The primary methyl group donor S-adenosylmethionine (SAM) is important for a plethora of cellular pathways including methylation of nucleic acids, proteins, and the 5′ cap structure of mRNAs, as well as biosynthesis of phospholipids and polyamines. In addition, because it is the cofactor for chromatin methylation, SAM is an important metabolite for the establishment and maintenance of epigenetic marks. Here, we demonstrate that cells halt proliferation when SAM levels become low. Cell cycle arrest occurs primarily in the G1 phase of the cell cycle and is accompanied by activation of the mitogen-activated protein kinase p38 (MAPK14) and subsequent phosphorylation of MAPK-activated protein kinase-2 (MK2). Surprisingly, Cdk4 activity remains high during cell cycle arrest, whereas Cdk2 activity decreases concomitantly with cyclin E levels. Cell cycle arrest was induced by both pharmacological and genetic manipulation of SAM synthesis through inhibition or downregulation of methionine adenosyltransferase, respectively. Depletion of methionine, the precursor of SAM, from the growth medium induced a similar cell cycle arrest. Unexpectedly, neither methionine depletion nor inhibition of methionine adenosyltransferase significantly affected mTORC1 activity, suggesting that the cellular response to SAM limitation is independent from this major nutrient-sensing pathway. These results demonstrate a G1 cell cycle checkpoint that responds to limiting levels of the principal cellular methyl group donor S-adenosylmethionine. This metabolic checkpoint might play important roles in maintenance of epigenetic stability and general cellular integrity.
In order to maintain DNA integrity and faithfully transmit genetic information, mammalian cells have evolved a plethora of cell cycle checkpoints to ensure cell cycle arrest when conditions are not suitable for cell division (Hartwell and Weinert, 1989). Limiting levels of low-molecular-mass nutrients was noted to inhibit cell proliferation more than thirty years ago (Holley and Kiernan, 1974; Pardee, 1974). The simplest explanation of this phenotype is substrate limitation; cells simply cannot grow when nutrient building blocks are short in supply. Alternatively, nutrient levels might be integrated in signaling pathways connected to cell cycle control as a means to protect cellular integrity during nutrient limitation. Metabolic checkpoints that respond to low glucose or low amino acid levels have been reported to be mediated by AMPK (AMP-activated kinase) through the p53 and mTORC1 (mammalian target of rapamycin complex 1) signaling pathways (Gwinn et al., 2008; Jones et al., 2005). Disruption of metabolic checkpoints mediated by the AMPK-mTORC1 pathway during either glucose or amino acid crisis has been shown to decrease cell viability.
Among the countless metabolites in cells, one particularly interesting metabolite with an undefined link to cell cycle is S-adenosylmethionine (SAM). SAM is synthesized from methionine and the adenosine moiety of ATP by methionine adenosyltransferase (MAT). The activated methyl group and the aminopropyl part of SAM are used in numerous cellular reactions including DNA, RNA, protein and lipid methylation, as well as polyamine synthesis, making SAM the most versatile metabolite second to ATP (Loenen, 2006). Most importantly, as the cofactor for all chromatin methylation, SAM is required for faithful maintenance and transmission of epigenetic marks. It is plausible that cells would develop a system that monitors SAM concentrations and stops S phase initiation if SAM levels are too low to support proper chromatin re-methylation. This idea is reminiscent of the SAM checkpoint proposed in the model organism S. cerevisiae (Kaiser et al., 2006). Consistent with this notion, targeted inhibition of MAT with a chemical inhibitor or shRNA knockdown was shown to inhibit leukemia cell proliferation and induce apoptosis (Attia et al., 2008; Jani et al., 2009), suggesting not only the existence of a SAM checkpoint in mammalian cells but also its potential as a therapeutic target. Furthermore, recent reports indicate breast and prostate cancer cells suffer a G1 cell cycle arrest when cultured in medium where methionine is replaced with its metabolic precursor homocysteine (Booher et al., 2012; Lu and Epner, 2000), probably as a consequence of reduced flux through the homocysteine-methionine-SAM metabolic axis, which results in insufficient SAM to support cell cycle progression (Booher et al., 2012).
To understand the signals and mechanism of the SAM checkpoint in mammalian cells, we used methionine-free medium, chemical inhibitor, and genetic tools to decrease intracellular SAM. Here, we demonstrate that SAM limitation induced robust G1 arrest with high Cdk4 and low Cdk2 activity, which was independent from the mTORC1 and polyamine pathways, but depended on p38 MAPK and its downstream checkpoint kinase MAPK-activated protein kinase-2 (MK2, also known as MAPKAPK2).
SAM depletion induces cell cycle arrest in G1
To analyze effects of SAM availability on cell cycle progression we used the IL3-dependent mouse pre-B-cell FL5.12 because they have well described and robust nutrient response pathways (Edinger and Thompson, 2002). In addition, genetically similar FL5.12 derivatives are available that are either tumorigenic owing to stable expression of the oncogenic fusion protein p190 BCR-Abl (p190 cells) (Li et al., 1999), or resistant to induction of apoptosis owing to stable expression of the anti-apoptotic factor Bcl-XL (BXL cells). Whereas the latter remain IL3-dependent, p190 cells can proliferate without IL3 (Neshat et al., 2000). We first tested the effect of methionine depletion on these cell lines. Methionine is the direct metabolic precursor of SAM (Fig. 1A) and its depletion is a convenient and efficient way to reduce intracellular SAM levels. As expected, all cell lines (FL5.12, p190, BXL) stopped proliferation immediately after they were shifted to methionine-free medium, and cell numbers rapidly decreased (Fig. 1B). The decrease in cell number was likely to be caused by apoptosis because BXL cells showed significantly higher viability compared to FL5.12 and p190 cells. Flow cytometric analyses showed that cells were primarily arrested in the G1 phase of the cell cycle with a smaller fraction arrested in G2/M (Fig. 1C). A comparable cell cycle arrest profile was observed when SAM levels were depleted through inhibition of methionine adenosyltransferase (MAT) (Fig. 1C, right panel) with cycloleucine (Lombardini and Talalay, 1970). Measurement of intracellular SAM concentrations revealed that SAM levels dropped rapidly after cells were shifted to methionine-free growth medium and were nearly undetectable after 4 hours (Fig. 1D). A similar rapid drop in cellular SAM was observed after cells were treated with cycloleucine. In contrast, SAM levels were unaffected in cells shifted to leucine-free medium (Fig. 1D), although leucine deprivation induced G1 arrest in cells (data not shown).
SAM depletion blocks entry into S phase despite high Cdk4 activity
To better characterize the effect of SAM depletion on cell cycle arrest, we monitored the ability of cells to replicate DNA after they were shifted to methionine-free medium or treated with cycloleucine (Fig. 2A). S phase was monitored by pulse-labeling with bromodeoxyuridine (BrdU). Both methionine depletion and inhibition of SAM synthesis with cycloleucine significantly prevented DNA replication (Fig. 2A). Flow cytometric analysis showed that cells accumulated in the G1 phase and there was no noticeable S phase population after SAM depletion (Fig. 1C) suggesting that the drop in BrdU incorporation is caused by arrest at the G1/S transition. To further determine the effect of SAM depletion on cell cycle progression we decided to follow a synchronous cell population. To this end, we pulse-labeled S phase cells with BrdU, then shifted cells to either methionine-free medium or treated them with cycloleucine, and followed the BrdU-labeled cells progressing through different cell cycle phases (Fig. 2B). Consistent with the cell cycle profile of the entire cell population after SAM depletion (Fig. 1C), the majority of cells that were shifted to methionine-depleted or cycloleucine medium progressed through S phase and mitosis, and arrested in G1 (Fig. 2B). Methionine depletion did reduce progression rate through S phase but did not block DNA-replication of cells that had committed to S phase, and a significant fraction of cells reached G1 after 12 hours. Cycloleucine did not affect the rate of S phase progression suggesting that the decreased DNA replication rate is a consequence of methionine depletion. However, SAM depletion did significantly delay cells in G2/M, although most cells eventually finished mitosis and arrested in G1 (Fig. 2B, data not shown). The delay in G2/M is probably due to slow progression from the G2 phase into metaphase, because cells pre-synchronized in metaphase with nocodazole progressed to the next G1 phase without delay when intracellular SAM was depleted (Fig. 2C). Taken together, these data demonstrate that at no point after SAM depletion can G1 cells re-enter S phase, indicating that SAM limitation induces a robust cell cycle arrest at the G1/S transition. We refer to this cell cycle arrest as the SAM checkpoint.
We next monitored some of the regulatory proteins important for G1/S transition. Cells were pre-synchronized in metaphase with a sequential thymidine–nocodazole block and then released into methionine-depleted medium or treated with cycloleucine (Fig. 3A). As expected cyclin B was present in metaphase but rapidly disappeared as cells progressed through the cell cycle. Most strikingly, SAM depletion by both methionine-free culture medium and cycloleucine treatment prevented phosphorylation of the retinoblastoma protein Rb in G1 (Fig. 3A). Two cyclin-dependent kinases (Cdks), Cdk4–cyclin-D and Cdk2–cyclin-E, phosphorylate Rb during G1 to enable entry into S phase (Malumbres and Barbacid, 2009). Levels of cyclin D1 were unaffected by SAM depletion (Fig. 3A). In agreement with constant cyclin D1 levels, Cdk4 activity as measured by Rb phosphorylation in vitro remained unaffected during SAM depletion (Fig. 3B). In contrast, the increase of cyclin E levels observed in control cells during G1, was absent when SAM levels were depleted (Fig. 3A), and accordingly Cdk2 activity in vitro dropped significantly (Fig. 3C). This is in contrast to previous results obtained with MDA-MB468 breast cancer cells where cyclin E levels remained high during methionine stress (Booher et al., 2012). This is probably due to dysregulation of cyclin E in these breast cancer cells owing to mutations in cyclin E regulators.
During growth factor withdrawal, degradation of the phosphatase Cdc25A causes downregulation of Cdk2 activity owing to the increase in inhibitory phosphorylation on Cdk2 (Khaled et al., 2005). Notably, Cdc25A levels were unchanged during SAM checkpoint activation and inhibitory Cdk2 tyrosine phosphorylation rapidly decreased during SAM depletion (Fig. 3D), indicating that the observed reduction in Cdk2 activity during SAM checkpoint activation (Fig. 3C) is not caused by inhibitory tyrosine phosphorylation. In addition, these results suggest that SAM checkpoint activation is caused by a pathway distinct from growth factor withdrawal, which is characterized by Cdc25A degradation and a concomitant increase in Cdk2 inhibitory tyrosine phosphorylation (Khaled et al., 2005). Consistent with this notion, SAM depletion readily induces G1 cell cycle arrest in the growth-factor-independent cell line p190 (Fig. 2B).
Knock-down of methionine adenosyltransferase MAT2A and MAT2B induces cell cycle arrest
SAM is synthesized from methionine and ATP by methionine adenosyltransferase. Mammalian MAT consists of two subunits, the catalytic subunit MAT2A and the regulatory subunit MAT2B (Fig. 4A). To further support our previous result that SAM depletion induces a SAM checkpoint activation and G1 cell cycle arrest, we generated doxycycline-inducible MAT2A and MAT2B dual knockdown cell lines (MATdkd) to genetically decrease intracellular SAM production. Induction of shRNA expression partially reduced MAT2A levels and dramatically decreased expression of MAT2B (Fig. 4B). To efficiently reduce intracellular SAM, we needed to reduce flux through the SAM synthesis pathway by lowering the methionine concentration to a more physiological level than that in tissue culture medium. Proliferation of control cells was not affected by the lower methionine levels during the time course. However, knockdown of MAT2A and MAT2B together prevented proliferation of cells under these conditions (Fig. 4C), and resulted in the same cell cycle phenotype, namely depletion of the S phase population and arrest in G1, as observed in response to SAM depletion by cycloleucine or methionine-free medium (Fig. 4D). Comparable results were observed with a different pair of shRNAs that also target MAT2A and MAT2B simultaneously (Fig. 4C).
SAM-depletion-induced cell cycle arrest is independent of mTORC1 signaling
The mTORC1 complex controls one of the major nutrient signaling pathways in eukaryotes. This pathway is particularly important in sensing amino acid availability. As expected, when cells were transferred to leucine-depleted growth medium, mTORC1 was inhibited, as demonstrated by reduced phosphorylation of the ribosomal subunit S6 (Fig. 5A). Surprisingly, depletion of intracellular SAM by culturing cells in methionine-free medium only transiently inhibited mTORC1 signaling. Moreover, inhibition of SAM synthesis with cycloleucine had no effect on S6 or S6 kinase phosphorylation, indicating that metabolic pathways around SAM are not monitored by mTORC1.
An extended timecourse confirmed that methionine-depleted medium had no persisting effects on S6 phosphorylation, suggesting that mTORC1 signaling is largely unaffected (Fig. 5B). In contrast, as expected, leucine deprivation dramatically reduced the phosphorylation of the mTORC1 downstream target ribosomal subunit S6 (Fig. 5B). mTORC1 is known to be activated by growth factor and nutrients through an IRS1–PI3K–PDK1–Akt pathway and feedback inhibits Akt activity through S6K-mediated IRS1 phosphorylation and proteasomal degradation (Easton et al., 2006). Accordingly, decreasing mTORC1 activity by leucine deprivation attenuated this feedback inhibition, which in turn resulted in Akt activation. Surprisingly, the phosphorylation of Akt Ser473 was also significantly increased during SAM depletion, despite constant mTORC1 activity. These results suggest that under these conditions other signaling pathways contribute to Akt activation.
The nutrient-insensitive RagBQ99L mutant cannot suppress SAM-depletion-induced cell cycle arrest
The Rag family small GTPases interact with mTORC1 in an amino-acid-dependent manner and are required for mTORC1 activation in response to intracellular amino acid levels (Sancak et al., 2008). Methionine, besides being the immediate metabolic precursor for SAM synthesis, is also an essential amino acid. Our previous result showed that depletion of SAM in methionine-free medium does not persistently affect mTORC1 activity (Fig. 5A,B). However, to further exclude the involvement of mTORC1 in the SAM checkpoint, we generated a cell line stably expressing RagBQ99L, a GTPase mutant that renders mTORC1 insensitive to amino acid levels (Sancak et al., 2008). As previously demonstrated (Sancak et al., 2008), phosphorylation levels of the mTORC1 downstream target ribosomal protein S6 was only slightly sensitive to leucine deprivation in RagBQ99L-expressing cells, while parental cells exhibit dramatic reduction of phosphorylated S6 (Fig. 5C). Next, we tested the cell cycle response of RagBQ99L cells to SAM depletion. RagBQ99L expressing cells showed robust cell cycle arrest in the G1 phase after SAM depletion with either methionine-free medium or cycloleucine (Fig. 5D). Together these results strongly suggest that the SAM checkpoint is independent of the major nutrient signaling pathway, which is controlled by mTORC1.
The SAM-checkpoint-induced G1 arrest in FL5.12 cells is distinct from the polyamine-depletion phenotype
In addition to serving as a cofactor for methylation reactions, SAM is also required for polyamine synthesis. Numerous studies have connected polyamine synthesis and increased expression of relevant enzymes in this pathway, such as ornithine decarboxylase (ODC) and S-adenosylmethionine decarboxylase (SAMDC or AdoMetDC), with tumor growth (Casero and Marton, 2007; Meyskens and Gerner, 1999; Seidenfeld et al., 1986). AdoMetDC consumes SAM to produce aminopropyl groups for polyamine synthesis. It was thus possible that SAM depletion decreases polyamine pools and induces polyamine-depletion phenotypes, which are characterized by Akt activation, p27-dependent G1 arrest and p53-dependent apoptosis (Koomoa et al., 2009; Koomoa et al., 2008; Wallick et al., 2005). However, we did not detect any significant upregulation of p21, p27 or p53 levels during SAM checkpoint activation (supplementary material Fig. S1A), nor could spermidine supplementation suppress the cell cycle arrest induced by SAM depletion (supplementary material Fig. S2A). In addition, FL5.12 cells treated with the ODC inhibitor difluoromethylornithine (DFMO), to block polyamine production, did not mimic the cell cycle arrest phenotype induced by SAM depletion (supplementary material Fig. S2B). Taken together, these results suggest that SAM depletion in FL5.12 cells induces a cell cycle arrest that is distinct from the effects of polyamine depletion.
The p38–MK2 pathway is required for SAM-depletion-induced cell cycle arrest
In addition to mTORC1, AMP-activated protein kinase (AMPK) regulates cellular energy homeostasis (Hardie et al., 2012). Recently, AMPK has been linked to cell cycle regulation, through mTORC1, p53, p27 and p38, in response to cellular metabolic cues (Gwinn et al., 2008; Jones et al., 2005; Liang et al., 2007; Sengupta et al., 2007; Zhuang and Miskimins, 2008). Our results have largely excluded mTORC1 as a crucial component of the SAM checkpoint pathway. Furthermore, p53 and p27 levels only increased after very extended periods of SAM depletion, long after cells had arrested at G1 (data not shown). Thus, p53 and p27 might contribute to the maintenance of cell cycle arrest after SAM depletion, but are probably not involved in the cell cycle arrest initiation in response to SAM depletion. These results prompted us to investigate whether the AMPK–p38 signaling pathway is activated during SAM depletion. To this end, we treated cells with MAPK inhibitors during SAM depletion induced by either culture in methionine-free medium or cycloleucine and monitored S phase entry by BrdU pulse labeling (Fig. 6A). Both p38 inhibitor SB202190 and MK2 inhibitor MK2III significantly restored S phase entry after SAM depletion, which is particularly clear when the cells were gated for early S phase (Fig. 6A). In contrast, even though the JNK inhibitor SP600125 also increased the total S phase population (Fig. 6A), this was an indirect effect due to slower DNA replication. Consequently, JNK inhibition did not suppress the block in G1/S transition, as evident by loss of early S phase cells (Fig. 6A). MK2 is a direct substrate for p38 phosphorylation and functions as a checkpoint kinase in parallel to Chk1 and Chk2 during UV-induced DNA damage (Manke et al., 2005). Our data suggests p38–MK2 signaling as an important component of SAM checkpoint activation. To test whether p38 is activated during SAM depletion, we monitored the p38-specific phosphorylation site Thr334 on MK2 after shifting cells to methionine-free medium. MK2 was rapidly phosphorylated on Thr334 during SAM depletion (Fig. 6B). MK2 phosphorylation was blocked by the p38 inhibitor SB202190, confirming p38 dependency (Fig. 6B). We have previously demonstrated that there are decreased levels of the DNA replication factor Cdc6 as a result of SAM checkpoint activation in the human breast cancer cell line MDA-MB 468 (Booher et al., 2012). Consistent with that study, Cdc6 levels were also decreased in FL5.12 cells during SAM depletion, and this phenotype could be partially reversed by treatment with the p38 inhibitor SB202190 (supplementary material Fig. S1A,B).
The p38 inhibitor experiments described above were performed in IL3-dependent murine pre-B cells, FL5.12. Similar results were observed with leukemic, IL3-independent FL5.12 cells that stably express BCR-Abl p190 (p190 cells). SAM depletion in p190 cells efficiently blocked S phase entry, and inhibition of p38 allowed a significant portion of the cells to overcome this block (Fig. 6C). Interestingly, inhibition of p38 to override the SAM checkpoint increased the proportion of sub-G1 cells, suggesting that cell cycle progression in low SAM levels is deleterious to cells and that the SAM checkpoint response is important for the maintenance of cellular integrity in both non-tumorigenic and tumorigenic cells (Fig. 6A,C). Accordingly, p38 inhibition during induction of the SAM checkpoint with methionine-free medium or the MAT inhibitor cycloleucine significantly increased cell death in a dose-dependent manner (supplementary material Fig. S2C).
We next asked whether the p38–MK2 pathway is also important for SAM checkpoint activation in human cells. To this end, we used human SupB15 cells, an acute lymphoblastic leukemia (ALL) cell line with BCR-Abl (p190) expression. Similar to murine cells, SAM depletion in SupB15 cells induced p38 activity as indicated by MK2 phosphorylation on Thr334 (Fig. 6D), and MK2 phosphorylation was blocked upon p38 inhibition with SB202190 (Fig. 6D). Importantly, inhibition of p38 allowed a significant number of SupB15 cells to enter S phase after SAM depletion (Fig. 6D). Finally, we further confirmed the importance of this pathway by extending our analyses to adherent cells. SAM depletion in human small cell lung carcinoma H1299 cells (p53-null) induced a G1 arrest (data not shown), and inhibition of MK2 by expression of the dominant kinase-dead MK2K76R mutant (Winzen et al., 1999) significantly increased the number of cells entering S phase during SAM checkpoint conditions (Fig. 6E). H1299 cells lack p53 tumor suppressor function, suggesting that the SAM checkpoint is independent of p53.
Cell cycle checkpoint activation in response to various environmental challenges is essential for the maintenance of cellular, genetic and epigenetic integrity of eukaryotic cells (Bartek and Lukas, 2003). Disruption of checkpoints due to inherited or acquired mutations has been recognized as an important contributor to human cancer. Since introduction of the concept of cell cycle checkpoints by Hartwell and Weinert (Hartwell and Weinert, 1989), research has largely been focused on molecular dissection of DNA damage, S phase and spindle checkpoints. In comparison, our understanding of checkpoints that monitor important cellular metabolites is in its infancy. In this study, we explore a pathway that monitors levels of the primary methyl-group donor SAM and its connections to cell cycle control. Conceptually, this pathway might define a checkpoint that is important for epigenetic stability because failing to stop cell cycle progression when SAM levels are insufficient to support chromatin methylation could lead to loss of chromatin methylation marks. Similar checkpoints monitoring other key metabolites are likely to exist.
Recently, metabolic checkpoints have emerged as potential therapeutic cancer targets (Gwinn et al., 2008; Laplante and Sabatini, 2012; Shackelford and Shaw, 2009). Tumor cells often adapt and reprogram their metabolism to fuel cell growth and proliferation and concomitantly acquire metabolic addictions that distinguish cancer cells from normal cells (Hanahan and Weinberg, 2011). Interestingly, addiction of cancer cells to a high flux through the methionine metabolism pathway has been known for over 35 years (Halpern et al., 1974). Recent studies in breast cancer cells suggest that SAM rather than methionine might be the limiting metabolite defining addiction to this metabolic pathway (Booher et al., 2012). Consistent with this idea, targeting methionine adenosyltransferase (MAT) with either a small molecule inhibitor or shRNA induces apoptosis in leukemia cells (Attia et al., 2008; Jani et al., 2009). The mechanisms of how cells induce cell cycle arrest and apoptosis in response to SAM limitation is currently unknown, but experiments in the yeast and breast cancer cell models indicate loss of pre-replication complexes from chromatin as a contributing factor (Booher et al., 2012; Su et al., 2005).
In this study, we define a cell cycle checkpoint induced by SAM limitation and identify p38 MAPK and its downstream checkpoint kinase MK2 as part of the signaling pathway for the mammalian SAM checkpoint. It has been proposed that the p38–MK2 pathway is a third cell cycle checkpoint module, parallel to ATR–Chk1 and ATM–Chk2, and it has been shown that it is essential for the survival of p53-null cells after DNA damage (Manke et al., 2005; Reinhardt et al., 2007; Reinhardt and Yaffe, 2009). DNA damage induces degradation of the G1/S-transition driver phosphatase Cdc25A in order to halt cell proliferation in G1 (Hassepass et al., 2003; Mailand et al., 2000). Inhibition of MK2 prevents degradation of Cdc25A after DNA damage, by an unknown mechanism, resulting in sustained cell proliferation despite DNA damage (Manke et al., 2005). Interestingly, p38-mediated degradation of Cdc25A has been suggested to control cell cycle arrest in response to growth factor withdrawal (Khaled et al., 2005). Whether MK2 is involved is unknown. Our study implicates the p38–MK2 module in G1 checkpoint arrest in response to SAM depletion. However, the p38–MK2 pathway appears to function through a distinct mechanism because Cdc25A levels remained constant throughout SAM checkpoint activation, Cdk2 phosphorylation of Tyr15 did not increase, and expression of the degradation-resistant Cdc25AS76A (Hassepass et al., 2003) did not override SAM-checkpoint-induced cell cycle arrest (data not shown). Furthermore, SAM checkpoint activation remains robust in growth-factor-independent cells expressing BCR-Abl p190, indicating that signaling pathways responding to growth factor withdrawal are different from those in SAM checkpoint activation.
Interestingly, p38 has previously been indirectly connected to cell cycle arrest in response to SAM depletion. Arsenic is an environmental toxin, a carcinogen and a cancer drug (de Thé and Chen, 2010; Kitchin and Conolly, 2010; Tseng, 2008). One of the main detoxification pathways for arsenic is methylation by human SAM-dependent arsenite methyltransferase, which consumes SAM and glutathione to neutralize intracellular arsenicals (Hayakawa et al., 2005). Exposure to arsenite decreases intracellular SAM levels (Reichard et al., 2007) and induces p38-dependent cell cycle arrest (Kim et al., 2002). It is thus conceivable that arsenite inhibits cell proliferation through the p38–MK2-activated SAM checkpoint we describe here.
In this study, we identify and characterize the cell cycle checkpoint response to limiting levels of SAM, and discovered the p38–MK2 pathway as an important link between SAM homeostasis and cell cycle arrest. Molecular mechanisms for how SAM levels are monitored are currently unknown. Our results suggest that the cellular response to SAM limitation is independent from the mTORC1 pathway and might define a distinct metabolite monitoring system. This is surprising because the mTORC1 pathway is the major molecular link between the metabolic state of cells and cellular functions. mTORC1 integrates many extracellular and intracellular inputs, including growth factors, stress, energy status, oxygen level and amino acids, with protein translation, lipid synthesis, cell growth, cell cycle and autophagy (Laplante and Sabatini, 2012). Interestingly, methionine depletion had only marginal effects on mTORC1 activity (Fig. 5A), and rendering mTORC1 insensitive to amino acid levels by expression of RagBQ99L did not bypass the induction of G1 cell cycle arrest in response to methionine depletion (Fig. 5C,D). These results suggest that intracellular methionine levels might be monitored through the downstream metabolite SAM, and integrated with cell cycle progression through the SAM checkpoint.
Methionine stress hypersensitivity is an almost universal metabolic characteristic of cancer cells and tumors (Guo et al., 1993; Kreis, 1979; Mecham et al., 1983; Poirson-Bichat et al., 1997; Stern et al., 1984; Tisdale et al., 1983) and was recently suggested to reflect a hypersensitive SAM checkpoint in cancer cells (Booher et al., 2012). Therefore, further understanding of the pathways connecting levels of SAM with cell proliferation will provide molecular insight into integration of metabolite homeostasis with cell cycle regulation and might lead to discovery of new cancer drug targets.
MATERIALS AND METHODS
Cell lines and reagents
Human SupB15, murine pre-B cells FL5.12, and FL5.12 derivatives are kind gifts from David Fruman (Molecular Biology & Biochemistry, University of California, Irvine) and Aimee Edinger (Develomental & Cell Biology, University of California, Irvine). Human H1299 cells were kind gifts from Wen-Hwa Lee (Biological Chemistry, University of California, Irvine). Cells were maintained in RPMI 1640 medium (R8999, US Biological, Swampscott, MA, USA) with 10% dialyzed FBS (Gemini, West Sacramento, CA, USA), 10 µM folic acid, 2.5 µM vitamin B12 (Fisher Scientific, Pittsburgh, PA, USA), 10 mM HEPES (Mediatech, Manassas, VA, USA), 500 pg/ml murine recombinant IL-3 (BD Pharmingen, San Jose, CA, USA) and 1% Penicillin-Streptomycin-Amphoterincin B solution (Mediatech). In the case of methionine-free medium, RPMI 1640 medium was replaced with RPMI 1640 medium deficient in methionine, cysteine, and glutamine (R9016, US biological) and was supplemented with L-cysteine and L-glutamine at the same concentration as in standard RPMI 1640 medium. Medium supplemented with spermidine contained 1 mM aminoguanidine to inhibit serum polyamine oxidase (Koomoa et al., 2008). MK2 inhibitor MK2III was from Calbiochem (EMD Millipore, KGaA, Darmstadt, Germany). Cell viability was measured with CellTiter-Glo® Luminescent Cell Viability Assay (Promega, Madison, WI); 2000 cells/well were used per assay. Antibodies against phospho-S6 (no. 5364), phosphor-Akt (no. 9271), phospho-p70 S6K (no. 9234), phospho-MK2 (no. 3041), total MK2 (no. 3042), Cyclin D1 (no. 2926) and Cdc25A (no. 3652) were from Cell Signaling Technology (Boston, MA, USA). Antibodies against α-tubulin and FLAG® were obtained from Sigma-Aldrich (Ontario, CA, USA). The retinoblastoma antibody was from BD Pharmingen (San Jose, CA, USA). Antibodies against cyclin B, cyclin E, Cdk2 (sc-163) and Cdk4 (sc-260) were purchased from Santa Cruz Biotechnology (Santa Cruz, CA, USA). Immunoblots were imaged on a Fuji LAS-4000 imaging system (Fujifilm, Tokyo, Japan).
Cells were shifted to conditional medium for indicated time period before labeling with 25 µM BrdU for 25 minutes. Cells were harvested, fixed with ice-cold 70% ethanol, and stored overnight at 4°C. Cells were denatured with 2 M HCl, neutralized with 0.1 M NaBr (pH 8.0), and blocked with PBS containing 5% FBS and 1% BSA before incubation with anti-BrdU antibodies (GTX26326, Genetex, Irvine, CA, USA) overnight. For BrdU-chase experiments, cells were labeled with BrdU prior to being shifted to conditional medium. BrdU immunostained cells were analyzed on a BD FACS Calibur Flow Cytometer (BD Biosciences, San Jose, CA, USA) and analyzed with Flowjo software (Tree Star Inc., Ashland, OR, USA).
Cdk2 and Cdk4 kinase activity assay
Cells were lysed in kinase extraction buffer (50 mM HEPES pH 7.5, 150 mM NaCl, 2.5 mM EDTA, 0.2% Triton X-100, 10% glycerol, 10 mM β-glycerophosphate, 2 mM NaF, 2 mM Na3VO4, 10 µg/ml leupeptin and 0.1 M phenylmethylsulfonyl fluoride) and incubated on a rotator at 4°C for 30 minutes. A total of 300 µg of total protein extracts were used per reaction. Kinases were immunopurified with either anti-Cdk2 or -Cdk4 antibodies and protein G-sepharose beads at 4°C overnight. Immuncomplexes were washed two times with kinase extraction buffer and twice with kinase buffer (50 mM HEPES pH 7.5, 10 mM MgCl2, 20 µM ATP). Immunocomplexes were resuspended in 25 µl kinase buffer, and 4 µg of the substrates histone H1 (Cdk2 kinase assay) or Rb (CDK4 kinase assay; a kind gift from Yu-Mei Chen, Biological Chemistry, University of California, Irvine), and 5 µCi of [γ-32P] ATP. The reactions were incubated at 30°C for 20 minutes. The reaction was stopped by adding 25 µl 2× concentrated Laemmli sample buffer, and products were separated by SDS-PAGE (10% gel). Gels were dried and kinase activity was detected by phosphoimaging and quantified by Bio-Rad Quantity One.
The pSLIK lentiviral vectors for knockdown of MAT were constructed as described previously (Shin et al., 2006). Briefly, oligonucleotides designed with BfuAI compatible protrusion (lower cased) were annealed and cloned into the BfuAI site in pEN_TGmirRc3 (ATCC, Manassas, VA, USA). Subsequent recombinations with pSLIKpuro were catalyzed with LR clonase (Invitrogen, Carlsbad, CA, USA). pSLIKpuro was generated from pSLIKhygro (Shin et al., 2006) by replacing the hygromycin resistance marker with a puromycin resistance cassette. The miR-shRNA sequence were designed by the RNAi codex algorithm (http://cancan.cshl.edu/RNAi_central/RNAi.cgi?type = shRNA).
The sequences used for shRNA are as follows (the mRNA-targeting sequence is underlined): luciferase (shRNA), 5′-agcgCCCGCCTGAAGTCTCTGATTAATAGTGAAGCCACAGA TGTATTAATCAGAGACTTCAGGCGGTtgcc-3′; mouse MAT2A (shRNA), 5′-agcgCGCAGTCACTCTAATCAATAACTAGTGAAGCCACAGATGTAGTTATTGATTAGAGTGACTGCAtgcc-3′; mouse MAT2B (shRNA), 5′-agcgCTCTTACTAAGTGATGTTTCATTAGTGAAGCCACAGATGTAATGAAACATCACTTAGTAAGATtgcc-3′.
Lentiviruses were generated by transfecting HEK293T cells with the pSLIK vectors together with packaging vectors pMDG, pCMVdeltaR8.91. Lentiviruses were collected 24 and 48 hours post-transfection for target cell infection. Cells were selected with 1 ug/ml puromycin 48 hours post viral infection.
Measurement of cellular SAM levels
SAM concentrations were measured following a protocol adapted from Wang et al. (Wang et al., 2001). Briefly, a Waters HPLC system with UV spectrometer was employed to carry mobile phases and detect SAM. Separation was performed on a PartiSphere C18 reverses phase analytical column (Waters, Milford, MA, USA). The mobile phase consisted of two solvents: solvent A, 8 mM octanesulfonic acid sodium salt, with pH adjusted with phosphoric acid to 3.0; and solvent B, 100% methanol. The column was equilibrated with 80% A and 20% B. Separation was obtained using a step gradient: 8 minutes at equilibration condition, 30 seconds to increase to 40% B, 12.5 minutes at 40% B, 30 seconds to decrease B to equilibration condition, 10 minutes at the equilibration condition. The flow rate was 1 ml/minutes and the detection was set at 254 nm. HPLC was performed at room temperature. SAM was identified by its retention time (17 minutes) and the co-chromatography with the standard. Quantification was based on integration of the area under the curve and was compared to a SAM standard curve from 0 to 10,000 pmol. Cell samples from 15-cm dishes were extracted with 500 µl 0.4 M HClO4 at room temperature, centrifuged at 16,000 g for 15 minutes, and 200 µl supernatant was used for each injection. The resulting pellets after centrifugation were lysed in Urea buffer (8 M Urea, 50 mM Tris-HCl pH 7.5, 150 mM NaCl) and protein content was measured with Bradford protein assay (#23236, Thermo Fisher Scientific Pierce, Rockford, IL, USA). Cellular SAM content was expressed as pmol SAM per mg protein.
We thank A. Edinger, D. Fruman, E. Lee and W. H. Lee for reagents and helpful suggestions. We are grateful to K. Yokomori and S. White for access to microscopes and HPLC, respectively. We thank H. Piwnica-Worms for Cdc25A and GSK3β constructs, M. Gaestel for MK2 constructs.
D.W.L. is responsible for execution and design of most experiments. B.P.C. contributed to execution of some experiments. P.K. is responsible for research direction, contributed to experimental design and wrote and revised the manuscript and figures, together with D.W. L.
This work was partially supported by the National Institute of Health [grant number GM66164]; and the University of California Cancer Research Coordination Committee (to P.K.). D.L. is supported by the California Institute for Regenerative Medicine ‘UCI CIRM Training Grant II’ [grant number TG2-01152]. Deposited in PMC for release after 12 months.
The authors declare no competing interests.