The protein alpha-synuclein (α-syn) is unusual because, depending on its conformation and the type of cell in which it is expressed, it is pro-death or pro-survival, triggering neurodegeneration in Parkinson’s disease and enhancing cell survival of some melanomas. To probe the function of α-syn in melanoma, we used CRISPR/Cas9 to knockout SNCA, the gene that codes for α-syn, in SK-Mel-28 melanoma cells. The SNCA-knockout clones in culture exhibited a decrease in the transferrin receptor 1 (TfR1), an increase in ferritin, an increase of reactive oxygen species and proliferated slower than control cells. These SNCA-knockout clones grafted into SCID mice grew significantly slower than the SK-Mel-28 control cells that expressed α-syn. In the excised SNCA-knockout xenografts, TfR1 decreased 3.3-fold, ferritin increased 6.2-fold, the divalent metal ion transporter 1 (DMT1) increased threefold, and the iron exporter ferroportin (FPN1) decreased twofold relative to control xenografts. The excised SNCA-KO tumors exhibited significantly more ferric iron and TUNEL staining relative to the control melanoma xenografts. Collectively, depletion of α-syn in SK-Mel-28 cells dysregulates cellular iron metabolism, especially in xenografts, yielding melanoma cells that are deficient in TfR1 and FPN1, that accumulate ferric iron and ferritin, and that undergo apoptosis relative to control cells expressing α-syn.
Clinical and epidemiological studies have revealed a co-occurrence of Parkinson’s disease (PD) and malignant melanoma1,2,3,4,5. PD patients typically have a two to fourfold higher risk of developing invasive melanoma than expected in age- and sex-matched control3, and, reciprocally, patients with invasive melanoma have a 1.4–2-fold higher risk of developing PD1,2. Several genes that are associated with PD, such as alpha-synuclein (protein: α-syn; gene: SNCA)6,7,8, are thought to confer an increased risk of melanoma4. α-Syn is frequently expressed in cell lines derived from tumors representing advanced melanoma6,9, and tissue microarray analysis and whole-genome expression profiling show elevated levels of α-syn in advanced stage melanomas10. Our focus in this study was the role of α-syn in malignant melanoma.
Numerous studies have shown that α-syn plays a key role in the pathobiology of PD11,12,13,14. α-Syn, which is 140 amino acid protein that is expressed at quite high levels in dopaminergic neurons, but that is also expressed in a variety of other tissues, is an intrinsically unfolded protein15 that adopts secondary structure in a context dependent fashion. When it binds to small lipid vesicles, α-syn converts from a random coil to a bent α-helical conformation16. Functionally, α-syn is involved in membrane and vesicular trafficking, as it senses membrane curvature17, regulates synaptic vesicle fusion with the presynaptic membrane18, and promotes endocytosis and exocytosis19,20. α-Syn has a hydrophobic internal domain that can promote fibrillization, and some of the soluble amyloid fibril seeds are thought to cause neurodegeneration that defines PD11,21,22.
α-Syn may also have a role in iron metabolism in the brain and other tissues23. For example, α-syn is expressed at different steps of erythropoiesis, especially in red blood cells, and the expression of SNCA is significantly correlated with the expression of the heme metabolism genes ALAS2, FECH, and BLVRB24. α-Syn enhances the intake of holo-transferrin (Tf)-transferrin receptor 1 (TfR1) complexes in neuronal and non-neuronal cells, indicating that it regulates the level of iron in some cells19,25, and it inhibits Snx3-retromer mediated recycling of iron-regulatory proteins in a yeast PD model26. Brain iron deposits are also a feature of PD27,28.
Our interest in this study was the connection between α-syn, iron metabolism and melanoma. Because iron is used in DNA synthesis, cell-cycle progression, iron-sulfur cluster biosynthesis, heme synthesis and energy production, cancer cells have a high demand for this metal, and cancers can often subvert the normal iron homeostasis at the systemic and cellular levels to acquire high levels of iron by increasing iron uptake and storage, decreasing iron export, or both (for a review see ref29). At the cellular level, the two iron regulatory proteins (IREB1/2)30 regulate the translation of several iron metabolic proteins, including TfR1, divalent metal ion transporter 1 (DMT1)31, ferritin, and ferroportin (FPN1)32, by binding to iron-responsive elements (IREs) in the 5′ and 3′ untranslated regions of the transcripts that encode these proteins. The dysregulation of cellular iron metabolism in cancer cells can come about from mutations in oncogenes and tumor suppressors, and often these mutations cause increased cell surface expression of TfR1 or decreased cell surface expression of FPN129.
Here we report that loss of α-syn expression in SK-Mel-28 cells dysregulates iron metabolic proteins, yielding cells with downregulated TfR1 and FPN1 and upregulated ferritin and DMT1. The results are consistent with loss of α-syn expression yielding melanoma cells with an overload of bio-unavailable ferric iron and a deficiency of bio-available labile iron; hence, the α-syn knockout melanoma cells, we propose, are functionally iron deficient.
Elevated SNCA transcript levels correlate with poorer survival for patients with melanoma
We analyzed the TGCA data set using the Xena genomics platform to determine whether elevated SNCA transcript levels from excised primary melanoma lesions correlate with decreased survival. The analysis of the TGCA data set (462 patients) yielded a significant association of better overall survival for patients with lower SNCA transcript level, while patients with high SNCA transcript level had worse overall survival (Fig. 1: 8.7 years [—] versus 5.3 years [—], p = 0.01242). We sought to determine herein the function of α-syn in melanoma cells.
Loss of α-syn decreases the level of TfR1
The SK-Mel-28 melanoma cell line, which expresses α-syn6, is a widely used cell line8,9,33,34,35 To understand the role of α-syn in melanoma, we used CRISPR/Cas9 technology to knockout SNCA in SK-Mel-28 cells (Supplementary Fig. S1 and Table S1). Several of these SK-Mel-28 SNCA-KO clones were used herein.
TfR1 and ferritin protein levels were probed in lysates of SK-Mel-28 SNCA-KO clones KO8, KO9 and SK-Mel-28 control cells. To ensure that any phenotypic changes in the KO clones were due to loss of α-syn expression, α-syn was re-expressed in each KO clone using lentiviral infection, and cell lines are referred to as KI8 and KI9. Each SNCA-KO clone exhibited a threefold increase in ferritin (p = 0.001) (Fig. 2a, lanes 2 & 3 vs 1; Fig. 2b) and a 1.8-fold decrease in TfR1 (p = 0.014, p = 0.006) relative to control cells (Fig. 2a, lanes 2 & 3 vs 1; Fig. 2c). Strikingly, re-expressing α-syn in the clones decreased ferritin and increased TfR1 levels, such that the levels of these two proteins were indistinguishable from those in control cells (Fig. 2a, lanes 4 & 5 vs 2 & 3; Fig. 2b,c).
We asked whether the decreased level of TfR1 in the SNCA-KO clones was due to the degradation of TfR1 molecules in the lysosome. If TfR1 molecules are proteolytically degraded in the lysosome, then inhibiting the activity of the lysosomal proteases with bafilomycin A1 (baf) will block the degradation. To this end, cells were treated for 5 h with baf (or dimethyl-sulfoxide, DMSO, as a control) and probed for TfR1, LC3-II, α-syn and α-tubulin by Western blotting (Fig. 2d). LC3-II is a lipidated form of LC3 that builds up in autophagosomes when autophagy is inhibited by baf. In the DMSO group, the level of TfR1 decreased by 40% (p = 0.0001) relative to control cells (Fig. 2d, lanes 2 vs 1; Fig. 2e); whereas, TfR1 showed no significant decrease relative to control cells in the baf + group (Fig. 2d, lanes 5 vs 4; Fig. 2e).
Quantitative PCR (qPCR) was also conducted to determine whether mRNA levels of several genes were affected in SNCA-KO clones. First, we found a modest 25% (p = 0.02), but significant, decrease in the TfR1 mRNA in KO8 cells compared to control and KI8 cells (Fig. 3a). Second, the mRNA levels of the iron responsive element binding proteins 1 and 2 (IREB1/2), which regulate the stability, and hence translation, of mRNAs of various iron-related proteins, were determined. The mRNA levels of IREB1/2 were unaffected by knocking out SNCA (Fig. 3b). Third, the mRNA level of the only mammalian iron exporter, FPN1, was increased by 200% in KO8 cells compared to the parental control cells, and upon re-expression of α-syn in the KO8 cells the mRNA level decreased to that of the control cells (Fig. 3c). (FPN1, see also: Dysregulation of cellular iron metabolism in SNCA-KO xenografts.) Overall, the data in Figs. 2 and 3 show that the decreased level of TfR1 in the SNCA-KO clones relative to control cells is a consequence of two phenomena: enhanced degradation in the lysosome and downregulated transcription.
Loss of α-syn expression suppresses cell proliferation in vitro
BrdU is an analog of thymidine, which can be incorporated into the newly synthesized DNA in replicating cells; thus, BrdU labeling is commonly used to detect DNA synthesis or cell proliferation36. A BrdU incorporation assay was used to determine whether knocking out α-syn affects proliferation in vitro. KO8 and KO9 clones and the corresponding KI clones were tested against the control SK-Mel-28 cells. The percentage of BrdU + cells was determined by fluorescence microscopy analysis, using DAPI to determine the number of total cells per field. On average, there was a significant (p = 0.01) decrease in BrdU incorporation in the two KO clones compared to SK-Mel-28 control cells, and the KI clones had BrdU incorporation values similar to the control cells (Fig. 4a,b).
Loss of α-syn expression suppresses melanoma tumor growth in a mouse xenograft model
We sought to determine whether the finding of suppressed proliferation in vitro translates to an in vivo model. To that end, in the same SCID mouse, we injected 1 × 106 SK-Mel-28 control cells in matrigel subcutaneously into the left flank in mice, and the same number of SK-Mel-28 SNCA-KO cells in matrigel were injected subcutaneously into the right flank. Clones KO3, KO6, KO8 and KO9 were tested. The animals were followed for 72 days and then sacrificed. Tumor volume curves for clones 6 and 8 are shown in Fig. 5a,d, respectively. Tumor volume data for KO3 and KO9 are given in Supplementary Fig. S3. The two KO clones grew much slower than the control cells (Fig. 5a,d), and, at the endpoint, average weight of the tumor formed from the KO clones was significantly (p = 0.001) less than the control tumors (Fig. 5b,c,e,f). Tumor sections were also evaluated by IHC to probe for α-syn and Ki-67 (Fig. 6), which is a nuclear protein associated with cell proliferation. KI-67 immunostaining is frequently used to evaluate cell proliferation in tissues37. For each KO clone tested, Ki-67 decreased significantly compared to the control tumor (Fig. 6a,b; Supplementary Fig. S4). IHC also showed complete lack of staining for α-syn in the KO clones. Overall, the data show that knocking out α-syn in melanoma cells suppresses the tumor growth at least partly by inhibiting tumor cell proliferation.
Dysregulation of cellular iron metabolism in SNCA-KO xenografts
Lysates of tumors excised from the SCID mice were western blotted to quantify the levels of ferritin, TfR1, DMT1 and FPN1. DMT1 isoform 2 localizes to endosomes, where it is activated at pH 5.5 to pump iron (in the ferrous state) from the lumen of endosomes into the cytosol38. FPN1 localizes to the plasma membrane, where it pumps iron (in the ferrous form)39 out of cells. Statistically significant changes in protein levels were identified in SNCA-KO xenografts, compared to controls, as follows: (i) ferritin increased 6.2 (± 0.5)-fold in xenografts 6, 8 and 9 (Fig. 7a,b); (ii) TfR1 decreased 3.3 (± 7)-fold in all four xenografts (Fig. 7a,c); (iii) DMT1 increased 2.9 (± 0.1)-fold in xenografts 6, 8 and 9 (Fig. 7a,d); and (iv) FPN1 decreased 1.9 (± 0.3)-fold in xenografts 6, 8 and 9 (Fig. 7e,f). Collectively, loss of α-syn affects the levels of both iron import (TfR1/DNM1) and iron export (FPN1) proteins. Moreover, because ferritin levels were significantly increased in the SNCA-KO clones compared to control cells, we hypothesized that knocking out α-syn dysregulates iron metabolism in such as manner as increase the concentration of non-labile, ferric iron.
Increased ferric iron in SNCA-KO xenografts
To test the hypothesis that loss of α-syn expression in SK-Mel-28 cells dysregulates the iron import–export balance towards ferric iron accumulation, excised xenograft sections were analyzed by Perls staining, which is a technique used to detect non-heme ferric iron (Fe3+), such as occurs in ferritin and hemosiderin, in tissue sections40. After treatment of the tissue with ferrocyanide and acid, deposits of iron appear as brown puncta. Puncta area readily visualized by light microcopy and the number of puncta per unit area quantified. Applying this technique to clones KO6, 8 and 9 and SK-Mel-28 control xenografts, we found significantly (p = 0.0001) more ferric iron deposits in each of the KO xenografts compared to control cells (Fig. 8a,b). Ferric iron deposits per unit area were typically three to fivefold higher than the density of iron deposits in the control xenografts.
Increased apoptosis in SNCA-KO xenografts
Apoptosis can be caused by iron deficit or iron overload41,42,43. Given that SNCA-KO xenografts exhibited increased levels of both ferric iron and ferritin relative to controls, we asked whether these xenografts also exhibited increased apoptosis. To that end, xenograft sections were analyzed for DNA fragmentation using the TdT-mediated, dUTP-biotin nick-end labeling (TUNEL) assay. The TUNEL assay is a method for detecting DNA fragmentation in cells, and it is frequently used to evaluate apoptosis in tissues37. TUNEL analysis of xenografts from KO6, 8 and 9 and controls revealed that the three KO clones showed significantly more DNA fragmentation per field than the controls (Fig. 9a,b). On average, the sections from the KO xenografts had two to threefold higher amounts of DNA fragmentation that the controls. Collectively, SNCA-KO xenografts had higher levels of both ferric iron and apoptotic TUNEL markers than the control xenografts (Figs. 8, 9).
In this study, we engineered SK-Mel-28 α-syn knockout cells (SK-Mel-28 SNCA-KO) to investigate the role, if any, played by α-syn protein in promoting proliferation (Fig. 1). Our results are consistent with the loss of SNCA significantly suppressing tumor growth, and the suppressed tumor growth is a consequence of a disturbance in iron metabolism. Aspects of this work are discussed below.
The synuclein family contains three (α, β, and γ-synuclein) highly conserved, small, soluble membrane-binding proteins44. α-Syn regulates membrane trafficking events 20,45, whereas much less is known about the function of β- and γ-syn. These proteins are highly expressed in brain and to a lesser extent in other tissues46. While α-syn has the greatest propensity to form soluble and insoluble neurotoxic aggregates and amyloid fibers that cause neurodegeneration, aggregated forms of β- and γ-syn may also contribute to some neurodegenerative diseases47,48. There is an intriguing connection of synucleins to cancer5,49, which suggests that neurodegeneration and cancer may share common mechanisms: (i) α-syn is highly expressed in melanoma cell lines6, and over-expressing α-syn promotes the proliferation of B16 murine melanoma cells50 as well as human SH-SY5Y neuroblastoma cells51. The mechanism by which α-syn promotes proliferation is unclear. (ii) β-syn is over-expressed in breast cancers52. (iii) γ-syn is abnormally expressed in various malignancies, but normal tissue, including breast, cervical, colon, prostate and ovarian cancers52,53. γ-syn promotes cancer cell migration and invasion54, and down regulating γ-syn expression by siRNA decreases cervical cancer proliferation in nude mice55. The role of synucleins in cancer is wide-open area of research.
We found that the SK-Mel-28 SNCA-KO cells in culture or implanted in mice exhibit significantly lower levels of TfR1 relative to control cells (Figs. 2a,c, 7a,c). In the mouse model, the SK-Mel-28 SNCA-KO melanoma xenografts compensate for the relatively low level of TfR1, which should cause iron deficiency, by decreasing the level of FPN1 (Fig. 7e,f), which decreases the efflux of iron out of cells, and increasing DMT1 (Fig. 7a,d), which, promotes ferrous iron export from endosomes into the cytosol (Fig. 10). We do not know why ferritin increases so dramatically in the SNCA-KO melanoma xenografts; nevertheless, the KO xenografts accumulate large amounts of ferritin/ferric iron, indicating a misregulation of iron inside the tumors. Our interpretation is that the SNCA-KO melanoma xenografts are overloaded with bio unavailable ferric iron bound to ferritin, and such cells, we speculate, probably have low amounts of bioavailable ferrous iron; hence, SNCA-KO melanoma cells are likely to be functionally iron deficient (Fig. 10). A functional iron deficiency, which could cause defects in DNA synthesis, cell cycle progression and energy production, likely causes the slow growth phenotype when the SK-Mel-28 SNCA-KO melanoma clones are engrafted into SCID mice (Figs. 5, S3). In support of our interpretation, when SK-Mel-28 cells are engrafted into SCID mice and the mice are treated with the iron chelator Dp44mT the chelator dramatically inhibits tumor growth33, which shows that depleting iron from melanoma cells inhibits their growth and proliferation.
FPN1 is transcriptionally upregulated in the SK-Mel-28 SNCA-KO clones in culture compared to control cells (Fig. 3c). Given that SNCA-KO xenografts accumulate ferric iron (Fig. 8), in our view, it is not surprising that cells overloaded with iron respond by upregulating the expression of an iron exporter. Curiously, however, the level of the FPN1 protein is decreased in SNCA-KO xenografts relative to the control xenografts. This decrease in FPN1 is most likely due to enhanced degradation of FPN1 in the lysosome. We suggest that both membrane proteins, TfR1 and FPN1, which cycle between the plasma membrane and locations within the cell, such as the trans-Golgi, are degraded faster in the SNCA-KO cells than in control cells. Overall, loss of α-syn expression accelerates the lysosomal degradation of TfR1, and likely FPN1.
Other studies have also shown that α-syn promotes the uptake of transferrin-bound iron (Tf-Fe3+)19,25. First, one study explored the effect of α-syn expression on the endocytosis of the fluorescent dye FM-464 on a neuronal cell line in cultural. α-Syn and physiological concentrations of certain polyunsaturated fatty acids (PUFAs) were shown to act synergistically to enhance the endocytosis of FM-46419. Additionally, α-syn alone, PUFA alone, or PUFA+ α-syn in an additive manner enhance clathrin-mediated endocytosis of a fluorescently tagged transferrin (Alex-488 Tf) in neuronal and non-neuronal cultured cells19. Overexpression of α-syn in MN9D neuronal cells caused a threefold increase in the TfR1 mRNA compared to control cells with no α-syn expression. Second, retinal epithelial (RPE) cells express α-syn, and Parkinson’s patients often experience ocular problems. Knocking down α-syn expression in retinal epithelial (RPE) cells significantly decreases the levels of both TfR1 and ferritin compared to control RPE cells25; whereas, overexpressing α-syn significantly increased the levels of these two proteins. Furthermore, knock down of α-syn appeared to shift TfR1 molecules into perinuclear vesicles, suggesting disrupted TfR1 recycling to the plasma membrane, and such vesicles are likely degraded in the lysosome25. We have shown that a subpopulation of TfR1 molecules are also degraded in the lysosome in SK-Mel-28 SNCA-KO melanoma cells (Fig. 2d,e).
Iron metabolism appears to be disrupted quite differently in the SK-Mel-28-SNCA-KO cells and homozygous SNCA-KO RPE cells. For example, loss of α-syn expression in the SK-Mel-28 cells yields a decrease in the level of TfR1 and an increase in the level of ferritin, generating a ferric iron overload. In contrast, loss of α-syn expression in RPE cells yields a decrease in levels of both TfR and ferritin, in this case, generating a ferric iron deficiency. These disparate results indicate that very different regulatory mechanisms are at work in these two types of cells.
In sum, knocking out α-syn expression in SK-Mel-28 cells has two effects on TfR1: the TfR1 mRNA is slightly but significantly decreased and degradation of TfR1 in the lysosome is enhanced relative to control cells that express α-syn. Whether TfR1 molecules are stuck on the plasma membrane due to a defect in endocytosis or stuck in Golgi vesicles due to a trafficking defect will be determined in future experiments. Overall, loss of α-syn in SK-Mel-28 cells dysregulates cellular iron metabolic proteins, leading to ferritin-ferric iron accumulation, and apoptosis.
Materials and methods
Animal maintenance and xenografts
All animals in this study received humane care in accordance with the guidelines set by the American Veterinary Medical Association, and all experiments were approved by the Institutional Animal Care and Use Committee of LSU Health Sciences Center in Shreveport (LSUHSC-S IACUC). Protocol #P-18-019. Female SCID-Beige mice (Taconic) were used at 7–8 weeks of age. Mice were maintained at LSU Health Sciences Center-Shreveport animal facility in sterile cages. Groups KO3, KO6, KO8, and KO9 contained 9, 7, 12, and 9 mice, respectively. To create xenografts, 1 × 106 SNCA-KO clones and SK-Mel-28 control cells, suspended in 50 µl of growth medium and mixed with 50 µl of matrigel (Corning #354234), were injected subcutaneously into the left and right back (2 grafts per each mouse) in SCID mice. Tumors were measured with digital calipers (3 times/week) and tumor volume calculated as: tumor volume (mm3) = (length × width2) × 0.523656. Mice were sacrificed by isoflurane overdose and death was confirmed by cervical dislocation.
Antibodies and reagents
α-Syn (610786) was purchased from BD Biosciences, transferrin receptor (13-6800) and ferroportin (PA522993) from Thermo Fisher Scientific, LC3-II (2775S) from Cell Signaling Technology, α-tubulin (T9026), HRP-conjugated anti-rabbit and anti-mouse antibodies (sc-516102, sc-2357), NRAMP (sc-166884), ferritin (sc-74513). α-Syn CRISPR/Cas9 knockout plasmid (sc-417273) from Santa Cruz Biotechnology. Bafilomycin A1 (B1793-10), 2′,7′-dichlorofluorescin diacetate (D6883) and DMSO (D8418) were obtained from Sigma. Penicillin–streptomycin (15140122) and phosphate-buffered saline (PBS-10010031) were from Gibco. Dulbecco's Modified Eagle's Medium (DMEM) (63844117), trypsin/EDTA (30-2101) and fetal bovine serum (30-2020) were purchased from American Type Culture Collection (ATCC, Manassas, VA).
Cell line and cell culture
The SK-MEL-28 cell line, which was purchased from ATCC, were authenticated at the University of Arizona Genetics Core via their STR Profiling Cell Authentication Service. Cells were cultured in DMEM supplemented with 10% fetal bovine serum (FBS) and 1% penicillin–streptomycin. The SK-MEL-28 cell line, and all knockout (KO) and knockin (KI) cell lines, were maintained in a humidified chamber with constant supply of 5% CO2 and 95% O2 at 37 °C.
CRISPR/Cas9-mediated gene knockout
CRISPR/Cas9 genome editing was used to target SNCA in SK-MEL-28 cells, α-syn CRISPR/Cas9 knockout plasmid containing 3 guide RNAs and GFP (as a marker for transfection) was purchased from Santa Cruz Biotechnology. Guide-RNA 1, 2 and 3 were complementary to exon 3, 4 and 5, respectively. Therefore, the Cas9 cut exon 3 and/or 4 and/or 5. Single cells expressing GFP were sorted in 96 well plates by fluorescence activated cell sorting. Further, we performed expansion of clones from single cells to 24 well, 12 well, 6 well plates, T25 and T75 flasks followed by validation of the SNCA knockout clones.
Re-expression of α-syn in SNCA KO clones
Lentivirus particles (> 107 IU/ml) expressing human α-syn under CMV promoter (pLenti-GIII-CMV-GFP-2A-Puro) were procured from Applied Biological Materials. Inc, Canada. SNCA KO cells were transduced at a multiplicity of infection 1 in a fresh DMEM with 10% (v/v) FBS and 8 µg/mL of polybrene (Sigma, St Louis, MO, USA) for 6 h. After 48 h the cells were selected with puromycin (0.5 µg/ml) for 7 days. The positively selected surviving cells were then sorted by FACS followed by expansion in 96 well plates, moved to 24 well, 12 well, 6 well plates, T25 flask and screened for the presence of α-syn by immunoblotting analysis.
RNA extraction, cDNA preparation and qPCR
Cells were harvested and total RNA of cells was extracted from SNCA knockout clones and control cells using E.Z.N.A column-based total RNA kit (Omega BioTek). Total RNA concentration was determined using Nanodrop spectrophotometer and 1 μg total RNA was used to prepare cDNA following the manufacturer’s protocol. cDNA was synthesized from total purified RNA by using iScript cDNA synthesis kit (Bio-Rad) according to the manufacturer’s protocol. qPCR reactions were performed using SYBR green PCR super mix reagent (Bio-Rad). β-actin was used as a housekeeping gene to normalize Ct values. The relative expression of each amplicon was analyzed by the delta Ct method. Primer sequences were SNCA (Forward: 5′-ACTGCTCCTCCAACATTTGTC-3′ and Reverse: 5′-AGGGTGTTCTCTATGTAGGCT-3′) and β-Actin (Forward: 5′-GGCATCCTCACCCTGAAGTA-3′ and Reverse: 5′-CAGAGGCGTACAGGGATAGC-3′). TaqMan primers for qPCR were SNCA (Hs00240906), TfR1 (Hs00951083-m1), IREB1 (Hs00158095-m1), IERB2 (Hs01021795-g1) and FPN1 (Hs00205888-m1) (ThermoFisher).
Cells were lysed in RIPA lysis buffer (50 mM Tris HCL, pH 7.4, 1% NP-40, 0.5% sodium deoxycholate, 0.1% SDS, 5 mM EDTA) followed by centrifugation (13,000 rpm/30 min/4 °C). the protein concentrations of the supernatants were determined using DC Protein Assay Kit (BIO-RAD 5000112), and all other steps performed as described26,57. Given that we typically detected multiple proteins from a single immunoblot, membranes were often cut into strips and the individual strips were hybridized with antibody.
Paraffin embedded tissue sections of 5 μm thickness were deparaffinized in xylene and then rehydrated in graded alcohol series (100%, 95%, 70%, 50%) solutions followed by heating in a microwave (20 min) for antigen retrieval using antigen unmasking solution (Vector Laboratories, H-3300-250). To inhibit endogenous peroxidases, sections were incubated with 0.3% H2O2 in methanol at room temperature and then cleared in PBS for 5 min. Slides were incubated in blocking solution (5% either horse (Vector Laboratories, s-2000) or goat (s-1000) serum in 1XPBS) for 30 min at room temperature. The sections were incubated overnight with mouse monoclonal α-synuclein antibody (1:500) and rabbit monoclonal Ki-67 antibody (1:500) in blocking solution at 4 °C. After the incubation, sections were washed in PBS and incubated with horse radish peroxidase (HRP) antibody conjugates (1:500) for 60 min at room temperature. Sections were washed with PBS and the antigen–antibody complexes were visualized using Vectastain Elite ABC Reagent (Vector Laboratories). The sections were developed using DAB (diaminobenzidine) substrate chromogen system (Vector Laboratories) and then counterstained with hematoxylin, dehydrated and mounted with di-n-butylphthalate-polystyrene-xylene (DPX) and the slides were visualized with a Nikon TE300 digital inverted microscope.
Perls staining was used to detect ferric iron deposits in xenograft sections. The Perls iron staining kit from Abcam (ab150674) was used according to the manufacturer's instructions. Briefly, sections were deparaffinized, hydrated and incubated in equal amounts of potassium ferrocyanide solution and hydrochloric acid solution for 30 min. Slides were washed with water followed by counter staining in nuclear fast red solution for 5 min. After washing, slides were dehydrated, mounted and imaged using a Nikon TE300 digital inverted microscope at 20× magnification. Image J software was used to count the number of Perls positive cells (black pigment) across 3 fields/section were represented graphically.
Terminal deoxynucleotidyl transferase dUTP nick end labeling (TUNEL) assay
In Situ Detection of Fragmented DNA was examined using an ApopTag peroxidase in situ Apoptosis Detection Kit (S7100) (Millipore, USA) according to the manufacturer’s instructions. The number of TUNEL positive cells in the xenografts were then evaluated using Image J software.
Bromodeoxyuridine (BrdU) assay
Cells were seeded onto coverslips in 6-well plates at a density of 3 × 106 cells/well and grown overnight prior to incubation with BrdU (3 μg/ml) for 3 h at 37 °C. Cells were fixed with 4% paraformaldehyde for 60 min at room temperature and then washed five times with PBS for 20 min. For immunocytochemical staining, the cells were treated with 0.4% Triton X-100 containing 2 M HCl in PBS for 30 min. After washing with PBS, cells were blocked with 5% horse serum in PBS for 1 h at room temperature and subsequently incubated with mouse monoclonal anti-BrdU antibody (sc-sc-32323, Santa Cruz Biotechnology) at a dilution of 1:200 overnight 4 °C. On the next day, cells were washed in PBS three times and incubated with goat anti-mouse IgG1-Alexa Fluor 488 (A-21121, Invitrogen) at a dilution of 1:100 for 2 h at room temperature in the dark. Following washing three times with PBS each 5 min at room temperature, cells were stained with DAPI (1 μg/ml) for 2–3 min at room temperature to stain nuclei. Fluorescent images were acquired at 20× magnification using a Nikon TE300 digital inverted microscope, and the number of BrdU positive cells were determined by a laboratory member with no knowledge of sample identity using Image J software.
Kaplan Meier survival analysis
The association between SNCA transcript level and melanoma survival was determined using the TCGA (The Cancer Genome Atlas) dataset. To download and obtain the survival data of patients with melanoma, we utilized UCSC Xena Browser (http://xenabrowser.net). UCSC Xena Browser showed that TCGA dataset contained 462 cases of melanoma with both genomic (e.g. SNCA mRNA expression) and clinical (e.g. survival rate) information. We then generated a Kaplan Meier survival analysis to analyze the relationship between SNCA gene expression and overall survival in patients with melanoma.
Experiments were repeated three times, unless noted otherwise. The statistical significance was determined by a two tailed Student's t-test or a one-way ANOVA with Dunnett posthoc test. All results were expressed as mean ± standard deviation (s.d.) and a statistical difference was accepted at the 5% level unless indicated otherwise. GraphPad prism software or KaleidaGraph was used to make plots.
Olsen, J. H., Friis, S. & Frederiksen, K. Malignant melanoma and other types of cancer preceding Parkinson disease. Epidemiology 17, 582–587. https://doi.org/10.1097/01.ede.0000229445.90471.5e (2006).
Gao, X., Simon, K. C., Han, J., Schwarzschild, M. A. & Ascherio, A. Family history of melanoma and Parkinson disease risk. Neurology 73, 1286–1291. https://doi.org/10.1212/WNL.0b013e3181bd13a1 (2009).
Bertoni, J. M. et al. Increased melanoma risk in Parkinson disease a prospective clinicopathological study. Arch. Neurol. 67, 347–352. https://doi.org/10.1001/archneurol.2010.1 (2010).
Bose, A., Petsko, G. A. & Eliezer, D. Parkinson’s disease and melanoma: Co-occurrence and mechanisms. J. Parkinsons Dis. 8, 385–398. https://doi.org/10.3233/jpd-171263 (2018).
Pan, T., Li, X. & Jankovic, J. The association between Parkinson’s disease and melanoma. Int. J. Cancer 128, 2251–2260. https://doi.org/10.1002/ijc.25912 (2011).
Matsuo, Y. & Kamitani, T. Parkinson’s disease-related protein, alpha-synuclein, in malignant melanoma. PLoS ONE https://doi.org/10.1371/journal.pone.0010481 (2010).
Inzelberg, R., Flash, S., Friedman, E. & Azizi, E. Cutaneous malignant melanoma and Parkinson disease: Common pathways?. Ann. Neurol. 80, 811–820. https://doi.org/10.1002/ana.24802 (2016).
Pan, T., Zhu, J., Hwu, W. J. & Jankovic, J. The role of alpha-synuclein in melanin synthesis in melanoma and dopaminergic neuronal cells. PLoS ONE https://doi.org/10.1371/journal.pone.0045183 (2012).
Turriani, E. et al. Treatment with diphenyl-pyrazole compound anle138b/c reveals that alpha-synuclein protects melanoma cells from autophagic cell death. Proc. Natl. Acad. Sci. USA 114, E4971–E4977. https://doi.org/10.1073/pnas.1700200114 (2017).
Smith, A. P., Hoek, K. & Becker, D. Whole-genome expression profiling of the melanoma progression pathway reveals marked molecular differences between nevi/melanoma in situ and advanced-stage melanomas. Cancer Biol. Ther. 4, 1018–1029. https://doi.org/10.4161/cbt.4.9.2165 (2005).
Spillantini, M. G. et al. Alpha-synuclein in Lewy bodies. Nature 388, 839–840 (1997).
Polymeropoulos, M. H. et al. Mutation in the alpha-synuclein gene identified in families with Parkinson’s disease. Science 276, 2045–2047. https://doi.org/10.1126/science.276.5321.2045 (1997).
Maries, E., Dass, B., Collier, T. J., Kordower, J. H. & Steece-Collier, K. The role of alpha-synuclein in Parkinson’s disease: Insights from animal models. Nat. Rev. Neurosci. 4, 727–738. https://doi.org/10.1038/nrn1199 (2003).
Goedert, M., Jakes, R. & Spillantini, M. G. The synucleinopathies: Twenty years on. J. Parkinsons Dis. 7, S53–S71. https://doi.org/10.3233/jpd-179005 (2017).
Weinreb, P. H., Zhen, W., Poon, A. W., Conway, K. A. & Lansbury, P. T. NACP, a protein implicated in Alzheimer’s disease and learning, is natively unfolded. Biochemistry 35, 13709–13715 (1996).
Chandra, S., Chen, X. C., Rizo, J., Jahn, R. & Sudhof, T. C. A broken alpha-helix in folded alpha-synuclein. J. Biol. Chem. 278, 15313–15318. https://doi.org/10.1074/jbc.M213128200 (2003).
Pranke, I. M. et al. alpha-Synuclein and ALPS motifs are membrane curvature sensors whose contrasting chemistry mediates selective vesicle binding. J. Cell Biol. 194, 88–102. https://doi.org/10.1083/jcb.201011118 (2011).
Burre, J. et al. alpha-Synuclein promotes SNARE-complex assembly in vivo and in vitro. Science 329, 1663–1667. https://doi.org/10.1126/science.1195227 (2010).
Ben Gedalya, T. et al. alpha-Synuclein and polyunsaturated fatty acids promote clathrin-mediated endocytosis and synaptic vesicle recycling. Traffic 10, 218–234. https://doi.org/10.1111/j.1600-0854.2008.00853.x (2009).
Logan, T., Bendor, J., Toupin, C., Thorn, K. & Edwards, R. H. alpha-Synuclein promotes dilation of the exocytotic fusion pore. Nat. Neurosci. 20, 681. https://doi.org/10.1038/nn.4529 (2017).
Goedert, M., Spillantini, M. G., Del Tredici, K. & Braak, H. 100 years of Lewy pathology. Nat. Rev. Neurol. 9, 13–24. https://doi.org/10.1038/nrneurol.2012.242 (2013).
Kalia, L. V. & Lang, A. E. Parkinson’s disease. Lancet 386, 896–912. https://doi.org/10.1016/s0140-6736(14)61393-3 (2015).
Belaidi, A. A. & Bush, A. I. Iron neurochemistry in Alzheimer’s disease and Parkinson’s disease: Targets for therapeutics. J. Neurochem. 139, 179–197. https://doi.org/10.1111/jnc.13425 (2016).
Scherzer, C. R. et al. GATA transcription factors directly regulate the Parkinson’s disease-linked gene alpha-synuclein. Proc. Natl. Acad. Sci. USA 105, 10907–10912. https://doi.org/10.1073/pnas.0802437105 (2008).
Baksi, S., Tripathi, A. K. & Singh, N. Alpha-synuclein modulates retinal iron homeostasis by facilitating the uptake of transferrin-bound iron: Implications for visual manifestations of Parkinson’s disease. Free Radic. Biol. Med. 97, 292–306. https://doi.org/10.1016/j.freeradbiomed.2016.06.025 (2016).
Patel, D. et al. Alpha-synuclein inhibits Snx3-retromer-mediated retrograde recycling of iron transporters in S. cerevisiae and C. elegans models of Parkinson’s disease. Hum. Mol. Genet. 27, 1514–1532. https://doi.org/10.1093/hmg/ddy059 (2018).
Dexter, D. T. et al. Increased nigral iron content in postmortem parkinsonian brain. Lancet 2, 1219–1220 (1987).
Dexter, D. T. et al. Alterations in the levels of iron, ferritin, and other trace metals in Parkinson’s disease and other neurodegenerative diseases affecting the basal ganglia. Brain 114, 1953–1975 (1991).
Torti, S. V., Manz, D. H., Paul, B. T., Blanchette-Farra, N. & Torti, F. M. In Annual Review of Nutrition, Vol. 38 (eds Stover, P. J. & Balling R.) 97–125 (2018).
Pantopoulos, K. In Redox-Active Metals in Neurological Disorders Vol. 1012 Annals of the New York Academy of Sciences (eds LeVine, S. M. et al.) 1–13 (2004).
Gunshin, H. et al. Cloning and characterization of a mammalian proton-coupled metal-ion transporter. Nature 388, 482–488. https://doi.org/10.1038/41343 (1997).
Donovan, A. et al. Positional cloning of zebrafish ferroportin1 identifies a conserved vertebrate iron exporter. Nature 403, 776–781 (2000).
Whitnall, M., Howard, J., Ponka, P. & Richardson, D. R. A class of iron chelators with a wide spectrum of potent antitumor activity that overcomes resistance to chemotherapeutics. Proc. Natl. Acad. Sci. USA 103, 14901–14906. https://doi.org/10.1073/pnas.0604979103 (2006).
Gandhirajan, R. K. et al. Cytochrome C oxidase inhibition and cold plasma-derived oxidants synergize in melanoma cell death induction. Sci. Rep. https://doi.org/10.1038/s41598-018-31031-2 (2018).
Kaur, U. & Lee, J. C. Unroofing site-specific alpha-synuclein-lipid interactions at the plasma membrane. Proc. Natl. Acad. Sci. USA 117, 18977–18983. https://doi.org/10.1073/pnas.2006291117 (2020).
Shen, T. et al. Ciclopirox inhibits cancer cell proliferation by suppression of Cdc25A. Genes Cancer 8, 505–516. https://doi.org/10.18632/genesandcancer.135 (2017).
Barzegar, M. et al. SKLB188 inhibits the growth of head and neck squamous cell carcinoma by suppressing EGFR signalling. Br. J. Cancer 117, 1154–1163. https://doi.org/10.1038/bjc.2017.298 (2017).
Ji, C. Y. & Kosman, D. J. Molecular mechanisms of non-transferrin-bound and transferring-bound iron uptake in primary hippocampal neurons. J. Neurochem. 133, 668–683. https://doi.org/10.1111/jnc.13040 (2015).
Drakesmith, H., Nemeth, E. & Ganz, T. Ironing out ferroportin. Cell Metab. 22, 777–787. https://doi.org/10.1016/j.cmet.2015.09.006 (2015).
Iezzoni, J. C. Diagnostic histochemistry in hepatic pathology. Semin. Diagn. Pathol. 35, 381–389. https://doi.org/10.1053/j.semdp.2018.10.003 (2018).
Wang, Z. J., Lam, K. W., Lam, T. T. & Tso, M. O. Iron-induced apoptosis in the photoreceptor cells of rats. Investig. Ophthalmol. Vis. Sci. 39, 631–633 (1998).
Xu, G. et al. Lipocalin-2 induces cardiomyocyte apoptosis by increasing intracellular iron accumulation. J. Biol. Chem. 287, 4808–4817. https://doi.org/10.1074/jbc.M111.275719 (2012).
Yang, F. et al. Inhibition of iron overload-induced apoptosis and necrosis of bone marrow mesenchymal stem cells by melatonin. Oncotarget 8, 31626–31637. https://doi.org/10.18632/oncotarget.16382 (2017).
Surguchev, A. A. & Surguchov, A. Synucleins and gene expression: Ramblers in a crowd or cops regulating traffic?. Front. Mol. Neurosci. https://doi.org/10.3389/fnmol.2017.00224 (2017).
Singh, P. K. & Muqit, M. M. Parkinson’s: A disease of aberrant vesicle trafficking. Annu. Rev. Cell Dev. Biol. 36, 237–264. https://doi.org/10.1146/annurev-cellbio-100818-125512 (2020).
Surguchov, A. Parkinson’s disease: Assay of phosphorylated alpha-synuclein in skin biopsy for early diagnosis and association with melanoma. Brain Sci. https://doi.org/10.3390/brainsci6020017 (2016).
Nishioka, K. et al. Association of alpha-, beta-, and gamma-Synuclein With Diffuse Lewy Body Disease. Arch. Neurol. 67, 970–975 (2010).
Sekigawa, A. et al. Distinct mechanisms of axonal globule formation in mice expressing human wild type alpha-synuclein or dementia with Lewy bodies-linked P123H beta-synuclein. Mol. Brain https://doi.org/10.1186/1756-6606-5-34 (2012).
Ahmad, M., Attoub, S., Singh, M. N., Martin, F. L. & El-Agnaf, O. M. A. gamma-synuclein and the progression of cancer. FASEB J 21, 3419–3430. https://doi.org/10.1096/fj.07-8379rev (2007).
Israeli, E. et al. alpha-Synuclein expression selectively affects tumorigenesis in mice modeling parkinson’s disease. PLoS ONE https://doi.org/10.1371/journal.pone.0019622 (2011).
Rodriguez-Losada, N. et al. Overexpression of alpha-synuclein promotes both cell proliferation and cell toxicity in human SH-SY5Y neuroblastoma cells. J. Adv. Res. 23, 37–45. https://doi.org/10.1016/j.jare.2020.01.009 (2020).
Bruening, W. et al. Synucleins are expressed in the majority ofbreast and ovarian carcinomas and in preneoplastics lesions of the ovary. Can. Biol. Ther. 88, 2154–2163 (2000).
Liu, C. Y. et al. Unconventional secretion of synuclein-gamma promotes tumor cell invasion. FEBS J. 281, 5159–5171. https://doi.org/10.1111/febs.13055 (2014).
Liu, C., Qu, L., Zhao, C. & Shou, C. Extracellular gamma-synuclein promotes tumor cell motility by activating beta 1 integrin-focal adhesion kinase signaling pathway and increasing matrix metalloproteinase-24,-2 protein secretion. J. Exp. Clin. Cancer Res. https://doi.org/10.1186/s13046-018-0783-6 (2018).
Zhang, C., Gu, L., Li, X. & Wang, J. Silencing of Synuclein-gamma inhibits human cervical cancer through the AKT signaling pathway. Cell Mol. Biol. Lett. https://doi.org/10.1186/s11658-019-0172-y (2019).
Janik, P., Briand, P. & Hartmann, N. R. The effect of estrone-progesterone treatment on cell proliferation kinetics of hormone-dependent GR mouse mammary tumors. Cancer Res. 35, 3698–3704 (1975).
Wang, S. et al. alpha-Synuclein disrupts stress signaling by inhibiting polo-like kinase Cdc5/Plk2. Proc. Natl. Acad. Sci. USA 109, 16119–16124. https://doi.org/10.1073/pnas.1206286109 (2012).
This study was supported by funds from the Feist-Weiller Cancer Center and the Chancellor of LSU Health Sciences Center to S.N.W.
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Shekoohi, S., Rajasekaran, S., Patel, D. et al. Knocking out alpha-synuclein in melanoma cells dysregulates cellular iron metabolism and suppresses tumor growth. Sci Rep 11, 5267 (2021). https://doi.org/10.1038/s41598-021-84443-y
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