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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Nature. Author manuscript; available in PMC Mar 25, 2013.
Published in final edited form as:
PMCID: PMC3607316
NIHMSID: NIHMS448813

AMPK regulates NADPH homeostasis to promote tumour cell survival during energy stress

Abstract

Overcoming metabolic stress is a critical step for solid tumour growth1,2. However, the underlying mechanisms of cell death and survival under metabolic stress are not well understood. A key signalling pathway involved in metabolic adaptation is the liver kinase B1 (LKB1)–AMP-activated protein kinase (AMPK) pathway2,3. Energy stress conditions that decrease intracellular ATP levels below a certain level promote AMPK activation by LKB1. Previous studies showed that LKB1-deficient or AMPK-deficient cells are resistant to oncogenic transformation and tumorigenesis46, possibly because of the function of AMPK in metabolic adaptation. However, the mechanisms by which AMPK promotes metabolic adaptation in tumour cells are not fully understood. Here we show that AMPK activation, during energy stress, prolongs cell survival by redox regulation. Under these conditions, NADPH generation by the pentose phosphate pathway is impaired, but AMPK induces alternative routes to maintain NADPH and inhibit cell death. The inhibition of the acetyl-CoA carboxylases ACC1 and ACC2 by AMPK maintains NADPH levels by decreasing NADPH consumption in fatty-acid synthesis and increasing NADPH generation by means of fatty-acid oxidation. Knockdown of either ACC1 or ACC2 compensates for AMPK activation and facilitates anchorage-independent growth and solid tumour formation in vivo, whereas the activation of ACC1 or ACC2 attenuates these processes. Thus AMPK, in addition to its function in ATP homeostasis, has a key function in NADPH maintenance, which is critical for cancer cell survival under energy stress conditions, such as glucose limitations, anchorage-independent growth and solid tumour formation in vivo.

The lack of LKB1 or AMPK activation rendered cancer cells more sensitive to cell death induced by glucose deprivation5,79 (Supplementary Fig. 1). However, the mechanism by which the failure to activate AMPK accelerates cancer cell death during energy stress remains to be explained. Our results demonstrate that the effect of AMPK does not involve p53 or mTORC1, which were implicated in the LKB1–AMPK-mediated regulation of cell survival during glucose deprivation8,10. In both control A549 cells (A549-Vect) and dominant-negative p53 (p53DN)-expressing A549 cells (A549-p53DN), LKB1 reconstitution restored AMPK activation, as measured by ACC phosphorylation, and inhibited glucose-starvation-induced cell death to a similar extent (Fig. 1a, b). mTORC1 inhibition with rapamycin also did not affect the sensitivity of A549 cells to glucose deprivation (Fig. 1b).

Figure 1
The failure to activate AMPK accelerates NADPH depletion, oxidative stress and cell death in the absence of glucose

Replacement of glucose with the non-metabolizable glucose analogues 2-deoxyglucose (2DG) or 5-thioglucose (5TG) revealed that only 2DG protected LKB1-deficient cancer cells (A549 and HeLa) from glucose-starvation-induced cell death (Fig. 1b and Supplementary Fig. 2b). Unlike 5TG, 2DG strongly induced the activation of AMPK, even in LKB1-deficient cells (Fig. 1a and Supplementary Fig. 2a). This activation occurred by means of a poorly understood mechanism that is dependent on hexokinase (Supplementary Fig. 3). The results suggest that, by activating AMPK, 2DG inhibits cell death during glucose deprivation. However, LKB1 reconstitution in A549 cells induced higher AMPK activation than 2DG (Fig. 1a), yet 2DG protected the cells slightly better than LKB1 (Fig. 1b), implying that 2DG could protect cells by both AMPK-dependent and AMPK-independent mechanisms.

Glucose limitations could induce oxidative stress by decreasing NADPH generation in the pentose phosphate pathway (PPP) (Fig. 1c). NADPH is required for the regeneration of reduced glutathione (GSH), which is used by glutathione peroxidase (GPX) to eliminate H2O2 (Fig. 1c). We therefore speculated as follows: first, that the failure to activate AMPK by glucose deprivation accelerates cell death through oxidative stress mediated by decreased PPP flux and NADPH/GSH generation; second, that AMPK activation under these conditions is required to inhibit cell death by decreasing oxidative stress; and third, that 2DG protects the cells by both AMPK activation and partial utilization in the PPP11 (Fig. 1c).

We first established that decreased PPP flux and increased oxidative stress are the cause of the cell death. Glucose-6-phosphate dehydrogenase (G6PD) knockdown accelerated cell death in low glucose (Fig. 1d) and even in the absence of glucose (Supplementary Fig. 4a, b). Glucose deprivation rapidly depleted NADPH/GSH and elevated the H2O2 level in control cells, which were further affected by G6PD knockdown (Supplementary Fig. 4c–e). Finally, the antioxidants N-acetylcysteine (NAC) and catalase inhibited cell death in LKB1-deficient or AMPK-deficient cells (Fig. 1e and Supplementary Figs 1c, 5 and 6).

We next examined the function of AMPK in redox regulation by using A549-Vect and A549-LKB1 cells. Unlike A549-Vect cells, A549-LKB1 cells maintained NADP+/NADPH and GSSG/GSH ratios and prevented the increase in the H2O2 level during glucose starvation (Fig. 1f, g and Supplementary Fig. 7). Expression of p53DN showed a faster depletion of NADPH and increase in H2O2 level (Fig. 1f, g), explaining increased cell death (Fig. 1e). The superoxide (O2) level was not increased (Fig. 1h), suggesting that the increased H2O2 level is due to NADPH depletion and impaired H2O2 detoxification. LKB1 reconstitution neither decreased the O2 level (Fig. 1h) nor changed that of catalase (Fig. 1a), further suggesting that NADPH maintenance is the predominant mechanism by which AMPK prevents oxidative stress. Consistently, LKB1 or AMPKα1 knockdown in MCF7 or H1703 cells significantly increased H2O2 levels, but not those of O2, during glucose deprivation (Supplementary Fig. 8). Similarly, AMPKα-knockout (AMPKα-KO) murine embryonic fibroblasts (MEFs) failed to maintain their NADP+/NADPH ratio and low H2O2 level after glucose starvation (Fig. 1i). Finally, as we had speculated, 2DG maintained NADPH, GSH and H2O2 levels and protected from cell death largely by means of AMPK activation and to a smaller extent by partial utilization in the PPP (Supplementary Fig. 4). This could explain why 2DG protects from cell death slightly better than LKB1 despite higher activation of AMPK by LKB1 (Fig. 1b). Thus, the combination of decreased NADPH generation by the PPP and impaired AMPK activation during glucose deprivation in LKB1-deficient or AMPK-deficient cells accelerates NADPH depletion and H2O2 elevation, eventually causing cell death.

Next we investigated the mechanism by which AMPK maintains the NADPH level in the absence of glucose. The intracellular NADPH level is determined by the difference between its production and its consumption. NADPH is generated from the PPP and mitochondrial metabolism, and is consumed mainly during H2O2 detoxification by GPX and peroxiredoxin (PRX) and fatty-acid synthesis (FAS) (Fig. 2a). Under limited glucose supply, the major NADPH source is mitochondrial metabolism, which is supported by fatty-acid oxidation (FAO). Metabolites provided by FAO to the tricarboxylic acid cycle generate malate and citrate, the substrates of NADPH-producing malic enzyme and isocitrate dehydrogenase, respectively. AMPK regulates fatty-acid metabolism through the phosphorylation and inhibition of ACC1 and ACC2, which in turn inhibit FAS and activates FAO, respectively12. Both ACC1 and ACC2 generate malonyl-CoA, the precursor of FAS and a potent inhibitor of carnitine palmitoyltransferase 1 (CPT1), the rate-limiting enzyme in FAO13 (Fig. 2a). We therefore reasoned that AMPK might regulate NADPH homeostasis by inhibiting ACC1 and ACC2.

Figure 2
ACC2 ablation recapitulates AMPK activation, maintaining the NADPH level and decreasing the H2O2 level during glucose deprivation

We first determined whether targeting ACC1 or ACC2 inhibits cell death, the accumulation of H2O2 and the depletion of NADPH observed during glucose deprivation. Targeting either ACC1 or ACC2 in A549 cells by short interfering RNAs (siRNAs) demonstrated that only ACC2 knockdown significantly inhibited cell death and H2O2 accumulation, without decreasing O2 (Supplementary Fig. 9). We therefore generated stable cell lines expressing ACC2-specific short hairpin RNA (shRNA) (Supplementary Fig. 10a). ACC2 knockdown in A549 cells maintained the NADP+/NADPH ratio (Fig. 2b) and the GSSG/GSH ratio (Fig. 2c), inhibited the accumulation of H2O2 (Fig. 2d) and prevented cell death (Fig. 2e). Similar results were obtained in HeLa, MCF7-LKB1sh and H1703-LKB1sh cells (Supplementary Fig. 10b–d). Targeting either ACC1 or ACC2 in AMPKα-KO MEFs significantly decreased the H2O2 level during glucose starvation (Supplementary Fig. 11). The inability of ACC1 knockdown in A549 cells to decrease the H2O2 level during glucose starvation was probably because FAS inhibition in these cells occurs to a similar extent regardless of LKB1 expression or ACC1 knockdown (Supplementary Fig. 12). In contrast, A549-LKB1 and A549-ACC2sh cells showed a marked increase in FAO, explaining why ACC2 knockdown was able to decrease H2O2 levels but ACC1 knockdown was not (Supplementary Fig. 12). Consistently, overexpression of the constitutively active ACC2(S212A) mutant significantly inhibited FAO and sensitized MCF7 cells to glucose-deprivation-mediated cell death, and partly blocked protection by 2DG in HeLa cells (Supplementary Fig. 13). Furthermore, short-term exposure to the FAS inhibitor C75, which also activates CPT1, mimicking the effects of AMPK on fatty-acid metabolism, lowered the NADP+/NADPH ratio and protected A549 and HeLa cells during glucose deprivation (Fig. 2b and Supplementary Fig. 14a, b). However, because C75 inhibits FAS downstream of ACC1, long-term treatment with C75 leads to the cytotoxic accumulation of malonyl-CoA14. Indeed, etomoxir, a CPT1 inhibitor, abrogated the short-term effect of C75 without affecting the effect of NAC (Supplementary Fig. 14c). These results indicate that the short-term protective effect of C75 was largely due to the activation of CPT1 and the acceleration of FAO. Furthermore, treatment with the ACC inhibitor TOFA protected from cell death, whereas the malate supplement alone could not (Supplementary Fig. 15a). However, the combination of TOFA and malate further protected from cell death (Supplementary Fig. 15a). These results suggest that malate alone is not sufficient to induce NADPH accumulation, because NADPH could still be consumed by FAS. Thus, when FAS is inhibited by TOFA, malate can promote sufficient NADPH accumulation to inhibit cell death during glucose deprivation. Finally, the protective effect of ACC2 knockdown was abrogated by buthionine sulfoximine, which depletes GSH, but not by nicotinamide (NAM), which inhibits Sirt1, excluding a possible involvement of the NAD+–Sirt1 pathway15 (Supplementary Fig. 15b).

Like glucose starvation, matrix detachment elicits energy stress followed by elevated H2O2 levels and cell death16. Indeed, matrix detachment inhibited glucose uptake in A549 cells (Supplementary Fig. 16), and markedly activated AMPK in A549-LKB1 cells (Fig. 3a). AMPK was also activated in A549 cells but to a much smaller extent than in A549-LKB1 cells (Fig. 3a), which is dependent on calmodulin-dependent protein kinase kinase (CaMKK; Fig. 3b). We therefore tested whether AMPK activation is required for redox regulation during matrix detachment and anchorage-independent growth, which is a hallmark of cancer cells. Matrix detachment significantly increased the H2O2 level in A549-Vect cells in comparison with A549-LKB1 cells, regardless of p53 status (Fig. 3c). CaMKK inhibition in A549 cells further elevated the H2O2 level during matrix detachment (Fig. 3d), supporting a key function for AMPK in redox regulation during this process. The results were confirmed in MCF7 cells with LKB1 knockdown or AMPKα1 knockdown (Supplementary Fig. 17). The impaired AMPK activation and the higher H2O2 level in matrix-detached A549 cells were correlated to the extent of NADPH depletion (Fig. 3e). The high NADP+/NADPH ratio in A549 cells was further increased after matrix detachment, whereas the low NADP+/NADPH ratio was maintained in A549-LKB1 cells (Fig. 3e).

Figure 3
AMPK-mediated inhibition of ACC1 is required to maintain the NADPH and reactive oxygen species levels after matrix detachment

We next investigated whether ACCs mediate the effect of AMPK during matrix detachment. Knockdown of ACC1 by siRNA, but not that of ACC2, blocked the increase in the H2O2 level by matrix detachment (Supplementary Fig. 18). We therefore used A549 cells expressing ACC1-specific shRNA (Supplementary Fig. 19) and confirmed that ACC1 knockdown markedly decreased the NADP+/NADPH ratio and H2O2 level (Fig. 3f, g). Finally, the ACC inhibitor TOFA, but not the mTORC1 inhibitor rapamycin, decreased the H2O2 level (Supplementary Fig. 20). LKB1 expression had a more pronounced effect on FAS inhibition than on FAO increase (Supplementary Fig. 21a). This effect was recapitulated by ACC1 knockdown (Supplementary Fig. 21b), explaining why ACC1 knockdown could decrease the H2O2 level.

We then assessed whether redox regulation by ACCs has a function in anchorage-independent growth. Consistent with previous observations16, we found that treatment of A549 cells and AMPKα-KO-RasV12 MEFs with NAC substantially increased the number of colonies (Fig. 4a and Supplementary Fig. 22). Inhibition of CaMKK markedly inhibited anchorage-independent growth, which was rescued by NAC treatment (Fig. 4a and Supplementary Fig. 22a). Targeting either ACC1 or ACC2 substantially increased the number of colonies on soft agar and recapitulated the effect of NAC (Fig. 4b, c and Supplementary Fig. 23). However, the average colony size was increased only by ACC1 knockdown (Fig. 4b, c), which may reflect the predominant function of ACC1 in controlling the H2O2 level after matrix detachment.

Figure 4
AMPK-mediated inhibition of ACC1 or ACC2 promotes anchorage-independent growth and solid tumour formation in vivo

To assess further the function of ACCs in anchorage-independent growth, we overexpressed the ACC1(S79A) and ACC2(S212A) mutants in two LKB1-proficient cell lines, MCF7 and H1703. Both mutants increased FAS and the H2O2 level after matrix detachment (Fig. 4d and Supplementary Fig. 24a), and potently inhibited anchorage-independent growth, which was partly rescued by NAC (Fig. 4e and Supplementary Fig. 24b, c). These results indicate that the inhibition of either ACC1 or ACC2 by AMPK is required for anchorage-independent growth by means of redox regulation. In contrast, ACC1 knockdown or ACC2 knockdown in LKB1-reconstituted HeLa cells inhibited anchorage-independent growth (Supplementary Fig. 25a). Thus, when AMPK is activated, further inhibition of ACC1 or ACC2 could not enhance tumorigenesis, instead attenuating it.

During the formation of a solid tumour, cells undergo metabolic stress including glucose deprivation and matrix detachment. Indeed, it has been shown that AMPKα-KO-RasV12 MEFs are severely impaired in their ability to form tumours in vivo6 and that AMPK is activated during the early stages of solid tumour formation17. Thus, to determine whether ACCs have a function in solid tumour formation in vivo, we performed xenograft assays using A549 and AMPKα-KO-RasV12 MEFs expressing shRNAs targeting ACC1 or ACC2. Knockdown of ACC1 or ACC2 significantly enhanced tumour formation in vivo (Fig. 4f, g); the latter had a more pronounced effect on tumour growth than the former. However, neither ACC1 knockdown or ACC2 knockdown in A549-LKB1 cells had much effect on tumour growth (Supplementary Fig. 25b), further suggesting that physiological inhibition of ACC by AMPK, but not enhanced inhibition, is required to promote solid tumour growth. To assess these results further, we performed orthotopic transplantation using MCF7 cells. The knockdown of either LKB1 or AMPKα1 in MCF7 cells significantly inhibited orthotopic tumour growth (Supplementary Fig. 26a). To test the function of ACC1 and ACC2 phosphorylation by AMPK in tumour growth, MCF7 cells expressing either ACC1(S79A) or ACC2(S212A) were subjected to orthotopic transplantation. Consistent with the in vitro results (Fig. 4e), ACC2(S212A) expression significantly inhibited solid tumour growth; ACC1(S79A) expression also inhibited tumour growth, although to a smaller extent, under two different experimental conditions (Fig. 4h and Supplementary Fig. 26b). Taken together, these results demonstrate that NADPH maintenance through AMPK–ACC1/ACC2 is critical for solid tumour growth in vivo (Fig. 4i). It was previously reported that ACC2 expression is significantly downregulated in papillary thyroid cancer18, supporting a tumour-suppressor function for ACC2 in certain contexts. Moreover, consistent with our results, it was shown that overexpression of CPT1 promotes solid tumour growth through the activation of FAO19.

Our results are not inconsistent with results showing that inhibition of FAS by the knockdown of fatty acid synthase (FASN) or ATP-citrate lyase (ACLY) inhibits tumorigenesis20,21 because, unlike the inhibition of ACC, the inhibition of FASN or ACLY exerts additional cytotoxic effects. These cytotoxic effects seem to be through the accumulation of malonyl-CoA but not through the direct inhibition of FAS itself14,22,23, and through the inhibition of acetylation without decreasing lipid contents24,25. Our results seem paradoxical because of the tumour suppressor activity of LKB1–AMPK, partly through mTORC1 inhibition3. We propose that during glucose limitations or matrix depletion, AMPK activation, at physiological levels, is required for NADPH homeostasis, which surpasses the requirement for mTORC1 activity. Combating energy stress conditions by AMPK is particularly important in the early stages of solid tumour formation when cells migrate to the lumen, or during metastasis when cells migrate from the primary tumour to a different location. However, AMPK activation is probably occurring in a temporal manner, because FAO could also increase the ATP level (Supplementary Fig. 27), which would eventually inhibit AMPK. Our results therefore do not necessarily contradict the possibility that prolonged and robust AMPK activation inhibits cancer cell proliferation. In fact, they suggest that a combination of metabolic inhibitors, such as 2DG or metformin, and ACC activators could synergistically decrease cancer cell survival by concurrently inhibiting mTORC1 and the pro-survival activity of AMPK. This combination could be more effective in LKB1-null cancer cells.

Our findings could explain why AMPK-deficient cells are resistant to oncogenic transformation4,6. At the organismal level our results may explain why patients with Peutz–Jeghers syndrome, who have an inherited deficiency of LKB1, and most mouse models of LKB1 deficiency develop only benign tumours4. Although somatic mutations in LKB1 are rare in most cancers, the mutations are prevalent in certain cancers, such as non-small cell lung carcinoma and cervical carcinoma3. In mouse models, deficiency in LKB1 also promotes Ras-induced lung tumorigenesis26. One possible explanation is that certain microenvironmental factors may enable AMPK activation in the absence of LKB1 through other upstream activators, such as CaMKK, as shown in Fig. 3b. In addition, LKB1 deficiency may affect other multiple downstream effectors of LKB1 (ref. 26) that could circumvent the requirement for the LKB1–AMPK pathway during the early stages of solid tumour formation.

AMPK is known to maintain intracellular ATP level under conditions of energy stress. Consistently, we found that AMPK maintains ATP level in addition to NADPH level under these conditions (Supplementary Fig. 27a). However, NAC, which protected from cell death, did not restore ATP level during glucose starvation (Supplementary Fig. 27b), indicating that NADPH maintenance rather than ATP maintenance is the predominant mechanism by which AMPK promotes cell survival during metabolic stress (Fig. 4j).

Our study shows that under conditions of energy stress, when NADPH generation from the PPP is impaired, AMPK activation is required for the maintenance of NADPH level by inhibiting ACC1 and/or ACC2 (Fig. 4i, j). This function of AMPK is critical for cancer cell survival during metabolic stress, which can occur in the solid tumour microenvironment.

METHODS

Cell culture, transfection, transduction and western blotting

MI5-4 CHO cells (a gift from J. Willson) were cultured in α-MEM supplemented with 2 mM glutamine and 10% FBS (Gemini). All other cells were cultured in DMEM (Invitrogen) containing 10% FBS. For the glucose starvation experiments, the cells were washed with PBS and cultured in glucose-free DMEM(Invitrogen) containing 10% dialysed FBS (Gemini). For suspension culture, the cells were plated on poly-HEMA (2-hydroxyethyl methacrylate)-coated plates. For the transient transfection of the siRNAs, 2 × 105 A549 cells or 105 AMPKα1/α2-DKO MEFs immortalized with SV40 large T (ref. 6) (a gift from B. Viollet) were plated in 6-cm plates 1 day before transfection with 500 pmol of siRNA using Lipofectamine 2000 (Invitrogen). At 48 h after transfection, the cells were replated in six-well plates for western blot analysis or in 12-well plates for measurements of cell death and reactive oxygen species. The infections with lentiviruses and retroviruses were conducted overnight, and infected cells were selected with blasticidin, puromycin or hygromycin under the following conditions: 25 µg ml−1 blasticidin for 6 days or 0.5 µg ml−1 puromycin for 3 days for A549 cells; 10 µg ml−1 blasticidin for 4 days for HeLa cells; 15 µg ml−1 blasticidin for 4 days or 1 µg ml−1 puromycin for 4 days for H1703 cells; 10 µg ml−1 blasticidin for 4 days or 1 µg ml−1 puromycin for 4 days for MCF7 cells; 10 µg ml−1 blasticidin for 4 days or 100 µg ml−1 hygromycin for 6 days for MEF-AMPKα-KO. For the western blot analyses, protein extracts were prepared in lysis buffer, as described previously27.

Reagents and antibodies

5-Thio-d-glucose was purchased from ICN Biomedical. DCF and DHE were purchased from Molecular Probes. [3H]Acetate, [9,10-3H]palmitate and 2-deoxy[3H]glucose were obtained from PerkinElmer. STO-609 and Ku-55933 were purchased from Calbiochem. All other chemicals were purchased from Sigma-Aldrich unless otherwise indicated. Antibodies against LKB1, AMPKα1/2, ACC, P-ACC and HK2 were purchased from Cell Signaling, and antibodies specific for ACC2, catalase and α-tubulin were purchased from Sigma-Aldrich. The G6PD antibody was purchased from Bethyl Lab, and the GSK3 antibody was from QCB.

Plasmids, RNA-mediated interference (RNAi) and viruses

The complementary DNAs encoding ACC1 and ACC2 were provided by M. R. Montminy. Site-directed mutagenesis of ACC1 (S79A) and ACC2 (S212) was performed with the QuickChange II XL Kit (Stratagene), as recommended by the manufacturer. The mutants were subcloned into the pLent6-D-TOPO vector (Invitrogen). SMART-pool siRNAs targeting human ACC1 and ACC2 and mouse ACC1 and ACC2 were purchased from Dharmacon (hACC1: 5′-gatgtgagcctgcggaata-3′, 5′-ccacttggctgagcgattg-3′, 5′-gcaattagattcgttgtca-3′, 5′-gatcttagcggaccaatat-3′, hACC2: 5′-gatacatgatcacggatat-3′, 5′-gaagagaggtctacacatc-3′, 5′-aggaagaggttgacagtta-3′, 5′-cctcgtagatgtggaatta-3′, mACC1: 5′-caagactgatggcgatatt-3′, 5′-gaaaatagactcacaacga-3′, 5′-ggaagttaatccagtatat-3′, 5′-tcaatgtgatgaatggata-3′, mACC2: 5′-gtggtgacgggacgagcaa-3′, 5′-gagattaagttccggaaga-3′, 5′-tcaattatctgaagcggga-3′, 5′-gaagagaggtctacacgtc-3′). The constructs (pENTR-U6) expressing an shRNA targeting LacZ, G6PD, ACC1 or ACC2 were generated with the BLOCK-iT U6 RNAi Entry Vector Kit (Invitrogen). The shRNA sequences used were 5′-GCCTCAGTGCCACTTGACA-3′ for hG6PD28, 5′-TACAAGGGATACAGGTATTTA-3′ for hACC1 2, 5′-GTGGAGCTGATTGTGGACATT-3′ for hACC2 1, 5′-GACGGCCTTAGACAATACAAA-3′ for hACC2 2, 5′-GCAGATTGCCAACATCCTAGA-3′ for mouse ACC1, and 5′-GTGGTGACGGGACGAGCAA-3′ for mouse ACC2. The shRNA expression cassettes were transferred to a lentiviral vector (plenti6) with the use of the BLOCK-iT Lentiviral RNAi Expression System (Invitrogen). The lentiviral constructs (pLKO.1) expressing shRNAs for a non-targeted control (5′-CAACAAGATGAAGAGCACCAA-3′) and hLKB1 (5′-GCCAACGTGAAGAAGGAAATT-3′) were purchased from Sigma-Aldrich. The lentiviral vector expressing the AMPKα1-specific shRNA with the sequence 5′-CTATGCTGCACCAGAAGTA-3′ was a gift from M. Karin, and was described previously29. All lentiviruses were produced with the BLOCK-iT Lentiviral RNAi Expression System (Invitrogen), as recommended by the manufacturer. To produce retroviruses expressing dominant-negative p53 (p53-DN) or constitutively active Ras (RasV12), the pBabe-Puro-GSE56 plasmid or the pBabe-hygro-RasV12 plasmid was transfected into amphotropic or ecotropic Phoenix cells, respectively, as described previously30.

Cell death assay

In most of the experiments, apoptotic cell death was measured by using DAPI staining, as described previously27,31. Cells were plated at a low density ((0.7–1) × 105 cells per well in a 12-well plate); on the next day, the cells were washed with PBS and cultured in glucose-free medium supplemented with dialysed FBS. At each time point, the cells were fixed by the direct addition of formaldehyde (final concentration 12%) to the culture medium. After overnight fixation, the cells were stained for 5 min with DAPI (1 µg ml−1), and then left in PBS. The cells were detected with fluorescence microscopy, and cells with condensed and/or fragmented chromatin indicative of apoptosis were counted as dead cells. For MCF7 cells, a trypan blue exclusion assay was performed to measure cell death.

Assays of reactive oxygen species

The intracellular levels of H2O2 and O2 were measured with DCF and DHE, respectively. Cells (105) were plated in a 12-well plate and treated with DCF or DHE for 30 min. The cells were then washed with PBS and collected as single-cell suspensions. Fluorescence was detected by flow cytometry.

NADPH, GSH and ATP assays

The intracellular levels of NADPH and total NADP (NADPH+NADP+) were measured with previously described enzymatic cycling methods, with modifications32,33. In brief, 1.8 × 106 cells were plated in 10-cm dishes; on the next day, the cells were lysed in 400 µl of extraction buffer (20 mM nicotinamide, 20 mM NaHCO3, 100 mM Na2CO3) and centrifuged. For NADPH extraction, 150 µl of the supernatant was incubated at 60 °C for 30 min. Next, 160 µl of NADP-cycling buffer (100 mM Tris-HCl pH 8.0, 0.5 mM thiazolyl blue, 2 mM phenazine ethosulfate, 5 mM EDTA) containing 1.3U of G6PD was added to a 96-well plate containing 20 µl of the cell extract. After a 1-min incubation in the dark at 30 °C, 20 µl of 10 mM glucose 6-phosphate (G6P) was added to the mixture, and the change in absorbance at 570 nm was measured every 30 s for 4 min at 30 °C with a microplate reader. The concentration of NADP+ was calculated by subtracting[NADPH] from [total NADP]. The intracellular levels of GSH and total glutathione (GSSG + GSH) were measured with the use of enzymatic cycling methods, as described previously34. The intracellular level of ATP was measured with an ATPlite assay kit (Perkin Elmer).

Metabolism assays

Fatty-acid synthesis and oxidation were measured as described previously35,36. In brief, 105 cells were seeded in a 12-well plate for 1 day. For the glucose starvation experiments, the cells were incubated in glucose-free medium for 2 h, and either [3H]acetate (for FAS) or [9,10-3H]palmitate (for FAO) was added for a further 3 h. For matrix detachment, 105 cells were seeded on poly-HEMA-coated 12-well plates for 2 h, and either [3H]acetate or [9,10-3H]palmitate was added for a further 3 h. For the measurement of FAS, total lipids were extracted from [3H]acetate-treated cells with chloroform/methanol. For the measurement of FAO, the medium from [9,10-3H]palmitate-treated cells was collected to recover 3H2O using Dowex 1X8-200 columns. 3H-labelled lipids and water were quantified by liquid scintillation counting. Glucose uptake was measured with 2-deoxy[3H]glucose.

Soft-agar assay

A total of 3 × 104 cells were suspended in DMEM (10% FBS, 5 mM glucose) containing 0.35% agarose and layered on solidified medium containing 0.7% agarose in six-well plates. For MCF7 cells, 1 mM sodium pyruvate was added to the medium. After solidification, the top layer was covered with the medium. When necessary, 2 mM NAC or 5 µg ml−1 STO-609 was added to each layer and the cover medium. The medium was replaced every week. Images were taken after 3–4 weeks and analysed with ImageJ software.

Xenograft assay

Male and female athymic nude mice (6–8 weeks old) were purchased from Charles River Laboratories. A549 cells (2 × 106 per 0.1 ml of PBS) or AMPKα-KO-MEFs-RasV12 cells (5 × 106 per 0.1 ml of PBS) expressing the LacZ-specific, ACC1-specific or ACC2-specific shRNA were injected subcutaneously into both the left and right flanks of each mouse. A xenograft assay using A549 cells was performed twice. MCF7 cells were injected orthotopically into the mammary fat pads (two positions per mouse) in two different conditions, namely the absence (Supplementary Fig. 25) and presence (Fig. 4g) of 10% Matrigel in cell suspensions. Before injection, 17β-oestradiol pellets (1.7 mg/pelleted, 60-day release; Innovative Research of America) were implanted in each mouse. The tumour size was measured every week, and the tumour volume was calculated with the equation V (in mm3) = a × b2/2, where a is the longest diameter and b is the shortest diameter. When the tumour size reached the end-point criterion (a diameter greater than 2 cm), the mouse was killed. All animal experiments were performed in accordance with the animal care policies of the University of Illinois at Chicago and were approved by the Animal Care Committee of the University of Illinois at Chicago.

Statistical analysis

All statistical analysis was performed with unpaired two-tailed Student’s t-tests, and all data are expressed as means and s.e.m. for at least three independent experiments, unless otherwise indicated.

Supplementary Material

Supp. Data

Acknowledgements

We thank B. Viollet for the AMPK-KO MEFs, M. R. Montminy for the ACC complementary DNA, and G. Hatzivassiliou for comments on the manuscript. This work was supported by grants CA090764, AG016927 and AG025953 from the National Institutes of Health, by the Chicago Biomedical Consortium with support from The Searle Funds at The Chicago Community, and by grant P60DK20595 to the Diabetes Research and Training Center, University of Chicago (to N.H.).

Footnotes

Supplementary Information is linked to the online version of the paper at www.nature.com/nature.

Author Contributions S.-M.J. and N.H. designed the experiments. S.-M.J. performed the experiments. N.S.C. provided advice. S.-M.J. and N.H. analysed the data and wrote the paper.

Reprints and permissions information is available at www.nature.com/reprints. The authors declare no competing financial interests. Readers are welcome to comment on the online version of this article at www.nature.com/nature

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