Background
Within recent years, it has been convincingly shown that propagating protein malconformation disease in the mouse brain can be achieved by inoculation of recombinant α-synuclein (α-SNC) or amyloid-β protein aggregates [
1]. Propagation ensued along anatomically connected fiber tracts and may reflect the propensity of Parkinson’s disease (PD) to progress along neuronal trajectories in the human brain as delineated by Braak et al. [
2]. These phenomenological studies are supported by a growing body of in vitro and in vivo experiments demonstrating interneuronal transmission of endogenously produced and secreted α-SNC [
1‐
7]. Once taken up, the internalized aggregates engage in proteopathic templating for the perpetuation of malconformation disease [
8]. Thus, there is great interest in understanding the mechanisms that govern the release of α-SNC monomers and aggregates under physiological and pathological conditions, because therapeutic modulation of extracellular α-SNC could be a way to prevent the propagation of PD once diagnosed. Several groups have documented neuronal α-SNC secretion [
3,
9‐
14], but knowledge of the mechanisms that govern secretion is limited. Both exocytosis of autophagosomes/amphisomes [
10] or late endosomes [
11] containing α-SNC have been proposed as vehicles of α-SNC secretion, but the regulatory mechanisms that drives exocytosis, rather than the classical trafficking pattern to lysosomal fusion and degradation, are largely unknown.
Nerve cells depend on autophagy for proteostasis and survival due to their post mitotic nature [
15]. In PD and other malconformation brain diseases, where pathology is associated with abnormal protein folding and aggregate accumulation, autophagy is activated [
16,
17] to compensate for the often compromised proteasomal function. While α-SNC is taken up by both macroautophagy and chaperone-mediated autophagy, modified or aggregated forms of α-SNC have also been found to partially inhibit the very same pathways [
16‐
21]. There is also mounting evidence that lysosomal function is compromised in PD and other brain diseases [
22]. Disturbed trafficking of hydrolases and other lysosomal proteins, including the vacuolar proton ATPase essential for acidification, results in a reduced complement of lysosomes and their enzymatic activities [
23‐
27]. In addition, the sequestration of fusion machinery or the aberrant sorting of PD-associated sorting receptors have been implicated [
25,
27,
28] altogether compromising the ability for an uninterrupted flow through the autophagosomal and endosomal pathways.
We have recently described how the small, disordered protein tubulin polymerization-promoting protein (p25α) perturbs the autophagosomal pathway in parkinsonergic nerve cell models. This small protein, normally expressed in oligodendrocytes, is ectopically expressed in dopaminergic neurons in PD, is co-localized with α-SNC in Lewy bodies, and has a strong propensity to aggregate α-SNC [
29]. Therefore, p25α upregulates autophagy and increases the autophagosomal uptake of α-SNC [
10]. However, through its inhibition of histone deacetylase 6 [
30], required for actin remodeling [
31], p25α also partially blocks fusion of autophagosomes and amphisomes, the fusion organelle of an autophagosome and a late endosome, with lysosomes [
10]. In turn, this greatly increases the secretion of α-SNC due to the exocytosis of amphisomes and/or autophagosomes. Accumulation of autophagosomes and amphisomes is cytotoxic [
32], and therefore secretion of α-SNC via exophagy can be regarded as a last resort to maintain proteostasis and cell viability [
10].
To study autophagy and exophagy of α-SNC in vitro, we have used the commonly known nerve cell lines PC12 and SH-SY5Y cells often used as cellular models of dopaminergic neurons. PC12 cells derive from a rat pheochromocytoma and can be differentiated to chatecholaminergic neuron-like cells in low serum and addition of nerve growth factor (NGF), while human neuroblastoma cell line SH-SY5Y can be differentiated to chatecholaminergic, but predominantly noradrenergic, nerve cells under low serum concentrations in the presence of either all-trans-retinoic acid (ATRA) or brain-derived neurotrophic factor (BDNF). We have transduced these cell lines to conditionally express α-SNC (wt or A30P) with or without concurrent p25α expression. During our travail, we observed that p25α expression in both cell types causes the persistent activation of cJUN-N-terminal kinase (JNK) in the absence of overt cell death [
10]. The JNK family consists of a number of isoforms divided into JNK1, JNK2, and JNK3 subtypes. JNK1 and JNK2 are expressed ubiquitously, but JNK3 is primarily expressed in the brain [
33]. All three individual JNK knockouts in mice are viable. While JNK1 is involved with neuronal housekeeping functions such a dendritic arborization, JNK2 and JNK3 are activated primarily in response to stressful conditions [
33]. Often protracted JNK activation will result in apoptosis but the anti- and pro-apoptotic functions of JNK isoforms are controlled by the mitogen-activated protein kinase kinase kinase dual leucine zipper kinase (DLK) [
34] and the subcellular distribution (nucleus versus cytosol) of activated JNK [
33,
35].
JNK is activated in response to inflammatory signaling. The transmission hypothesis of malconformation disease propagation does however not address the role of microglia, the resident central nervous system (CNS) immune cells, which are essential for development and progression of neurodegenerative diseases [
36]. In the mature brain, microglia exist in a surveying state [
37] but any deviation from CNS homeostasis, immunological stimuli, or signaling from neurons can activate microglia [
36,
37]. However, protracted activation of microglia, basically due to their inability to eradicate the initiating stimulus, causes neurotoxic effects by excess production of cytotoxic factors such as superoxide [
38] and tumor necrosis factor α (TNFα) [
39]. Notably, aggregated α-SNC has recently been shown to activate microglia through Toll-like receptor 2 (TLR2) [
40] and complement receptor 3 (CR3) [
41] signaling.
In the present work, we demonstrate that activation of neuronal stress kinases JNK2 and/or JNK3 is essential for the exophagosomal release of α-SNC from differentiated PC12 and SH-SY5Y nerve cells. We find that JNK is activated not only as a consequence of endogenous stress relating to lysosomal fusion deficiency but also following inflammatory signaling from co-cultured microglia, which were themselves activated by the α-SNC secreting neurons. In both instances, activated JNK supports an augmented secretion of α-SNC from neurons. In a broader scope, our results suggest that inflammatory microglia also in vivo could modulate release of proteotoxic α-SNC aggregates from neurons and thereby disease propagation, in a manner mechanistically different from the well-documented bystander damage to neighboring neurons in later phases of disease.
Methods
Antibodies and chemical reagents
Antibodies used were mouse monoclonal anti-α-synuclein antibody (BD Transduction Laboratories, Franklin Lakes, NJ); rabbit polyclonal anti-phospho-SAPK/JNK (Thr183/Tyr185) antibody (#9251, Cell Signaling, Danvers, MA); rabbit polyclonal anti-phospho-cjun (#2592, Epitomics, San Francisco, CA); mouse monoclonal anti-β-actin (A-1978, Sigma-Aldrich, St Louis, MO); rabbit polyclonal anti-p25α antibody (Enzo Life Sciences, Farmingdale, NY); mouse monoclonal anti-FLAG tag antibody (#A00187-200, Genscript, Aachen, Germany); mouse monoclonal anti-FLAG tag antibody (clone M2, Sigma-Aldrich); mouse monoclonal anti-JNK1 antibody (F-3) (sc-1648, Santa Cruz Biotechnology, Dallas, TX); rabbit polyclonal anti-JNK2 antibody (#4672, Cell Signaling); rabbit monoclonal anti-JNK3 antibody (#2305, Cell Signaling); mouse monoclonal anti-CHOP antibody (Abcam, ab11419); rabbit polyclonal anti-Nrf2 antibody (sc-22810, Santa Cruz); rat monoclonal anti-cluster of differentiation 11b (CD11b) antibody (MCA711, AbD Serotec, Puchheim, Germany); and rabbit polyclonal anti-TLR2 antibody (sc-10739, Santa Cruz). Salubrinal, SP600125, phorbol 12-myristate 13-acetate (PMA), lipopolysaccharide serotype O:55 (LPS), doxycycline, puromycine, Triton X-100, Tween-20, NADH, sodium pyruvate, trichloroacetic acid (TCA), phosphatase and protease inhibitors, and H2O2 were all from Sigma. Human and rat tumor necrosis factor (TNF)α, rat interleukin (IL)34, rat transforming growth factor (TGF)β1, rat interferon (IFN)β1, human brain-derived neurotrophic factor (BDNF), and granulocyte macrophage-colony stimulating factor (GM-CSF) were all from Peprotech (Rocky Hill, NJ). Alexa 488-, 568-, or 633-conjugated goat anti-mouse or anti-rabbit antibodies were from Molecular Probes (Life Technologies, Grand Island, NY); horseradish peroxidase (HRP)-conjugated swine or goat anti-mouse or rabbit secondary antibodies were from Dako (Glostrup, Denmark); ToPro-3 iodide for nucleus staining was from Molecular Probes.
Cell culture and neuronal differentiation
The rat pheochromocytoma cell line PC12 (ATCC) was seeded on collagen-coated culture dishes and cultured in DMEM containing 10 % horse serum, 5 % fetal calf serum, and 1 % penicillin and streptomycin at 37 °C in 5 % CO
2. For experiments, PC12 cells were seeded at a density of 45,000 cells/cm
2 and differentiated in DMEM containing 2 % horse serum, 1 % penicillin and streptomycin, and 100 ng/ml nerve growth factor (NGF) 2.5S subunit, (Serotec, Raleigh, NC) for 2 days before transgene expression was induced for an additional 2 days. Human neuroblastoma SH-SY5Y cells were cultured in DMEM containing 10 % fetal calf serum and 1 % penicillin and streptomycin at 37 °C in 5 % CO
2. For experiments, SH-SY5Y cells were serum starved at high cell density for 5 days and then reseeded and differentiated with 10 μM all-trans-retinoic acid (ATRA) or 10 μg/ml BDNF in serum-free medium for 6–8 days to obtain a neuron-like phenotype. Transgene expression was induced in the last 48 h before experimentation. PC12 cells conditionally (tet-on) expressing human α-SNC w/wo p25α have previously been established and described, as have SH-SY5Y cells stably expressing α-SNC A30P w/wo conditional expression of p25α [
10]. Purification and culture of primary microglia from neonatal rats was performed as previously described [
42]. The murine microglial cell line Ra2 (licensed by the Japan Science and Technology Agency, Patent ID US6.673,6,5; JP3410738; EP10/602,234) was kindly provided by Dr. Makoto Sawada (Dept. of Brain Function, Nagoya University, Nagoya, Japan) and maintained in MEM with 10 % FCS, 1 ng/ml GM-CSF, and 5 μg/ml bovine insulin [
10]. Ra2-gp91
phox cells with gp91phox under the control of an elongation factor (EF) promotor have previously been described [
42]. In all instances, doxycycline (100-200 ng/ml) was used to induce transgene expression for a minimum of 48 h.
Lentivirus production and transduction
Lentivectors SIN-W-PGK-ASK1-K709R and SIN-W-PGK-Flag-Δ169c-Jun [
43] were a generous gift of Dr. Deglon (CEA, Institute of Biomedical Imaging and Molecular Imaging Research Center, Orsay, France). Lentiviral vectors pLKO.1 JNK1 shRNA (TRCN0000055115), pLKO.1 JNK2 shRNA (TRCN0000012590), and pLKO.1 JNK3 shRNA (TRCN0000012634) were all from Open Biosystems (Dharmacon, Lafayette, CO). Control vector pLKO.1 scrambled (Scr) shRNA was from Sigma (#SHC002). Lentiviral particles for infection were produced as previously described [
44] before superinfection of PC12 cells conditionally expressing α-SNC alone (PC12 α-SNC) or with p25α (PC12 α-SNC/p25α) and SH-SY5Y cells expressing α-SNC
A30P alone (SH-SY5Y α-SNC
A30P) or with conditional p25α expression (SH-SY5Y α-SNC
A30P/p25α). Cells stably expressing scrambled shRNAs were selected with 0.2 μg/ml puromycin for at least 5–7 days before beginning differentiation and experimentation. To generate Ra2 microglia constitutively expressing the encoded H
2O
2 sensor HYPER3 [
45] (generously provided by Dr. Belousov, Shemyakin-Ovchinnikov Institute of Bioorganic Chemistry, Moscow, Russia), complementary DNA (cDNA) was PCR-cloned into the BamHI/XhoI-restricted lentiviral vector pHR-cPPT.CMV.W expressing cDNA under the control of the constitutive cytomegalovirus (CMV) promotor.
Transient transfections with constitutive active JNK isotypes
Plasmids expressing Flag-tagged constitutively active versions of JNK1-3 (pCDNA3 Flag MKK7B2Jnk1a1, pCDNA3 Flag MKK7B2Jnk2a2 and pCDNA3 Flag MKK7B2Jnk3a1) and kinase dead mutant JNK1 (pCDNA3 Flag MKK7B2JNK1a1(AFP)) are described in [
46] and were obtained through Addgene (Cambridge, MA). Transient transfection was performed with differentiated SH-SY5Y α-SNC
A30P cells utilizing the Lipofectamine 2000 (Life Technologies) reagent according to the manufacturer’s instructions. Conditioned medium was collected, and cells were lysed for analysis by western blotting for p-JNK, Flag, and α-SNC, respectively, after an overnight transfection period.
Western blotting (WB)
Cells were lysed in lysis buffer (100 mm NaCl, 50 mm Tris-HCl, 1 mm EGTA, 10 mmMgCl
2, pH 7.2) containing 1 % Triton X-100, phosphatase, and protease inhibitor mixture for 5 min at room temperature and thereafter kept on ice. Cell lysates were centrifuged at 16,100×
g for 5 min at 4 °C, and protein concentrations of the supernatant were determined with D
c protein assay (Bio-Rad, Copenhagen, Denmark), before the addition of Laemmli buffer and loading of equivalent protein quantities on SDS-polyacrylamide gels. Following transfer to PVDF membranes, western blotting was performed using chemiluminescent HRP detection substrate (Millipore, Hellerup, Denmark). Specifically, for p-JNK in differentiated PC12 cells exposed to Ra2-conditioned medium (Fig.
6e,
f), Ra2 cells were changed to HBSS ± LPS (0.5 μg/ml) ± NGF for 6 h before conditioned HBSS was collected from Ra2 monoculture and centrifuged 6000 rpm at 4 °C for 3 min prior to transfer to differentiated PC12 cell monoculture for a 6-h incubation. After 6 h, PC12 conditioned medium was recovered and cells lysed and prepared for western blot as described. All western blot bands were quantified with ImageJ or Image Lab.
Trichloroacetic acid protein precipitation
Conditioned medium was harvested and centrifuged at 800×g for 5 min, 4 °C, before 20 % (v/v) trichloroacetic acid (TCA) was added to the supernatant and incubated on ice for 10 min. The protein precipitates were pelleted by centrifugation (16,100×g, 10 min, 4 °C) and washed four to five times in ice-cold acetone until the pellet appeared clear white. The pellets were dried at 95 °C for 20 min, dissolved in ×2.5 Laemmli buffer, boiled for 20 min at 95 °C, and subsequently processed for western blotting.
Microglia oxidant production
Differentiated PC12 neurons contained in six-wells (ca. 60 % confluency) were incubated with 750.000/well Ra2 microglia expressing HYPER3 in PC12 medium MEM with additives (as described above). Cells were co-cultured overnight without (control) or with 100 ng/ml LPS. The next day, cells were flushed off the culture vessel with HBSS and immediately analyzed by flow cytometry on a Beckton Dickinson FACSaria using the 488 nm laser for excitation of HYPER3. To take advantage of ratiometric HYPER3 measurements, we also performed a microtiter-based fluorescence assay. In this format, conditioned medium from PC12 cells was applied to adherent Ra2 microglia expressing HYPER3 contained in ELISA wells (50,000/well) for 2 hours before the analysis of HYPER3 fluorescence using a FLEX station at 37 °C with excitation at 485/420 nm and emission at 516 with cutoff filter set at 495 nm. HYPER3 measurements were performed with Ra2 microglia receiving only PC12 conditioned medium (basal) or in addition also 100 ng/ml PMA. Exogenous H2O2 (100 μM) and DTT (100 mM) were used to obtain maximal oxidation or reduction of the HYPER3 probe for comparison.
Lactate dehydrogenase (LDH) assay
To evaluate cell death during our experiments, we collected a small fraction of the aspirated media to be used for LDH assay. Samples were stored at 4 °C until assay was performed and maximally 4–6 days. Aspirated media were centrifuged 6000 rpm, 5 min, at 4 °C to remove cell debris before applying 25-μl sample in duplicate to a 96-well plate. Two hundred microliters freshly prepared reagent solution (0.08 M Trizma Base, 0.2 M NaCl, 148.5 μg/ml NADH, and 93.5 μg/ml sodium pyruvate, ph 7.2) was added, and immediately, Abs340nm was measured for approximately 20 min at room temperature (1 reading each 20–30 s). The slope of the resulting Abs340nm change over time was calculated and normalized to protein amounts for each sample. All measurements were related to total cellular content of LDH obtained by the addition of 0.1 % Triton X-100 to control wells to release all LDH to medium.
Immunofluorescence/confocal microscopy
PC12/Ra2 co-cultures were washed once in Hanks’ balanced saline solution and fixed in a phosphate buffer containing 2 % paraformaldehyde, pH 7.4, for 30 min. Immunofluorescence was essentially performed as previously described [
44], and images were acquired with a Zeiss LSM510 confocal laser scanning microscope with a C-Apochromat ×63, 1.4 NA oil immersion objective, using the argon 488-nm and the helium/neon 543- and 633-nm laser lines for excitation of Alexa 488, 568, and 633, respectively. Confocal sections of 0.8–1.0 μm were collected and saved as 512 × 512-pixel or 1024 × 1024-pixel images at 12-bit resolution. The same microscopy settings were used for obtaining all images relating to the same series of experiments, and images were prepared and compiled without digital manipulation.
Statistical analyses
Comparison between two groups was done by Student’s t test. Comparisons of more than two groups were done by one- or two-way ANOVA with either Tukey’s (comparing every mean with every other mean) or Dunnett’s correction (comparing every mean with a control mean) for multiple comparisons. A p value <0.05 was considered statistically significant. All data are graphically represented as means + SEM or given as means ± SD. For Western blotting, all calculations were performed with actin-normalized integrated optic density (IOD) where applicable or with raw IOD values. Statistical evaluation was performed with Graphpad Prism.
Discussion
Within just a few years, a substantial body of evidence has emerged to support the idea that α-synucleinopathy can spread through the brain via release of proteotoxic α-SNC species from an affected neuron and uptake by a neighboring neuron [
55]. Once internalized, these species can confer misfolding disease through proteopathic templating and thereby perpetuate the disease. The mechanism of neuronal α-SNC release is under intense investigation, and both late endosomes [
11] and amphisomes [
10], the organelles derived from fusion between autophagosomes and late endosomes, have been proposed as vesicular carriers of α-SNC to the surroundings by exocytosis. Note that exosomes, small intra-luminal vesicles contained within late endosomes and purported to contain or bind misfolded protein, are released in both cases. In the current study, we pinpoint active (phosphorylated) JNK in differentiated nerve cells as a pivotal regulator of α-SNC secretion by exophagy in response to both internal and external stress factors. With respect to the latter, we specifically show that classically activated microglia, and their inflammatory mediators such as TNFα, substantially augment α-SNC secretion from neurons.
Active JNK is required for exophagy of α-SNC from differentiated neurons
We find that p25α, which partially inhibits fusion of late autophagosomal elements with lysosomes [
10], caused persistent phosphorylation and activation of JNK accompanied by phosphorylation of downstream target cJUN to a much higher degree than α-SNC expression alone. However, pharmacological (SP600125) or genetic (JNK2/3 shRNA) JNK knockdown decreased, whereas constitutive active JNK signaling (MKK7B-JNK fusion constructs) increased α-SNC release from nerve cells regardless of p25α expression.
JNK1 has many “house-keeping” functions, while JNK2 and JNK3 are preferentially activated in response to cellular stress [
33]. The mixed lineage kinase DLK is involved in the regulation of the pro-apoptotic versus physiological functions of the JNKs [
34]. We show that knockdown of JNK2 in PC12 cells and JNK3 in SH-SY5Y cells significantly and robustly downregulated α-SNC release from cells co-expressing p25α (Fig.
3). Notably, JNK3 is not expressed in PC12 cells, and a certain degree of redundancy between JNK isoforms has been noted in global knockout studies in rodents [
33] perhaps explaining the dependency on JNK2 in these cells. Conversely, of the constitutively active JNK1, JNK2, and JNK3 fusion constructs expressed in differentiated SH-SY5Y cells, JNK2 and JNK3 most effectively increased α-SNC secretion and, if any, JNK3 appeared to be the most efficient signaling JNK entity in relation to α-SNC release, as well as activation of endogenous JNK. Although JNK target cJUN was consistently phosphorylated in p25α-expressing cells, we find that its transcriptional activity is not required for the JNK effect on α-SNC secretion, as co-expression of dominant-negative cJUN did not alter α-SNC secretion (Fig.
4). This indicates that JNK2 and JNK3 modify the activity of cytosolic targets to effect increased exophagy.
Salubrinal inhibited both JNK activation and α-SNC secretion in PC12 nerve cells. However, expression of dominant-negative ASK1-K709R, which inhibits signaling through the classical ER-stress IRE1α-TRAF2-ASK1 signaling axis terminating in p38-mitogen-activated protein kinase and JNK activation [
47], failed to decrease phosphorylation of JNK. For the same reasons, oxidative stress, which also signals through ASK1, is not the cause of JNK activation in p25α-expressing cells [
50]. Instead, we consider that the mechanism of JNK activation following p25α-associated stress relates to the perturbation of lysosomal fusion with amphisomes [
10]. Thus, in both PC12 and SH-SY5Y cells, bafilomycin, which more efficiently than p25α inhibits lysosomal fusion reactions, caused profound JNK activation (and α-SNC secretion). These observations are perhaps supported by drosophila studies showing JNK activation in response to accumulation of dysfunctional late endosomes [
56]. The association of JNK isoforms with vesicular compartments through protein scaffolds or adaptor proteins that bind to either kinesin and dynein microtubule motors is well noted [
57], and both cargo association [
58‐
60] and mobility are regulated by JNK activity [
59]. Thus, JNK3 in part determines directional organelle mobility in zebra fish axons [
61] and has also been associated with aberrant directional cargo transport in response to pathogenic huntingtin as a basis of neurodegeneration [
62]. The lack of retrograde movement of prelysosomal and lysosomal compartments may in turn directly favor exocytosis of these elements, because the fate of any endosomal, and presumably autophagosomal element, is to a large part determined by its distribution in the cell [
63]. This agrees well with the observation that Rab8 overexpression, which dramatically increases α-SNC release from PC12 nerve cells [
10], immobilizes LC3-positive autophagosomes/amphisomes at the cell periphery (unpublished data; FV).
Differences in subcellular distribution of JNK activity, isoform activation, and temporal activation patterns likely also explain the lack of strict correlation between JNK activation and α-SNC secretion under different stress conditions. For example, exogenous oxidative stress increases α-SNC secretion without any overt JNK activation in both cell lines, and in SH-SY5Y cells, ER stress imposed with tunicamycin and thapsigargin similarly increases α-SNC release under conditions where JNK activity is actually depressed. On the other hand, ER stress in PC12 cells increased both JNK activation and α-SNC secretion in a dose-dependent manner. However, we did not investigate the dependency of release on either JNK (isoforms) or autophagy in these alternative stress conditions. For now, we therefore specifically conclude that the increase in α-SNC secretion following either amphisome accumulation associated with lysosomal fusion deficiency or (select) cytokine signaling relies on the ability of JNK2 and JNK3 activation to promote exophagy of α-SNC.
Reciprocal interactions between microglia and neurons activate microglia and increase α-SNC release from neurons
Microglia are essential for the development of full-blown neurodegenerative disease, but their contribution has mainly been relegated to the terminal phase of disease, where classically activated microglia exert neurotoxic effects by the production of reactive oxygen species [
38] and other pro-inflammatory mediators [
64]. However, in animal models as well as humans, microglia activation is widespread in the brain years or even decades before clinical symptoms. Differentiated PC12 nerve cells expressing α-SNC activated oxidant production of either resting or LPS-primed microglia in co-culture, as reported previously [
65], and this was enhanced by the p25α co-expression in nerve cells, which increases α-SNC release. Microglial oxidant production was not only increased in direct co-culture, also passive transfer of neuron-conditioned media was able to induce increased microglial ROS production. While we have not sought to identify the neuronal factors responsible for microglia activation, it is reasonable to assume that the microglia are responding to released α-SNC oligomers and aggregates, which have recently been shown to engage TLR2 [
40] and CR3 [
41] scavenger receptors to activate microglia. In agreement herewith, we observe that internalized α-SNC in microglia colocalize in part with TLR2, and to a smaller degree with CD11b.
Activated microglia produce a range of inflammatory molecules that are neurotoxic at high concentrations. We show that classically activated (LPS; M1 activation), but not resting, microglia increase neuronal JNK phosphorylation and α-SNC secretion (in the absence of neuronal p25α expression). In co-culture, LPS-activated primary microglia from neonatal rats caused NGF-differentiated PC12 cells to secrete almost fourfold more α-SNC compared to controls. Passive transfer of conditioned media from microglial monocultures to neuronal monocultures allowed us to establish that the increased α-SNC secretion was accompanied by neuronal JNK phosphorylation. This experiment also excludes oxidants (because of their limited half-life) as the microglia-derived factor that directly influences neuronal p-JNK and α-SNC release. Thus, the potentiation of α-SNC secretion we observe in neurons exposed to conditioned medium from Ra2 microglia overexpressing gp91phox is likely a property of an altered microglial redox balance, which eventually supports inflammatory mediator expression [
52]. One such classical factor secreted from activated microglia is TNFα [
39,
52]. TNFα dose- and time-dependently significantly increased α-SNC secretion from both differentiated PC12 and SH-SY5Y cells by approximately two- to fourfold, and this correlated with JNK activation, again in the absence of p25α expression. Further, the increased α-SNC secretion afforded by TNFα required JNK, as shRNA knockdown of JNK2 in PC12 cells and JNK3 in SH-SY5Y cells reduced TNFα-induced α-SNC secretion. We note that JNK2 and JNK3 knockdown also under non-stimulated conditions (control cells) decrease α-SNC secretion in PC12 and SH-SY5Y cells, respectively, suggesting a basal mechanism. TNFα can be toxic to neurons at concentrations similar to the ones used here [
66], but in our hands, there appeared no relevant toxicity (measured by LDH release and flow cytometric probes of cell death and membrane permeability), and morphological differentiation remained unaltered (or even slightly enhanced). The ability to induce an augmented release of α-SNC from PC12 nerve cells is not unique to TNFα or pro-inflammatory mediators: of a handful of cytokines tested with known neuronal receptors, anti/non-inflammatory cytokines TGFβ1 and IFNβ1, both increased α-SNC secretion from neurons in monoculture.
A few studies have documented that cytokines can induce autophagy [
67], but we do not know how TNFα, or activated microglia for that matter, induce augmented neuronal α-SNC secretion by exocytosis of amphisomes. We do, however, implicate activated stress kinases JNK2 or JNK3 as essential components in the process. Of note, JNK activity is increased in post-mortem brains from PD patients [
68]. Intriguingly, modest JNK inhibition in animal models of PD ameliorates motoric symptoms via unknown mechanisms [
69,
70] that may relay to microglia activation [
71] and/or conceivably to a mechanism as proposed above.
Rationally, any alterations in the exophagosomal release of α-SNC from neurons following exogenous stimulation would ultimately have to impinge on either autophagosomal uptake of α-SNC or on exocytosis of amphisomes. Future work is directed at understanding how JNK and cell non-autonomous mechanisms determine the burden of α-SNC released into the surroundings.
Competing interests
The authors declare that they have no competing interests.
Authors’ contributions
DPC designed, carried out, and analyzed the cytokine exposure, co-culture experiments, and JNK shRNA transductions and transfections. PE designed, carried out, and analyzed the experiments with SP600125 and salubrinal. IR helped in carrying out essentially all experiments. FV conceived the study, helped design all experiments, and carried out and analyzed ASK1, cJUN, H2O2, and thapsigargin and tunicamycin experiments. DPC and FV drafted the manuscript, and PE and IR commented the draft. All authors read and approved the final manuscript.