and mimics some aspects of MSA. In accordance with NIH guidelines for the humane treatment of animals, mice were euthanized (at 6 months of age) by deep anesthesia with chloral hydrate. Brains were removed and divided sagitally. One hemibrain was post-fixed in phosphate-buffered 4% paraformaldehyde (pH 7.4) at 4°C for 48 h and sectioned at 40 µm with a Vibratome 2000 (Leica, Germany), while the other hemibrain was snap frozen and stored at −70°C for western blot analysis.

Immunocytochemistry

S87-P in transgenic mice

To investigate the distribution of the phosphorylated α-syn epitopes brains from non-TG and TG mice, serially-sectioned, free-floating, blind-coded vibratome sections were incubated overnight at 4°C with either the mouse monoclonal antibody against α-syn (syn-1, 1:500, Transduction Laboratories), rabbit polyclonal anti- human α-syn specific antibody (Chemicon, 1:500), mouse monoclonal against S129-P α-syn and the rabbit polyclonal against S87-P α-syn, as described previously (Masliah et al., 2000). Incubation with the primary antibody was followed by anti-mouse IgG or goat anti-rabbit IgG (1:100, Vector) followed by avidin D-HRP and DAB. Sections were analyzed with and Olympus bright field video microscope. For each case, three sections were analyzed and the results were averaged and expressed as mean pixel intensity.

Analysis of injected rat brains

For Immunofluorescence, slices were washed overnight in PBS and incubated 30 min in H2O2 for 30 min at room temperature, then blocked in a solution of 5% Bovine Serum Albumin (BSA, Sigma), 10% Normal Goat Serum (NGS, Vector Laboratories, Burlingame, CA, USA) and 0.1% Triton X-100 (AppliChem, Darmstadt, Germany) in PBS, during 2hrs at room temperature. Slices were then incubated overnight at 4°C with the primary anti-TH (1:500; AB152; Millipore, MA, USA) and anti-Human α-syn (1:500; LB509, Zymed laboratories, CA, USA) antibodies in blocking buffer and subsequently incubated for 2hrs at room temperature with secondary antibodies conjugated to Alexa Fluor-488 or Alexa Fluor-568 (1:1000; Molecular Probes, Invitrogen AG, Basel, Switzerland). Slices were finally washed and mounted on glass slides using DABCO mounting solution (Sigma-Aldrich). For the enzymatic revelation, slices were washed overnight in PBS and incubated in phenylhydrazine (Aldrich; Steinheim, Germany) for 1h at 37°C and blocked in a solution of 5% BSA, 10% NGS and 0.1% Triton X-100 in PBS, during 2 h at room temperature. Slices were incubated overnight at 4°C with the primary antibody anti-P Ser 87 (1:100) and then incubated for 2hrs with the biotinylated secondary antibody (1:200; Vector Laboratories, Burlingame, CA, USA) followed by incubation in avidin–biotin–peroxidase complex (Vector Laboratories, Burlingame, CA, USA) for 30min at room temperature. Sections were finally revealed with 3,3′-diaminobenzidine solution (DAB) and mounted on glass slides with Merckoglas mounting medium (Merck; Darmstadt, Germany).

Double labeling and confocal microscopy

To determine the co-localization between α-syn immunolabeled-neurons and CK1, 40 µm-thick vibratome sections from α-syn TG mice were immunolabeled with the rabbit polyclonal antibodies against α-syn (Chemicon, affinity purified polyclonal, 1:500) (Masliah and Rockenstein, 2000) and CK1δ ((C-18); Santa Cruz Biotechnology, 1:100). The CK1 positive cells were detected with the Tyramide Signal Amplification™-Direct (Red) system (1:100, NEN Life Sciences, Boston, MA) while α-syn immunoreactive was detected with the goat anti-rabbit fluorescein isothiocyanate (FITC) antibody (Vector, 1:75). This system allows the simultaneous detection of signals from antibodies from the same species. All sections were processed under the same standardized conditions. The immunolabeled blind-coded sections were serially imaged with the laser scanning confocal microscope (LSCM, MRC1024, BioRad). For each mouse, a total of three sections were analyzed and for each section, four fields in the frontal cortex and hippocampus were examined.

Detection of S87-P in Lewy Bodies

Lewy body enrichment was conducted as previously described (Gai et al 2000). Fresh frozen brain tissues were from 3 diffuse Lewy body disease cases (sex/age at death/postmortem interval (hr): m/80/6, m/74/24, f/81/12). Grey matter was dissected temporal cortex comprising of the superior, middle, inferior, and fusiforml gyri from a 1 cm thick coronal slice at the level of caudal amydgaloid, and homogenized in 4 volumes of homogenization buffer (HB) (0.32 M sucrose, 50 mM Tris-HCl at pH 7.4, 5 mM EDTA, leupeptin 1 mg/ml, pepstatin 1 mg/ml, phenylmethylsulfonyl fluoride 17.4 mg/ml), and homogenized in a Dounce homogeniser (Wheaton, NJ) by 10 strokes of pestle A and 10 strokes of pestle B. The homogenate was filtered through glass wool and centrifuged for 10 min at 1000 × g. The pellet was adjusted to 6 ml with HB and Percoll to 14% (vol/vol) of Percoll concentration. The suspension was overlaid on 2.4 ml of 35% Percoll (vol/vol in HB) and centrifuged for 30 min at 35,000 × g. The material between the sample-35% Percoll interface was collected and washed once in TBS (50 mM Tris–HCl buffered saline pH 7.4 and protease inhibitors) by centrifugation for 10 min at 4000 × g. The above procedures were conducted either on ice or at 4°C. The pellet was resuspended in 10 volumes of TBS and smeared onto gelatin-coated slides and air-dried at room temperature.

The smears were fixed for 10 min with 2% paraformaldehyde with 0.2% picric acid in phosphate buffered saline, followed by 3×5 min washes with TBS-azide (20 mM Tris-HCl, 0.15M NaCl, 0.1% sodium azide, pH 7.4), blocked for 60 min with 20% normal horse serum (NHS) in TBS-azide, incubated overnight with primary antibody pairs constituted in 1% NHS TBS-azide. Primary antibodies were affinity-purified sheep anti-α-syn (Gai et al 1999) used at 5µg/ml, affinity purified rabbit anti-S87-P α-syn, and mouse monoclonal11A5 anti-pS129 α-syn (Anderson et al 2006). Omitting primary antibodies were used as negative controls. Omitting Following 3×5 min washes with TBS-azide, the smears were incubated for 1 hr with Alexa 594 or Alexa 488 conjugated donkey anti-sheep, donkey anti-rabbit, or donkey anti-mouse (Molecular Probes). The smears were washed 3×5 min washes with TBS-azide, and coverslipped with 20 µl of Vectashield mounting medium, sealed with nail polish, and examined using a Leica TCS SP5 Spectral Confocal Microscope.

Cloning, Expression, and Purification of α-Syn Variants

The S129E, S129A, S87A and S87E α-syn mutants were generated using site-directed mutagenesis employing complementary internal mutagenic primers and two-step PCR. All cDNA sequences were confirmed by sequencing. All proteins used in these studies were expressed as previously described (Kessler et al., 2003), except those used for NMR studies (see below). Cell lysis (Microfluidics Corporation M110-EHI) was followed by ammonium sulfate precipitation [30% (w/v) solution], anion exchange chromatography (Amersham Biosciences Q Sepharose) in 10 mM Tris-HCl/1 mM EDTA/pH 8.0, and cation exchange chromatography (Amersham Biosciences S Sepharose) in 10 mM sodium acetate/1 mM EDTA/pH 4.0. The final homogeneity of each preparation was determined by densitometric analysis of Coomassie-stained SDS-PAGE gel scans (NIH Image 1.61/ppc program). Purified preparations were lyophilized from ammonium bicarbonate buffer (100 mM) (buffer exchange achieved by Amersham Biosciences G25 chromatography) and stored at −20°C until use. For the NMR studies, expression and purification of unlabelled and 15N-labeled α-syn were performed as described (Eliezer et al., 2001; Hoyer et al., 2002). To enable attachment of a spin label, a single Cys was introduced intọ α-syn at position 18 (A18C). The nitroxide spin label chosen for reaction with the Cys-containing mutant was MTSL (1-oxy-2, 2, 5, 5-tetramethyl-D-pyrroline-3-methyl)-methanethiosulfonate (Toronto Research Chemicals, Toronto, Ontario, Canada). MTSL has already been shown to efficiently react with α-syn Cys mutants and the reaction was carried out as described previously (Bertoncini et al., 2005).

In vitro Phosphorylation and Dephosphorylation assays

WT or mutant α-syn was phosphorylated by CK1delta (specific activity 2,000,000 U/mg) (NEB) at concentrations of 1.446 mg/ml (unless otherwise stated), in the presence of 1.09 mM ATP (Sigma), 1× reaction solution supplied with the enzyme and 1200U of CK1/145 µg of α-syn. The phosphorylation reaction was incubated at 30°C for the stated time points and the reaction was stopped with ethylenediaminetetraacetic acid (EDTA) disodium salt (5 mM final concentration) (Axon Lab). The progress of the reaction was monitored by RP-HPLC and mass spectrometry (Wilkins et al., 1999). α-Syn dephosphorylation was performed with Calf Intestinal Alkaline Phosphatase (CIAP) (Promega, Madison USA). Briefly, α-syn previously phosphorylated at both S87 and S129 by CK1 was incubated 1h at 37°C with CIAP at the concentration of 200 U/µl (2000U/µg of protein) in 1× CIAP buffer. The reaction was stopped by adding the loading buffer and the progress of the phosphorylation reaction was monitored by western blot using antibodies against S87-P and S129-P.

Fibrillization Studies

To probe the effect of CK1 mediated phosphorylation on the aggregation of α-syn, 100 µM WT and mutant α-syn that were first phosphorylated and then subjected to fibrillization conditions, at 37°C with continuous shaking for the indicated time points. The unphosphorylated controls were treated under the same conditions as the phosphorylated samples, but CK1 was not added to them. The extent of fibril formation was monitored by ThT fluorescence assay and by determining the amount of soluble monomeric and oligomeric α-syn in solution at indicated time point during the aggregation process (Paleologou et al., 2008).

Gel Electrophoresis (SDS-PAGE) and Immunoblotting

α-Syn samples were diluted in loading buffer and separated on 12% SDS 1 mm gel. Gels were stained with Simply Blue Safe stain (Invitrogen) or silver stained (Invitrogen) according to manufacturer’s instructions. For western blots, membranes were probed with the primary antibody [mouse monoclonal anti- α -syn (121–125) (211) at a dilution of 1:500 (Santa Cruz Biotechnology) or mouse antị-α-syn (15–123) at a dilution of 1:1000 (BD Transduction), or mouse monoclonal anti-S129-P α -syn at a dilution of 1:5000 (Wako), or rabbit polyclonal anti-S87-P α -syn at a dilution of 1:100] at RT for 1–2 hours. Following incubation with the secondary antibody (i.e. goat anti-mouse ALEXA Fluor 680) protected from the light at RT, for 1 h and washing with PBST (4×), the immunoblots were scanned in a Li-COR scanner at a wavelength of 700 nm. The western blot analysis for brain homogenates was carried out as following. Brain homogenates that include the frontal cortex and the striatum were separated by ultracentrifugation as previously described into cytosolic and membrane fractions (Masliah and Rockenstein, 2000). Samples from both cytosolic and membrane fractions were separated on 12% or 4–12% SDS-PAGE gels (NuPAGE, Invitrogen) and transferred onto 0.22 µM nitrocellulose membranes (Schleicher & Schunell, Keene, NH) using 1× 3-[Cyclohexylamino]-1-propaneosulfonic acid (CAPS) transfer buffer containing 20% methanol. Membranes were blocked with 3% milk in PBS containing 0.1% Tween-20 (Sigma) (PBS-T), followed by incubation in primary antibody (1:1000) in PBS-T overnight at 4 °C. The primary antibodies used were as follows: rabbit polyclonal against total α-syn (Chemicon); mouse monoclonal against S129-P α-syn (courtesy of Dr. T Iwatsubo, Tokyo University), rabbit polyclonal against S87-P α-syn and mouse monoclonal against α-actin (Chemicon International, Temecula, CA). Membranes were further incubated with goat anti-mouse or anti-rabbit IgG secondary antibodies conjugated to horseradish peroxidase (1:5000, American Qualex, San Clemente, CA) and visualized by enhanced chemiluminescence (ECL, NEN Life Sciences, Boston, MA) and exposed to film. For determinations of levels of immunoreactivity, ECL treated membranes were analyzed in the VersaDoc imaging system (Bio-Rad, Hercules, CA) using the Quantity One software (Bio-Rad).

Preparation of Large Unilamellar Vesicles (LUV) and Small Unilamellar Vesicles (SUV) and α-syn-liposome complexes

1-Palmitoyl-2-Oleoyl-sn-Glycero-3-[Phospho-rac-(1-glycerol)] (Sodium salt) (POPG) (Avanti Polar Lipids Inc.) was purchased in chloroform which was removed by evaporation and lyophilization. The residual phospholipid was hydrated with 50 mM HEPES (Fluka), 150 mM NaCl (Fluka), pH 7.4 solution, giving rise to a phospholipid suspension of 10 mg/ml. To increase the efficiency of LUVs formation, 10 cycles of freezing in dry ice and thawing at 37°C water bath were carried out. SUVs were prepared by extrusion through a 100 nm polycarbonate membrane (Avestin Inc.) according to manufacturer’s instructions. The SUVs were stored at 4°C and used within 3–5 days. The appropriate amount and volume of α -syn in PBS or sodium phosphate, pH 7.5 was mixed with the appropriate volume of POPG to generate a mass ratio of α -syn:POPG of 1:20. The α-syn-liposome complex was incubated for 2 h at RT prior to CD spectroscopy.

Circular Dichroism (CD)

The average secondary structure of monomeric α-syn in the presence and absence of 1-Palmitoyl-2-Oleoyl-sn-Glycero-3-[Phospho-rac-(1-glycerol)] (Sodium salt) (POPG) (Avanti Polar Lipids Inc.) vesicles was determined by CD spectroscopy using a Jasco 810 Spectrometer. The Far UV-CD spectra (190–250 nm, integration time of 2 seconds for 0.2 nm) were collected at RT in a 1 mm path length quartz cuvette containing 0.1 mg/mL of α-syn in PBS or sodium phosphate buffer and vesicles were prepared as described in (see supporting materials).

Transmission Electron Microscopy (TEM)

For EM studies, WT or mutant α-syn samples were deposited on Formvar-coated 200 mesh copper grids (Electron Microscopy Sciences) at a concentration of 25 µM. Grids were washed with two drops of water and stained with two drops of freshly prepared 0.75% (w/v) uranyl acetate (Electron microscopy sciences). Specimens were inspected on a Philip CMX 10 electron microscope, operated at 100 kV. Digitized photographs were recorded with a slow scan CCD camera (Gatan, Model 679).

Nuclear magnetic resonance (NMR)

NMR samples of free α-syn contained ~ 0.1 mM 15N-labeled WT or mutant α-syn in 90% H2O/10% D2O, 50 mM phosphate buffer at pH 7.4, 100 mM NaCl. NMR experiments were acquired on Bruker Avance 600 and 700 MHz NMR spectrometers. The temperature was set to 15°C. NMR data were processed and analyzed using NMRPipe (Delaglio et al., 1995) and Sparky 3 (T. D. Goddard and D. G. Kneller, SPARKY 3, University of California, San Francisco) and NMRView (Johnson and Blevins, 1994). Spectra were referenced indirectly to DSS and ammonia using the known chemical shift of water (Wishart et al., 1995). Tentative assignments for the spectra of mutant and phosphorylated proteins were obtained by transferring each previously assigned cross peak in the 1H -15N heteronuclear single quantum coherence (HSQC) spectrum of the WT protein to the nearest unassigned cross peak in each new spectrum. Subsequently, they were verified by 3D HNHA and 3D NOESY-HSQC spectra (Bax and Grzesiek,, 1993). 3J(HN,Hα) scalar couplings were measured using intensity modulated HSQC experiments (Permi et al., , 2000). 15N R spin relaxation rates were measured with a pulse sequence based on Farrow et al. (Farrow et al., 1994) on a Bruker Avance 600 MHz spectrometer. Relaxation delays were set to 8, 48, 64, 128 and 184 ms. The spin lock frequency was 2.5 kHz. Relaxation times were calculated by fitting an exponential function to the decaying signal integrals. Steady-state heteronuclear 15N{1H} -NOE values are reported as the ratio of peak heights in paired spectra collected with and without an initial period (4 s) of proton saturation during the 5-s recycle delay. Pulse field gradient NMR experiments were acquired on unlabeled WT and mutant α-syn (concentration of 200 µM) dissolved in 99.9 % D2O, 50 mM phosphate buffer pH 7.4 and containing dioxane (concentration ~ 20 mM) as an internal radius standard and viscosity probe (Wilkins et al., 1999). Twenty one-dimensional 1H spectra were collected as a function of gradient amplitude employing the PG-SLED sequence (Jones et al., 1997; Wilkins et al., 1999). Each experiment was repeated at least two times. The gradient strength was increased from 1.69 to 33.72 Gauss/cm, in a linear manner. Signals corresponding to the aliphatic region of the 1H spectra (3.3-0.5 ppm) were integrated and diffusion data (signal intensity versus gradient strength) were fitted to Gaussian functions using XWINNMR (Bruker Instruments, Karlsruhe, Germany). Stokes radii of α-syn were calculated from the apparent diffusion coefficients of α-syn and dioxane, and the known Stokes radius of dioxane (Jones et al., 1997). Errors in stokes radii estimated from repeat measurements are about 0.5 Å.

The in situ phosphorylation assay was performed in a Shigemmi NMR tube, at 15 °C, with a sample containing 100 µM 15N-labeled WT or mutant α-syn and 2 mg/ml CK1 (specific activity 2,000,000 U/mg) (New England Biolabs) in the standard phosphorylation buffer. After addition of 1.5 mM ATP solution, a series of 1H-15N HSQCs was started on a Bruker 600 MHz spectrometer. Each HSQC was measured with 16 scans per increment for 90 minutes.

For NMR studies of micelle-bound α-syn, lyophilized protein was dissolved in sample buffer (100 mM NaCl, 10 mM Na2HPO4, pH 7.4 in 90%/10% H2O/D2O) with 40 mM deuterated SDS (Cambridge Isotope). Spectra were recorded on either Varian INOVA 600 MHz (Weill Cornell) or a Bruker Avance 800 MHz (New York Structural Biology Center) spectromteres at sample temperature of 40 °C. 2D and 3D double and triple resonance data, including HSQC, HNCACB, CBCACONH, HNCO, HNCACO and HSQC-NOESY-HSQC, were collected using standard pulse sequences. A mixing time of 150 ms was used for the NOESY experiment. Typical spectral widths were 10, 20, 8 and 53 PPM in the proton, nitrogen, CO and C dimensions. Data were processed using NMRPipe (Delaglio et al., 1995) and analyzed using NMRView (Johnson, 1994).

Results

Characterization of α-syn phosphorylation in TG models of synucleinopathies and human brain from AD, LBD, and MSA patients

In order to determine the physiological and pathological relevance of S87 phosphorylation, we generated a rabbit polyclonal antibody, anti-S87-P, against a synthetic peptide that corresponds to amino acid residues 81–93 of human α-syn, with S87 being phosphorylated. Figure 1A demonstrate that our anti-S87-P antibody specifically detects serine 87 phosphorylated forms (S87-P) of α-syn, and reveals the absence of immunoreactivity against either unphosphorylated, S129A or S129-P α-syn. To rule out the possibility that the lack of immunoreactivity of S87A is due to a loss of the epitope rather than lack of phospohorylation, the specificity of the antibody was verified by probing its immunoreactivity toward diphosphorylated α-syn (S87-P/S129-P) after phosphatase (CIAP) treatment. Phosphatase treatment resulted in the loss of immunoreactivity toward both anti S87-P and anti-S129-P antibodies (Fig. 1B), consistent with the loss of the phosphate group on both residues. Thus, providing further verification of the specificity of both antibodies.

Figure 1
Specificity of anti-S87-P antibody

To probe the specificity of our S87-P antibody and determine if phosphorylation at this residue occurs in vivo, we characterized the level of S87-P in slices from rat brains injected on one side with an AAV2/6 viral vector over-expressing the S129A variant of α-syn A30P (Fig. 1 C–H, n=3). As a control, we also examined tissues from rat brains injected a mutant form of the same protein, in which phosphorylation at S87 was blocked by a serine to aspartate substitution at position 87 (S87D/S129A–A30P) (Fig. 1 I–N, n=3). In both cases, the uninjected side served as an additional control to assess the level of background signal due to non-specific interactions and antibody cross-reactivity with other proteins. We detected a strong staining against human A30P α-syn in the injected substantia nigra (Fig. 1E, K) compared to the non-injected side (Fig. 1F, L). However, anti-S87-P staining was exclusively detected in the substantia nigra over-expressing human S129A α-syn (Fig; 1G) and no labelling was detectable, neither in the non-injected side (Fig. 1H, N) nor in the substantia nigra over-expressing the S87D/S129A mutant (Fig. 1M). These findings demonstrate conclusively that phosphorylation at serine 87 does occur in vivo, at least under conditions of increased α-syn expression (corresponding to an approximate doubling of the total α-syn level in nigral tissue extracts (Azeredo da Silveira et al. 2009)) and validate the specificity of our antibody on brain tissue. However, it is not possible to determine the overexpression levels in individual neurons.

α-Syn in LBs is phosphorylated at S87-P and S87-P levels are increased in human brains from AD, LBD, MSA patients

Having established the specificity of the antibody, anti-S87-P, together with anti-α-syn and anti-S129-P antibodies, was tested in human brain (frontal cortex) homogenates from control, AD, LBD and MSA cases. Immunoblot analysis of cortical samples, from control or diseased human brains, showed a native α-syn band at 14 kDa in the cytosolic fractions (Fig. 2A), which was significantly increased in the AD, LBD, and MSA cases relative to the control (Fig 2A, G). In the membrane fractions increased α-syn levels is detected in the LBD and MSA cases, with higher molecular weigh species being present in the LBD cases only (Fig. 2B, G). Anti-S87-P antibody detected a weak band at 14 kDa in the control cases. This band became more pronounced in the diseased brains notably in the LBD cases (Fig. 2D, H), where it was accompanied by a weaker band at around 17 kDa. The antibody against S129-P detected a band at 14 kDa as well as higher MW bands (Fig. 2 E, F, I). With both antibodies against phosphorylated α-syn most of the immunoreactivity was detected in the membrane fractions in the LBD and MSA cases but not in the controls and AD cases (Fig. 2 C, D, E, F). Several α-syn immureactive bands at molecular weights of 38 kDa and higher were detected in the control samples from LBD cases. These bands were more abundant in the membrane fractions and showed clear immureactivity towards the anti-S129-P, but at best weak reactivity to the anti-S87-P antibody.

Figure 2
Comparison of the levels of phosphorylated α-syn immunoreactivity by immunoblot in human brains from controls, AD, LBD and MSA cases

To further investigate the pathological relevance of S87 phosphorylation, we assessed S87-P levels in Lewy body samples from three diffuse Lewy body (DLB) cases. Lewy bodies were intensely labelled by the sheep anti-α-syn antibody. Therefore, the signal gain was set low (50% of S87-P α-syn signal) to show characteristic homogenous and concentric patterns, with little background or neuroile labelling (Fig. 3 left column). The S87-P α-syn immunoreactivity was less intense but readily detected in all Lewy bodies (more than 500 Lewy bodies were analyzed by confocal microscopy). The S87-P α-syn labelling appeared smooth within Lewy bodies (Fig. 3 B and E). In addition, granular S87-P α-syn labellings of 0.2–0.5µm size were also detected, more obvious in Lewy body periphery, neural processes, and neuropil (Fig. 3 A and D). No such labelling was seen when anti- S87-P α-syn antibody was omitted. These granular labellings may be complexes or cellular particles containing more concentrated S87-P α-syn. Figure. 3 J and K illustrate the relative intensities for α-syn (red line), S87-P α-syn (green) and DNA (blue) labelings across a Lewy body. However, it must be noted that fluorescence intensity depends on many factors, including the dye used, the affinity of each antibody for its epitope, the accessibility of the epitope, etc.

Figure 3
Analysis of the colocalization of S87-P and α-syn in Lewy bodies isolated from fresh brain of DLB cases

The localization of S87-P α-syn in Lewy bodies suggests it is an integrated part of the inclusions. We further examined whether S87-P α-syn is enriched in buffer insoluble fractions in brains of synucleinopathies and Alzheimer’s disease. The buffer insoluble fractions contained numerous Lewy bodies and glial inclusions and were further solublized in 5%SDS/Urea. As shown in Figure 3 L to O, S87-P α-syn reactivity was more prominent in 5%SDS/Urea fraction, compared to total α-syn reactivity. Figure 3M demonstrates that the level of S87-P in these fractions is higher in diseased brains relative to control cases.

The levels of S87-P are increased in brains of transgenic (TG) models of synucleinopathies

To further assess if S87 phosphorylation is a pathological event, we assessed its levels in brain homogenates from TG mouse experimental models of PD/LBD and MSA (Fig. 4). As expected the highest levels of α-syn expression were observed in the mThy1 α-syn TG mice followed by the PDGF α-syn and the MBP-α-syn TG both in the cytosolic (Fig. 4 A, C, E) and membrane fractions (Fig. 4 B, D, F). Bands reflecting monomers (at 14 kDa) and the oligomers (at 38–62 kDa) were detected. Consistent with the finding in the human brain homogenates, antibodies against S87-P detected a band at 14 kDa, which were significantly more abundant in the membrane fraction of the mThy1 α-syn TG mice (Fig. 4D). With antibody against S129-P, a strong 14 kDa band was detected in the cytosolic fraction of both the mThy1 α-syn and MBP α-syn TG mice (Fig. 4E). S129-P α-syn was detected at 14 and 42 kDa in the membrane fractions of the α-syn TG mice (Fig. 4F). Consistent with the western blots, immunocytochemical analysis with the antibody against total α-syn showed immunoreactivity in the neuropil corresponding to nerve terminals in the non TG mice (Fig. 5A). In the PDGF and mThy1-α-syn TG mice abundant accumulation of α-syn was detected in the neuronal cell bodies while in MBP α-syn TG mice immunoreactivity was associated with oligodendrocytes (Fig. 5B–D). With S129-P antibody abundant α-syn immunoreactivity was detected in the three lines of α-syn TG mice (Fig. 5E–H). With the S87-P antibody abundant immunoreactivity was observed in the neuronal cell bodies of the mThy1-α-syn TG (but not in the PDGF-α-syn) mice and in the inclusions in the oligodendrocytes in the MBP-α-syn TG mice (Fig. 5K, L).

Figure 4
Comparison of the levels of phosphorylated α-syn immunoreactivity by immunoblot in brains of α-syn models of LBD
Figure 5
Patterns of phosphorylated α-syn immunoreactivity in brains of α-syn models of LBD

S87-P colocalization with CK1

Among the various kinases reported to phosphorylate α-syn in vitro, CK1 and the dual specificity tyrosine regulated kinase 1A (Dyrk1A) are the only two that phosphorylate α-syn at S87. To determine the co-localization between S87-P immunolabeled-neurons and CK1, 40 µm-thick vibratome sections from the temporal cortex of α-syn TG mice and LBD/PD patients were immunolabeled with the antibodies against S87-P and CK1. Figure 6 demonstrates a great degree of colocalization of S87-P and CK1 in neuronal inclusions in Tg mice (Fig. 6A) and in Lewy body like structures in LBD/PD diseased brains (Fig. 6B), consistent with in vitro observations and suggesting that CK1 may by directly involved in modulating α-syn phosphorylation in vivo. These findings are consistent with previous cell culture studies implicating CK1 in the phosphorylation of α-syn at S129 and S87 (Okochi et al., 2000).

Figure 6
Colocalization of S87-P and CK1 within inclusions in the thy1-α-syn TG mice and LBD/PD diseased brains

Serine→Glutamate substitution or phosphorylation at S87 inhibits the fibrillization of WT and mutant (S129A and S129E) α-syn

Having verified the pathological relevance of S87 phosphorylation, we sought to understand the role of S87 phosphorylation in modulating the structure and aggregation properties of α-syn. Towards this goal, we compared the structural, oligomerization, fibrilization and membrane binding properties of monomeric WT α-syn to those of the phosphorylation mimics (S87E) as well as the purified in vitro S87-phosphorylated form of α-syn using NMR, CD, SEC, SDS-PAGE, ThT, and TEM.

Phosphorylation at S87 is sufficient to block α-syn fibrillization

Recent studies from our laboratory demonstrated that CK1 mediated phosphorylation blocks α-syn fibrillization (Paleologou et al., 2008). In vitro CK1 phosphorylation of WT α-syn followed by tryptic digestion and mapping of phosphorylation sites revealed that CK1 phosphorylates α-syn at multiple sites (S87, T92, S129), with S87 and S129 being the major phosphorylation sites (supplemental material and figures 2 and 3). To determine the relative contributions of phosphorylation at S87 to the CK1-induced inhibition of α-syn fibril formation, we examined the effect of CK1-mediated phosphorylation on the fibrillization of the S129A and S129E, both of which cannot be phosphorylated at S129. Prephosphorylation of both variants with CK1 results in significant retardation of α-syn fibrillization and a reduction in amyloid fibril formation relative to the unphosphorylated forms of both proteins (supplemental Fig. 3). S129A, S129E and the WT α-syn formed significant amounts of amyloid fibrils, whereas prephosphorylated forms of S129E (S129E/S87P) and WT (S129P/S87P) showed predominantly soluble oligomeric species. S129A rapidly forms short protofibrillar/fibrillar structures, consistent with its marked increased propensity to fibrillize (Paleologou et al., 2008). However, the amount of fibrils formed by prephosphorylated S129A is significantly less than that observed for unphosphorylated S129A.

To further prove that inhibition of α-syn fibrillogenesis is due to phosphorylation at S87, we prepared and purified the S87-P phosphorylated forms of S129A and S129E α-syn and compared their aggregation properties to those of the corresponding unphosphorylated forms of α-syn. The phosphorylated (S87-P) and unphosphorylated α-syn forms of each protein were separated by RP-HPLC and their purities were verified by MALDI-TOF mass spectrometry. We consistently observed that the mono (S87-P) and diphosphorylated (S87-P/T92-P) forms of S129A and S129E species did not form fibrils even after 48 h, whereas the unphosphorylated forms of these proteins exhibited extensive fibril formation after 24 h of incubation (Fig 7A). These observations were confirmed by SEC and TEM studies, which revealed the absence of any fibrillar aggregates and presence of predominantly monomers in the S129A/S87-P and S129E/S87-P samples (Fig. 7 B, C). Interestingly, monophosphorylated S129E/S87-P appears to form significantly less oligomeric/protofibrillar-like aggregates than S129A/S87-P, suggesting that the presence of both phosphate and Glu substitutions at S87 and S129, respectively results in a greater inhibition of α-syn fibrillization.

Figure 7
Phosphorylation at S87 inhibits S129A α-syn aggregation propensity

In the fibrillar state, only S129 undergoes phosphorylation by CK1 in vitro

According to the solid state NMR data α-syn residue 87 is in a region that is part of the rigid structure of the fibrils and within one of the beta-strands participating in the formation of the fibril structure (Kloepper et al., 2007; Heise et al., 2008; Vilar et al., 2008), suggesting that it might not be subject to phosphorylation after fibril formation has occurred. To determine if S87 is accessible and can undergo phosphorylation in the fibrillar state, we generated monomer-free fibrillar samples of WT α-syn and subjected them to in vitro phosphorylation with CK1. Phosphorylation was assessed by western blotting using antibodies against α-syn, S87-P and S129-P. We observed that only S129 undergoes phosphorylation by CK1, suggesting that S87, within α-syn fibrils, is not accessible or exists in a conformation that is not recognized by CK1 (supplemental Fig. 5).

The phosphomimic S87E aggregates slower than WT and S87A α-Syn

Selective phosphorylation and/or overexpression of S87-P in vivo is currently not possible, as CKI phosphorylates at both S87 and S129 and DYRK1A mediated phosphorylation at S87 is less efficient. Therefore, future efforts to assess the role of S87 phosphorylation in modulating the normal biology and aggregation of α-syn in vivo are likely to rely on the use of the phosphomimics S87E and S87A. Recent studies from our group (Paleologou et al., 2008) and others (Waxman and Giasson, 2008; McFarland et al., 2009) demonstrate that substitution of S129 by glutamate or aspartate does not reproduce the effect of phosphorylation at this site on α-syn structure and aggregation properties in vitro. Having established that S87-P is sufficient to inhibit α-syn oligomerization and fibrillogenesis, the 87 mutants S87A and S87E were generated to assess whether the phosphorylation mimic S87E is likely to mimic S87 phosphorylation in vivo. Comparison of the fibrillization of WT, S87A and S87E α-syn showed that S87A aggregated at a similar rate and to similar levels as WT α-syn, whereas for S87E the observed aggregation rate was slower than those of the WT and S87A proteins (Fig. 7D). TEM images further confirmed these findings, as both WT and S87A formed dense networks of fibrils as opposed to S87E, which formed a few short fibrils after 72 h of aggregation (Fig. 7F). In accordance with these findings, the consumption of monomeric protein over time monitored by SEC and SDS-PAGE analysis also revealed a significant decrease in monomeric WT and S87A (Fig. 7 B, E), whereas the levels of the monomeric S87E α-syn remained virtually unchanged over the 72 h of aggregation, providing further evidence that S87E does not aggregate.

α-Syn is disordered independent of phosphorylation at S87

Serine 87 lies in the hydrophobic NAC region of α-syn, suggesting that the introduction of a negative charge through the substitution of serine by glutamate at this position is unfavourable and may alter the secondary structure and hydrodynamic properties of monomeric α-syn. Figure 8A demonstrates that WT, S87A and S87E α-syn exhibit virtually identical random coil and α-helical CD spectra in solution and upon binding to synthetic membranes, respectively. Given that α-syn exists predominantly in a random coil conformation, subtle changes in the secondary structure of the protein are unlikely to be discernable by CD studies. Therefore, to further elucidate the consequences of phosphorylation on the structure and dynamics of monomeric α-syn, high-resolution NMR studies were also conducted. For all proteins, the resonances in 1H-15N HSQC spectra were sharp and showed only a limited dispersion of chemical shifts, reflecting a high degree of backbone mobility (Fig. 8B). Upon phosphorylation of WT α-syn by CK1, the resonances of S87 and S129 were strongly attenuated at the position seen in the proton-nitrogen correlation (HSQC) of the unphosphorylated protein, but new signals appeared in the region, in which resonances of phosphorylated amino acids are usually found (supplemental Fig. 4A). For S129D α-syn, phosphorylation at S129 was blocked so that only the resonance of S87 was attenuated at its original position and appeared at its phosphorylated position (Fig. 8B). Other chemical shift changes induced by phosphorylation were generally small. In addition, steady-state heteronuclear 15N[1H]-NOEs (Fig. 8C), 15N R relaxation rates and 3J(HN,Hα) couplings (supplemental Fig. 4) were very similar for unphosphorylated and phosphorylated α-syn, indicating that phosphorylation at S87 has no apparent effect on the secondary structure of α-syn.

Figure 8
α-syn is disordered independent of phosphorylation at S87

Pulse field gradient NMR experiments allow accurate determination of the diffusion coefficient of a molecule. From the diffusion coefficient, a hydrodynamic radius Rh can be calculated that provides an estimation of the overall dimensions of a biomolecule (Farrow et al., 1994). For WT and S129D α-syn, we determined hydrodynamic radii of 28.2 Å and 28.1 Å, respectively (Fig. 8D). The phosphorylation mimic S87E did not change the hydrodynamic radius of α-syn. On the other hand, phosphorylation of S129A and S129D α-syn at S87 increased Rh by 2.6 and 1.9 Å (Fig. 8D). Addition of 8 M urea to phosphorylated S87A α-syn further increased the Rh value to 36.2 Å. If α-syn were a true random coil, a hydrodynamic radius of 36.9 Å would be expected (Kohn et al., 2004). Interestingly, phosphorylation of S129 appears to have a more dramatic effect on the hydrodynamic radius of monomeric α-syn as it results in an increase of Rh by ~ 5.0 Å. This result is consistent with our previous studies demonstrating disruption of the intramolecular interactions between the C and N-terminal regions of α-syn upon phosphorylation at S129 and suggest that phosphorylation at S87 may only partially disrupt this interaction (Paleologou et al., 2008).

Phosphorylation at S87 results in changes in protein conformation upon membrane binding

In the presence of SDS micelles, the lipid-binding domain of α-syn adopts a conformation consisting of two helical segments, which have been previously characterized using NMR (Eliezer et al., 2001; Bussell and Eliezer, 2003; Chandra et al., 2003; Ulmer and Bax, 2005). A comparison of proton-nitrogen correlation spectra of micelle-bound phosphorylated WT (S87-P and S129-P) α-syn and its unphosphorylated counterpart shows that the resonances of S87 and S129 of the phosphorylated protein are dramatically shifted. In addition to local changes, many resonances of amino acids in the vicinity of S87-P were also shifted (79, 81, 83, 84, 85, 86, 88, 89, 91, 92, 93, 94, 95, 96) (Fig. 9A). Most of these amino acids are part of the second helix that α-syn adopts upon binding to micelles. Relatively less extensive shifts were observed in the resonances of amino acids close to S129, consistent with our previous studies of the effects of phosphorylation at this site (Paleologou et al., 2008). Similar changes in the vicinity of S87-P were made when comparing the HSQC spectra of S129A/S87-P (Fig. 9B) and S129E/S87-P (Fig. 9C) and their unphosphorylated counterparts, strongly suggesting that changes occur in the environment of the second helix are a result of S87 phosphorylation.

Figure 9
Phosphorylation at S87 results in changes in protein conformation upon membrane binding

In order to quantify the chemical shift changes between the phosphorylated and unphosphorylated micelle-bound proteins, the resonances of each form of S129A α-syn were directly assigned using triple resonance methods. Graphs of the resulting weighted average of the amide proton and nitrogen chemical shift changes between the phosphorylated and unphosphorylated proteins are shown (Fig. 9E) for S129A /S129A–S87-P. A similar graph was generated for S129E/S129E–S87-P (Fig. 9F) by transferring the S129A assignments. The data demonstrate clearly that relatively large chemical shift changes take place at sites close to S87 in both phosphorylated proteins, with more minor changes spanning the region between residues 60 and 80. Chemical shift changes observed upon comparing micelle-bound unphosphorylated S129A or S129E with WT α-syn were restricted to the immediate sites of the mutation and were essentially identical to those previously observed for the free protein (Paleologou et al., 2008), indicating that the mutations themselves do not cause long-range effects.

To better understand the effects of S87 phosphorylation on the micelle-bound structure of α-syn, we analyzed both sequential HN-HN NOE and Cα chemical shift data. The NOE data (Fig. 10A) reveal a decrease in signal intensity, when compared with those previously obtained for the WT protein, in the second half of the second micelle-bound helix, coinciding with the location of the phosphorylated S87 residue and suggesting a possible decrease in the stability of the helical structure in this region. Accordingly, secondary Cα chemical shift data (Fig. 10B) also show smaller positive amplitudes in this region when compared with previous observations for the unphosphorylated WT protein. Interestingly, these structural effects are similar to those observed for the protein β-syn, a close homologue of α-syn, which is however missing 11 residues from the NAC region (Sung and Eliezer, 2006, 2007).

Figure 10
The effects of S87 phosphorylation on the micelle-bound structure of α-syn

To further probe the effect of phosphorylation on α-syn-membrane interactions, we compared the CD spectra of mono- (S129A/S87-P) and diphosphorylated S129A (S129A/S87-P,T92-P) to that of S129A and WT α-syn in solution and upon binding to POPG vesicles. Although the effect of phosphorylation at S87 and T92 at the monomer is not discernable by Far-UV/CD (Fig. 10C), both mono- (S129A/S87-P) and diphosphorylated (S129A/S87-P,T92-P) exhibit reduced α-helical propensity in the presence of synthetic vesicles with diphosphorylation having the most dramatic affect (Fig. 10D).

Discussion

α-Syn S87 phosphorylation occurs in vivo and is increased in synucleinopathies

Phosphorylation is an important reversible post-translational modification that regulates the structural and functional properties of proteins in health and disease. The role of phosphorylation in modulating the aggregation and fibrillogenesis of tau and α-syn is currently a subject of intense investigation and pathways involved are being pursued as viable targets to prevent or slow down the progression of AD and PD (Glicksman et al., 2007; Wen et al., 2008; Rezai-Zadeh et al., 2008). While hyperphosphorylation of tau at different sites has been well characterized and the role of tau phosphorylation in AD pathology was investigated in several mouse models of AD, a thorough mapping and investigation of all phosphorylation sites within α-syn and of the kinases involved remains to be accomplished. Several kinases phosphorylate α-syn at S129 (Okochi et al., 2000; Pronin et al., 2000; Fujiwara et al., 2002; Takahashi et al., 2003a; Chen and Feany, 2005; Kim et al., 2006; Qing et al., 2009; Inglis et al., 2009; Mbefo et al., 2009) and S87 (Okochi et al., 2000; Pronin et al., 2000), as well as Y125 (Ellis et al., 2001; Nakamura et al., 2001; Hasegawa et al., 2002; Takahashi et al., 2003a), Y133 (Ellis et al., 2001; Negro et al., 2002) and Y136 (Ellis et al., 2001; Negro et al., 2002) in vitro. However, only phosphorylation at S129 has been shown to correlate with the pathology of PD and related α-synucleinopathies. Here we demonstrate that α-syn is phosphorylated at S87 in vivo and the level of S87-P is increased in brains of TG models of synucleinopathies and human brains from AD, LBD, and MSA patients. To determine if α-syn in LBs is also phosphorylated at S87, we performed immunofluorescence stainings of LBs isolated from fresh human brains using our anti S87-P antibody. S87-P immunoreactivity was consistently detected in homogeneous presumably earlier stages of formation as well as mature LBs, suggesting S87-P α-syn occurs throughout the life span of LB development.

Both S87 nor S129 phosphorylation are found in LB, but are they not responsible for LB formation

Previous studies from our group and others demonstrated that phosphorylation at S129 blocks, rather than inhibit α-syn fibrillization. Herein, we show that phosphorylation at S87 also inhibits α-syn fibrillization in vitro. Together, these findings suggest that phosphorylation at these residues should inhibit, rather than promote LB formation in vivo. Our findings that S129, but not S87, undergoes phosphorylation by CK1 in the fibrillar state is consistent with the solid state NMR results and favour the hypothesis that phosphorylation at S129 is a late event that occurs after α-syn fibrillization and/or during the development and maturation of LBs. The increased level of S129-P is consistent with its being further away from the core of the fibrils and in a region that is highly disordered and thus more accessible to phosphorylation by kinases. The co-localization of several kinases (Arawaka et al., 2006; Ryu et al., 2007) and α-syn within LBs combined with recent studies from our group (Mbefo et al., 2009) and by Waxman and Giasson (Waxman and Giasson, 2008) demonstrating that aggregated α-syn species are better substrate for CK1, CK2 and the Polo Like Kinases (PLK 1–3) suggest that S129 phosphorylation could easily occur subsequent to LB formation. When combined with our own observations that S129 phosphorylation actually inhibits α-syn fibrillization (also confirmed by a recent study by Waxman and Giasson (Waxman and Giasson, 2008)), these observations provide strong support for the hypothesis that phosphorylation at S129 is in fact not a prerequisite for LB formation and more likely occurs after α-syn fibrillization (Fig. 10B).

Recent studies by Fournier et al, using our anti-S87-P antibody, demonstrated that S87-P was only observed in the TBS soluble fractions, whereas S129-P was observed in both soluble and SDS fractions from healthy and symptomatic mice overexpressing α-syn or α-syn and Parkin (Fournier et al., 2009). These results combined with the presence of S87 in a β-strand conformation within the core of fibrils are consistent with our results showing the inhibition of α-syn fibrillization upon phosphorylation of this site and the lack of phosphorylation in the pre-formed fibrillar state, but do not explain how this residue becomes phosphorylated within LBs. These observations could be explained if α-syn within LBs exists in different aggregated and/or fibrillar states some of which may possess different core-structure than α-syn fibrils formed in vitro. From the Lewy body data we have gathered, it appears that s87P has been incorporated in Lewy bodies at early (with homogeneous morphology) as well as later (concentric morphology) stages of maturation. Alternately, the Lewy bodies we typically observe may perhaps reflect later events of the disease process and are likely generated from small α-syn aggregates originating in sites where α-syn turnover is most active, for instance at synapses. Small α-syn aggregates may be retrogradely transported through axons, sometimes leading to the formation of Lewy neurites. We did not detect S87-P in Lewy neurites, suggesting that S87 phosphorylation is indeed a later event occurring after the formation of early aggregates. Thus, S87 phosphorylation may occur subsequent to early α-syn aggregation, but prior to the formation of the mature amyloid fibril form, in which S87 is no longer accessible to the responsible kinases. Further studies will be required to determine the aggregation states of S87-P immunoreactive material within LBs and to determine the kinetics of, and interplay between, S87 and S129 phosphorylation during the evolution of LBs.

S → E mutation at S87 or S129 mimic only some aspects of phosphorylation

Recent studies by two independent research groups demonstrated that AAV mediated overexpression of the S129A in the substantia nigra of rats results in both increased aggregation and loss of dopaminergic neurons relative to overexpression of WT and S129D α-syn (Gorbatyuk et al., 2008; Azeredo da Silveira et al., 2009). Thus it appears that the increased in vivo aggregation caused by the S129A mutation (which also promotes α-syn aggregation in vitro) may lead to toxicity that is unrelated to its effect in blocking phosphorylation at S129. To properly probe the role of phosphorylation in vivo it is essential that mutants designed to abolish phosphorylation should exhibit aggregation properties similar to that of the WT protein. Similarly, phosphorylation mimicking mutations should reproduce the structural and functional consequences of α-syn phosphorylation. Neither the S129A nor S129D/E mutants fulfill these criteria as demonstrated by both the in vivo studies cited above and our own recent in vitro studies. In contrast, as we show here, the S87A and S87E mutants come closer to fulfilling these criteria. Figure 7 demonstrates that S87A exhibits similar fibrillization properties as the WT protein, whereas S87E does not form fibrils, suggesting S→E substitution at S87 reproduces the effect of phosphorylation on α-syn aggregation. Together these findings suggest that overexpression of S87E and S87A mutants should facilitate the elucidation of the role of phosphorylating this residue on modulating α-syn oligomerization and fibrillogenesis in vivo

Nevertheless, the fact that phosphorylation at S87 (S87-P), but not the phosphomimic S87E, induced significant changes in the conformation of membrane bound α-syn which coincided with a slight reduction in the propensity of S87-P to form α-helical structure upon binding to membranes, suggest that S87E may not recapitulate phosphorylation-dependent protein-membrane interactions. Our findings demonstrate that detailed and careful biophysical characterization of the phosphorylated proteins and their phosphomimics can assist in designing and interpreting in vivo studies aimed at elucidating the role of phosphorylation in health and disease.

Potential role of S87 and S129 in regulating phosphorylation dependent protein-protein interactions

Phosphorylation of proteins represents an important molecular switch for regulating protein-protein and protein-ligand interactions and thus protein function. The C-terminal region of α-syn has been implicated in the majority of α-syn interactions with proteins (Jensen et al., 1999; Giasson et al., 2003; Fernandez et al., 2004) and metal ions (Paik et al., 1999; Brown, 2007) and phosphorylation in this region is likely to influence the affinity of α-syn for other proteins and thereby alter the biochemical and biological processes regulated by its interactions. Indeed, McFarland and colleagues recently showed differences in the set of proteins pulled down by S129- or Y125-phosphorylated forms of α-syn.

S87 lies in the NAC region, which is crucial in mediating α-syn fibrillization, and our results accordingly demonstrate that S87 phosphorylation exerts a profound effect on α-syn aggregation. Interestingly, our results also show that S87 phosphorylation alters the conformation of membrane bound α-syn and decreases its affinity to lipid vesicles (Fig. 10), probably by destabilizing the helical conformation and decreasing the lipid-binding affinity of the protein around the phosphorylation site (Figs. 9 & 10). S87 is also located in a region involved in the interactions of α-syn with at least some proteins, such as the enzyme PLD2 (Payton et al., 2004). Thus, phosphorylation at position S87 may offer further opportunities, beyond phosphorylation in the C-terminal tail region, for regulating synuclein protein-protein, as well as protein-membrane interactions. Further studies of the effects of S87 phosphorylation in vivo will be required to evaluate this hypothesis.

Conclusions

The results presented here indicate that phosphorylation of α-syn at S87 clearly occurs in vivo and is increased in synucleinopathies. However, the role of α-syn S87 phosphorylation in disease is unlikely to encompass directly increasing the fibrillization or deposition of the protein as phosphorylation at this residue blocks rather than promotes α-syn fibrillization. Whether phosphorylation enhances or protects against α-syn toxicity in vivo remains controversial. Previous studies aimed at addressing this question in the case of S129 phosphorylation are based on overexpression of the phosphomimics (S129E /D), which do not reproduce all aspects of phosphorylation, and have yielded contradictory results (Chen and Feany 2005; Gorbatyuk et al., 2007; Azezredo Da Silveira et al., 2009; McFarland et al., 2009). Our work here suggests that S87E should provide a more robust phosphomimic, at least as regards its effects on a-syn aggregation. To date, emphasis has been placed on trying to elucidate the role of phosphorylation in modulating α-syn aggregation and toxicity. However, α-syn phosphorylation at S87 may also influence the normal function of the protein, either by perturbing the membrane-bound conformation of the protein as suggested by our data, or by modulating protein-protein interactions, as has already been shown for other phosphorylation sites. The identification of the natural kinases and phosphatases involved in regulating α-syn phosphorylation at S87 (and S129) should facilitate studies of its effects on both synuclein toxicity and function and is of crucial importance both to understanding the role of phosphorylation in the pathogenesis of PD and to the identification of novel targets to treat PD and related synucleinopathies.

Supplementary Material

Supp1

Acknowledgment

We Thank Dr. Omar Elagnaf and Dr. Ruth Luthi-Carter for critical review of the manuscript. Financial support for these studies was provided by the Swiss Federal Institute of Technology Lausanne (HAL, KEB, AWS), a grant from the Swiss National Science Foundation (HAL, EP, AS, 310000-110027), by the Max Planck society (MZ, COF), a DFG Heisenberg scholarship to (ZW 71/2-1 & 3-1), and by NIH/NIA grant AG019391, the Irma T. Hirschl Foundation, the Michael J. Fox Foundation and a gift from Herbert and Ann Siegel (to D.E.) and Marie curie fellowship (AO). D.E. is a member of the New York Structural Biology Center, supported by NIH grant GM66354 which is a STAR center supported by the New York State Office of Science, Technology and Academic Research, by NIH grant P41 GM66354, and which received funds from NIH, USA, the Keck Foundation, New York State, and the NYC Economic Development Corporation for the purchase of 900 MHz spectrometers.

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