Glycogen Synthase Kinase 3 and 3 Mediate a Glucose-Sensitive ...

MOLECULAR AND CELLULAR BIOLOGY, June 2007, p. 4328–4339 0270-7306/07/$08.00⫹0 doi:10.1128/MCB.00153-07 Copyright © 2007, American Society for Microbiology. All Rights Reserved.

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Glycogen Synthase Kinase 3␣ and 3␤ Mediate a Glucose-Sensitive Antiapoptotic Signaling Pathway To Stabilize Mcl-1䌤 Yuxing Zhao,1 Brian J. Altman,1 Jonathan L. Coloff,1 Catherine E. Herman,1,2 Sarah R. Jacobs,1 Heather L. Wieman,1 Jessica A. Wofford,1 Leah N. Dimascio,1 Olga Ilkayeva,1,2 Ameeta Kelekar,3 Tannishtha Reya,1 and Jeffrey C. Rathmell1,2,4* Department of Pharmacology and Cancer Biology,1 Sarah W. Stedman Nutrition and Metabolism Center,2 and Department of Immunology,4 Duke University Medical Center, Durham, North Carolina 27710, and Department of Laboratory Medicine and Pathology, University of Minnesota, Minneapolis, Minnesota 554553 Received 26 January 2007/Returned for modification 2 March 2007/Accepted 9 March 2007

Glucose uptake and utilization are growth factor-stimulated processes that are frequently upregulated in cancer cells and that correlate with enhanced cell survival. The mechanism of metabolic protection from apoptosis, however, has been unclear. Here we identify a novel signaling pathway initiated by glucose catabolism that inhibited apoptotic death of growth factor-deprived cells. We show that increased glucose metabolism protected cells against the proapoptotic Bcl-2 family protein Bim and attenuated degradation of the antiapoptotic Bcl-2 family protein Mcl-1. Maintenance of Mcl-1 was critical for this protection, as glucose metabolism failed to protect Mcl-1-deficient cells from apoptosis. Increased glucose metabolism stabilized Mcl-1 in both cell lines and primary lymphocytes via inhibitory phosphorylation of glycogen synthase kinase 3␣ and 3␤ (GSK-3␣/␤), which otherwise promoted Mcl-1 degradation. While a number of kinases can phosphorylate and inhibit GSK-3␣/␤, we provide evidence that protein kinase C may be stimulated by glucose-induced alterations in diacylglycerol levels or distribution to phosphorylate GSK-3␣/␤, maintain Mcl-1 levels, and inhibit cell death. These data provide a novel nutrient-sensitive mechanism linking glucose metabolism and Bcl-2 family proteins via GSK-3 that may promote survival of cells with high rates of glucose utilization, such as growth factor-stimulated or cancerous cells. rate of glycolysis is an attribute of cancer cells that has been appreciated for many years (55), with tumor cells exhibiting high rates of glucose uptake and utilization but moderate rates of mitochondrial oxidation (49). More recently, the high rates of glucose uptake into cancer cells have been exploited in positron emission tomography to image many types of tumors in patients (18). Increased glycolysis can stem from tumor hypoxia (19), and a number of oncogenes (4, 10, 20, 40, 44, 52) have been shown to directly promote glucose metabolism. In addition, genes directly involved in glucose utilization, such as glucose transporter 1 (Glut1) and hexokinases 1 and 2 (HK1 and HK2), which catalyze the uptake and phosphorylation of glucose to glucose-6-phosphate, respectively, are often overexpressed in cancer cells and have been correlated with poor prognosis (50, 59). Despite ample evidence for altered glucose metabolism in cancer cells, the specific impact that this form of metabolism may have on cell fate has been obscured by the myriad of other signaling and transcriptional events that can occur in cellular transformation. The ability to maintain glucose metabolism may play a key role in cancer cell resistance to death upon growth factor deprivation. We have shown that overexpression of Glut1 and HK1 is sufficient to delay loss of plasma membrane integrity of growth factor-withdrawn cells (44). These findings suggested the existence of a glucose-dependent signaling pathway that could delay or prevent apoptosis. While glucose-sensitive signaling to initiate insulin secretion in pancreatic beta cells is relatively well understood (22), glucose-dependent signaling pathways that may regulate apoptosis are less certain. In support of such a pathway, pretreatment of cells with high extra-

Maintenance of tissue homeostasis requires balanced cell death and proliferation. A key factor that determines this balance is the availability of cell extrinsic growth signals (9, 42). In the absence of such signals, a cell death program that is regulated by proteins of the Bcl-2 family is initiated. In the hematopoietic system, cytokines, such as interleukin-3 (IL-3), provide signals to prevent the activation of programmed cell death (27). Prior to commitment to death, however, cytokine-deprived cells undergo a program of cellular atrophy (45). During atrophy, surface glucose transporters, such as Glut1, become internalized and degraded in lysosomes (14, 45), leading to reduced glycolytic flux and mitochondrial membrane potential (53). Ultimately, loss of glucose metabolism leads to cell death (7, 8, 20, 45). Conversely, maintenance or enhanced glucose uptake has been shown to protect hematopoietic cells (44, 53), neurons (47), and cardiomyocytes (32). Thus, control of glucose metabolism may play a key role in regulation of cell fate. While amino acid sensing is well known to occur via mTOR/ Raptor protein complexes (58), nutrient-sensing pathways that may respond to changes in glucose metabolism and affect cell survival are poorly understood. In contrast to normal cells, in which glucose metabolism is regulated by growth factors (16, 53), cancer cells often both maintain enhanced glucose utilization and resist cell death even in the absence of growth factors (19, 21). An increased * Corresponding author. Mailing address: Department of Pharmacology and Cancer Biology, DUMC Box 3813, Durham, NC 27710. Phone: (919) 681-1084. Fax: (919) 668-6044. E-mail: jeff.rathmell @duke.edu. 䌤 Published ahead of print on 19 March 2007. 4328

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GSK-3 MEDIATES ANTIAPOPTOTIC GLUCOSE SIGNALING

cellular glucose concentrations or hyperglycemia has been shown to enhance de novo synthesis of diacylglycerol and promote protein kinase C (PKC) activation to protect cardiomyocytes and neurons from ischemic injury. The mechanism of this protection, however, is not clear (29, 38, 46, 57). The Bcl-2 family of proteins includes both pro- and antiapoptotic proteins (12) and are likely candidates to mediate regulation of cell death by glucose metabolism. Some evidence has previously suggested that Bcl-2 family proteins may be sensitive to cell metabolic status because the proapoptotic Bcl-2 family member Bax can become activated upon glucose deprivation (7, 53). The mechanism linking the Bcl-2 family and glucose metabolism, however, is not certain yet likely utilizes critical regulatory Bcl-2 family proteins. In hematopoietic cells, induction and translocation to mitochondria of the proapoptotic BH3-only protein Bim have been shown to play an important role in many cell death pathways (6). The antiapoptotic Bcl-2 family protein Mcl-1 also plays a vital role in cell survival and binds Bim on mitochondria to inhibit Bim-induced activation of the proapoptotic protein Bax. Conditional gene targeting has shown that Mcl-1 is required for the survival of both B and T cells (36). Mcl-1 levels are highly regulated by proteolytic degradation, and phosphorylation of Mcl-1 by GSK-3 in cytokine-deprived cells has recently been shown to play an important role in targeting Mcl-1 for ubiquitination and degradation (31, 62). Cellular activation or transformation leads to signaling and transcriptional as well as metabolic events that may affect Bcl-2 family members and cell death. To address how the increased glucose uptake and catabolism characteristic of activated lymphocytes or cancer cells may influence the Bcl-2 family in the absence of other signaling or transcriptional events, we have analyzed the death of cells in which only glucose uptake and metabolism are promoted. Using this approach, we describe a novel glucose-responsive antiapoptotic signaling pathway. In this pathway, enhanced glucose uptake led to inhibitory phosphorylation of GSK-3, most likely via PKC activity, to stabilize the antiapoptotic Bcl-2 family protein Mcl-1. This novel nutrient-sensing pathway may provide a critical mechanism to connect glucose utilization to the Bcl-2 family of proteins via diacylglycerol-induced activation of PKC isoforms to inhibit GSK-3 and set a threshold for apoptosis of cells with high rates of glucose metabolism.

MATERIALS AND METHODS Cells. FL5.12 cells, BAF3 cells, and 32D cells were cultured in RPMI medium supplemented with 0.5 ng/ml recombinant mouse IL-3 (BD Pharmingen and Pepro Tech, Rocky Hill, NJ) as previously described (5). Glut1/HK1-expressing FL5.12 cells were generated after selection of clones stably expressing Glut1 and HK1 and have been previously described (44). Transient transfections were performed by nucleofection (Kit V; Amaxa Biosystems). Stable expression of the short hairpin RNA interference vector (shRNAi) was achieved by retroviral transfection with pKDGFP shRNAi. Stable clones were identified after cell sorting for green fluorescent protein (GFP)-positive cells and Western analysis for gene expression. For growth factor withdrawal, cells were washed three times in phosphate-buffered saline (PBS) prior to resuspension in RPMI medium lacking IL-3. To inhibit protein synthesis, cells were cultured in medium containing 25 ␮g/ml of cycloheximide. Glycolysis was measured as described previously (43). Plasmid constructs. Bim isoforms were cloned from FL5.12 mRNA using SuperScript One-Step reverse transcription-PCR with Platinum Pfx (Invitrogen) according to the manufacturer’s protocol and subcloned into pEF6 (Invitrogen).

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Hemagglutinin (HA)-tagged Mcl-1 (generously provided by H. J. Brady, University College, London) was cloned into pEF6. Bim and Mcl-1 shRNAi plasmids were constructed using previously described approaches (15). shRNAi sequences were as follows: Bim, GATCTGCGCCCGGAGATACGGATTCCTCGAGCA ATCCGTATCTCCGGGCGCAGATC; Mcl-1, AATGGTTCGATGAAGCTTT CCCTCGAGCGAAAGCTTCATCGAACCATT (34), and GFP, GATCCGTT CAACTAGCAGACCATTCCTCGAGCAATGGTCTGCTAGTTGAACGG ATC. Sequences were cloned under control of the hU6 promoter in pCR2.1 and pKD vectors as described previously (15). The GSK-3␤ shRNAi construct was kindly provided by David Turner (University of Michigan) (60). EGFP-PKDCRD and EGFP-PKD-CRD-P155/287G constructs were kindly provided by Martin Spitaler and Doreen Cantrel (University of Dundee, United Kingdom). pCMV-FLAG-ubiquitin was kindly provided by Michael Ehlers (Duke University). Mass spectral analysis of organic acids. Intracellular organic acids were analyzed as described previously (24). Briefly, cells were washed in PBS, lysed in 0.1 M HCl, and cleared by centrifugation. A cocktail of stable-isotope internal standards was added, and lysates were then extracted in ethyl acetate, dried, and converted to methyl esters, with the addition of trimethyl silyl esters with ethoxyamine hydrochloride. Organic acids were then analyzed by capillary gas chromatography/mass spectrometry. Cell fractionation. To isolate mitochondria, cells were washed once in PBS, resuspended in mitochondrial isolation buffer (20 mM HEPES [pH 7.5], 10 mM KCl, 5 mM MgCl2, 1 mM EDTA, 1 mM EGTA, 250 mM sucrose, protease inhibitors), and forced by syringe to pass through a 5-␮m polycarbonate filter membrane. Unbroken cells and nuclei were pelleted by centrifugation at 800 ⫻ g for 10 min at 4°C. The supernatant was subjected to an additional centrifugation at 16,000 ⫻ g for 10 min at 4°C. The pellet was collected as heavy membrane and mitochondrial fractions, and the supernatant was used as the cytosolic fraction. Clonogenic assay. Cells were withdrawn from IL-3 for 0, 12, 18, 24, and 48 h; washed; and recultured in medium containing IL-3 in 96-well plates at concentrations of 1/3, 1, or 3 cells per well. The frequency of colonies on each plate after 7 days was determined as the mean and standard error of colony number relative to cell input for each plate (n ⫽ 5). Western blots. Cells were lysed in radioimmunoprecipitation assay buffer with protease inhibitors (BD Pharmingen) and phosphatase inhibitors (Sigma) on ice for 10 min and precleared by centrifugation. Protein concentrations were determined by bicinchoninic acid protein assay (Bio-Rad), and 25 ␮g of protein was subjected to 4 to 20% sodium dodecyl sulfate-polyacrylamide gel electrophoresis (Bio-Rad). Antibodies used were rabbit anti-Bax (Cell Signaling), rabbit antiBim (BD Pharmingen), rabbit anti-Bcl-2 (BD Pharmingen), mouse anti-cytochrome c (BD Pharmingen), rabbit anti-Glut1 (Abcam), rabbit anti-phosphoGSK-3(Ser9/21) (Cell Signaling), rabbit anti-GSK-3␤ (Cell signaling), mouse anti-phospho-Akt (Ser473), rabbit anti-Mcl-1 (Santa Cruz and Biolegend), rabbit anti-Cox IV, rabbit antiubiquitin (Santa Cruz), rat anti-HA (Roche), rabbit anti-FLAG (Sigma), and mouse antiactin (Sigma). Rabbit anti-phospho-Mcl1(Ser159) was a kind gift of D. Green (St. Jude Children’s Research Hospital, Memphis, TN) and U. Maurer (Institut fu ¨r Molekulare Medizin und Zellforschung, Germany). Secondary antibodies were anti-rabbit and anti-mouse horseradish peroxidase-labeled antibodies (BD Pharmingen) and anti-rabbit infrared-labeled antibody and were detected with ECL-Plus (Amersham, Biosciences) or the Odyssey infrared imaging system (Licor). All images were uniformly contrasted, and some were digitally rearranged for ease of viewing (rearranged lanes indicated by spaces). Immunoprecipitation. Cells were harvested and lysed in CHAPS buffer {50 mM Tris [pH 7.5], 10% glycerol, 1% 3-[(3-cholamidopropyl)-dimethylammonio]1-propanesulfonate [CHAPS], 150 mM NaCl, 1 mM EDTA, proteasome inhibitor}. Lysates were precleared, antibodies (rabbit anti-Bax [clone 6A7; BD Pharmingen], rabbit anti-Bim [BD Pharmingen], and rat anti-HA [Roche]) were added, and the mixtures were rotated at 4°C for 1 h. Anti-rabbit immunoglobulin G beads (ebioscience) or protein A/G beads (Santa Cruz) were then added to the lysates and incubated overnight. Beads were washed with 1% CHAPS buffer three times, and proteins were eluted by boiling the beads in sodium dodecyl sulfate loading buffer. Fluorescence microscopy. To image GSK-3 phosphorylation in primary bone marrow cells, cells were cytospun, fixed on the slides in 4% paraformaldehyde, washed in PBS–0.1% Tween, and blocked with 20% normal goat serum. Slides were stained with anti-nerve growth factor receptor (NGFR)–biotin (BD Pharmingen) and anti-phospho-GSK-3 (Cell Signaling) or an isotype control, followed by anti-rabbit–Alexa 546 (Molecular Probes), antistreptavidin–FITC (BD Pharmingen), and DAPI (4⬘,6⬘-diamidino-2-phenylindole). To image cells expressing GFP fusion proteins, cells were fixed with 1% paraformaldehyde in PBS

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FIG. 1. Glut1/HK1 expression increases glucose metabolism and delays commitment to cell death. (A) Glycolytic flux was measured in control (Neo) and Glut1/HK1 cells in the presence or absence of IL-3. (B) Tandem mass spectrometry-based analysis of organic acids in control and Glut1/HK1 cells cultured in the presence or absence of IL-3 for 6 h. (C) Clonogenicity of multiple individual control, Glut1/HK1, and Bcl-xL cells cultured in the absence of IL-3 for the indicated times, followed by readdition of IL-3. (D) Control and Glut1/HK1 cells were IL-3 withdrawn and cultured in 10 mM glucose, 10 mM 2DOG plus 1 mM methylpyruvate, or 5 mM glucose plus 5 mM 2DOG, and viability was determined by PI exclusion. (E) Bax activation was analyzed by immunoprecipitation (I.P.) of active Bax from cells cultured in the presence or absence of IL-3 for 10 h followed by Western blotting for total Bax. (F) Cytochrome c release in control (Neo), Glut1/HK1, and Bcl-xL cells after IL-3 withdrawal. Cells were cultured in the presence or absence of IL-3 for the indicated times, fractionated to isolate cytosolic and mitochondrial proteins, and analyzed by Western blotting for cytochrome c. Values are means and standard deviation (n ⫽ 3) (A, B, and D) or means and standard errors of the means (n ⫽ 5) (C). N, Neo control; GH, Glut1/HK1; X, Bcl-xL.

and viewed with a Zeiss LSM410 confocal microscope (Zeiss, Thornwood, NY) and Metamorph software. Glut1-transgenic mice and primary cell culture. Full-length rat Glut1 was cloned into the pLck.E2 vector, which we have used previously for T-lymphocytespecific transgene expression (43). Transgenic animals were made in and were a generous gift of the Abramson Family Cancer Research Institute transgenic facility at the University of Pennsylvania. Mice were backcrossed five generations to C57BL6/J mice and cared for at Duke University. T cells were purified by negative selection, and glucose uptake and in vitro survival in neglect were measured as described previously (3, 43). Bone marrow cells were cultured in 5 ng/ml recombinant IL-3-containing RPMI 1640 medium. Media with IL-3 were changed every 2 days. On day 4, cells were infected in retrovirus supernatant (MSCV-Glut1-IRES-NGFR or vector control) at a concentration of 1 ⫻ 106 cells/ml for 24 h at 37°C, and they were analyzed by immunofluorescence 2 days later.

RESULTS Glut1 and HK1 signal to delay Bcl-2 family-mediated commitment to cell death after growth factor withdrawal in a manner that requires glucose hydrolysis. To determine how changes in glucose metabolism may signal to affect cell death pathways, we analyzed the effects of Glut1 and HK1 expression (Glut1/HK1 cells) (44) on cell death by using the FL5.12

hematopoietic precursor cell line. FL5.12 cells are nontransformed and are strictly dependent on the cytokine IL-3 for maintenance of glucose uptake and survival. Expression vectors for Glut1 and HK1 (pSFFV-Glut1 and pcDNA3-HK1, respectively) were previously cotransfected into FL5.12 cells, and stable clones were identified by Geneticin selection and immunofluorescence labeling (44). Analysis of Glut1/HK1 cells, therefore, provided a means to directly identify glucosestimulated antiapoptotic signaling pathways independent of other transformation- or oncogene-induced antiapoptotic mechanisms. Expression of Glut1 and HK1 promoted and maintained enhanced glycolysis during IL-3 withdrawal (Fig. 1A), and mass spectrometry-based quantification of intracellular organic acids showed dramatically increased production of lactate that was maintained in the absence of IL-3 (Fig. 1B). In contrast, Krebs cycle intermediates were only modestly increased or were reduced in Glut1/HK1 cells. Although expression of Glut1 and HK1 does not direct coordinate control over entire metabolic pathways, Glut1/HK1 cells displayed a highly glycolytic phenotype in the presence of IL-3 and shortly after IL-3 withdrawal, similar to what has been observed in many cancer cells (49).

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We have previously shown that Glut1/HK1-expressing cells exhibit delayed cell permeability to the vital fluorescent dye propidium iodide (PI) upon IL-3 withdrawal (44). Permeability to PI, however, may be delayed by maintenance of cellular energetics and continued production of ATP (56) and thus may not reflect a true change in the commitment point of death. To more rigorously test the survival capacity of Glut1/ HK1 cells upon IL-3 withdrawal, we performed limiting-dilution clonogenicity analysis on individual control or Glut1/HK1 clones following restoration of IL-3 to cells withdrawn from IL-3 for various periods of time (Fig. 1C). Consistent with results obtained by PI exclusion (44), control cells rapidly lost their ability to recover and grow with readdition of IL-3, whereas Glut1/HK1 maintained significant clonogenic survival, albeit not to the same extent as cells expressing the antiapoptotic Bcl-2 family protein Bcl-xL. The survival advantage of Glut1/HK1 cells over control cells required a hydrolyzable glucose source, as the nonhydrolyzable 2-deoxyglucose (2DOG) failed to enhance cell survival even in the presence of methyl pyruvate (a cell-permeable form of pyruvate to provide a mitochondrial substrate) (Fig. 1D). These findings suggest that glucose may initiate an antiapoptotic signaling pathway requiring glucose hydrolysis to delay commitment to cell death. Commitment to cell death upon growth factor withdrawal in hematopoietic cells occurs at the point of mitochondrial disruption by Bax and Bak and release of cytochrome c into the cytosol. To identify the stage at which glucose metabolism may delay cell death commitment, Bax activation and cytochrome c release were analyzed in Glut1/HK1 cells. Control and Glut1/ HK1 cells were deprived of IL-3 for 10 h, and Bax was immunoprecipitated from cell lysates by using an active Bax conformation-specific antibody (Fig. 1E). No active Bax was detectable in cells cultured in the presence of IL-3. Upon IL-3 withdrawal, activated Bax was readily observed in control cells but not in Glut1/HK1 cells. Cytosolic and mitochondrial cell fractions from control, Glut1/HK1, and Bcl-xL cells were also analyzed by immunoblotting to observe mitochondrial disruption and release of cytochrome c (Fig. 1F). Mitochondria in control cells began to lose integrity 10 h after IL-3 withdrawal, with decreased cytochrome c in the mitochondrial fractions and the appearance of cytochrome c in cytoplasmic fractions. In contrast, cytochrome c release was delayed in Glut1/HK1 cells, and cytosolic cytochrome c was readily detectable only after 12 h of IL-3 withdrawal. By this time, control cells had released the majority of the cytochrome c into the cytosol. Cells overexpressing Bcl-xL maintained mitochondrial integrity throughout the time analyzed. Caspase activation in Glut1/ HK1 cells was also reduced upon IL-3 withdrawal, as precipitation of caspase 3 in Glut1/HK1 cells with biotinylated zVAD, a broad caspase inhibitor that binds to active caspases, yielded only 40% of that obtained in control cells upon IL-3 withdrawal (data not shown). These results indicate that increased glucose metabolism delayed commitment to cell death after growth factor withdrawal upstream of Bax activation and cytochrome c release. Bim is necessary and sufficient for cytokine withdrawalinduced apoptosis, yet glucose metabolism promotes resistance to Bim toxicity. Antiapoptotic glucose signaling in Glut1/ HK1 cells delayed Bax activation and cytochrome c release upon IL-3 withdrawal, suggesting regulation of the Bcl-2 family

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members by glucose hydrolysis. Gene-targeting studies have shown that the proapoptotic BH3-only Bcl-2 family member Bim plays a pivotal role in apoptosis of hematopoietic cells upon cytokine withdrawal (6). In FL5.12 cells, the three isoforms of Bim (BimEL, BimL, and BimS) were induced and were important for efficient apoptosis upon IL-3 withdrawal, as cells with decreased Bim expression by shRNAi partially resisted IL-3 deprivation-induced apoptosis (Fig. 2A and B). To test if glucose metabolism affected Bim induction, we cultured control, Glut1/HK1, and Bcl-xL cells in IL-3 or withdrew cells from IL-3 for 10 h. Transcriptional induction of Bim RNA was analyzed by RNase protection (Fig. 2C), and total Bim protein levels were determined by immunoblotting (Fig. 2D). All three Bim isoforms were induced at the RNA level, and BimEL and BimL were upregulated at the protein level in all three cell lines upon IL-3 withdrawal. Endogenous BimS protein was undetectable in all conditions (data not shown). For reasons that are not clear, Glut1/HK1 and Bcl-xL cells had somewhat higher levels of total cellular Bim RNA and protein induction following IL-3 deprivation. Nevertheless, apoptosis was delayed in Glut1/HK1 cells (Fig. 1C). Mitochondrial levels of Bim are critical for Bim to promote apoptosis, and increased glucose metabolism may have affected Bim translocation to mitochondria (41). To analyze Bim translocation, mitochondria were isolated from control, Glut1/HK1, and Bcl-xL cells deprived of IL-3 for the indicated times and were immunoblotted for Bim protein levels. Despite somewhat higher total Bim levels, Glut1/HK1 and Bcl-xL cells showed similar Bim translocation to mitochondria compared to control cells, (Fig. 2E). To determine if Bim protein associations were altered by Glut1/HK1 expression, Bim was immunoprecipitated from control and Glut1/HK1 cells and analyzed by immunoblotting for associations with Bcl-2 and Mcl-1 (Fig. 2F). While IL-3 withdrawal increased the amount of immunoprecipitated Bim, no differences between control and Glut1/HK1 cells were observed in Bcl-2 coimmunoprecipitation. Mcl-1 was also precipitated with Bim in both cell lines, although total Mcl-1 levels were reduced in IL-3-withdrawn control cells. Bim induction was greater and Bim translocation to mitochondria and association with other Bcl-2 family proteins appeared normal in Glut1/HK1 cells, yet Glut1/HK1 cells resisted cell death upon IL-3 withdrawal. To determine if increased glucose metabolism could prevent Bim cytotoxicity downstream of induction and translocation to mitochondria, control or BimL-expressing plasmids were transfected into control, Glut1/HK1, and Bcl-xL cells in the presence of IL-3 and cell viability was monitored. Expression of BimL was similar in all three cell lines, with moderately higher expression in Glut1/ HK1 and Bcl-xL cells relative to control cells (Fig. 2G). BimL led to significant death of control cells, while Bcl-xL-expressing cells were more resistant. Glut1/HK1 cells showed intermediate resistance to BimL (Fig. 2H). Similar results were obtained with BimS (data not shown). These data suggested that increased glucose metabolism acted on the Bcl-2 family proteins at the mitochondria to prevent Bim toxicity and promote cell survival. Increased glucose metabolism stabilizes Mcl-1 to protect cells against IL-3 withdrawal-induced apoptosis. Although RNase protection showed no differences in mRNA levels of multiple Bcl-2 family members upon IL-3 withdrawal (data not

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FIG. 2. Bim is necessary for death and is induced normally in Glut1/HK1 cells, yet Bim toxicity is inhibited. (A and B) Cells were transfected with control (GFP) or Bim shRNAi and analyzed in the presence or absence of IL-3 for Bim expression (A) and survival (B). (C and D) Bim RNA (C) and protein (D) induction after IL-3 withdrawal in control (Neo), Glut1/HK1, and Bcl-xL cells. Cells were cultured in the presence or absence of IL-3 for 10 h. Bim RNA levels were determined by RNase protection assay, and protein levels were determined by Western blotting. (E) Control (Neo), Glut1/HK1, and Bcl-xL cells were cultured in the presence or absence of IL-3 for the indicated times. Bim levels in mitochondrial fractions were determined by Western blotting. (F) Control (Neo) and Glut1/HK1 cells were cultured in the presence of or withdrawn from IL-3 for 10 h. Bim was immunoprecipitated, and the precipitates were analyzed by immunoblotting for Bim, Bcl-2, and Mcl-1. (G and H) Control (Neo) or BimL plasmid was transiently transfected into control (Neo), Glut1/HK1, and Bcl-xL cells. Bim expression was determined by Western blotting (G), and cell viability was determined by PI exclusion (H). Values are means and standard deviations (n ⫽ 3) (B and H). N, Neo control; GH, Glut1/HK1; X, Bcl-xL.

shown), mitochondrial protein levels of the antiapoptotic protein Mcl-1 were found to be affected by glucose metabolism. Mitochondria were purified from control and Glut1/HK1-expressing cells that were cultured in the presence or absence of IL-3 and analyzed for Mcl-1 and Bcl-2 expression levels (a representative gel is shown in Fig. 3A, and quantification from three similar independent experiments is shown in Fig. 3B). Mitochondrial Bcl-2 expression remained constant in the presence or absence of IL-3 and was used as a loading and normalization control. Mitochondrial Mcl-1 protein levels, in contrast, decreased in control and Bcl-xL-expressing cells upon IL-3 withdrawal. Glut1/HK1 cells, however, maintained mitochondrial Mcl-1 levels even upon IL-3 withdrawal. Notably, reduction of Mcl-1 levels in Bcl-xL-expressing cells indicated

that Mcl-1 loss occurred independent of mitochondrial disruption, cytochrome c release, and caspase activity. To determine the loss of Mcl-1 over time after IL-3 withdrawal, total cellular lysates from control, Glut1/HK1, and Bcl-xL cells deprived of IL-3 for the indicated times were analyzed by immunoblotting for Mcl-1 and actin to obtain the relative ratio of cellular abundance of Mcl-1 to that of actin (Fig. 3C). In both control and Bcl-xL-expressing cells, the ratio of Mcl-1 to actin decreased over time when cells were withdrawn from IL-3. This relative loss of Mcl-1 protein was attenuated, however, in Glut1/HK1 cells. Genetic experiments have indicated that the complete loss of Mcl-1 leads to the death of hematopoietic cells in vivo (35, 36). IL-3 withdrawal, however, resulted in only a partial loss of

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FIG. 3. Maintenance of Mcl-1 protein level is critical for protection of Glut1/HK1 cells upon IL-3 withdrawal. (A and B) Control, Glut1/HK1, and Bcl-xL cells were cultured in the presence or absence of IL-3 for 10 h, and mitochondria were isolated. (A and B) Representative gel (A) and quantitated averages and standard deviations of mitochondrial Mcl-1 levels using Bcl-2 as a normalization control (B). (C) Control (Neo), Glut1/HK1, and Bcl-xL cells were withdrawn from IL-3, and the total cellular Mcl-1/actin ratio was determined over time. (D and E) Control and Glut1/HK1 cells were transiently transfected with control (GFP) or Mcl-1 shRNAi, and then Mcl-1 protein level was determined by immunoblotting (D) and cell viability was observed by PI exclusion (E). Values are means for cell survival from triplicate samples; error bars indicate standard deviations. N, Neo control; GH, Glut1/HK1; X, Bcl-xL.

Mcl-1. We sought, therefore, to determine how moderate changes in Mcl-1 protein level that occur upon IL-3 withdrawal may influence sensitivity to apoptosis. Mcl-1 protein levels were decreased using shRNAi to approximately 50% in control and Glut1/HK1 cells to mimic the levels of Mcl-1 that occur in growth factor withdrawal (Fig. 3D). In the presence of cytokine, this reduced level of Mcl-1 in Mcl-1 shRNAi-treated cells was not sufficient to promote spontaneous activation of Bax or cell death (Fig. 3E and data not shown). Upon withdrawal from cytokine, however, cells expressing shRNAi for Mcl-1 displayed an increased rate of Bax activation and more rapid cell death. This rapid cell death required Bim induction, as simultaneous shRNAi of Bim led to a partial rescue of Mcl-1deficient cells (data not shown). Importantly, Mcl-1-deficient Glut1/HK1 cells underwent programmed cell death at the same high rate as Mcl-1-deficient control cells. Increased glucose catabolism, therefore, appeared to delay apoptosis upon growth factor withdrawal via regulation of the antiapoptotic Bcl-2 family protein Mcl-1 to prevent a sudden change in Mcl-1 levels that may allow Bim-mediated Bax activation and apoptosis. Expression of Glut1 and HK1 attenuates Mcl-1 protein degradation after growth factor withdrawal. Ubiquitination and proteasomal degradation play critical roles in control of Mcl-1 levels (62). To determine the effect of Glut1/HK1 expression on the degradation of Mcl-1, we cultured control and Glut1/

HK1 cells in the absence of IL-3 for 8 h, treated cells with cycloheximide to block new protein synthesis, and observed Mcl-1 degradation. In whole-cell (Fig. 4A) or mitochondrial (a representative gel is shown in Fig. 4B, and quantification from three similar independent experiments is shown in Fig. 4C) extracts, the Mcl-1 was more rapidly degraded in control cells than in Glut1/HK1 cells. To further confirm delayed Mcl-1 degradation, control and Glut1/HK1 cells expressing HAtagged Mcl-1 were transfected with FLAG-tagged ubiquitin and withdrawn from IL-3. Immunoprecipitation of HA–Mcl-1 followed by immunoblotting for FLAG-ubiquitin showed that Mcl-1 ubiquitination was reduced in Glut1/HK1 cells (Fig. 4D). Antiapoptotic glucose signaling, therefore, appeared to inhibit growth factor withdrawal-induced apoptosis via a glucose-sensitive attenuation of Mcl-1 protein ubiquitination and degradation. Inhibition of GSK-3 kinase activity by glucose metabolism protects Mcl-1 levels and attenuates cell death. Mcl-1 protein degradation is regulated in part through Mcl-1 phosphorylation by GSK-3 on serine 159 and subsequent Mcl-1 ubiquitination by the BH3 domain containing ubiquitin ligase Mule (31, 62). We therefore analyzed phosphorylation of Mcl-1 S159 and found it decreased relative to that in control cells in two independent clones expressing Glut1 alone or with HK1 (Fig. 5A), suggesting reduced GSK-3 kinase activity in glycolytic cells. As GSK-3␣/␤ activity is negatively regulated by phosphor-

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FIG. 4. Glucose uptake attenuates Mcl-1 ubiquitination and degradation after growth factor withdrawal. (A, B, and C) Control and Glut1/HK1 cells were withdrawn from IL-3 for 8 h and then treated with cycloheximide (CHX) to observe Mcl-1 degradation. (A) Total cellular Mcl-1 as a fraction of starting levels prior to CHX treatment. (B and C) Representative gels (B) and quantitated averages and standard deviations from three independent experiments (C) of mitochondrial Mcl-1 levels, using Bcl-2 as a normalization control, before (⫺) and after (⫹) CHX treatment. (D) HA-Mcl-1-expressing control and Glut1/HK1 cells were transiently transfected with FLAG-ubiquitin (FLAG-Ub) and withdrawn from IL-3 for 10 h. The proteasome inhibitor MG-132 (20 ␮M) was added in the last hour of culture. Lysates were immunoprecipitated with anti-HA and probed with anti-FLAG, anti-HA, or anti-heavy chain immunoglobulin. N, Neo control; GH, Glut1/HK1.

ylation on serines 21 and 9, respectively, total GSK-3␤ and phospho-GSK-3␣/␤ levels were determined by immunoblotting in control and Glut1 and/or HK1 cells (Fig. 5B). Increased levels of phospho-GSK-3 occurred in multiple independently derived FL5.12 cell clones in which Glut1 and hexokinase 1 were expressed individually or together (Fig. 5B). Phosphorylation of GSK-3 appeared to be specific for GSK-3 and did not represent increased overall cellular signaling activity, as levels of phospho-Akt (serine 473) were similar in all cell lines (Fig. 5B) and comparable levels of phospho-STAT5, the STAT3 and STAT5 target Pim1, phospho-mTOR, and phospho-p70S6 kinase were observed in control and Glut1/HK1 cells (data not shown). Enhanced phosphorylation of GSK-3 was maintained upon IL-3 withdrawal and was also observed in Glut1/HK1expressing 32D and BAF3 early hematopoietic cell lines (Fig. 5C). Our data support and extend previous findings on the role of GSK-3␣/␤ in regulation of Mcl-1 (31) to include regulation of GSK-3 by glucose metabolism. Inhibition of GSK-3 in control cells increased maintenance of Mcl-1 (Fig. 5D) and provided protection from cell death (Fig. 5E) upon growth factor deprivation to extents comparable to those observed in Glut1/HK1 cells. In addition, RNAi of GSK-3␤, leading to an approximately 50% decrease in GSK-3␤ protein with unchanged GSK-3␣ levels, increased Mcl-1 protein levels (Fig. 5F) and attenuated cell death upon IL-3 withdrawal similarly to the

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case for Glut1/HK1 cells (Fig. 5G). GSK-3 phosphorylation and inhibition of Mcl-1 protein degradation, therefore, appears to represent a critical point in a nutrient-sensing pathway linking glucose metabolism to cell survival. Glut1 expression increases the phospho-GSK-3 level, protects Mcl-1, and attenuates cell death in primary hematopoietic cells. Having demonstrated increased phospho-GSK-3 levels and maintenance of Mcl-1 in Glut1/HK1-expressing bone marrow-derived myeloid and pro-B-cell lines, we next tested the ability of increased glucose uptake to regulate phosphoGSK-3 in primary bone marrow-derived hematopoietic cells. Primary murine bone marrow cells were isolated, cultured in IL-3, infected with control or Glut1-expressing retrovirus, and analyzed by immunofluorescence for phospho-GSK-3. Similar to the case for cell lines, Glut1 expression in primary bone marrow cells led to enhanced levels of phospho-GSK-3 (Fig. 6A). We also generated a transgenic mouse with expression of Glut1 specifically in T lymphocytes. Purified peripheral T cells from Glut1-transgenic mice had increased Glut1 expression (Fig. 6B) and resting glucose uptake (Fig. 6C). Importantly, freshly isolated T cells from Glut1-transgenic mice had increased levels of phospho-GSK-3 compared to T cells purified from littermate nontransgenic mice (Fig. 6D) that was partially maintained upon in vitro culture in the absence of stimulation (Fig. 6E, Neglect). In accordance with GSK-3-mediated regulation of Mcl-1 protein levels, Mcl-1 protein levels decreased when T cells were neglected in vitro (Fig. 6F). This was attenuated by inhibition of GSK-3 or by expression of the Glut1 transgene (Fig. 6F and G). In addition, Glut1-transgenic T cells showed increased resistance to cell death when cultured in vitro in the absence of growth factor or cytokine stimulation (Fig. 6H). Increased phospho-GSK-3, protection of Mcl-1, and resistance to growth factor withdrawal-induced cell death, therefore, appear to be general events in primary hematopoietic cells with increased glucose uptake. PKC activity may be responsible for GSK-3 phosphorylation and glucose-stimulated signaling for protection from cell death. GSK-3␣/␤ can be phosphorylated on serines 21 and 9 by a number of kinases, including PKA, PKC, and Akt (26). To identify candidate kinases by which glucose catabolism may stimulate phosphorylation of GSK-3, we treated control and Glut1 cells with inhibitors to each kinase and observed phospho-GSK-3 levels (Fig. 7A). Inhibition of Akt by the phosphatidylinositol 3-kinase (PI3K) inhibitor LY294002 or of PKA by the inhibitor H89 did not decrease phosphorylation of GSK3␣/␤ at serines 21 and 9 in Glut1/HK1 cells but did appear to increase GSK-3 phosphorylation in control cells. PI3K/Akt and PKA are, therefore, not major GSK-3 kinases responsible for glucose-stimulated GSK-3 phosphorylation. The mechanism of this increased GSK-3 phosphorylation by these inhibitors is not clear, but it is likely due to compensation by other kinases activated under the stress of inhibitor treatment. In contrast, the global PKC inhibitor (Ro31-8220) led to a near-complete loss of phospho-GSK-3 in both control and Glut1/HK1 cells (Fig. 7A), suggesting that PKC isoforms were critical GSK-3 kinases. This effect was not dependent on other described nutrient-sensing kinase pathways, such as mTOR (58) and CamK II (33), as the mTOR/Raptor inhibitor (rapamycin) and CamK II inhibitor (KN93) also had no effect on phosphoGSK-3 levels in Glut1/HK1 cells and increased phospho-

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FIG. 5. GSK-3 phosphorylation is increased in Glut1- and HK1-expressing cells and regulates both Mcl-1 degradation and cell death. (A) Mcl-1-expressing control, Glut1, or Glut1/HK1 cells were analyzed for phospho-S159 and total Mcl-1. Ratios are shown. (B) Multiple FL5.12 clones expressing Glut1 and/or HK1 were analyzed for phospho-Akt, phospho-GSK-3, and total GSK-3␤ by immunoblotting. (C) Control and Glut1/HK1 FL5.12, 32D, and BAF3 cells were cultured in IL-3 or withdrawn from IL-3 for 6 hours, and phospho-GSK-3 and total GSK-3␤ were determined by immunoblotting. Ratios are shown. (D and E) Cells were treated with GSK-3 inhibitor (10 ␮M SB216763), followed by immunoblotting for Mcl-1 and actin (ratios are shown) (D) and determination of cell viability upon IL-3 withdrawal (E). (F and G) FL5.12 cells were transiently transfected with shRNAi for GFP or GSK-3␤. Cells were analyzed by immunoblotting for GSK-3␤, Mcl-1, and actin in the presence or absence of IL-3 (ratios are shown) (F), and cell survival upon IL-3 withdrawal was determined by PI exclusion (G). Values are means from triplicate samples; error bars indicate standard deviations. M, hMcl-1; N, Neo control; G, Glut1; H, HK1; GH, Glut1/HK1.

GSK-3 levels in control cells (Fig. 7A), possibly due to compensatory increases in PKC activity similar to those of other kinase inhibitors. To further examine a role for PKC isoforms in phospho-GSK-3␣/␤, control and Glut1/HK1 cells were subjected to treatment with a variety of PKC inhibitors with differing specificities (Fig. 7A). With the exception of Go6983 and Rottlerin, which inhibit primarily conventional PKCs and PKC␦, respectively, each provided at least partial inhibition of GSK-3 phosphorylation, suggesting that PKC isoforms may play prominent roles in phosphorylation of GSK-3 in response to enhanced glucose metabolism. Diacylglycerol acts as secondary messenger for conventional and novel PKC activation, and its level and distribution can be

altered by glucose metabolism (28, 38, 39). To determine if increased glucose metabolism affected diacylglycerol to promote PKC activity, cells were transfected with a diacylglycerol binding reporter construct. Control and Glut1/HK1 cells were transfected with a diacylglycerol binding domain of the PKCrelated kinase PKD (PKC␮)-CRD fused to GFP (PKD-CRDGFP) or with a mutant in which the PKD-CRD was altered to attenuate its ability to bind diacylglycerol (PKD-CRD-GFP P155/287G). Cell membrane localization of PKD-CRD-GFP was significantly higher in Glut1/HK1 cells than in control cells, whereas no difference was observed in PKD-CRD-GFP P155/287G-transfected cells (representative confocal images are shown in Fig. 7B, and quantitation from three independent

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FIG. 6. Glut1 expression increases GSK-3 phosphorylation, Mcl-1 level, and survival in primary hematopoietic cells. (A) Bone marrow cells were cultured in IL-3, infected with retrovirus to express Glut1 and truncated hNGFR as a marker on day 4, and stained by immunofluorescence for phospho-GSK-3 (red), hNGFR (green), and DAPI on day 7. (B to E) Glut1 protein levels were analyzed by immunoblotting (B), glucose uptake was measured (C), and phospho-GSK-3 levels were determined by immunoblotting (D) and quantified (E) in purified T lymphocytes from nontransgenic (Non) and Glut1-transgenic (Glut1) littermates freshly after purification or after 1 day of culture in the absence of stimulation (neglect). (F) Mcl-1 levels were determined by immunoblotting of freshly isolated, neglected, or GSK-3 inhibitor (10 ␮M SB216763 [SB])-treated nontransgenic T cells. Ratios are shown. (G) Mcl-1/actin ratio quantitated from nontransgenic and Glut1-transgenic T cells after isolation (fresh), neglect, or culture in GSK-3 inhibitor (SB). (H) Purified T cells from nontransgenic and Glut1-transgenic littermate mice were cultured without stimulation (neglect), and cell survival determined after 2 days. Values shown are the means from triplicate samples; error bars indicate standard deviations.

experiments is shown in Fig. 7C). These data indicate that chronically elevated glucose metabolism in Glut1/HK1 cells may increase or alter localization of diacylglycerol and provide a possible mechanism for altered PKC localization or activation. To determine if enhanced PKC activity in Glut1/HK1 cells was required for antiapoptotic glucose signaling and increased survival, we examined the effect of PKC inhibition in cell death upon IL-3 withdrawal. Glut1/HK1 cells were withdrawn from IL-3 and were untreated or treated with PKC inhibitor alone or with GSK-3 inhibitor, and Mcl-1 levels were determined by immunoblotting (Fig. 7D). Inhibition of PKC led to a sharp reduction in Mcl-1 protein levels that simultaneous inhibition of GSK-3 could partially rescue. In addition, inhibition of PKC prevented Glut1/HK1-mediated protection from cell death and reduced the survival of IL-3-withdrawn Glut1/HK1 cells to a level equivalent to that of control cells (Fig. 7E). This loss of Glut1/HK1-mediated protection appeared to be due to activation of GSK-3, as increases in the rate of cell death caused by PKC inhibition could be reversed by simultaneous inhibition of GSK-3. Together, these data suggest that a signaling pathway via PKC and GSK-3 is sensitive to glucose metabolism and is active in highly glycolytic cells, such as growth factor-stimulated or cancer cells. Ultimately, this glucose-dependent signaling pathway protects cells from apoptosis by attenuating degradation of Mcl-1 and thus inhibiting toxicity from the proapoptotic proteins, such as Bim.

DISCUSSION A decreased glucose metabolic rate and initiation of apoptosis are sequential processes that occur when nontransformed cells are withdrawn from growth factors. Cancer cells, however, maintain both glucose metabolism and cell viability when they are growth factor deprived (49). The relationship between these two features of cancer cell physiology has been unclear. Here we show that increased glycolysis is sufficient to initiate an antiapoptotic signaling pathway to delay commitment to cell death upon growth factor withdrawal. This antiapoptotic signaling pathway appears to be mediated, at least in part, through maintenance of Mcl-1 protein levels via PKC-mediated inhibition of GSK-3. This pathway was activated in both cell lines and primary cells expressing Glut1 and/or hexokinase, which suggests that the coordinate upregulation of glucose metabolic pathways that is promoted by growth factors may play a previously undefined yet critical role in the survival of growth factor-stimulated or cancer cells. Nutrient-induced signaling pathways have been shown to play important roles in many aspects of cell physiology. The mTOR/Raptor protein complex has been clearly implicated in amino acid sensing for regulation of protein synthesis, cell growth, and autophagy (30). Metabolic stress, such as may occur when ATP levels become depleted, can promote activation of AMP kinase via increased intracellular levels of AMP, which can both inhibit protein synthesis (23) and activate p53

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FIG. 7. PKC activity is necessary for GSK-3 phosphorylation and may be stimulated by altered diacylglycerol distribution in Glut1/HK1 cells. (A) Control and Glut1/HK1 FL5.12 cells were cultured in IL-3 in the presence of various kinase inhibitors (PKC, 10 ␮M Ro31-8220 [Ro]; PI3K, 10 ␮M LY294002 [LY]; PKA, 10 ␮M H89; CamK II, 10 ␮M KN93; mTOR, 25 nM rapamycin [Rap]; PKC, 10 ␮M GF 109203X; PKC, 2 ␮M Go6976; PKC, 10 ␮M Go 6983; PKC, 20 ␮M Rottlerin [Rott]) for 1 h, and phospho-GSK-3 levels were determined by immunoblotting. (B and C) Control and Glut1/HK1 cells transiently transfected to express PKD-CRD-GFP or PKD-CDR-GFP P155/287G were imaged by confocal microscopy (B), and cells with membrane-targeted GFP were blindly quantified (means and standard deviations from three independent experiments are shown) (C). (D) Glut1/HK1 cells were withdrawn from IL-3 for 3 hours in vehicle alone (Ctrl), PKC inhibitor (2 ␮M Ro31-8220 [Ro]), or PKC inhibitor plus GSK-3 inhibitor (10 ␮M SB216763 [SB]), and Mcl-1 and actin levels were detected by immunoblotting. Ratios are shown. (E) Control and Glut1/HK1 cells were withdrawn from IL-3 and cultured in the absence or presence of PKC (10 ␮M Ro31-8220 [Ro]) or GSK-3 (10 ␮M SB216763 [SB]) inhibitor, and cell survival was observed over time. Ratios are shown. N, Neo control; GH, Glut1/HK1.

to inhibit cell cycle progression (25). Here we provide evidence of a novel glucose-sensitive signaling pathway. This pathway was stimulated by expression of Glut1 and/or HK1 and appeared to require glucose catabolism, as the nonhydrolyzable glucose analog 2DOG was incapable of providing this glucoseinduced survival signal. Elevated glucose metabolism led to phosphorylation of GSK-3␣/␤ on serines 21 and 9 in cells to maintain Mcl-1 protein levels and inhibit Bim-induced apoptosis in hematopoietic cells. While PKC activation in response to hyperglycemia has been thought to play a potential antiapoptotic role (1, 28, 38, 39), to our knowledge this is the first description of a similar pathway in cells with intrinsically high glucose uptake, such as growth factor-stimulated or cancer cells, and the first to connect this pathway to GSK-3 and the Bcl-2 family of proteins. The approach utilized here to examine the effects of glucose metabolism on cell death in the absence of other signaling or oncogenic events revealed a pathway that may be of broad importance in both cell survival and growth. While the antiapoptotic effects of Glut1 and HK1 expression were not long term, this survival advantage nevertheless provided a significant clonogenic survival advantage over control cells (Fig. 1C) and likely underestimated the overall role that sustained glucose utilization may play in preventing cell death. Indeed, cytokine withdrawal ultimately leads to the loss of expression

of both glycolytic and pentose phosphate pathway enzymes, which is not prevented by expression of Glut1 and HK1 (data not shown and reference 44). Thus, in contrast to the case for growth factor-stimulated or cancer cells, which coordinately upregulate and maintain entire metabolic pathways (49), expression of Glut1 and HK1 alone allows only a temporary increase in glucose metabolism after IL-3 withdrawal. In addition, while this analysis focused on the effects of this glucose signaling pathway on hematopoietic cell death, PKC isoforms and GSK-3 have multiple functions, and glucose-stimulated PKC activity and GSK-3 inhibition may affect other aspects of cell survival and growth to promote cancer progression or proliferation of growth factor-stimulated cells of multiple tissues. Addressing the contribution of glucose-stimulated signaling will be an important consideration for future studies of growth and survival of cancer cells as well as of stimulated lymphocytes, which show a robust increase in glucose uptake and utilization after antigenic stimulation (2, 13, 17). There has been additional evidence to suggest that glucosemediated pathways may regulate apoptosis. In hepatocytes and pancreatic ␤-cells, glucokinase may reside in a protein complex with the BH3-only protein Bad, where Bad phosphorylation by PKA can regulate glucose-stimulated insulin secretion and cell death induced by glucose deprivation (11). It has also recently been shown that NADPH levels can regulate phosphorylation

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of caspase 2 and mitochondrial release of cytochrome c via CamK II in Xenopus egg extracts (33). Each of these models is not mutually exclusive with the antiapoptotic glucose-signaling pathway proposed here. In particular, NADPH levels may play a key role in metabolic signaling to PKC if acyl coenzyme A synthesis is required for de novo diacylglycerol generation. As we did not, however, observe any effect of PKA or CamK II inhibition on phospho-GSK-3 levels in Glut1/HK1 cells and Glut1/HK1 expression increased clonogenicity upon IL-3 withdrawal, our results likely identify a novel PKC-mediated glucose signaling pathway. It is also possible that Glut1/HK1 inhibited cell death in part by enhanced availability of metabolic substrates and generation of cytosolic NADH and ATP that may be cytoprotective as energy sources. The glucose-initiated signaling pathway described here may act in concert with and in the context of each of these other pathways and direct metabolic effects to prevent cell death of glycolytic cells. Altered diacylglycerol levels or distribution and prevention of GSK-3 phosphorylation by PKC inhibitors suggest that this nutrient-signaling pathway is initiated by glucose-mediated effects on diacylglycerol and PKC localization or activity. Conventional and novel PKC isoforms are regulated by phosphorylation, calcium, and diacylglycerol (51). While they are not calcium or diacylglycerol regulated, atypical PKCs (PKC␨ and PKC␫) are regulated by other kinases, including PKCs (61), or lipids (37, 48). In principle, increased glucose metabolism may affect intracellular calcium levels or kinase and phosphatase pathways that promote PKC activity. Using a biosensor for diacylglycerol, we show here that increased glucose metabolism leads to altered diacylglycerol levels or localization. Increased extracellular levels of glucose have been shown to enhance de novo synthesis of diacylglycerol in a variety of cell types, and this can stimulate activity of multiple PKC isoforms (38, 54, 57) that can be protective in both cardiac and neuronal ischemia (29, 46). Basal de novo generation of diacylglycerol and related lipids depends on both glucose and the availability or synthesis of fatty acids and thus incorporates several aspects of cell metabolism to indicate nutrient status. This pathway may, therefore, be ideally situated to regulate nutrient-stimulated survival and may regulate basal PKC activity not just in cells in the presence of high extracellular glucose but also in cells with high intrinsic glucose uptake and utilization. For decades it has been known that cancer cells have increased rates of glycolysis and that growth factors and lymphocyte activation stimulate glucose metabolism. Due to mutation or activation of specific transcriptional programs that may affect apoptosis, however, it has been impossible to discern the effects of glycolysis on apoptosis. In this study, we directly analyzed the effects of increased glucose utilization on apoptosis by expressing only essential glycolytic genes in nontransformed cell lines and primary lymphocytes. Our results demonstrate the existence of a novel antiapoptotic signaling pathway stimulated by glucose metabolism that can set a threshold for apoptotic death. While regulation of Mcl-1 levels appeared to be the critical regulator of cell death in the systems used here, GSK-3 has also been shown to influence a variety of targets to regulate cell function and fate (26). Thus, glucose-regulated PKC activation and inhibition of GSK-3 may affect a variety of cell types through distinct mechanisms. This study indicates that the long-acknowledged glycolytic metabo-

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lism of cancer cells and activated lymphocytes may directly influence cell survival and reveals a novel pathway for possible therapeutic intervention. ACKNOWLEDGMENTS We thank Sally Kornbluth (Duke University), Christopher Newgard (Duke University), Leta Nutt (Duke University), David R. Plas (University of Cincinatti), W. Kimryn Rathmell (University of North Carolina at Chapel Hill), Dennis Thiele (Duke University), Craig B. Thompson (University of Pennsylvania), and Tso-Pang Yao (Duke University) for helpful comments. We thank the Sarah W. Stedman Center for Nutrition and Metabolism for technical assistance. Glut1transgenic mice were a generous gift of Craig Thompson and the Abramson Family Cancer Research Institute (University of Pennsylvania). We are grateful for reagents provided by H. J. Brady (University College, London), D. Turner (University of Michigan), M. Spitaler and D. Cantrell (University of Dundee), M. Ehlers (Duke University), U. Maurer (Institut fu ¨r Molekulare Medizin und Zellforschung), and D. Green (St. Jude Children’s Research Hospital). This work was funded by a Howard Temin KO1 Career Development Award from the National Cancer Institute (to J.C.R.), a Sidney Kimmel Foundation for Cancer Research Scholar Award (to J.C.R.), a V Foundation for Cancer Research Scholar Award (to J.C.R.), and R01 AI063345 (to J.C.R.). REFERENCES 1. Babazono, T., J. Kapor-Drezgic, J. A. Dlugosz, and C. Whiteside. 1998. Altered expression and subcellular localization of diacylglycerol-sensitive protein kinase C isoforms in diabetic rat glomerular cells. Diabetes 47:668– 676. 2. Bental, M., and C. Deutsch. 1993. Metabolic changes in activated T cells: an NMR study of human peripheral blood lymphocytes. Magn. Reson. Med. 29:317–326. 3. Bentley, J., D. Itchayanan, K. Barnes, E. McIntosh, X. Tang, C. P. Downes, G. D. Holman, A. D. Whetton, P. J. Owen-Lynch, and S. A. Baldwin. 2003. Interleukin-3-mediated cell survival signals include phosphatidylinositol 3-kinase-dependent translocation of the glucose transporter GLUT1 to the cell surface. J. Biol. Chem. 278:39337–39348. 4. Bentley, J., I. Walker, E. McIntosh, A. D. Whetton, P. J. Owen-Lynch, and S. A. Baldwin. 2001. Glucose transport regulation by p210 Bcr-Abl in a chronic myeloid leukaemia model. Br. J. Haematol. 112:212–215. 5. Boise, L. H., M. Gonzalez-Garcia, C. E. Postema, L. Ding, T. Lindsten, L. A. Turka, X. Mao, G. Nunez, and C. B. Thompson. 1993. bcl-x, a bcl-2 related gene that functions as a dominant regulator of apoptotic cell death. Cell 74:597–608. 6. Bouillet, P., D. Metcalf, D. C. Huang, D. M. Tarlinton, T. W. Kay, F. Kontgen, J. M. Adams, and A. Strasser. 1999. Proapoptotic Bcl-2 relative Bim required for certain apoptotic responses, leukocyte homeostasis, and to preclude autoimmunity. Science 286:1735–1738. 7. Chi, M. M., J. Pingsterhaus, M. Carayannopoulos, and K. H. Moley. 2000. Decreased glucose transporter expression triggers BAX-dependent apoptosis in the murine blastocyst. J. Biol. Chem. 275:40252–40257. 8. Ciofani, M., and J. C. Zuniga-Pflucker. 2005. Notch promotes survival of pre-T cells at the beta-selection checkpoint by regulating cellular metabolism. Nat. Immunol. 6:881–888. 9. Conlon, I., and M. Raff. 1999. Size control in animal development. Cell 96:235–244. 10. Dang, C. V. 1999. c-Myc target genes involved in cell growth, apoptosis, and metabolism. Mol. Cell. Biol. 19:1–11. 11. Danial, N. N., C. F. Gramm, L. Scorrano, C. Y. Zhang, S. Krauss, A. M. Ranger, S. R. Datta, M. E. Greenberg, L. J. Licklider, B. B. Lowell, S. P. Gygi, and S. J. Korsmeyer. 2003. BAD and glucokinase reside in a mitochondrial complex that integrates glycolysis and apoptosis. Nature 424:952– 956. 12. Danial, N. N., and S. J. Korsmeyer. 2004. Cell death: critical control points. Cell 116:205–219. 13. Doughty, C. A., B. F. Bleiman, D. J. Wagner, F. J. Dufort, J. M. Mataraza, M. F. Roberts, and T. C. Chiles. 2006. Antigen receptor-mediated changes in glucose metabolism in B lymphocytes: role of phosphatidylinositol 3-kinase signaling in the glycolytic control of growth. Blood 107:4458–4465. 14. Edinger, A. L., and C. B. Thompson. 2002. Akt maintains cell size and survival by increasing mTOR-dependent nutrient uptake. Mol. Biol. Cell 13:2276–2288. 15. Fox, C. J., P. S. Hammerman, R. M. Cinalli, S. R. Master, L. A. Chodosh, and C. B. Thompson. 2003. The serine/threonine kinase Pim-2 is a transcriptionally regulated apoptotic inhibitor. Genes Dev. 17:1841–1854. 16. Frauwirth, K. A., J. L. Riley, M. H. Harris, R. V. Parry, J. C. Rathmell, D. R.

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17. 18. 19. 20.

21. 22. 23. 24.

25. 26. 27. 28. 29. 30. 31.

32. 33.

34.

35. 36. 37.

38. 39. 40.


Plas, R. L. Elstrom, C. H. June, and C. B. Thompson. 2002. The CD28 signaling pathway regulates glucose metabolism. Immunity 16:769–777. Frauwirth, K. A., and C. B. Thompson. 2004. Regulation of T lymphocyte metabolism. J. Immunol. 172:4661–4665. Gambhir, S. S. 2002. Molecular imaging of cancer with positron emission tomography. Nat. Rev. Cancer 2:683–693. Gatenby, R. A., and R. J. Gillies. 2004. Why do cancers have high aerobic glycolysis? Nat. Rev. Cancer 4:891–899. Gottlob, K., N. Majewski, S. Kennedy, E. Kandel, R. B. Robey, and N. Hay. 2001. Inhibition of early apoptotic events by Akt/PKB is dependent on the first committed step of glycolysis and mitochondrial hexokinase. Genes Dev. 15:1406–1418. Hanahan, D., and R. A. Weinberg. 2000. The hallmarks of cancer. Cell 100:57–70. Henquin, J. C. 2000. Triggering and amplifying pathways of regulation of insulin secretion by glucose. Diabetes 49:1751–1760. Inoki, K., T. Zhu, and K. L. Guan. 2003. TSC2 mediates cellular energy response to control cell growth and survival. Cell 115:577–590. Jensen, M. V., J. W. Joseph, O. Ilkayeva, S. Burgess, D. Lu, S. M. Ronnebaum, M. Odegaard, T. C. Becker, A. D. Sherry, and C. B. Newgard. 2006. Compensatory responses to pyruvate carboxylase suppression in islet betacells: preservation of glucose-stimulated insulin secretion. J. Biol. Chem. 281:22342–22351. Jones, R. G., D. R. Plas, S. Kubek, M. Buzzai, J. Mu, Y. Xu, M. J. Birnbaum, and C. B. Thompson. 2005. AMP-activated protein kinase induces a p53dependent metabolic checkpoint. Mol. Cell 18:283–293. Jope, R. S., and G. V. Johnson. 2004. The glamour and gloom of glycogen synthase kinase-3. Trends Biochem. Sci. 29:95–102. Khaled, A. R., and S. K. Durum. 2002. Lymphocide: cytokines and the control of lymphoid homeostasis. Nat. Rev. Immunol. 2:817–830. Koya, D., and G. L. King. 1998. Protein kinase C activation and the development of diabetic complications. Diabetes 47:859–866. Malliopoulou, V., C. Xinaris, I. Mourouzis, A. D. Cokkinos, N. Katsilambros, C. Pantos, E. Kardami, and D. V. Cokkinos. 2006. High glucose protects embryonic cardiac cells against simulated ischemia. Mol. Cell. Biochem. 284:87–93. Martin, D. E., and M. N. Hall. 2005. The expanding TOR signaling network. Curr. Opin. Cell Biol. 17:158–166. Maurer, U., C. Charvet, A. S. Wagman, E. Dejardin, and D. R. Green. 2006. Glycogen synthase kinase-3 regulates mitochondrial outer membrane permeabilization and apoptosis by destabilization of MCL-1. Mol. Cell 21:749– 760. Morissette, M. R., A. L. Howes, T. Zhang, and J. Heller Brown. 2003. Upregulation of GLUT1 expression is necessary for hypertrophy and survival of neonatal rat cardiomyocytes. J. Mol. Cell Cardiol. 35:1217–1227. Nutt, L. K., S. S. Margolis, M. Jensen, C. E. Herman, W. G. Dunphy, J. C. Rathmell, and S. Kornbluth. 2005. Metabolic regulation of oocyte cell death through the CaMKII-mediated phosphorylation of caspase-2. Cell 123:89– 103. Oishi, K., S. Kamakura, Y. Isazawa, T. Yoshimatsu, K. Kuida, M. Nakafuku, N. Masuyama, and Y. Gotoh. 2004. Notch promotes survival of neural precursor cells via mechanisms distinct from those regulating neurogenesis. Dev. Biol. 276:172–184. Opferman, J. T., H. Iwasaki, C. C. Ong, H. Suh, S. Mizuno, K. Akashi, and S. J. Korsmeyer. 2005. Obligate role of anti-apoptotic MCL-1 in the survival of hematopoietic stem cells. Science 307:1101–1104. Opferman, J. T., A. Letai, C. Beard, M. D. Sorcinelli, C. C. Ong, and S. J. Korsmeyer. 2003. Development and maintenance of B and T lymphocytes requires antiapoptotic MCL-1. Nature 426:671–676. Pandian, S. S., A. A. Sneddon, C. S. Bestwick, S. McClinton, I. Grant, K. W. Wahle, and S. D. Heys. 2001. Fatty acid regulation of protein kinase C isoforms in prostate cancer cells. Biochem. Biophys. Res. Commun. 283:806– 812. Peter-Riesch, B., M. Fathi, W. Schlegel, and C. B. Wollheim. 1988. Glucose and carbachol generate 1,2-diacylglycerols by different mechanisms in pancreatic islets. J. Clin. Investig. 81:1154–1161. Pinton, P., T. Tsuboi, E. K. Ainscow, T. Pozzan, R. Rizzuto, and G. A. Rutter. 2002. Dynamics of glucose-induced membrane recruitment of protein kinase C beta II in living pancreatic islet beta-cells. J. Biol. Chem. 277:37702–37710. Plas, D. R., J. C. Rathmell, and C. B. Thompson. 2002. Homeostatic control of lymphocyte survival: potential origins and implications. Nat. Immunol. 3:515–521.

4339

41. Puthalakath, H., D. C. Huang, L. A. O’Reilly, S. M. King, and A. Strasser. 1999. The proapoptotic activity of the Bcl-2 family member Bim is regulated by interaction with the dynein motor complex. Mol. Cell 3:287–296. 42. Raff, M. C. 1992. Social controls on cell survival and cell death. Nature 356:397–400. 43. Rathmell, J. C., R. L. Elstrom, R. M. Cinalli, and C. B. Thompson. 2003. Activated Akt promotes increased resting T cell size, CD28-independent T cell growth, and development of autoimmunity and lymphoma. Eur. J. Immunol. 33:2223–2232. 44. Rathmell, J. C., C. J. Fox, D. R. Plas, P. Hammerman, R. M. Cinalli, and C. B. Thompson. 2003. Akt-directed glucose metabolism can prevent Bax conformation change and promote growth factor-independent survival. Mol. Cell. Biol. 23:7315–7328. 45. Rathmell, J. C., M. G. Vander Heiden, M. H. Harris, K. A. Frauwirth, and C. B. Thompson. 2000. In the absence of extrinsic signals, nutrient utilization by lymphocytes is insufficient to maintain either cell size or viability. Mol. Cell 6:683–692. 46. Raval, A. P., K. R. Dave, D. Mochly-Rosen, T. J. Sick, and M. A. PerezPinzon. 2003. Epsilon PKC is required for the induction of tolerance by ischemic and NMDA-mediated preconditioning in the organotypic hippocampal slice. J. Neurosci. 23:384–391. 47. Ravikumar, B., A. Stewart, H. Kita, K. Kato, R. Duden, and D. C. Rubinsztein. 2003. Raised intracellular glucose concentrations reduce aggregation and cell death caused by mutant huntingtin exon 1 by decreasing mTOR phosphorylation and inducing autophagy. Hum. Mol. Genet. 12:985–994. 48. Selbie, L. A., C. Schmitz-Peiffer, Y. Sheng, and T. J. Biden. 1993. Molecular cloning and characterization of PKC iota, an atypical isoform of protein kinase C derived from insulin-secreting cells. J. Biol. Chem. 268:24296– 24302. 49. Semenza, G. L., D. Artemov, A. Bedi, Z. Bhujwalla, K. Chiles, D. Feldser, E. Laughner, R. Ravi, J. Simons, P. Taghavi, and H. Zhong. 2001. The metabolism of tumours: 70 years later. Novartis Found Symp. 240:251–260, 260– 264. 50. Smith, T. A. 2000. Mammalian hexokinases and their abnormal expression in cancer. Br. J. Biomed. Sci. 57:170–178. 51. Tan, S. L., and P. J. Parker. 2003. Emerging and diverse roles of protein kinase C in immune cell signalling. Biochem. J. 376:545–552. 52. Valverde, A. M., P. Navarro, M. Benito, and M. Lorenzo. 1998. H-ras induces glucose uptake in brown adipocytes in an insulin- and phosphatidylinositol 3-kinase-independent manner. Exp. Cell Res. 243:274–281. 53. Vander Heiden, M. G., D. R. Plas, J. C. Rathmell, C. J. Fox, M. H. Harris, and C. B. Thompson. 2001. Growth factors can influence cell growth and survival through effects on glucose metabolism. Mol. Cell. Biol. 21:5899– 5912. 54. Vary, T. C., and C. J. Lynch. 2006. Meal feeding stimulates phosphorylation of multiple effector proteins regulating protein synthetic processes in rat hearts. J. Nutr. 136:2284–2290. 55. Warburg, O. 1956. On the origin of cancer cells. Science 123:309–314. 56. Waterhouse, N. J., J. C. Goldstein, O. von Ahsen, M. Schuler, D. D. Newmeyer, and D. R. Green. 2001. Cytochrome c maintains mitochondrial transmembrane potential and ATP generation after outer mitochondrial membrane permeabilization during the apoptotic process. J. Cell Biol. 153:319–328. 57. Whiteside, C. I., and J. A. Dlugosz. 2002. Mesangial cell protein kinase C isozyme activation in the diabetic milieu. Am. J. Physiol. Renal Physiol. 282:F975–F980. 58. Wullschleger, S., R. Loewith, and M. N. Hall. 2006. TOR signaling in growth and metabolism. Cell 124:471–484. 59. Younes, M., R. W. Brown, M. Stephenson, M. Gondo, and P. T. Cagle. 1997. Overexpression of Glut1 and Glut3 in stage I nonsmall cell lung carcinoma is associated with poor survival. Cancer 80:1046–1051. 60. Yu, J. Y., J. Taylor, S. L. DeRuiter, A. B. Vojtek, and D. L. Turner. 2003. Simultaneous inhibition of GSK3alpha and GSK3beta using hairpin siRNA expression vectors. Mol. Ther. 7:228–236. 61. Zhang, J., P. Z. Anastasiadis, Y. Liu, E. A. Thompson, and A. P. Fields. 2004. Protein kinase C (PKC) betaII induces cell invasion through a Ras/Mek-, PKC iota/Rac 1-dependent signaling pathway. J. Biol. Chem. 279:22118– 22123. 62. Zhong, Q., W. Gao, F. Du, and X. Wang. 2005. Mule/ARF-BP1, a BH3-only E3 ubiquitin ligase, catalyzes the polyubiquitination of Mcl-1 and regulates apoptosis. Cell 121:1085–1095.