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We have previously shown that doxorubicin sensitizes prostate cancer cells to TNF-Related Apoptosis Inducing Ligand (TRAIL). Sensitization correlated with decreased expression of the anti-apoptotic protein cFLIPS. The decrease in cFLIPS could not be explained by transcriptional regulation or increased degradation, leading us to focus on translational mechanisms. In this study, we found that doxorubicin caused strong and sustained phosphorylation of elongation factor 2 (EF-2), which interferes with protein elongation. Phosphorylation of EF-2 appeared to occur in a kinase-independent manner. Treatment with hydrogen peroxide recapitulated the events observed after doxorubicin treatment. In addition, cells treated with hydrogen peroxide expressed less XIAP and survivin which, like cFLIPS, are short half-life proteins with an anti-apoptotic function while expression levels of DR5, caspases-8, -9, -3, and Bax are maintained. The doxorubicin-mediated decrease in cFLIPS and XIAP as well as TRAIL-induced apoptosis was prevented by pretreatment with an iron chelator, indicating that expression of these proteins was affected by free radical generation upon interaction of iron with doxorubicin. In conclusion, our data suggest that free radicals can affect the phosphorylation of EF-2 resulting in a net loss of short half-life proteins such as cFLIPS and XIAP, leaving a cell more vulnerable to apoptotic stimuli.
Doxorubicin (brand named Adriamycin) has been a staple of chemotherapy for decades. Cancer patients who receive doxorubicin treatment can expect multiple side effects which may include hair loss, anemia, nausea, reduced immunity, and general fatigue . In severe cases, doxorubicin side effects may include cardiac toxicity [2, 3]. The mechanism of doxorubicin action has been linked to DNA damage, topoisomerase inhibition, and iron sequestration with subsequent free radical generation [4–7]. Although the DNA damaging aspects of doxorubicin are the most widely accepted explanation of the drug’s effects, both therapeutic and detrimental, the free radical hypothesis has been revisited recently by several groups. When doxorubicin is administered it binds to cellular iron, generating free radicals including hydrogen peroxide through Fenton chemistry . These free radicals are believed to directly degrade the anti-apoptotic protein cFLIP, rendering the treated cells more vulnerable to apoptosis . This free radical mechanism hypothesis is summarized in Figure 1.
cFLIP is a caspase-8 homolog and has as many as 11 splice variants . Two variants have been well characterized, called cFLIPL and cFLIPS based on the length of the mRNA and protein product. Previously, we have described a link between doxorubicin treatment and the downregulation of the short isoform of cFLIP . cFLIPS is enzymatically inactive and binds to caspase-8 preventing homo-dimer formation and the autocatalytic cleavage step required for caspase activation . By inhibiting the activation of caspase 8, FLIPS plays an important role in preventing death-ligand induced apoptosis.
We have previously demonstrated that upon doxorubicin treatment, prostate carcinoma cells which are resistant to the death ligand TNF Related Apoptosis Inducing Ligand (TRAIL) become TRAIL-sensitive, which correlated with a decrease in cFLIPS levels . In addition, PC3 cells can be sensitized with simple downregulation of cFLIPS through siRNA, suggesting that the myriad other actions of doxorubicin may be superfluous to this sensitization process . Identifying this key protein change, we wished to determine how doxorubicin was accomplishing the downregulation of cFLIPS.
The regulation of cFLIPS by doxorubicin does not appear to be mediated at the levels of transcription or proteasomal degradation . Therefore, in this study we examined the possibility of translational control of cFLIPS. Protein translation consists of several discrete steps, each mediated by a set of specific translation factors. The initiation step of translation involves loading ribosomes with mRNA and the complexing of these loaded ribosomes into aggregates known as polysomes . The elongation step of translation follows the ribosomal loading and is mediated by Elongation Factor 2 (EF-2), which moves the mRNA forward through the ribosome from codon to codon as the nascent protein grows. EF-2 activity is largely determined by its phosphorylation status; phosphorylation deactivates the enzyme and is typically controlled by a dedicated kinase (EF-2 kinase) . However, EF-2 is also vulnerable to oxidative phosphorylation via free radical activity .
Normally, phosphorylation of EF-2 occurs when the cell is resource starved or when the cell is undergoing mitosis [17, 18]. The resulting decrease in protein synthesis is an important mechanism that allows the cell to conserve energy or direct energy to other cellular functions. Recent research has demonstrated that free radical treatments, which would presumably force a phosphorylation state of EF-2, result in a significant G2/M phase arrest . Interestingly, doxorubicin treatment also results in a G2/M phase arrest . This correlation suggests that free radical production by doxorubicin may play a role in causing a G2/M arrest although the effect has long been thought to result from doxorubicin-induced DNA damage .
In this study, we demonstrate that free radical generation is sufficient to explain doxorubicin-mediated sensitization to TRAIL. We have expanded the current model of doxorubicin-mediated events to include translational regulation and discuss the possible clinical ramifications of the data.
The human prostate cancer cell line PC3 was purchased from ATCC and maintained in RPMI 1640 media supplemented with 10% FBS and antibiotic/antimycotic from Gibco, Grand Island, NY, at 37°C with 5% CO2. Doxorubicin, Desferoxamine (DFO) and hydrogen peroxide were obtained from the MUSC pharmacy. KillerTRAIL was purchased from Axxora, San Diego CA.
After overnight plating, PC3 cells were treated with increasing concentrations of doxorubicin or 10 μg/ml cycloheximide (as a positive control) for 4–24 hours as indicated in Figure 2. Cells were incubated in methionine-deficient RPMI1640 containing 10% FBS one hour prior to adding 50 μCi of L-[35S]-Methionine (in vivo cell labeling grade) (Amersham, Piscataway, NJ). After a 2 hours pulse, the medium was removed, cells rinsed with PBS and protein prepared in RIPA buffer (1% NP-40, 0.1% SDS and 0.5% deoxycholate in PBS) containing freshly added protease inhibitors (P8340, Sigma, St. Louis, MO). To separate unreacted amino acid from protein products, 10 μl lysate was spotted on Whatman 3mm paper for TCA precipitation. TCA-precipitated 35S-labeled protein was quantitated by scintillation counting. All assays were performed in duplicate.
PC3 cells were left untreated or treated with 250 ng/ml doxorubicin for 20 hours and then rinsed three times on ice with ice-cold phosphate-buffered saline to which 100 μg/ml cycloheximide was added to arrest polypeptide chain elongation. Cells were scraped from the plates in 10 ml of phosphate-buffered saline/cycloheximide, pelleted by centrifugation, and resuspended in 1 ml of resuspension buffer (10 mM Tris, pH 7.5, 250 mM KCl, 2 mM MgCl2, 0.5% (v/v) Triton X-100). The resuspended cells were homogenized with 18 strokes of a glass A pestle Dounce homogenizer and transferred to a chilled 1.5-ml microtube. 150 μl of a solution containing 10% (v/v) Tween 80, 5% (w/v) deoxycholate was added, and the homogenate was vortexed and incubated on ice for 15 min. The lysates were then layered on a 15–50% sucrose gradient containing 200mM Tris (pH 7.5), 2.5M KCl, and 100mM MgCl2, and ultracentrifuged at 35000 RPM for 100 minutes at 4°C. Traces were obtained by running the gradients through an ISCO fractionator with upward displacement, set to continuously monitor at 254 nm. Polysome data shown is representative of two independent experiments.
PC3 cells were plated 5 × 105 per well in 6 well plates for all experiments with the exception of the TRAIL toxicity experiment (Figure 6) in which cells were plated 1.5 × 105. After 24 hours, media was changed and cells were treated as indicated. Following treatment, cells were scraped into media and centrifuged at 1500 rpm for 5 minutes at 4°C. Supernatant was discarded and protein was prepared in RIPA buffer containing freshly added mammalian protease and phosphatase inhibitor cocktails (P8340, P2850, P5726, Sigma, St. Louis, MO). Lysates were then centrifuged for 20 minutes at 13,000 rpm at 4°C and supernatants for western blot analysis stored at −20°C. Protein was separated on 4–12% Bis/Tris NuPage gels in MES buffer, transferred to nitrocellulose for 90 minutes at 30 V and blocked in 5% milk. Sources of antibodies were as follows: Antibodies against cleaved PARP, Bax, XIAP, Survivin, EF-2, phospho-EF-2, and EF-2 kinase were purchased from Cell Signaling Technologies, Danvers, MA. The NF-6 hybridoma supernatant against FLIP was generously provided by Dr. Marcus Peter, University of Chicago. Antibodies against DR5, caspase-8 and caspase-3 were purchased from Axxora, San Diego, CA. Anti-actin was purchased from Sigma. After blocking, membranes were probed with primary antibody overnight at 4°C (1;1000 or 1:2000 in TBS-Tween with 5% milk), except NF-6, which was used at room temperature at 1:5 in TBS-Tween without milk. Following three washes with TBS-Tween, membranes were incubated with the anti-mouse (1:5000) or anti-rabbit (1:50000) HRP-conjugated secondary antibodies (SantaCruz Biotechnologies, Santa Cruz, CA) for 1 hour at room temperature in TBS-Tween with 5% milk. Membranes were washed three times in TBS-Tween followed by chemiluminescent detection of the secondary conjugates with DuraWest Supersignal (Pierce, Rockford, IL). In some cases membranes were stripped with Re-Blot mild solution (Chemicon, Temecula, CA) and reprobed. All Western blot data shown is representative of at least three independent experiments.
PC3 cells were plated in triplicate at 1 × 104/well in a 96 well plate. Cells were left untreated, treated with 100 ng/ml TRAIL, treated with 25 μM hydrogen peroxide, or a combination of both. Caspase activity was determined at 4 hours using the Apo-ONE homogeneous Caspase-3/7 assay (Promega, Madison WI) according to manufacturer’s instructions. The fluorescence readings were taken on a FluostarOptima plate reader with 485nm excitation and 530nm emission wavelengths (BMG technologies, Durham, NC). Background fluorescence was determined by incubating media with substrate alone and subtracting these values from wells containing cells. Percent increase was determined by dividing the fluorescence intensity from TRAIL treated samples by their respective control either media or hydrogen peroxide alone.
PC3 cells were plated at 3 ×105/well in 6-well plates. Cells were serum starved for 60 hours and then treated with 250 ng/ml doxorubicin or 25 μM hydrogen peroxide in normal growth media. After two hours of treatment, normal growth media replaced the treatment media. The cells were harvested after 24 hours for cell cycle analysis by incubating the cells with Cell Stripper (Mediatech, Inc, Herndon, VA) at 37°C for 5–10 minutes. Cells were then transferred to a 15 ml conical tube containing their spent media and any non-adherent cells and centrifuged at 4°C and 1500 rpm for 5 minutes. Supernatant was discarded and the cells resuspended in 100 μL PBS. 2 mL ice-cold 70% ethanol was added drop-wise to each sample while vortexing and the samples were incubated at 4°C for one hour. Cells were then repelleted and washed with PBS twice. The pellets were resuspended in 100 μL of PBS followed by addition of 100 μL of RNAase (1 mg/mL) and 200 μL of propidium iodide (0.1 mg/ml). Samples were incubated in the dark for 30 minutes before quantification on a FACalibur (Beckton Dickinson, Bedford, MA) in the MUSC flow cytometry core facility. A minimum of 10,000 events was scored for each sample. Data were analyzed with the CellQuest software.
Our previous study indicated that a doxorubicin dose as low as 250 ng/ml could effectively downregulate cFLIPS but that the effect is not mediated by transcriptional control or by ubiquitination . Therefore, we next investigated translational control. To assess the effect of doxorubicin on protein synthesis, we initially performed S35-methionine incorporation assays. As shown in Figure 2A, unlike our positive control cycloheximide, which nearly completely inhibited incorporation of the radiolabel by four hours, a high dose of doxorubicin (1000 ng/ml) did not globally affect incorporation of 35S-methionine at four or seven hour time points. However, within 24 hours doxorubicin suppressed 35S-methionine incorporation to a similar extent as cycloheximide. Based on morphological analysis and our earlier data demonstrating that exposure of PC3 cells to doxorubicin does not induce apoptosis nor significantly affect viability within 24 hours, reduced incorporation of 35S-methionine was attributed to inhibition of protein synthesis rather than cell death [22, 23]. The lack of doxorubicin-mediated inhibition of 35S-methionine incorporation at the earlier time points suggests that protein synthesis may be affected indirectly as a consequence of other cellular events. A dose response curve demonstrates that 250 ng/ml doxorubicin reduces incorporation of 35S-methione by about half within 20 hours of treatment (Figure 2B). These experiments confirm that treatment of PC3 cells with doxorubicin results in global downregulation of protein synthesis in a dose and time-dependent manner. We hypothesized that cFLIPS, a protein with a reported half-life of about 40 minutes , would disappear quickly, giving the impression that it had been preferentially downregulated, when in fact it was merely an early indication of a systemic change. Therefore, we changed the focus of our investigation from cFLIPS-specific translational control to global translational control.
To examine initiation of translation, PC3 cells treated with 250 ng/ml doxorubicin or left untreated for 20 hours were harvested and spun through a sucrose gradient for polysome profile analysis. A loss of polysome formation was expected if doxorubicin negatively affected initiation of translation. However, as shown in Figure 3A, traces obtained from polysome analysis of untreated and doxorubicin treated samples were similar, indicating that doxorubicin treatment does not result in loss of polysome formation. Therefore, we chose to focus next on translation elongation.
In order to investigate the possible effect of doxorubicin on elongation we probed doxorubicin-treated lysates for phosphorylation of EF-2. As shown in Figure 3B, EF-2 was strongly phosphorylated 16 hours after initiation of doxorubicin treatment and remained phosphorylated until 24 hours. We also investigated the effect of doxorubicin on EF-2 kinase, the enzyme responsible for phosphorylation of EF-2. As shown in Figure 3B, the levels of EF-2 kinase are in fact downregulated at the same time that phosphorylation of EF-2 is strongest. EF-2 kinase has a half-life of six hours and expression levels may therefore be quickly affected by inhibition of translation . These data suggested that a kinase-independent mechanism might explain the continued and increased EF-2 phosphorylation induced by doxorubicin.
Oxidative phosphorylation does not require the action of a kinase and free radicals have been shown to phosphorylate EF-2 at relatively high doses . We show here that the free radical source hydrogen peroxide can both phosphorylate EF-2 and downregulate cFLIPS in PC3 cells (Figure 4A). The hydrogen peroxide dose curve indicates that at doses as low as 25 μM, the protein profile of doxorubicin treatment is recapitulated. This profile, as we have shown in previous work  and in Figure 3B, is characterized by a reduction in cFLIPS, preservation of cFLIPL and strong phosphorylation of EF-2. We therefore hypothesized that hydrogen peroxide could, like doxorubicin, sensitize PC3 cells to TRAIL. As shown in Figure 4B, microscopic analysis of PC3 cells reveals that combined treatment with hydrogen peroxide and TRAIL results in apoptotic morphology and loss of cells. The apoptotic nature of cell death was confirmed in a caspase-3/7 activity assay. The TRAIL-induced increase in caspase-3/7 activity was nearly three times higher in cells that were co-treated with hydrogen peroxide (Fig. 4C).
Doxorubicin treatment results in numerous cellular responses including G2/M arrest and free radical generation [27, 28]. We wished to perform a direct comparison of the effect of 25 μM hydrogen peroxide or 250 ng/ml doxorubicin on cell cycle distribution in order to examine the possible contribution of free radicals to G2/M arrest seen upon doxorubicin treatment. As shown in Figure 4D, after 24 hours of treatment, cells treated with doxorubicin are almost fully arrested in G2/M. Cells treated with hydrogen peroxide have a 60% increase in G2/M and are trending strongly away from G1 phase (Figure 4D).
We have shown that treatment with hydrogen peroxide results in phosphorylation of EF-2, decreased levels of cFLIPS and sensitization to TRAIL. Therefore, we wished to determine the effect of hydrogen peroxide treatment on other proteins in the apoptotic pathway. Because several anti-apoptotic proteins have extremely short half-lives, we predicted their expression to decrease upon hydrogen peroxide-induced EF-2 phosphorylation. In contrast, we predicted that pro-apoptotic proteins would be spared due to their typically longer half-lives [29–32]. The TRAIL-induced apoptotic pathway involves several steps including ligand-receptor binding, activation of the initiator caspase-8, Bax oligomerization at the mitochondria, and subsequent apoptosome formation involving activation of caspases-9 and 3. Antagonists of this pathway include cFLIP (caspase-8 inhibition), Bcl-2 (inhibition of Bax oligomerization), XIAP (inhibition of caspases-9 and –3) and survivin (inhibition of caspase-3).
As expected, following treatment with hydrogen peroxide, the protein machinery for apoptosis, including the TRAIL receptor DR5, caspases-8, -9, and -3, and Bax, was preserved (Fig 5A). The anti-apoptotic counterparts of these proteins, however, did not maintain their basal levels upon EF-2 phosphorylation in response to hydrogen peroxide. In addition to cFLIPS, XIAP (half-life of 120 minutes) and survivin (half-life of 30 minutes) disappeared from cells upon treatment [33, 34] (Figure 5a). Bcl-2 and Mcl-1, which antagonize apoptotic proteins at the mitochondrial level, were below detection limits in these cells (data not shown). Thus, caspases in hydrogen peroxide treated PC3 cells are essentially unopposed.
We next directly tested the idea that doxorubicin downregulates short half-life proteins through free radicals formation following association with intracellular iron (as shown in Figure 1). We pre-treated PC3 cells with increasing doses of the iron chelator desferoxamine (DFO) for two hours before treating with 250 ng/ml doxorubicin for 24 hours. Figure 5B shows the dose-dependent rescue of the anti-apoptotic proteins cFLIPS and XIAP from doxorubicin-induced downregulation.
We further pursued the observation that DFO pretreatment protects against the doxorubicin-mediated downregulation of FLIPs and XIAP by testing the TRAIL vulnerability of PC3 cells treated with both DFO and doxorubicin. We have shown previously that doxorubicin pretreatment sensitizes cells to TRAIL (11) and predicted that pretreatment with DFO would have a protective effect due to preservation of anti-apoptotic proteins. To test this hypothesis, cells were pretreated with DFO for three hours, cultured in the presence of doxorubicin for an additional 16 hours and then exposed to TRAIL for 2 hours. As shown in Fig. 6A, DFO pretreatment strongly inhibited the apoptotic response to doxorubicin and TRAIL. Analysis of protein lysates revealed that after only two hours of TRAIL treatment, the doxorubicin treated cells already showed strong cleavage of caspase-8, caspase-3, and PARP. DFO exerted a protective effect on cleavage of these proteins. Importantly, we also confirmed that phosphorylation of EF2 was reduced when an iron chelator precludes doxorubicin interaction with endogenous iron, supporting the hypothesis that protein translation machinery plays an important role in determining the response of a cell to TRAIL by modulating the expression of anti-apoptotic proteins.
We show that doxorubicin treatment of PC3 carcinoma cells halts protein translation and that this effect does not occur at initiation but elongation of translation and is mediated by phosphorylation of EF-2. The effect of doxorubicin on EF-2 phosphorylation, loss of cFLIPS and enhanced sensitivity to TRAIL was recapitulated by treatment with hydrogen peroxide. Cell cycle distribution in hydrogen peroxide treated cells also trended towards G2/M arrest. Free radical generation did not only result in reduced levels of cFLIPS but also in the loss of XIAP and survivin, which like cFLIPS have short half-lives and function as antagonists in the apoptotic pathway. Pro-apoptotic proteins including DR5, caspases-8, -9, and –3 as well as Bax were not affected by hydrogen peroxide treatment. Overall these data suggest that free radical generation, phosphorylation of EF-2 and subsequent inhibition of protein elongation results in a preferential loss of short half-life proteins with anti-apoptotic function leaving a cell vulnerable to apoptotic stimuli. Doxorubicin treatment accomplishes this sensitization by generating free radicals upon association with iron, since decreased expression of cFLIPS and XIAP was abrogated by pre-treatment with an iron chelator. Our data suggest that the phosphorylation status of EF-2 is exquisitely sensitive to oxidative stress and inactivation of EF-2 by phosphorylation quickly results in a lowering of defenses against apoptosis. This built-in sensitivity to abnormal free radical abundance may be an important self-diagnostic capability of cells that naturally results in a vulnerable physiological state. Our proposed model of how doxorubicin affects cancer cells is more comprehensive than has been elucidated previously (Figure 6). The inclusion of the EF-2 arm of this pathway opens a new area of inquiry into the role of free radicals in controlling cancer growth.
A rigorous conversation about free radicals, antioxidants, and cancer therapies is well underway and timely. Currently, highly concentrated doxorubicin therapy is sometimes coupled with iron chelation therapy. The iron chelation prevents free radical formation as demonstrated in a variety of studies and confirmed here [3, 9]. The purpose of the dual therapy is to protect cardiac myocytes which are particularly sensitive to free radical damage, perhaps due to a reduced intrinsic ability to process free radicals as compared to other normal cells such as cardiac fibroblasts . The danger inherent in this approach is that the iron chelators may have the potential to be cancer-protective as well as cardiac-protective. Interestingly, our DFO dose curve and TRAIL sensitization studies (Figures 5B and and6)6) show that a relatively high concentration of DFO is required to protect PC3 cancer cells (at least 40 μM) while cardiac cells are protected by doses as low as 10 μM . These results suggest that there may be a therapeutic window for DFO, which would be important to quantify in order to give patients the maximally effective treatment. Dexrazoxane (DRZ), another iron chelating agent, has been evaluated for cardiac-protective effects when used in combination with ABVE (doxorubicin, bleomycin, vincristine and etoposide) therapy in children with Hodgkin’s disease . The authors found that secondary acute myeloid leukemia and myelodysplastic syndrome occurred more frequently among children in the DRZ arm of the study, which approached but did not reach statistical significance. Two patients in the DRZ group also developed secondary solid tumors earlier than expected. The authors concluded that “the incidence of and the time of onset of the specific leukemias and solid tumors noted after DRZ with doxorubicin and etoposide heightens our concern about using DRZ to reduce long-term cardiopulmonary toxicity in the context of ABVE-based therapy”. Our data suggest a mechanism for this observation that should be considered when designing further studies on amelioration of side effects associated with doxorubicin.
Debate about the role of free radicals in cancer development is ongoing. Our proposed model of doxorubicin’s toxic effect on cancer cells is counter-intuitive to the long-standing belief that free radicals typically cause cancer rather than facilitate eradication of cancer. However, a recent study in Cancer Cell revealed that the ROS-forming compound beta-phenylethyl isothiocyanate, found in vegetables such as broccoli and cabbage, actually destroys cancer in a mouse model through a ROS-mediated mechanism . Another recent mouse model of cancer treatment, which unexpectedly hinged on ROS production is the use of manganese superoxide dismutase (MnSOD) in combination with TRAIL. The MnSOD produces hydrogen peroxide, which was reported to activate caspase-8 and downregulate Bcl-2 . Our data suggest that anti-apoptotic proteins in addition to Bcl-2 may also have been down-regulated by this approach and that caspase-8 activation may have been the result of reduced c-FLIP expression. Furthermore, a group which focused specifically on TRAIL activation of caspase-8 in prostate cancer cells recently published their finding that caspase activation could be blocked by the antioxidants Vitamin C or catalase . Our data suggest the antioxidants may be preventing EF-2 phosphorylation, thereby protecting the cell by preserving anti-apoptotic proteins such as cFLIPS, XIAP, and survivin.
In addition to illuminating a therapeutic mechanism of doxorubicin, our data suggest that EF-2 phosphorylation plays a role in the side effects caused by the drug. For instance, anemia and nausea may be attributed in part to cell cycle arrest in cells, which normally proliferate (blood cells and gut epithelial cells, respectively). Several studies have shown that iron chelators and antioxidants may help to ameliorate such doxorubicin-induced side effects [41–43]. Early work on EF-2 suggested that EF-2 phosphorylation may impact cell cycling by downregulating protein synthesis and thereby clearing the cell of short-half life proteins such as cyclins . The authors of this study state that, “Temporary inhibition of translation may trigger the transition of a cell from one physiologic state into another because of the disappearance of short-lived repressors.” We propose that this mechanism is common between cell cycle modulation and TRAIL sensitization. In this paper we connect phosphorylation of EF-2 by doxorubicin to TRAIL sensitization via changes in the profile of apoptosis-related proteins and also conclude that the phosphorylation of EF-2 by free radicals may contribute to the cell cycle arrest seen upon doxorubicin treatment.
Our model also clarifies some of our previous findings. For instance, we have recently shown that downregulation of cFLIPS was sufficient to sensitize PC3 cells to TRAIL . Because these cells have such low levels of Bcl-2 and Mcl-1, cFLIPS may be the critical determinant of its apoptotic phenotype. In other cell systems, the global downregulation of anti-apoptotic proteins may be required to sensitize cells to TRAIL. We also previously demonstrated that cFLIPS was decreased sufficiently after four hours of doxorubicin treatment to allow TRAIL-induced apoptosis to occur . However, levels of cFLIPS rebounded by 24 hours, suggesting the effect of doxorubicin on inhibition of protein elongation is transient and reversible. Since translational control is an excellent modifier of the protein profile of a cell, we see EF-2 as an interesting new target for cancer researchers.
The authors would like to gratefully acknowledge Drs. David Kurtz and Semyon Rubinchik for their thoughtful comments on the draft manuscript. Thanks also to Rick Peppler for performing the flow cytometry. Dr. Marcus Peter kindly provided the NF-6 antibody. This work was supported by National Institutes of Health (NIH RO1 CA102218).
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