Summary
Recent research suggests that altered redox control of melanoma cell survival, proliferation, and invasiveness represents a chemical vulnerability that can be targeted by pharmacological modulation of cellular oxidative stress. The endoperoxide artemisinin and semisynthetic artemisinin-derivatives including dihydroartemisinin (DHA) constitute a major class of antimalarials that kill plasmodium parasites through induction of iron-dependent oxidative stress. Here, we demonstrate that DHA may serve as a redox chemotherapeutic that selectively induces melanoma cell apoptosis without compromising viability of primary human melanocytes. Cultured human metastatic melanoma cells (A375, G361, LOX) were sensitive to DHA-induced apoptosis with upregulation of cellular oxidative stress, phosphatidylserine externalization, and activational cleavage of procaspase 3. Expression array analysis revealed DHA-induced upregulation of oxidative and genotoxic stress response genes (GADD45A, GADD153, CDKN1A, PMAIP1, HMOX1, EGR1) in A375 cells. DHA exposure caused early upregulation of the BH3-only protein NOXA, a proapototic member of the Bcl2 family encoded by PMAIP1, and genetic antagonism (siRNA targeting PMAIP1) rescued melanoma cells from apoptosis indicating a causative role of NOXA-upregulation in DHA-induced melanoma cell death. Comet analysis revealed early DHA-induction of genotoxic stress accompanied by p53 activational phosphorylation (Ser 15). In primary human epidermal melanocytes, viability was not compromised by DHA, and oxidative stress, comet tail moment, and PMAIP1 (NOXA) expression remained unaltered. Taken together, these data demonstrate that metastatic melanoma cells display a specific vulnerability to DHA-induced NOXA-dependent apoptosis and suggest feasibility of future antimelanoma intervention using artemisinin-derived clinical redox antimalarials.
Keywords: Malignant melanoma, Dihydroartemisinin, PMAIP1, Reactive oxygen species, Oxidative stress, Apoptosis
Introduction
Metastatic melanoma, a malignant tumor originating from neural crest-derived melanocytes, causes the majority of skin cancer-related deaths [1, 2]. The poor prognosis associated with metastatic melanoma and the dearth of pharmacological treatment options create an urgent need for more efficacious chemotherapeutic intervention. Recent research suggests a causative involvement of altered redox homeostasis and reactive oxygen species (ROS)-dependent signaling in the control of melanoma cell survival, proliferation, and invasiveness [1, 3–7].
Accumulative experimental evidence indicates that several prooxidant chemotherapeutics cause cytotoxic deviations from redox homeostasis that cannot be tolerated by malignant cells, already exposed to high constitutive levels of ROS, but do not compromise viability of non-transformed cells [1, 8–10]. A rapidly increasing number of investigational redox chemotherapeutics has been evaluated in clinical studies including motexafin gadolinium, darinaparsin, arsenic trioxide, NOV-002, PX-12, disulfiram, and elesclomol as recently reviewed [1, 10, 11].
The sesquiterpene endoperoxide artemisinin and other semisynthetic artemisinin-derivatives including dihydroartemisinin (DHA) constitute an important class of FDA-approved antimalarial drugs that kill plasmodium parasites through induction of iron-dependent oxidative stress [12]. Lead optimization has led to the development of a whole range of 1,2,4-trioxane-based, semisynthetic artemisinin-derivatives with shared endoperoxide pharmacophore including DHA, artemether, arteether, and artesunate, representing the most potent and rapidly acting group of antimalarials available today. Recent research has demonstrated that artemisinin-based endoperoxide drugs may serve as experimental prooxidant cancer chemotherapeutics displaying significant activity in cell-based, animal, and human studies [11, 13–15], but only a limited number of prior experimental studies has examined artemisinin-based agents targeting melanoma [16–18]. Interestingly, a clinical case report on two patients with metastatic uveal melanoma presented preliminary evidence in support of a potential therapeutic benefit associated with artesunate chemotherapy [13].
Based on our earlier research aiming at the identification of experimental redox chemotherapeutics targeting melanoma [19, 20], we decided to further examine the antimelanoma activity of artemisinin-based chemotherapy focusing on DHA, a clinically used prototypical semisynthetic artemisinin-derivative with increased stability based on lactone group reduction. Here, we report for the first time that DHA displays activity as a selective redox chemotherapeutic targeting cultured human metastatic melanoma cells without compromising viability of primary epidermal melanocytes and that pronounced upregulation of the BH3-only protein NOXA is required for DHA-induced caspase-dependent elimination of melanoma cells.
Materials and methods
Chemicals
All chemicals were purchased from Sigma Chemical Co (St. Louis, MO, USA).
Cell culture
G-361, A375, and LOX human melanoma cells and dermal neonatal foreskin Hs27 fibroblasts from ATCC (Manassas, VA, USA) were cultured as published recently [19–21]. Primary human epidermal melanocytes (adult skin, lightly pigmented: HEMa-LP from Cascade Biologics, abbreviated HEMa) were cultured using Medium 154 medium supplemented with HMGS-2 growth supplement. Cells were maintained at 37°C in 5% CO2, 95% air in a humidified incubator.
Transmission electron microscopy
Cells were fixed in situ with 2.5% glutaraldehyde in 0.1 M cacodylate buffer (pH7.4), postfixed in 1% osmium tetroxide in cacodylate buffer and then processed and analyzed as published recently [22].
Human stress and toxicity pathfinder™ RT2 profiler™ PCR expression array
After pharmacological exposure, total cellular RNA (3×106 A375 cells) was prepared according to a standard procedure using the RNeasy kit (Qiagen, Valencia, CA, USA). Reverse transcription was performed using the RT2 First Strand kit (Superarray, Frederick, MD, USA) and 5 μg total RNA as described previously [20]. The RT2 Human Stress and Toxicity Pathfinder™ PCR Expression Array (SuperArray) profiling the expression of 84 stress-related genes was run and analyzed as published earlier [20, 21, 23]. Expression values were averaged across three independent array experiments, and standard deviation was calculated for graphing.
CDKN1A, DDIT3, GADD45A, HMOX1, and PMAIP1 expression analysis by real time RT-PCR
For expression analysis by real time RT-PCR, total cellular RNA (3×106 cells) was prepared using the RNEasy kit from Qiagen (Valencia, CA, USA) and processed according to published standard procedures [21, 23]. After reverse transcription, real time RT-PCR was performed using an Applied Biosystems 7000 SDS and Applied Biosystems’ Assays On Demand primers specific to CDKN1A (assay ID Hs00355782_m1), DDIT3 (assay ID Hs00358796_g1), GADD45A (assay ID Hs00169255_m1), HMOX1 (assay ID Hs00157965_m1), PMAIP1 (assay ID Hs00560402_m1), and GAPDH (assay ID Hs99999905_m1). Gene-specific product was normalized to GAPDH and quantified using the comparative (ΔΔCt) Ct method as described in the ABI Prism 7000 sequence detection system user guide [23]. Expression values were averaged across three independent experiments, and standard deviation was calculated for graphing.
siRNA-Transfection targeting PMAIP1 expression
A375 cells were transiently transfected with a 100 nmol pool of four small interfering RNA (siRNA) oligonucleotides (oligos) targeting PMAIP1 or a 100 nmol pool of four nontargeting siRNA oligos using the DharmaFECT 1 transfection reagent (Dharmacon RNA Technologies, Lafayette, Colorado, USA) following a standard procedure [20]. The sequences of siGENOME PMAIP1 SMARTpool (PMAIP1 siRNA) (Gen-Bank: NM 021127) were AAACUGAACUUCCGGCAGA, AUUCUGUAUCCAAACUCU, CUGGAAGUCGAGU GUGCUA, and GCAAGAACGCUCAACCGAG.
Immunoblot analysis of NOXA, PUMA, HO-1, CHOP, and p21
Sample preparation, SDS-PAGE, transfer to nitrocellulose, and development occurred as described earlier [20, 21]. Gel percentages were 12% (HO-1, p21, CHOP) and 15% (NOXA, PUMA). The following primary antibodies were used: mouse anti-CHOP monoclonal antibody (2895S; 1:1,000; Cell Signaling Technology, Danvers, MA); rabbit anti-HO-1 polyclonal antibody (SPA-896F, 1:5,000; Stress-gen Bioreagents, Ann Arbor, MI); monoclonal mouse anti-NOXA IgG (OP180; 1:1,000; EMD Chemicals, Gibbstown, NJ); polyclonal rabbit anti-PUMA antibody (4976; 1:1,000; Cell Signaling Technology) and mouse anti-p21 monoclonal antibody (2946; 1:2,000; Cell Signaling Technologies).
Cell death analysis
Viability and induction of cell death (early and late apoptosis/necrosis) were examined by annexin-V-FITC (AV)/propidium iodide (PI) dual staining of cells followed by flow cytometric analysis as published previously [19].
Flow cytometric detection of cleaved procaspase-3, phospho-p53 (Ser15), and phospho-H2A.X
Treatment-induced proteolytic caspase-3 activation and formation of phospho-p53 (Ser15) and phospho-H2A.X were examined in cultured A375 human melanoma cells using antibodies directed against cleaved/activated caspase-3 (Asp 175), phospho-p53 (Ser15), and phospho-histone H2A.X (Ser139) (Alexa Fluor 488 conjugates, Cell Signaling, Danvers, MA, USA) followed by flow cytometric analysis as published recently [19, 23].
Detection of intracellular oxidative stress by flow cytometric analysis
Induction of intracellular oxidative stress by DHA was analyzed by flow cytometry using 2′,7′-dichlorodihy-drofluorescein diacetate (DCFH-DA) as a sensitive non-fluorescent precursor dye according to a published standard procedure [19].
Determination of reduced cellular glutathione content
Intracellular reduced glutathione was measured using the GSH-Glo Glutathione assay kit (Promega; San Luis Obispo, CA) as described recently [23]. Data are normalized to GSH content in untreated cells and expressed as means ± SD (n=3).
Mitochondrial transmembrane potential
Mitochondrial transmembrane potential (Δψm) was assessed using the potentiometric dye 5,5′,6,6′-tetrachloro-1,1′,3,3′-tetraethyl-benzimidazolyl-carbocyanine iodide (JC-1) following our published flow cytometric procedure [19].
Cell Glo ATP assay
ATP content per 10,000 cells was determined using the CellTiter-Glo luminescent assay (Promega, Madison, WI, USA) according to the manufacturer’s instructions as published earlier [23]. Data are normalized to ATP content in untreated cells (expressed as means ± SD (n=3).
Comet assay (alkaline single cell electrophoresis)
The alkaline comet assay was performed on A375 melanoma and HEMa cells according to the manufacturer’s instructions (Trevigen, Gaithersburg, MD, USA) as published in detail recently [23]. Cells were stained with SYBR™ Green and then visualized and analyzed using a fluorescence microscope (fluorescein filter) and CASP software. At least 75 tail moments for each group were analyzed in order to calculate the mean ± S.D. for each group.
Statistical analysis
Unless indicated differently, the results are presented as mean ± S.D. of at least three independent experiments. All data were analyzed employing one-way analysis of variance (ANOVA) with Tukey’s post hoc test using the Prism 4.0 software. Differences were considered significant at p≤0.05. Means without a common letter differ (p<0.05).
Results
DHA induces cell death in human A375 metastatic melanoma cells but not in primary epidermal melanocytes
First, induction of cell death by DHA was assessed by flow cytometric analysis of annexinV-FITC/propidium iodide-stained metastatic melanoma cell lines (A375, G361, LOX), primary human fibroblasts (Hs27), and primary epidermal melanocytes (HEMa) (Fig. 1). Exposure to DHA (10 and 40 μM, 48 h) dose-dependently induced pronounced cell death in metastatic melanoma cells (Fig. 1a–d), but no impairment of viability was observed in primary epidermal melanocytes (Fig. 1a and d) and fibroblasts (Fig. 1c and d) exposed to DHA concentrations up to 100 μM.
Fig. 1.
DHA induces death in human metastatic melanoma cells but not in primary epidermal melanocytes. a Induction of cell death by exposure to DHA (40 μM, 48 h); flow cytometric analysis. The numbers indicate viable (AV−, PI−) in percent of total gated cells (mean ± SD, n=3). Representative light microscopy pictures taken after 48 h exposure to DHA are shown in panels I–IV. (I–II: A375; III–IV: HEMa; I and III: control; II and IV: DHA) b Dose response relationship of induction of A375 cell death (DHA 5–40 μM, 48 h). c Induction of cell death (DHA, 40 μM, 48 h) in G361 cells versus Hs27 dermal fibroblasts. d LD50 values as assessed by AV-PI flow cytometry
Array analysis reveals upregulation of oxidative and genotoxic stress response gene expression in A375 melanoma cells exposed to DHA
Next, modulation of stress and toxicity response gene expression was examined in A375 cells exposed to DHA (40 μM, 48 h exposure) using the RT2 Human Stress and Toxicity Profiler™ PCR Expression Array technology (SuperArray, Frederick, MD) (Fig. 2a). Out of 84 stress-related genes contained on the array DHA-induced expression changes in A375 cells affected 21 genes by at least two-fold over untreated control cells as summarized in Fig. 2b. More than fivefold upregulation was detected affecting the p53-regulated DNA damage inducible genes growth arrest and DNA-damage-inducible, alpha (GADD45A; 6-fold), cyclin-dependent kinase inhibitor 1 (CDKN1A; 6-fold), and DNA damage inducible transcript 3 (DDIT3/GADD153; 8-fold). Moreover, pronounced upregulation of genes encoding the antioxidant enzyme heme oxygenase-1 (encoded by HMOX1; 6-fold), the oxidative stress-responsive transcription factor and tumor suppressor early growth response protein 1 (encoded by EGR1; 5-fold), and the cytokine granulocte-macrophage colony stimulating factor 2 (CSF2; 6-fold) was observed.
Fig. 2.
Stress response gene expression in DHA-treated A375 metastatic melanoma cells. a The scatter blot (left panel) depicts differential gene expression as detected by the RT2 Human Stress and Toxicity Profiler™ PCR Expression Array technology (DHA: 40 μM, 48 h). Upper and lower lines: cut-off indicating twofold up-or down-regulated expression, respectively. Arrays were performed in three independent repeats and analyzed using the two-sided Student’s t test. b The table summarizes expression changes by at least twofold (p<0.05)
DHA induces oxidative stress in A375 melanoma cells
Led by upregulated expression of oxidative stress response genes after 48 h continuous exposure (HMOX1, EGR1; Fig. 2), we further examined the occurrence of cellular oxidative stress and redox alterations in DHA-treated A375 melanoma cells (Fig. 3).
Fig. 3.
DHA-induced oxidative stress in metastatic melanoma cells. a DHA-modulation (40 μM, 3��24 h exposure) of heme oxygenase-1 (HMOX1) mRNA (top panel; quantitative RT-PCR; mean ± SD, n=3) and protein (HO-1) levels (immunobot analysis, bottom panel) in A375 cells (b) Modulation of intracellular reduced glutathione in A375 cells, normalized to protein content (mean ± SD, n=3). c–e DHA-induction of intracellular oxidative stress. Cells were exposed to DHA (1–40 μM; up to 24 h). c A375 cells. One representative experiment (left panel) and quantitative analysis of three independent repeat experiments (right panel; mean ± SD) are displayed. d A375 and G361 cells versus HEMa and Hs27 cells (40 μM DHA; mean ± SD, n=3). e A375 melanoma cells exposed to the combined action of DHA (40 μM, 24 h) and small molecule modulators [NAC (10 mM), DFO (20 μM), zVADfmk (40 μM); mean ± SD, n=3]
Time course analysis of HMOX1 expression was performed by quantitative RT-PCR and detection revealing pronounced upregulation within 12 h continuous exposure (Fig. 3a). In addition, in A375 cells exposed to DHA (20 and 40 μM) significant depletion of intracellular reduced glutathione levels was observed at a similar time point (12 h; Fig. 3b). A dose-dependent elevation of intracellular oxidative stress could be observed in A375 cells exposed to DHA (10–40 μM, 24 h) as assessed by 2′,7′-dichloro-dihydrofluorescein diacetate detection of intracellular peroxide levels using flow cytometry (Fig. 3c). Over a 24 h treatment period (DHA, 40 μM), DCF fluorescence intensity increased approximately fivefold and was significantly upregulated within 12 h continuous exposure (Fig. 3d). Similar results were observed in other melanoma cell lines (G361; Fig. 3d). In contrast, DCF fluorescence intensity remained unaltered in primary melanocytes (HEMa) and Hs27 fibroblasts exposed to DHA (40 μM; 24 h; Fig. 3d), suggesting that DHA treatment does not induce oxidative stress in cells that are resistant to DHA-induced cell death (Fig. 1d). Further DCF-based analysis revealed that DHA-induced intracellular oxidative stress was blocked if A375 cells were pretreated with the thiol-antioxidant N-acetyl-L-cysteine (NAC, 10 mM, 24 h pretreatment followed by 40 μM DHA, 24 h) or the iron chelator deferoxamine (DFO, 20 μM, 1 h pretreatment followed by 40 μM DHA, 24 h) (Fig. 3e). In contrast, treatment with the pan-caspase inhibitor zVADfmk that was able to protect A375 cells against DHA-induced cell death (as detailed further in Fig. 4b) did not suppress elevation of cellular DCF fluorescence suggesting that DHA-induction of intracellular oxidative stress is an early event that does not occur downstream of caspase activation and cellular disintegration.
Fig. 4.
DHA-induced A375 and G361 melanoma cell apoptosis. a A375 cells [DHA-treated (40 μM, 24 and 48 h)] were examined by transmission electron microscopy (direct magnification: 8,800 x). The left panel depicts cell viability as determined by flow cytometry (mean ± SD, n=3). b Modulation of A375 and G361 cell death by exposure to DHA (40 μM, 48 h) in the presence or absence of small molecule modulators; three left panels: representative experiment using A375 cells [The numbers indicate viable (AV−, PI−) in percent of total gated cells (mean ± SD, n=3)]. The two bar graphs (right) summarize viability data. c DHA-induced (10 and 40 μM, 24 h) caspase-3 activation as examined in A375 cells by flow cytometric detection. Data (mean ± SD, n=3) are summarized in the bar graph. d A375 cell viability after preincubation (24 h) with BSO (1 mM) followed by DHA (20 μM, 48 h; mean ± SD, n=3). e A375 cell ATP levels after DHA treatment (20 and 40 μM, 1–24 h). f Mitochondrial transmembrane potential (△ψm) in response to DHA (40 μM; 6–24 h) in JC-1 stained A375 cells; one representative experiment out of three repeats is depicted
DHA-induced A375 melanoma cell apoptosis with mitochondrial impairment and caspase 3 activation is antagonized by iron chelation and antioxidant intervention
An apoptotic mode of DHA-induced A375 cell death was suggested by flow cytometric detection of annexin V-positivity, a cellular marker indicative of early stages of apoptosis that involve phosphatidylserine externalization at the plasma membrane level (Fig. 1a and b and Fig. 4b and d). Further morphological evidence in support of DHA-induced apoptosis was obtained employing transmission electron microsocopy that revealed early membrane blebbing (24 h exposure) followed by nuclear condensation (48 h exposure), both established hallmarks of cellular apoptosis (Fig. 4a) [24]. Consistent with caspase-dependent execution of DHA-induced cell death, cell viability was maintained upon cotreatment with the pancaspase inhibitor zVADfmk, an effect also observed with G361 melanoma cells (Fig. 4b).
Further flow cytometric analysis using a cleaved-procaspase 3-directed Alexa488-conjugated antibody revealed proteolytic activation of this executioner caspase that occurred dose dependently (10–40 μM DHA, 24 h; Fig. 4c). Consistent with a causative involvement of cellular oxidative stress in DHA-induced melanoma cell apoptosis, antioxidant pretreatment (NAC, 10 mM, 24 h preincubation) significantly diminished cytotoxicity of DHA (Fig. 4b), and significant sensitization towards DHA-induced cytotoxicity (20 μM, 24 h exposure) was observed in A375 cells that were pre-exposed to the prooxidant inhibitor of glutathione biosynthesis L-buthionine-S,R-sulfoximine (BSO, 1 mM; 24 h preincubation; Fig. 4d) [20]. Furthermore, iron chelation (DFO, 20 μM, 1 h pretreatment) efficiently suppressed DHA-induced cytotoxicity in A375 and G361 melanoma cells (Fig. 4b), and DHA-dependent proteolytic caspase 3 activation was completely blocked by DFO in A375 cells (Fig. 4c).
Further flow cytometric analysis using the sensor dye JC-1 revealed an early impairment of mitochondrial integrity as obvious from dramatic loss of transmembrane potential (Δψm) that occurred within 12 h in DHA exposed A375 cells (Fig. 4f). In the context of mitochondrial impairment, DHA-induced energy crisis was evident from cellular ATP depletion in A375 cells that reached the level of statistical sigificance within 12 exposure time (40 μM DHA; Fig. 4e). None of these DHA-induced changes observed in A375 cells (AV-PI positivity, EM morphological changes, procaspase 3 cleavage, loss of Δψm and ATP) was observed in melanocytes or Hs27 fibroblasts that maintained full viability during the course of the experiment (up to 48 h continuous exposure to DHA, 40 μM, Fig. 1a and d, and data not shown).
DHA-induced early upregulation of PMAIP1 (NOXA) expression occurs in A375 and G361 melanoma cells but not in primary melanocytes
Our expression array data indicated that DHA exposure occurred with transcriptional upregulation of PMAIP1 encoding the proapoptotic BH3-only regulator protein NOXA (Fig. 2). We therefore examined DHA-induced PMAIP1 expression at the mRNA and protein level as a function of exposure time in A375 and G361 melanoma cells versus primary melanocytes (Fig. 5a–f). Time course analysis revealed significant upregulation of PMAIP1 transcript levels that occurred in both melanoma cell lines within 6 h continuous exposure (DHA, 40 μM) but was not observed in melanocytes (Fig. 5a–c). Immunoblot detection of NOXA confirmed DHA-induction of PMAIP1 expression at the protein level in A375 and G361 cells (Fig. 5d–f). In contrast, NOXA protein levels remained undetectable in melanocytes (Fig. 5f, left panel). In parallel with dramatic upregulation of NOXA protein levels as an early response to DHA exposure observed in melanoma cells, immunoblot detection in A375 cells also revealed a moderate upregulation of the proapoptotic BH3-only mediator PUMA that remained unchanged in DHA-treated melanocytes (Fig. 5d and f).
Fig. 5.
NOXA (PMAIP1) expression in DHA-induced A375 melanoma cell apoptosis. a–c DHA-modulation (40 μM, up to 24 h) of PMAIP1 mRNA levels in A375 (panel a), G361 (panel b), and HEMa cells (panel c) by real time RT-PCR analysis (mean ± SD, n=3). d NOXA and PUMA upregulation in A375 cells exposed to 40 μM DHA (3–24 h); immunobot analysis. e NOXA upregulation in G361 cells exposed to 40 μM DHA (3–24 h); immunobot analysis. f NOXA and PUMA upregulation in A375 versus HEMa cells exposed to 40 μM DHA (6 and 12 h); immunobot analysis. g PMAIP1 knockdown in untreated wildtype (wt), control siRNA treated (siControl), and PMAIP1 siRNA treated (siPMAIP1) A375 cells was confirmed after DHA exposure (40 μM, 48 h) by NOXA immunoblot detection. h Induction of death by exposure to DHA (40 μM, 48 h) assessed by flow cytometry of A375 cells after siControl and siPMAIP1 treatment. Numbers indicate viable (AV−, PI−) in percent of total gated cells. One representative experiment of three similar repeats is shown
Genetic antagonism of PMAIP1 (NOXA) expression protects A375 metastatic melanoma cells from DHA-induced apoptosis
Based on the established key role of NOXA in the mitochondrial pathway of apoptosis [25–27], we then tested the hypothesis that upregulation of PMAIP1 expression may be causatively involved in DHA-induced A375 melanoma cell apoptosis. To this end, genetic target modulation using a siRNA approach targeting PMAIP1 expression was employed. First, efficacy of PMAIP1 knockdown (siPMAIP1) was confirmed at the protein level (Fig. 5g). Immunoblot detection revealed that DHA-induced upregulation of NOXA protein levels, as observed earlier in wildtype A375 control cells (Fig. 5d, f, g), could be blocked by prior transfection using the siPMAIP1 oligonucleotides (Fig. 5g, right panel), but was not suppressed when transfection occurred using non-targeting siRNA control reagent (siControl; Fig. 5g, middle panel).
Next, the effect of siRNA intervention targeting PMAIP1 upregulation on DHA-induced apoptosis was examined in A375 cells (Fig. 5h). Flow cytometric analysis revealed pronounced cellular protection against DHA-induced cytotoxicity (40 μM, 48 h) that was only observed in siPMAIP1-tranfected (approximately 82% survival) but not in siControl-transfected (approximately 45% survival) cells, suggesting that NOXA is a key mediator of DHA-induced apoptosis in A375 melanoma cells.
DHA impairs genomic integrity with early activational phosphorylation of p53 (p53-Ser15) in A375 melanoma cells but not in primary epidermal melanocytes
Our array-based observation that DHA treatment induced genotoxic stress response gene expression (GADD45A, CDKN1A, and DDIT3; 48 h exposure; Fig. 2) led us to examine if early induction of DNA damage may contribute to DHA-apoptogenicity in A375 metastatic melanoma cells. First, GADD45A, CDKN1A, and DDIT3 expression was examined at the transcriptional level by time course analysis using quantitative RT-PCR that revealed pronounced upregulation within 6 h (GADD45A, DDIT3) or 12 h (CDKN1A) continuous exposure (Fig. 6a–c). DHA-induced expression changes at the protein level were observed by immunoblot detection of CHOP (encoded by DDIT3/GADD153), a transcription factor that can be upregulated in response to genotoxic stress and ER stress. Using the established ER stress inducer thapsigargin (300 nM, 24 h) as a positive control, CHOP upregulation was observed within 12 continuous exposure to DHA, whereas p21 (encoded by CDKN1A) displayed increases that occurred only upon 24 h continuous exposure (Fig. 6d and e, respectively).
Fig. 6.
DHA-induced genotoxic stress in A375 melanoma cells. DHA-modulation (40 μM, up to 24 h exposure) of GADD45A (panel a), DDIT3 (panel b), and CDKN1A (panel c) mRNA levels (mean ± SD, n=3). DHA-modulation (40 μM, up to 24 h exposure) of CHOP (encoded by DDIT3; panel d) and p21 (encoded by CDKN1A; panel e) protein levels by immunoblot analysis; thapsigargin (TG): 300 nM, 24 h. f A375 and HEMa cells were exposed to DHA (10–40 μM, 3–12 h), and DNA damage was detected using the comet assay; positive control: H2O2 (100 μM, 30 min); representative comet images (left panels) and quantitative analysis of average tail moments (bar graph). g Induction of γ-H2A.X in DHA-treated A375 cells (40 μM, up to 48 h). h Early activational p53 phosphorylation (Ser15) as assessed by flow cytometric analysis [DHA 40 μM; 1–6 h; with or without DFO (20 μM)]. One representative experiment out of three similar repeats is shown (left panel), and data (mean ± SD, n=3) are summarized in the bar graph
DHA-dependent induction of genotoxic stress was examined using alkaline single cell electrophoresis (comet assay) [23]. As evident from formation of nuclear comets in A375 cells, significant induction of genotoxic stress was detectable within 3 h exposure to low micromolar concentrations of DHA (10 μM) (Fig. 6f). At higher concentrations (40 μM), DHA treatment induced comets with average tail moments that exceeded control levels more than three fold within 6 h of exposure (Fig. 6f). In contrast, analogous comet analysis performed in human epidermal melanocytes exposed to DHA (10 and 40 μM, up to 12 h exposure time) did not reveal any impairment of genomic integrity (Fig. 6f).
DHA-induced impairment of genomic integrity was also examined by flow cytometric analysis of the nuclear phosphorylated histone variant H2A.X (γ-H2A.X, Ser 139), a sensitive marker of DNA double-strand breaks (Fig. 6g) [28]. In A375 cells, no induction of γ-H2A.X was observed in response to DHA exposure at time points and concentrations (10 μM, 3 h) that caused a significant increase in average tail moment demonstrating that DHA-induced early impairment of genomic integrity does not involve the generation of double strand breaks.
DNA damage is known to induce activational phosphorylation of tumor suppressor protein p53 at Ser15 that occurs by genotoxic stress-responsive kinases [29]. Consistent with an involvement of p53 activation that may occur upstream of GADD45A, DDIT3, and CDKN1A upregulation, early activational phosphorylation [phospho-p53 (Ser15)] was observed in response to DHA within 3 h exposure time (Fig. 6h). In contrast, treatment with DHA did not cause any changes in p53-Ser15 phosphorylation status in human epidermal melanocytes (Fig. 6h), a finding consistent with the absence of DHA-induced DNA comets observed above (Fig. 5c).
Discussion
Recent research has demonstrated that the redox antimalarial artemisinin and its semisynthetic derivatives including DHA may display anticancer activity. Here, we have demonstrated for the first time that DHA may serve as a potent redox chemotherapeutic that selectively induces melanoma cell apoptosis without compromising viability of primary human melanocytes. These results are consistent with earlier research demonstrating that induction of cellular oxidative stress with mitochondria-dependent apoptosis plays a major role in the anticancer activity of artemisinins [12, 15, 30, 31]. Earlier experimentation has also demonstrated that expression of antioxidant genes including thioredoxin reductase and catalase is an important determinant of artesunate activity against tumor cells further establishing the importance of redox mechanisms underlying artemisinin apoptogenicity directed against cancer cells [32].
In our experiments focusing on A375 human metastatic melanoma cells, expression array analysis revealed DHA-induced upregulation of oxidative and genotoxic stress response genes (GADD45A, GADD153, CDKN1A, PMAIP1, HMOX1, EGR1) in A375 melanoma cells (Fig. 2 and Fig. 6a–c), consistent with early activational phosphorylation of p53 (Ser15) as detected by flow cytometry (Fig. 6h) [36,38]. Direct experimental evidence indicating early induction of DHA-genotoxicity within 3 h continuous exposure was then obtained employing single cell electrophoresis (comet assay) that detects impairment of genomic integrity by visualizing DNA unwinding under alkaline conditions that may result from single or double strand breaks, AP-site formation, or nucleotide excision repair [23]. In this context it should be mentioned that induction of DNA damage by the artemisinin-derivative artesunate has been observed earlier in Chinese hamster ovary (CHO-9) cells but comet assay-based assessment was only performed upon 24 h continuous exposure without inclusion of earlier timepoints [33]. Moreover, recent microarray analysis of LOX IMVI melanoma cells exposed to a synthetic artemisinin-dimer has documented DHA-induced upregulation of DNA damage response gene expression [18]. However, the molecular mechanism underlying DHA genotoxicity in A375 melanoma cells remains unresolved at this point, and we are currently testing the hypothesis that oxidative DNA base modification and free radical-induced single strand breaks are involved in DHA genotoxicity in melanoma cells.
Pronounced upregulation of the BH3-only protein NOXA, a proapoptotic member of the Bcl2 family encoded by PMAIP1, occurred within 6 h DHA-exposure at the transcriptional and protein level (Fig. 5) [25–27]. In addition, moderate upregulation of PUMA, another BH3-only proapoptotic protein, was also detected in DHA-exposed A375 cells (Fig. 5d and f), but neither NOXA nor PUMA levels were increased in HEMa cells exposed to DHA (Fig. 5f). In the context of therapeutic induction of melanoma cell apoptosis by small molecule intervention, it is important to note that upregulation of the BH3-only protein NOXA upstream of mitochondrial membrane permeabilization and cytochrome C release has recently emerged as a promising key mechanism underlying potent apoptogenicity of various investigational drugs targeting metastatic melanoma [25–27]. The causative role of NOXA in DHA-induced apoptotic elimination of melanoma cells was then established by demonstrating that genetic antagonism (siRNA targeting PMAIP1 expression) rescued melanoma cells from DHA-induced apoptosis (Fig. 5).
Importantly, PMAIP1 and PUMA are established target genes subject to transcriptional control by p53 in melanoma cells [27]. Detection of early p53-Ser15 activational phosphorylation as observed in our experiments (Fig. 6h) may indeed indicate that PMAIP1 and PUMA upregulation occurs downstream of DHA-induced p53 activation in A375 melanoma cells, a hypothesis to be substantiated by further experimentation. Importantly, another report has recently demonstrated the causative role of PMAIP1 upregulation in DHA-induced apoptosis of Jurkat T lymphoma cells [31].
It will also be interesting to examine the possibility that induction of ER stress, suggested by upregulation of CHOP protein levels observed after 12 h continuous exposure (Fig. 6d), contributes to DHA-induced cytotoxicity in A375 cells as observed earlier in the context of artemisinin-dimers [18].
It is remarkable that in primary human epidermal melanocytes, cell viability was not compromised by DHA exposure (Fig. 1a and d), and comet tail moment (Fig. 6f), NOXA expression (Fig. 5c and f), and cellular oxidative stress (Fig. 3d) remained unaltered by DHA exposure. The mechanistic basis underlying differential DHA cytotoxicity directed against melanoma versus melanoytes remains unresolved at this point. Intracellular activation of the endoperoxide-pharmacophore is thought to occur by redox-active labile iron, the common pharmacodynamic basis underlying both antimalarial and anticancer activity [11, 12]. Indeed, the susceptibility of tumor cells to artemisinin and its derivatives can be enhanced by co-administration of ferrous iron, and oral co-administration of dihydroartemisinin and ferrous sulfate retarded implanted fibrosarcoma tumor growth in rats [34]. Cancer cells display increased rates of iron uptake that supports rapid proliferation [35], and recent data strongly suggest that altered iron homeostasis with increased cellular levels of redox active iron in oncogenic Ras-transformed cells represents a chemical Achilles heel targeted by iron-activated prooxidant intervention [36]. The specific vulnerability of melanoma cells to DHA, not observed in melanocytes, may therefore result from increased intracellular availability of redox active labile iron, a hypothesis to be tested by future experimentation.
Development of more efficacious therapeutic modalities targeting early and late stages of malignant melanoma is ongoing [37]. Our data demonstrate that metastatic melanoma cells display a specific vulnerability to DHA-induced NOXA-dependent apoptosis suggesting that further preclinical and clinical evaluation of anti-melanoma intervention using artemisinin-derived redox antimalarials is warranted.
Acknowledgments
Supported in part by grants from the National Institutes of Health [R01CA122484, ES007091, ES006694, Arizona Cancer Center Support Grant CA023074].
Footnotes
Declaration of interest The authors report no conflicts of interest. The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Cancer Institute or the National Institutes of Health.
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