Identification of artesunate as a specific activator of ferroptosis in pancreatic cancer cells
1 Lysosomal Systems Biology, German Cancer Research Center (DKFZ), Heidelberg, Germany
2 Systems Biology of Cell Death Mechanisms, German Cancer Research Center (DKFZ), Heidelberg, Germany
3 Department of Surgery, Heidelberg University Hospital, Heidelberg, Germany
4 BioQuant, University of Heidelberg, Germany
Correspondence to: Anne Hamacher-Brady, email: email@example.com
Correspondence to: Nathan R Brady, email: firstname.lastname@example.org
Keywords: artesunate, necroptosis, ferroptosis, KRas, pancreatic cancer, cell death
Received: February 20, 2015
Accepted: April 28, 2015
Published: May 2, 2015
This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Oncogenic KRas reprograms pancreatic ductal adenocarcinoma (PDAC) cells to states which are highly resistant to apoptosis. Thus, a major preclinical goal is to identify effective strategies for killing PDAC cells. Artesunate (ART) is an anti-malarial that specifically induces programmed cell death in different cancer cell types, in a manner initiated by reactive oxygen species (ROS)-generation. In this study we demonstrate that ART specifically induced ROS- and lysosomal iron-dependent cell death in PDAC cell lines. Highest cytotoxicity was obtained in PDAC cell lines with constitutively-active KRas, and ART did not affect non-neoplastic human pancreatic ductal epithelial (HPDE) cells. We determined that ART did not induce apoptosis or necroptosis. Instead, ART induced ferroptosis, a recently described mode of ROS- and iron-dependent programmed necrosis which can be activated in Ras-transformed cells. Co-treatment with the ferroptosis inhibitor ferrostatin-1 blocked ART-induced lipid peroxidation and cell death, and increased long-term cell survival and proliferation. Importantly, analysis of PDAC patient mRNA expression indicates a dependency on antioxidant homeostasis and increased sensitivity to free intracellular iron, both of which correlate with Ras-driven sensitivity to ferroptosis. Overall, our findings suggest that ART activation of ferroptosis is an effective, novel pathway for killing PDAC cells.
Pancreatic ductal adenocarcinoma (PDAC) is an incurable form of cancer. Standard therapies increase survival rates by less than six months  and PDAC is predicted to increase in incidence . PDAC is driven by constitutively-active KRas mutations [3, 4], which result in metabolic reprogramming [5-7] and resistance to apoptosis . PDAC is highly resistant to death receptor and mitochondrial modes of apoptotic programmed cell death . Moreover, death receptor activation is an important source of cancer-promoting inflammation signaling  and promotes metastasis . Thus, the discovery of efficient strategies to kill pancreatic cancer cells remains an outstanding goal in programmed cell death (PCD) research, and considerable efforts are being made to identify general, as well as patient-specific, molecular targeting strategies [11, 12].
A complementary strategy, which we apply here, is to determine the mechanisms and mode of PCD activated by small molecules which induce efficient cancer cell death . Here we focused on artesunate, a water-soluble derivative of the natural compound artemisinin, an effective anti-malarial , with well-understood pharmacokinetics [15, 16]. ART specifically induces cell death and blocks clonogenicity in a variety of cancer types [13, 17, 18, 19], including PDAC cells . Importantly, ART-mediated cytotoxicity is dependent on increased reactive oxygen species (ROS) generation and the presence of iron [13, 21-23], and activates different modes of PCD, including apoptosis [13, 17, 21, 24] , necroptosis , and lysosomal pro-death signaling [13, 19, 21].
Recent studies have revealed that oncogenic KRas mutations reprogram tumor cells to states dependent on enhanced glucose  and glutamine metabolism , which are required to support the upregulated antioxidant capacity needed for tumor growth . Importantly, drug screening studies have recently uncovered that Ras transformation renders cells sensitive to a ROS-induced, non-apoptotic, iron-dependent mode of cell death [26, 27]. This mode of programmed necrosis, termed ferroptosis, is characterized by loss of redox homeostasis, increased lipid peroxidation, and inhibition by the small molecule ferrostatin-1 . Intriguingly, PDAC redox homeostasis is dependent on cystine uptake via the xc− transporter , which is a key participant in ferroptosis , suggesting an inherent sensitivity of PDAC to this iron-dependent mode of programmed necrosis.
Therefore, in the study presented here, we investigated the selectivity and mode of cell death activated by ART in PDAC cell lines. We report that ART induces an iron- and ROS-dependent cell killing and a block to clonogenicity in PDAC cell lines containing both wild-type and mutant KRas, but not control non-neoplastic HPDE cells. We report that co-treatment with either the ROS scavenger trolox, the inhibitor of ferroptosis, ferrostatin-1, or the iron chelator deferoxamine block ART cytotoxicity, while loading lysosomes with iron-saturated holo-transferrin enhances ferroptotic PDAC cell death. Moreover, our analysis of patient-derived mRNA expression data suggests that PDAC tumors in vivo can contain pathway adaptations that have been shown to sensitize Ras-transformed cells to ferroptosis. Overall, our findings suggest ART-mediated activation of the ferroptotic mode of necrotic cell death as a promising and highly effective pathway for killing PDAC cells.
ART induces iron-catalyzed, ROS-mediated PCD specifically in pancreatic cancer cells
We first measured levels of ART-induced cell death at 24 and 48 hours of treatment in PDAC cell lines expressing wild-type KRas (BxPC-3) or constitutively active KRasG12D (Panc-1) . HPDE pancreatic duct epithelial cells  were used as a non-neoplastic control cell line to assess PDAC specificity of ART-induced PCD. PDAC cells were treated under nutrient deprivation conditions  to mimic the metabolic stress of PDAC [33, 34], while non-neoplastic HPDE cells were treated in fully supplemented medium. ART (50 µM) induced significant cell death at 24 hours in all PDAC cell lines, increasing at 48 hours (Figure 1A). Co-addition of the lysosomal iron chelator deferoxamine mesylate (DFO; 0.1 mM)  fully blocked cell death, demonstrating iron-dependency of ART-induced cell death in PDAC cells. Conversely, increasing lysosomal free iron by co-treatment with iron-saturated, diferric holo-transferrin (HTF; 20 µg/ml) significantly increased Panc-1 cell death at 24 and 48 hours of treatment. Control pancreatic duct epithelial HPDE cells were insensitive to all conditions, indicating tumor cell-specificity of death induction.
Next, to determine ART effects on long-term cell survival and proliferation we performed colony formation assays  following 24 hours of drug treatments. Consistent with cell death results, ART reduced clonogenic growth of Panc-1 cells, and this proliferative arrest was amplified by co-treatment with HTF (Figure 1B). Importantly, DFO rescued clonogenic growth inhibition induced by ART (Figure 1C), further highlighting a central role for lysosomal iron in ART-mediated effects.
HTF is endocytosed and trafficked to lysosomes , and we previously demonstrated that ART targets endolysosomes to the perinuclear region . We therefore sought to determine if ART impacted HTF uptake in PDAC cells by measuring uptake of iron-loaded transferrin conjugated to Alexa Fluor 546 (HTF546, 5 µg/mL). In control cells, HTF546 entered cells and accumulated in endolysosomes distributed throughout the cytosol (Figure 1D). In cells treated with ART, HTF546 uptake was unaltered, as demonstrated by endolysosomal localization inside the cytosol. Moreover, within 6 hours HTF546-containing endolysosomes prominently formed clusters at perinuclear regions, consistent with previously demonstrated ART-induced perinuclear clustering of endolysosomes in breast cancer cells . This perinuclear accumulation of HTF546 was also observed following 24 hour pre-treatment with ART, further demonstrating that ART treatment does not impair the lysosomal uptake of HTF (Figure 1E).
Next, we determined whether PDAC cell death was dependent on ART-induced ROS generation [13, 17, 18], via imaging-coupled flow cytometry to measure ROS in parallel to cell death induction. At 24 hours ART/HTF treatment induced significant cell death (~60%), while ART alone did not induce significant levels of cell death (Figure 2A). Importantly, ROS generation by ART/HTF correlated with cell death, and the ROS scavenger trolox (TX; 0.5 mM)  significantly blocked cell death and reduced ROS levels (Figure 2B). Furthermore, TX rescued cell proliferative functions of ART-treated Panc-1 cells (Figure 2C). In contrast, treatment with TNF (43 ng/ml) and actinomycin D (ActD; 1 µg/ml), a combination known to induce apoptotic cell death in pancreatic cancer cells , resulted in TX-insensitive cell death (Figure 2D), demonstrating pathway specificity.
These results identify that ART specifically induces rapid ROS-mediated PDAC cell killing and long-term growth arrest, in a lysosomal iron-dependent manner.
ART induces a MOMP- and caspase-3 independent mode of cell death
We previously described that ART activated mitochondrial apoptosis in breast cancer cells . We therefore examined different parameters of mitochondrial outer membrane permeabilization (MOMP), and downstream caspase activation in PDAC cells. Consistent with findings in breast cancer cells, ART induced mitochondrial fragmentation in Panc-1 cells at 24 hours of treatment (Figure 3A, 3C, 3D). However, Panc-1 cells maintained mitochondrial membrane potential under ART treatment, as shown by maintained TMRM fluorescence (Figure 3A). Furthermore, in Panc-1 cells ART did not induce mitochondrial translocation of GFP-Bax (Figure 3B), and did not trigger cytochrome c (Figure 3C) or Smac release (Figure 3D), all markers for MOMP activation . Finally, use of a GFP-based caspase-3 activity sensor , which as expected reported TNF/ActD activation of caspase-3, demonstrated absence of caspase-3 activation by ART (Figure 3E). These findings demonstrate that, unlike breast cancer cells, Panc-1 cells resist ART-mediated activation of MOMP, and do not undergo neither caspase-dependent apoptosis, suggesting that in PDAC cells ART activates an alternative mode of PCD.
ART does not activate necroptosis, but activates ferroptosis in PDAC cells
ART was reported to activate necroptotic cell death in schwannoma cells . We thus tested whether treatment with necrostatin-1 (Nec-1, 20 µM), a RIPK1 inhibitor , would reduce ART-induced PDAC cell death. Nec-1 reduced, but did not fully block, ART killing at 48 hours (Figure 4A). Therefore, we treated cells with the potent, more specific inhibitor of necroptosis, necrostatin-1s (Nec-1s, 20 µM) . Nec-1s did not suppress cell death induction by ART (Figure 4A), suggesting that Nec-1 inhibition of ART-induced cell death was due to recently reported non-specific effects of the inhibitor , and evidencing that ART-induced Panc-1 cell death is non-necroptotic.
Interestingly, it was recently described that iron-dependent ROS production in Ras-transformed cells can activate programmed necrosis in the form of ferroptosis . We therefore treated cells with the ferroptosis-inhibitor ferrostatin-1 (Fer-1, 20 µM), which resulted in full suppression of PDAC cell death at 48 hours of ART and ART/HTF treatment (Figure 4B). To further explore the induction of ferroptosis by ART, we performed colony formation assays with Panc-1 cells, following treatment with ART, ART/Nec-1 or ART/Fer-1. Nec-1 did not increase clonogenic growth under ART treatment, while Fer-1 rescued cells from ART-induced block to proliferation (Figure 4C), further suggesting ART activation of ferroptotic cell death. The small molecule erastin specifically induces ferroptosis by blocking the xc- cystine/glutamate antiporter leading to glutathione depletion . We thus analyzed the ability of erastin to induce ferroptosis in Panc-1 cells, at 10, 50 and 100 µM erastin concentrations, in absence and presence of HTF. Notably, at 24 hours 10 µM erastin induced significant cell death only with the addition of HTF. 50 µM erastin induced significant cell death alone, and was further increased by HTF co-treatment. 100 µM erastin induced maximal cell death, without further increase by HTF co-treatment (Figure 4D). We then characterized erastin (50 µM)-induced cell death in Panc-1 cells at 48 hours. Co-treatment with Fer-1, TX or DFO blocked cell death (Figure 4E). Importantly, Nec-1, but not Nec-1s, blocked erastin-induced Panc-1 cell death. These findings further indicate that Nec-1 exerts non-specific activity during ferroptosis, but not apoptosis, as neither Nec-1, Nec-1s nor Fer-1 blocked TNF/ActD induced cell death (Figure 4F).
Ferroptosis was discovered as a pathway for killing cells transformed by mutationally-active Ras [26, 27]. Thus, we next compared HTF/ART-induced cell death and impact of Fer-1 in wild-type KRas (COLO357 and BxPC-3) and KRasG12D mutant (AsPC-1) PDAC cell lines [31, 45] (Figure 5). COLO357 cells were overall less responsive to HTF/ART. Cell death was significantly induced in BxPC-3 (WT KRas) at 48 hours by HTF/ART and blocked by Fer-1. AsPC-1, which express KRasG12D were most responsive to HTF/ART treatment, and Fer-1 blocked cell death fully, at all measured time-points. Notably, at 24 hours, ART alone induced significant cell death weakly in BxPC-3 and more potently in AsPC-1 cells. HTF enhanced killing only in KRasG12D mutant AsPC-1 cells. The necroptosis inhibitor Nec-1s had no impact on cell death under any conditions.
Overall, these findings demonstrate that erastin and ART activate ferroptosis in PDAC cell lines in an iron- and ROS-dependent manner, and that ART-induced ferroptosis is most efficient in mutationally-active KRas expressing PDAC cell lines while Fer-1 block of cell death is independent from KRas mutation status.
ROS signaling and lipid peroxidation during ART-induced ferroptosis
We next sought to characterize ferroptosis signaling in ART-treated Panc-1 cells. Iron-dependent ROS generation during ferroptosis is the central stressor for cellular damage and death . Thus, we determined the impact of increased ROS by measuring the Nrf2-mediated antioxidant response . Western blot analysis revealed that HO-1 expression increased in response to ART and ART/HTF (Figure 6A), indicating activation of ROS-mediated signaling pathways. To determine whether, similar to TX, Fer-1 blocks ferroptosis through ROS scavenging, we measured ROS generation in parallel to cell death in Panc-1 cells treated with ART/HTF without or with Fer-1. Surprisingly, imaging-coupled flow cytometry results indicated that Fer-1 blocked ART-induced loss of cell survival without blocking ART-induced ROS generation (Figure 6B).
We therefore asked if Fer-1 might act via blocking of localized ROS production in ART-treated Panc-1 cells, as Fer-1 was shown to inhibit lipid peroxidation during ferroptotic cell death [28, 47, 48]. Lipid peroxidation was measured using BODIPY C11 (581/591), a specific sensor for intracellular lipid peroxidation which undergoes a shift in fluorescence emission from red to green upon oxidization . Panc-1 cells were treated for 24 hours with ART alone or in combination with TX or Fer-1 and then incubated with BODIPY C11 (581/591). Quantitative, single-cell analysis revealed a shift from non-oxidized to oxidized BODIPY C11 (581/591) in response to ART, evidencing increased lipid peroxidation (Figure 6C). Both TX and Fer-1 significantly reduced lipid peroxidation induced by ART.
Characterization of PDAC in vivo potential for ferroptosis
While the above findings confirm that PDAC cell lines are insensitive to apoptosis, we here demonstrate that PDAC cells appear sensitized to ferroptotic cell death, induced by either ART/HTF or erastin treatments. We thus sought to determine whether cell culture-based understanding of factors contributing to apoptosis resistance and ferroptosis sensitivity are present in PDAC patient mRNA expression profiles. To that end, we analyzed the Badea dataset, which compares mRNA expression of 36 patient-matched tumor and normal pancreatic tissues samples .Iron and oxidative response
Gene expression analysis revealed altered iron (Figure 7A) and ROS/glutathione (Figure 7B) homeostasis in patient PDAC tissues. In cell lines, Ras transformation results in increased levels of transferrin receptor (TFRC) and decreased levels of ferritin components . TFRC, imports transferrin, and ferritin is responsible for the storage of intracellular iron, and serves as an important anti-oxidant . Consistent with these findings, in the patient PDAC tissues, expression of TFRC is increased, while expression of transferrin (TF) and ferritin light chain (FTL) is decreased (Figure 7A). Glutathione peroxidase 4 (GPX4) is an inhibitor of ferroptosis that is dependent on GSH levels and high levels confer resistance to ferroptosis activation . In the Badea dataset, the expression of GPX4, as well as other antioxidant enzymes are increased (Figure 7B), consistent with increased dependency on anti-oxidant system in PDAC . Apoptosis resistance
Similarly, clustering apoptosis pathway gene sets of normal and tumor samples demonstrated a global apoptosis de-regulation in PDAC (Figure 7C-7D). Notably, TNFR and FAS death receptors are up-regulated in PDAC samples suggesting a pro-tumorigenic function (Figure 7C). This is consistent with the findings that TNFR expression promotes inflammation , and increased CD95 expression is responsible for PDAC metastasis . Alterations in the mitochondrial pathway were also observed. For example, anti-apoptotic Bcl2 members MCL-1 expression was significantly increased, while Bcl-xL had unchanged expression in PDAC patients (Figure 7D). Ferroptotic genes
Finally, we analyzed a set of six genes shown to be required for ferroptotic death , RPL8 (ribosomal protein L8), ATP5G3 (ATP synthase F0 complex subunit C3), IREB2 (iron response element binding protein 2), CS (citrate synthase), ACSF2 (acyl-CoA synthetase family member 2), and EMC2/TTC35 (ER Membrane Protein Complex Subunit 2). While IREB2, CS, ACSF2, and EMC2 showed no significant differences between normal and tumor tissues, RPL8 and ATP5G3 were significantly reduced in tumor tissues, due to patient heterogeneity. These findings suggest that patient profiling may be useful to suggest sensitivity to ferroptotic treatment strategies.
Previously it was shown that ART activates ROS generation [13, 21-23], and lysosomal pro-death signaling [13, 19, 21], resulting in downstream activation of apoptosis [13, 17, 24] or necroptosis  pathways, in a cancer type-dependent manner. In this study we report that in PDAC cells, ART activates a form of cell death that is distinct from canonical, caspase-mediated apoptosis, and necroptosis. Instead, ART activates an iron- and ROS-dependent form of programmed necrosis, known as ferroptosis , with most effective ART-mediated death induction in PDAC cells expressing mutationally-active KRas.
The ferroptotic mode of programmed necrosis was recently discovered as an apoptosis-independent form of cell death in Ras-transformed cells [26, 27]. Ferroptosis is characterized by increased levels of lipid peroxidation, which can be caused by compound-mediated inhibition of the lipid peroxidase GPX4, via glutathione (GSH) depletion or through direct inhibition . Here we show that the recently characterized ferroptosis-inducer erastin, which inhibits the cystine/glutamate antiporter system xc− , activated ferroptosis also in Panc-1 cells, demonstrating the sensitivity of PDAC cells to ferroptotic cell death. This finding is consistent with the reported dependency of PDAC on system xc−  in order to maintain redox homeostasis.
While mitochondrial apoptosis is critical for efficient chemotherapy induction of PCD in many cancer types , PDAC cells are highly resistant to apoptosis initiation and execution , and killing of PDAC cells represents an ongoing challenge in PCD research. Thus, the here described sensitivity of PDAC cancer cells to ferroptosis suggests an alternative pathway to selectively kill pancreatic cancer cells, especially considering that mutationally-active KRas mutations drive the majority of PDAC [7, 53, 54]. Importantly, we found that transferrin co-treatment increased ferroptotic cell death induced by both ART and erastin. Moreover, transferrin increased ART-mediated cell death to highest levels in Panc-1 and AsPC-1 PDAC cells, which have constitutively active KRas mutations , but did not alter the cell death response in BxPC-3 or COLO357 cells, which express wild type KRas [31, 45]. Indeed, iron-dependent killing of Ras-transformed cells offers a simple explanation for treatment specificity. Transferrin receptors are increased in PDAC patient tumor tissues [55, 56], and our analysis of the Badea dataset demonstrates TFRC up-regulation and down-regulation of ferritin in PDAC patients, recapitulating metabolic reprogramming by Ras which sensitizes transformed cells to ferroptosis . Therefore, our cell culture findings suggest that, while PDAC cells are insensitive to apoptotic and necroptotic signaling, KRas mutation may render PDAC cells pre-sensitized to iron-dependent ROS-induction followed by ferroptotic cell death. Furthermore, our analysis of the Badea dataset not only indicates the high resistance of PDAC to apoptosis induction in vivo, but also a high degree of patient heterogeneity. It is possible, that certain patients may be more sensitized to induction of ferroptotic PDAC cell death.
At present, the only clinically-approved inducer of ferroptosis is the Raf kinase inhibitor sorafenib [57, 58], whose effectiveness in ferroptosis induction is limited by specific concentration ranges . ART is well tolerated in malaria patients and pharmacokinetics have been characterized [15, 16]. Based on cell culture findings and patient-derived mRNA expression data, both indicating altered iron handling and antioxidant capacity in PDAC, we propose ART as a candidate for in vivo ferroptosis induction for targeted killing of PDAC cells.
MATERIALS AND METHODS
Cell culture reagents were obtained from Invitrogen, Sigma, Lonza, and Pan Biotech. Electron microscopy-grade paraformaldehyde was obtained from EMS. Complete EDTA-free protease inhibitor and PhosSTOP phosphatase inhibitor cocktails were purchased from Roche. Alexa Fluor 546 Human Transferrin, tetramethylrhodamine methyl ester and 2’,7’-dichlorodihydrofluorescein diacetate were obtained from Invitrogen. Artesunate, holo-transferrin, ferrostatin-1, erastin and puromycin were purchased from Sigma. Trolox and actinomycin D were obtained from Calbiochem. Deferoxamine mesylate was purchased from EMD Bioscience. Necrostatin-1 was purchased from Santa Cruz Biotechnology. Necrostatin-1s was obtained from BioVision. TNF was a kind gift from BASF (Mannheim, Germany).
Human pancreatic adenocarcinoma cell lines Panc-1, COLO357, AsPC-1 and BxPC-3 (obtained from the Department of General Surgery, University of Heidelberg, Germany), and the human embryonic kidney 293T cell line were maintained in DMEM supplemented with 10% FBS, L-glutamine, non-essential amino acids and penicillin/streptomycin/amphotericin B. The human pancreatic duct epithelial HPDE cell line  was maintained in KGM medium supplemented with bovine pituitary extract, hEGF, insulin, hydrocortisone, gentamicin and amphotericin B (Lonza). Fully supplemented media are referred to as full medium (FM).
Treatments of PDAC cell lines with artesunate (50 µM), holo-transferrin (20 µg/ml), erastin (10-100 µM), TNF (43 ng/ml) and actinomycin D (1 µg/ml), ferrostatin-1 (20 µM), necrostatin-1 (20 µM), necrostatin-1s (20 µM), deferoxamine mesylate (0.1 mM), and trolox (0.5 mM) were performed in glucose-containing Hank’s Balanced Salt Solution (in mM: 1.3 CaCl2, 0.5 MgCl2, 0.4 MgSO4, 5.3 KCl, 0.4 KH2 PO4, 4.2 NaHCO3, 137.9 NaCl, 0.3 Na2 HPO4, 5.6 D-glucose) to mimic the metabolically challenged conditions found in PDAC [33, 34]. Drug treatments of non-neoplastic HPDE cells were performed in full medium.
Lentivirus-mediated gene transfer
For lentiviral gene transfer, a pCDH-puro-CMV lentiviral vector carrying the super folding (sf) GFP-tagged caspase-3 sensor (GC3A1), pCDH-CMV-GC3AI , was transfected into 293T cells together with pCMVdeltaR8.91 (packaging vector) and pMD2.G (VSV-G envelope protein expression vector) using calcium-phosphate transfection. Cells were infected with virus particle-containing supernatants at 50% confluency, and selected and maintained with puromycin (1 µg/mL). For experiments, cells were plated in puromycin-free medium.
Colony formation assay
75,000 cells per well were seeded in 24-well plates and treated with the indicated drug combinations for a time period of 24 hours. Detached, dead cells were removed and after trypsinization, 300 cells per well were seeded into new 12-well plates and grown in full medium for 11 days to allow formation of colonies. Colony formation was inspected by widefield microscopy prior to fixation and staining with 1% (w/v) crystal violet in 25% MeOH for 20 minutes. Images were acquired using a Canon EOS 600D DSLR camera and colonies containing more than 50 cells were scored using the segmentation editor of Fiji software (http://fiji.sc/Fiji).
High-resolution fluorescence microscopy
Widefield fluorescence microscopy was performed with a DeltaVision RT microscope system (Applied Precision) using a 60x objective. Cells were plated in 8-well microscopy µ-slides (iBidi), treated as indicated and subjected to either live-cell imaging or fixed with 4% paraformaldelhyde in PBS. For live-cell imaging, cells were stained with tetramethylrhodamine methyl ester (TMRM, 50 nM) for 20 minutes at 37°C or with BODIPY C11 (581/591) (0.5 mM) for 30 minutes at 37°C. Holo-transferrin uptake was monitored in live cells stained with Alexa Fluor 546 Human Transferrin (HTF546, 5 µg/ml) for the indicated amount of time. For immunofluorescence, fixed cells were permeabilized with 0.3% Triton-X in PBS, blocked with 3% BSA and incubated with antibodies against cytochrome c (BD Bioscience, no. 556432) or SMAC (Santa Cruz Biotechnology, no. sc-22766) at room temperature for 2 hours. Fluorescent staining was performed for 1 hour at room temperature using highly cross-absorbed Alexa Fluor 488 or Alexa Fluor 546 secondary antibodies (Invitrogen). Images of representative cells were captured using the Z-axis scan function. Acquired images were deconvolved (Softworx, Applied Precision). Image analysis and preparation was performed using ImageJ (rsbweb.nih.gov/ij/) and Fiji (http://fiji.sc/Fiji). Representative images shown are total intensity projections of 5 µm thick Z-axis scans. For detection of lipid peroxidation, mean green intensity (oxidized BODIPY C11 (581/591)) was divided by mean red intensity (reduced BODIPY C11(581/591)) per cell.
Imaging-coupled flow cytometry
To assess cell death in parallel to ROS levels, Panc-1 cells were treated as indicated, and incubated with propidium iodide (PI, 0.5 µg/ml) and 2’,7’-dichlorodihydrofluorescein diacetate (H2 DCFDA, 2 μM) for 1 hour at 37°C. Cells were then trypsinized and analyzed by imaging-coupled flow cytometry using the Imagestream X (Amnis). DCF and PI were simultaneously excited using the 488 nm and 546 nm lasers, respectively. Image analysis was performed using IDEAS 4.0 (Amnis). Briefly, single, in-focus cells were selected yielding 1000-2000 cells per condition for analysis. The percentage of PI-negative cells (survival) and the mean DCF values of PI-negative cells are reported.
Fluorescence plate reader cell death assay
20,000 cells were seeded per well in 96-well plates and on the following day treated with the indicated drugs. At 24 and 48 hours, cells were stained with the cell exclusion dyes Yo-Pro-1 iodide 491/509 (0.1 µM) or propidium iodide (PI, 1 µg/ml) for 30 minutes at 37°C. Fluorescence read-out was performed using a Tecan Infinite M200 plate reader (Tecan) at 488 nm for Yo-Pro-1 stained cells or at 546 nm for PI stained cells. Cell death is presented as fold changes in Yo-Pro-1 or PI fluorescence intensity normalized to control conditions. To substract background, acquired intensities from non-stained wells were subtracted from stained wells prior to normalization:
, ITreat, (Intensity of stained, treated cells; ICon, Intensity of stained, control cells; IBack, Intensity of non-stained control cells).
600,000 cells per well of a 6-well plate were plated and on the following day subjected to the indicated drug treatments. At 24 hours whole cell lysates were prepared using RIPA lysis buffer containing protease and phosphatase inhibitors. Dosed protein samples were electrophoresed using Bis-Tris NuPAGE gels (Invitrogen) and transferred to nitrocellulose using the iBlot dry blotting system (Invitrogen). Subsequently, membranes were blocked and incubated with antibodies against GAPDH (Santa Cruz Biotechnology, no. sc-25778) and HO-1 (Cell Signaling Technology, no. 5853S). HRP-conjugated secondary antibodies (GeneTex, GTX213110-01) were used for digital chemiluminescence detection. Blots shown are representative of three independent experiments. Densitometric band quantifications were performed using ImageJ (http://rsbweb.nih.gov/ij/). Briefly, the integrated intensities of target protein bands were measured and normalized to the integrated intensity of GAPDH loading control under the same condition.
The probability of statistically significant increases or decreases between conditions of at least three independent experiments was determined using the Student’s t-test. One-tailed paired t-tests were performed to test treatment versus control (*) while two-tailed, paired t-tests were performed to test co-treatment versus ART (#) or ART/HTF (§). Values are expressed for bar graphs and line graphs as mean ± SEM. Single cell data is presented as dot plot with mean ± SEM. Statistical significances and number of measurements are indicated in figure legends.
Gene set analysis
Gene set analysis was performed using R2 platform (r2.amc.nl) on the dataset from Badea et al. . Tumor samples are indicated by green boxes while normal tissue samples are presented as red boxes. Differential expression is calculated based on the zscore showing an up-regulation (red) and down-regulation (green) clustered in heatmaps.
We gratefully acknowledge M-S Tsao (University of Toronto) for providing HPDE cells and B Li (Tianjin Medical University) for providing pCDH-CMV-GC3AI. This work was supported by the German Cancer Research Center (DKFZ), through SBCancer within the Helmholtz Alliance on Systems Biology funded by the Initiative and Networking Fund of the Helmholtz Association (NRB); and the e:Bio grant #0316191 (LysoSys) of the Federal Ministry of Education and Research (BMBF), Germany (AH-B). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
CONFLICTS OF INTEREST
The authors declare no conflict of interest.
N.E. performed experiments, analyzed data and prepared figures. L.R. and J.H. contributed to assay development and experiments. A.H.-B. and N.R.B. conceived the study, performed experiments and analyzed data. N.E., A.H.-B. and N.R.B. wrote the manuscript.
ActD, Actinomycin D; ART, Artesunate; DFO, Deferoxamine; Fer-1, Ferrostatin-1; HTF, Holo-Transferrin; Nec-1, Necrostatin-1; Nec-1s, Necrostatin-1s; PDAC, pancreatic ductal adenocarcinoma; PCD, programmed cell death; TX, Trolox; TNF, Tumor Necrosis Factor
Last Modified: 2016-06-03 19:28:01 EDT