|XBP-1u suppresses autophagy by promoting the degradation of FoxO1 in cancer cells.|
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|PMID: 23277279 Owner: NLM Status: Publisher|
|Autophagy is activated to maintain cellular energy homeostasis in response to nutrient starvation. However, autophagy is not persistently activated, which is poorly understood at a mechanistic level. Here, we report that turnover of FoxO1 is involved in the dynamic autophagic process caused by glutamine starvation. X-box-binding protein-1u (XBP-1u) has a critical role in FoxO1 degradation by recruiting FoxO1 to the 20S proteasome. In addition, the phosphorylation of XBP-1u by extracellular regulated protein kinases1/2 (ERK1/2) on Ser61 and Ser176 was found to be critical for the increased interaction between XBP-1u and FoxO1 upon glutamine starvation. Furthermore, knockdown of XBP-1u caused the sustained level of FoxO1 and the persistent activation of autophagy, leading to a significant decrease in cell viability. Finally, the inverse correlation between XBP-1u and FoxO1 expression agrees well with the expression profiles observed in many human cancer tissues. Thus, our findings link the dynamic process of autophagy to XBP-1u-induced FoxO1 degradation.Cell Research advance online publication 1 January 2013; doi:10.1038/cr.2013.2.|
|Ying Zhao; Xue Li; Mu-Yan Cai; Ke Ma; Jing Yang; Jingyi Zhou; Wan Fu; Fu-Zheng Wei; Lina Wang; Dan Xie; Wei-Guo Zhu|
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|Type: JOURNAL ARTICLE Date: 2013-1-01|
|Title: Cell research Volume: - ISSN: 1748-7838 ISO Abbreviation: Cell Res. Publication Date: 2013 Jan|
|Created Date: 2013-1-1 Completed Date: - Revised Date: -|
Medline Journal Info:
|Nlm Unique ID: 9425763 Medline TA: Cell Res Country: -|
|Languages: ENG Pagination: - Citation Subset: -|
|Key Laboratory of Carcinogenesis and Translational Research of Ministry of Education, Department of Biochemistry and Molecular Biology, Peking University Health Science Center, Beijing 100191, China.|
|APA/MLA Format Download EndNote Download BibTex|
Journal ID (nlm-ta): Cell Res
Journal ID (iso-abbrev): Cell Res
Publisher: Nature Publishing Group
Copyright © 2013 Shanghai Institutes for Biological Sciences, Chinese Academy of Sciences
Received Day: 14 Month: 11 Year: 2012
Revision Received Day: 21 Month: 11 Year: 2012
Accepted Day: 22 Month: 11 Year: 2012
Print publication date: Month: 04 Year: 2013
Electronic publication date: Day: 01 Month: 01 Year: 2013
pmc-release publication date: Day: 1 Month: 4 Year: 2013
Volume: 23 Issue: 4
First Page: 491 Last Page: 507
PubMed Id: 23277279
Publisher Item Identifier: cr20132
|XBP-1u suppresses autophagy by promoting the degradation of FoxO1 in cancer cells Alternate Title:FoxO1 degradation by interacting with XBP-1u|
1Key Laboratory of Carcinogenesis and Translational Research of Ministry of Education, Department of Biochemistry and Molecular Biology, Peking University Health Science Center, Beijing 100191, China
2State Key Laboratory of Oncology in South China, Sun Yat-Sen University Cancer Center, Guangzhou, Guangdong 510060, China
2Peking-Tsinghua University Center for Life Sciences, Peking University, Beijing 100871, China
*Tel: +86-10-82802235 E-mail: email@example.com
Autophagy is a process of intracellular degradation that delivers cytoplasmic constituents to the lysosome for the maintenance of homeostasis and bioenergetics in mammalian cells1,2,3,4. Autophagy is activated under a number of stressful conditions, including serum starvation and oxidative stress, as well as several conditions that lead to increased protein misfolding1,5. Through the induction of autophagy, mammalian cells are able to obtain an influx of free amino acids and other essential nutrients. However, autophagy is rarely persistently activated in response to stress, but is instead activated in a dynamic manner to avoid autophagy-induced cell death. For example, autophagy commonly occurs during the first few hours of serum starvation, when it provides an initial burst of free amino acids for the synthesis of essential proteins; however, this autophagic process is rarely observed after the first 4-8 h of serum starvation in normal rat kidney cells or mouse fibroblasts6,7.
Several regulators have been reported to be important for the induction of autophagy, including beclin1, mammalian target of rapamycin (mTOR) and the FoxO family members8,9,10,11,12. Mammalian FoxO transcription factors, including FoxO1, FoxO3a, FoxO4 and FoxO6, are homologs of Caenorhabditis elegans abnormal dauer formation-16 (DAF-16) and Drosophila dFoxO13,14,15,16. FoxO transcription factors are involved in several important biological processes, such as cell cycle arrest, DNA repair, apoptosis, glucose metabolism and aging13,17. Recent reports have also raised the possibility that FoxO family members are involved in the induction of autophagy via both transcription-dependent and -independent pathways10,11,12,18. Loss of FoxO protein is also responsible for the attenuation of autophagy in Drosophila, mouse muscle cells and several cancer cell lines10,11,12,19.
As FoxO family proteins are key regulators of multiple important biological processes, factors that influence the fate of FoxO1 are of great interest to researchers. It has been reported that the FoxO proteins are degraded via the proteasomal pathway in response to insulin and growth factors. Additionally, the oncoprotein S-phase kinase-associated protein 2 (Skp2) has been shown to ubiquitinate FoxO1 and promote its degradation20. FoxO1 is also degraded by the ubiquitin-proteasome pathway in Fao hepatoma cells, a process mediated by COP1 — a RING-finger E3 ubiquitin ligase21. Finally, the ubiquitin E3 ligase MDM2 can bind to FoxO1 or FoxO3 to promote the polyubiquitination and degradation of these proteins22,23. In addition to the factors mentioned above, X-box-binding protein-1s (XBP-1s) has recently been reported to interact with FoxO1 and cause the ubiquitin-dependent proteasomal degradation of FoxO1 in MEF cells24, although the mechanism of FoxO1 degradation induced by XBP-1s is not fully understood.
XBP-1s is a transcriptional activator of the unfolded protein response (UPR) and is also a critical factor for the regulation of genes involved in cell survival25,26. Unconventional splicing of the XBP-1 mRNA can result in two alternate proteins, XBP-1s (the spliced form) and XBP-1u (the unspliced form). Following endoplasmic reticulum (ER) stress, the XBP-1 pre-mRNA is cleaved by the activated inositol-requiring enzyme 1 (IRE1) to form the “mature” (i.e., spliced) XBP-1 mRNA, which encodes XBP-1s27; XBP-1s can then bind to ER stress-response elements to induce the transcription of ER chaperones28. In addition to regulating the UPR, XBP-1 has also been implicated in the regulation of autophagy in the murine nervous system29. XBP-1 deficiency resulted in increased levels of FoxO1 and enhanced macroautophagy in cellular and animal models of Huntington's disease, although the authors did not interpret how XBP-1 deficiency is related to autophagy, and how FoxO1 level is negatively correlated with XBP-1 level30.
In this study, our results demonstrate that FoxO1 turnover is highly associated with the dynamic autophagy process. Phosphorylation of XBP-1u by ERK is required for XBP-1u binding to FoxO1, which leads to localization of FoxO1 to the 20S proteasome for degradation. Interestingly, we also identified an inverse correlation between XBP-1u and FoxO1 expression in 229 cases of human colorectal cancer tissues. The relationship between XBP-1u and FoxO1 expression was also found to be highly correlated with p62 status in these cancer tissues, which suggests that XBP-1 is a critical protein for the promotion of tumor development.
Starvation caused by the removal of all amino acids or treatment with Earle's balanced salt solution (EBSS) induces very rapid autophagy31, which makes it difficult to study the dynamics of this process. To induce a long-term autophagic model, we used glutamine-free medium to starve human cancer cells. As shown in Figure 1A, autophagy was induced in the human colon cancer HCT116 cell line in response to glutamine starvation, which reached a peak at 24 h, as measured by p62 degradation and LC3-II accumulation, two common autophagic hallmarks. Interestingly, p62 degradation and LC3-II accumulation gradually returned to normal levels by 36 h post treatment (statistical data shown in Supplementary information, Figure S8). Autophagy was also directly observed by electron microscopy, which was used to monitor the formation of autophagosomes, as well as by fluorescent microscopy, which was used to observe LC-3-immunopositive punctate signals. Numerous vesicular structures with double membranes were commonly observed when HCT116 cells were incubated in glutamine-free medium for 12-24 h, but not after 48 h (Figure 1B). Under the same treatment conditions, punctate LC3 signals were consistently observed in the HCT116 cells. This staining significantly decreased by 36 h after glutamine starvation (Figure 1C and 1D), indicating that the observed autophagy was a dynamic process. Therefore, we sought to determine the key regulators controlling these changes. As FoxO1 acetylation is involved in regulating the autophagic process10, we first measured FoxO1 levels in the treated cells. As shown in Figure 1A (lower panels), FoxO1 levels gradually decreased in response to glutamine starvation. Surprisingly, we found that FoxO1 acetylation increased by 2 h after glutamine starvation and reached a peak at 24 h after treatment, as detected with a co-immunoprecipitation assay (Figure 1A, lower panels, and 1D). FoxO1 acetylation was highly correlated with its interaction with Atg7 (Figure 1A, lower panels) and the autophagic changes induced by glutamine starvation in the HCT116 cells (Figure 1D). To measure the overall rates of long-lived protein degradation, HCT116 cells were pre-labeled with [3H]-leucine 48 h prior to glutamine starvation in the presence or absence of 3-methyladenine (3-MA), an inhibitor of autophagy. Figure 1E shows that glutamine starvation significantly enhanced the overall degradation of proteins in HCT116 cells in a time-dependent manner. However, the 3-MA-sensitive degradation gradually decreased by 36 h after glutamine removal in HCT116 cells, indicating that the long-lived protein degradation by 36 h after glutamine starvation maybe depend on other forms of autophagy but not on macroautophagy6.
To determine whether this phenomenon occurs in other cell lines, we also assayed FoxO1 protein levels and acetylation status in A549 and HeLa cell lines under glutamine-starvation conditions (FoxO1 was highly expressed in A549 and HeLa cells, but virtually no expression was detected in H1299 cells10). Similar to what we observed in the HCT116 cells, FoxO1 levels gradually decreased whereas FoxO1 acetylation increased following treatment, which were correlated with changes in p62 degradation and LC3-II accumulation in both cell lines (Figure 1F and 1G). These data suggest that the dynamic autophagic process is likely to be associated with FoxO1 acetylation.
To determine whether the reduction in FoxO1 protein levels was the result of protein degradation or gene repression, we measured FoxO1 mRNA levels using real-time PCR. Glutamine starvation had no effect on FoxO1 mRNA levels (Figure 2A), indicating that protein degradation was likely responsible for the decrease in FoxO1 protein levels after glutamine starvation.
To determine the pathways involved in FoxO1 degradation, we pretreated HCT116 cells with a panel of inhibitors, the proteasome inhibitor MG132, the calpain inhibitor calpeptin and the lysosome inhibitor chloroquine (CHQ). MG132 significantly blocked the glutamine starvation-induced reduction of FoxO1 levels (Figure 2B) whereas calpeptin and CHQ had no effect on FoxO1 degradation (Figure 2C). These results suggest that FoxO1 is degraded by the proteasomal pathway in response to glutamine starvation.
Next, to determine whether FoxO1 is degraded in the nucleus or the cytoplasm, we ectopically expressed FoxO1 in H1299 cells, a cell line that normally has very low levels of FoxO110. We generated plasmids to express flag-tagged wild-type FoxO1 (WT) or mutated FoxO1 (3A) in which the residues T24, S256 and S319 of FoxO1 were each changed to alanine. The mutant protein FoxO1 (3A) was predominantly localized to the nucleus. As shown in Figure 2D, a significant decrease in FoxO1 (WT) protein levels was observed in response to glutamine starvation, whereas FoxO1 (3A) protein levels were unchanged. To further characterize this process, nuclear and cytoplasmic fractions were prepared from glutamine-starved HCT116 cells and then subjected to immunoblotting with a FoxO1 antibody. As shown in Figure 2E, degradation of endogenous FoxO1 was only observed in the cytoplasmic fraction. Taken together, these data demonstrate that glutamine starvation-induced FoxO1 degradation occurs in the cytoplasm and not in the nucleus.
Finally, to determine whether ubiquitination is required for FoxO1 degradation, plasmids expressing flag-tagged FoxO1 or a HA-ubiquitin were co-transfected into H1299 cells; FoxO1 ubiquitination was detected by co-immunoprecipitation with an anti-flag antibody followed by immunoblotting with an anti-HA antibody. Contrary to our expectations, we were unable to detect any polyubiquitinated FoxO1 in H1299 cells in response to glutamine starvation (Figure 2F). Therefore, we investigated whether the 20S proteasome plays a role in FoxO1 degradation. As assayed by co-immunoprecipitation, flag-tagged FoxO1 was physically associated with the 20S proteasome (Figure 2G), which was further confirmed by an in vitro protein degradation assay (Figure 2H). These data suggest that FoxO1 is degraded by 20S proteasome.
Several possible molecules have been reported to be involved in the degradation of FoxO proteins, including Skp220, MDM222 or XBP-1s24. To determine whether these proteins are associated with FoxO1 degradation in response to glutamine starvation, we designed several siRNA fragments against these proteins. Using RNAi technique, we excluded Skp2 and MDM2 as the molecules required for FoxO1 degradation in response to glutamine starvation (data not shown). We next tested the role of XBP-1 in FoxO1 degradation by transfecting plasmids encoding XBP-1u or XBP-1s into HCT116 cells. XBP-1s is a nucleus-localized protein and XBP-1u is predominately localized in the cytoplasm (Supplementary information, Figure S1A). As shown in Figure 3A, the FoxO1 protein level was markedly reduced by overexpression of XBP-1u, but not by overexpression of XBP-1s. In addition, knockdown of XBP-1u significantly abrogated glutamine starvation-induced reduction of FoxO1 protein in HCT116 cells (Figure 3B and Supplementary information, Figure S1B). We also performed a rescue experiment using a plasmid specifically expressing mutated XBP-1u to validate the XBP-1u's activity in the induction of FoxO1 degradation in HCT116 cells. The XBP-1u expressing plasmid rescued the reduction of FoxO1 degradation by XBP-1u RNAi in the absence of glutamine (Figure 3C), further showing that XBP-1u is responsible for the cytosolic FoxO1 degradation in response to glutamine starvation.
To confirm the role of XBP-1u in the degradation of FoxO1, we first tested whether XBP-1u interacts with FoxO1 using a co-immunoprecipitation assay. As shown in Figure 3D, endogenous FoxO1 interacted with XBP-1u in the presence of MG132 in the HCT116 cells after glutamine starvation. Next, to test whether the interaction between XBP-1u and FoxO1 was direct, an in vitro GST pull-down assay was carried out using bacterially expressed proteins. Wild-type FoxO1 protein that was translated in vitro was incubated with GST fusion proteins of full-length, C- or N-terminal XBP-1u; western blotting was then performed using an anti-FoxO1 antibody. As shown in Figure 3E, the C-terminal region of XBP-1u interacted with FoxO1. To examine the subcellular localization of the FoxO1 and XBP-1u interaction, we transfected H1299 cells with plasmids expressing GFP-FoxO1 and flag-XBP-1u, and performed immunofluorescence assays using an anti-flag antibody. We found that the majority of wild-type FoxO1 was present in the cytoplasm where it co-localized with XBP-1u in the absence or presence of glutamine (Figure 3F and Supplementary information, Figure S1C). These results suggest that FoxO1 interacts with XBP-1u in the cytoplasm upon glutamine starvation.
Moreover, FoxO1 degradation by the 20S proteasome was enhanced by incubation with full-length XBP-1u protein. In contrast, N-terminal XBP-1u protein, which was not observed to directly interact with FoxO1, did not affect FoxO1 degradation by the 20S proteasome (Figure 3G and Supplementary information, Figure S2). Furthermore, we examined the effects of XBP-1u on the FoxO1/20S proteasome interaction. As shown in Figure 3H, the 20S proteasome fraction was able to interact with FoxO1 as demonstrated by a GST-FoxO1 pull-down assay. The addition of in vitro translated full-length XBP-1u, but not N-terminal XBP-1u, facilitated the FoxO1/20S proteasome interaction. Taken together, these data suggest that the interaction between XBP-1u and FoxO1 is required for degradation of FoxO1 by the 20S proteasome.
Prior to degradation, FoxO1 is usually post-translationally modified by phosphorylation32,33. Therefore, we used two well-characterized kinase inhibitors, PD098059, an inhibitor of ERK, and SB203580, an inhibitor of p38, to investigate which cellular signaling pathway might be involved in XBP-1u-mediated FoxO1 degradation. HCT116 cells were pre-incubated with PD098059 or SB203580 for 30 min followed by incubation with or without glutamine in the presence of inhibitor for further 24 h. Blockage of ERK by PD098059 completely inhibited glutamine starvation-induced FoxO1 degradation; SB203580 did not inhibit degradation (Figure 4A). To further confirm the role of ERK in FoxO1 degradation, HCT116 cells were transfected with non-specific or ERK-specific siRNA, and FoxO1 degradation was assayed. The efficiency of the RNAi against ERK was significant, and as expected, upon glutamine starvation, FoxO1 was degraded in the cells transfected with the control siRNA. In contrast, FoxO1 remained at a higher level in the cells transfected with the ERK siRNA (Figure 4B and Supplementary information, Figure 3A), suggesting that ERK plays a critical role in FoxO1 degradation.
To determine whether ERK directly phosphorylates FoxO1 to induce FoxO1 degradation, a plasmid encoding a mutated FoxO1 (9A) in which the nine putative ERK phosphorylation sites in FoxO1 were mutated to alanine, or a plasmid encoding wild-type FoxO1 (WT), were separately transfected into H1299 cells. Both FoxO1 (WT) and FoxO1 (9A) were degraded after glutamine starvation (Figure 4C), indicating that ERK-mediated FoxO1 degradation does not result from direct phosphorylation of FoxO1 by ERK.
As FoxO1 interacted with XBP-1u during glutamine starvation, we could not rule out the possibility that ERK might directly phosphorylate XBP-1u, and that in turn, phosphorylated XBP-1u might play a role in FoxO1 degradation. Indeed, we found that glutamine starvation induced phosphorylation of both endogenous and overexpressed XBP-1u in HCT116 cells, as shown by a co-immunoprecipitation assay (Figure 4D and Supplementary information, Figure S3B). Using the software program GPS2.1, we identified two residues in XBP-1u, Ser61 and Ser176, as putative ERK target sites. Therefore, we generated a plasmid encoding a mutated XBP-1u (S61/176A) in which the two serine residues were changed to alanine. After transfection into HCT116 cells, we confirmed that glutamine starvation did not induce XBP-1u (S61/176A) phosphorylation (Figure 4E and Supplementary information, Figure S3C). The purified XBP-1u and ERK1 were then incubated in vitro to investigate whether ERK is responsible for XBP-1u phosphorylation. As shown in Figure 4F, XBP-1u was significantly phosphorylated by ERK1. These data suggest that ERK activity may be required for XBP-1u to modulate degradation of FoxO1.
To test whether the phosphorylation of XBP-1u by ERK has any effect on the interaction of XBP-1u and FoxO1, HCT116 cells were treated with or without the ERK inhibitor PD098059 and then exposed to glutamine starvation. Figure 5A and Supplementary information, Figure S4A show that PD098059 significantly disrupted the interaction between FoxO1 and XBP-1u. To test whether the decreased interaction between FoxO1 and XBP-1u was due to changes in XBP-1u localization, we collected nuclear and cytoplasmic fractions from HCT116 cells that had been treated with or without PD098059 prior to glutamine starvation. Figures 5B, 5C and Supplementary information, Figure S4B show that the majority of cytoplasmic XBP-1u translocated into the nucleus in the presence of PD098059 during glutamine starvation. To further investigate the role of phosphorylation in the nuclear export of XBP-1u, the XBP-1u (WT), XBP-1u (S61A), XBP-1u (S176A) or XBP-1u (S61/176A) plasmids were separately transfected into H1299 cells, followed by immunostaining and/or nuclear/cytoplasmic extraction. As shown in Figures 5D, 5E and Supplementary information, Figure S4C, XBP-1u (S61/176A) was localized to both the nucleus and the cytoplasm, whereas XBP-1u (WT) was mainly localized to the cytoplasm. The interaction of the 20S proteasome and XBP-1u was also disrupted when XBP-1u (S61/176A) was expressed in the presence or absence of glutamine (Figure 5F and Supplementary information, Figure S4E), indicating that Ser61 and Ser176 are essential for XBP-1u interaction with the 20S proteasome. Furthermore, XBP-1u mutants lacking ERK phosphorylation sites (S61/176A) or lacking 20S proteasome binding sites (1-204 aa) were also tested for their ability to destabilize FoxO1. Overexpression of XBP-1u (WT), but not the XBP-1u (S61/176A) or XBP-1u (1-204 aa) (Figure 5G), induced a decrease in FoxO1 protein levels. In addition, both single mutated XBP-1u (S61A) and XBP-1u (S176A) also induced a modest degradation of FoxO1, but much less than WT XBP-1u (Supplementary information, Figure S4D). These data indicate that dephosphorylation of XBP-1u promotes XBP-1u translocation from the cytoplasm to the nucleus and attenuates its interaction with the 20S proteasome, which leads to a decrease in FoxO1 degradation.
As FoxO1 is essential for the induction of autophagy in response to serum starvation or oxidative stress10, we tested whether XBP-1u suppresses autophagy via induction of FoxO1 degradation. As shown in Figure 6A and Supplementary information, Figure S5A, overexpression of XBP-1u significantly decreased FoxO1 protein levels, and blocked the accumulation of LC3-II and degradation of p62 induced by glutamine starvation. Similarly, the number of LC3 puncta significantly decreased when glutamine-starved HCT116 cells were transfected with XBP-1u, but not with XBP-1s (Figure 6B). To further clarify the role that endogenous XBP-1u plays in the induction of autophagy, an XBP-1 RNAi plasmid was transfected into HCT116 cells to establish stable XBP-1-knockdown cell lines; a non-specific RNAi plasmid was used as a negative control. These cell lines were separately cultured in glutamine-free medium for up to 48 h. Cell lysates were extracted for western blotting to detect changes in p62 degradation and LC3-II accumulation. LC3-II levels dropped by 36 h after glutamine starvation in cells containing normal XBP-1 levels (Figure 1A), whereas in XBP-1-knockdown cells, LC3-II levels did not drop until 72 h after glutamine starvation (Figure 6C and Supplementary information, Figure S5B, statistical data shown in Supplementary information, Figure S8). Additionally, glutamine starvation-induced p62 degradation was markedly reduced in XBP-1-knockdown HCT116 cells compared with control cells (Figure 6C, statistical data shown in Supplementary information, Figure S8). Consistently, even at 48 h after glutamine starvation, the number of autophagic cells did not drop in the XBP-1-knockdown cell lines as observed by fluorescent or electron microscopy (Figure 6D and 6E). We also performed the long-lived protein degradation assay in XBP-1-knockdown HCT116 cells. The 3-MA-sensitive degradation was persistently increased after glutamine removal (Figure 6F). In contrast, in FoxO1/XBP-1 double knockdown HCT116 cells, glutamine starvation did not induce p62 degradation or LC3-II accumulation (Figure 6G). These data indicate that downregulation of XBP-1 promotes autophagy and that this function requires FoxO1.
It is well known that autophagic death is a non-apoptotic form of programmed cell death. To investigate whether autophagy induced by XBP-1 knockdown has an effect on the overall survival of cancer cells, we tested the viability of HCT116 cells with or without XBP-1 knockdown under conditions of glutamine starvation. As expected, following glutamine starvation for 72 h, cell viability was significantly decreased in XBP-1-knockdown HCT116 cells compared with wild-type HCT116 cells (Figure 7A). Interestingly, cell death was inhibited in HCT116 cell lines that were stably transfected with the XBP-1- and FoxO1-RNAi plasmids, suggesting that XBP-1 knockdown-induced cell death upon glutamine starvation is dependent on FoxO1 (Figure 7A). To determine which type of cell death was occurring after XBP-1 knockdown, the autophagy inhibitor 3-MA or the apoptosis inhibitor Z-VAD-fmk were used. The cell death was greatly suppressed by 3-MA, verifying the role of autophagy in cell death caused by XBP-1 knockdown upon glutamine starvation (Figure 7B). These data suggest that persistent induction of autophagy induces cell death, which likely results from excessive degradation of cell components essential for survival.
To investigate the expression profiles of XBP-1, FoxO1 and p62 in CRCs, we conducted immunohistochemical (IHC) staining for XBP-1u, FoxO1 and p62 on a CRC-TMA containing 229 CRC specimens. Using the criteria described in Materials and Methods, high expression of cytoplasmic XBP-1, FoxO1 and p62 was observed in 120 (52.4%), 107 (46.7%) and 119 (52.0%) of the 229 CRC cases, respectively. Representative IHC stainings of XBP-1u, FoxO1 and p62 are shown in Figure 7C and 7D. A correlation analysis demonstrates that the expression levels of XBP-1u in CRCs are inversely correlated with the expression levels of FoxO1 (P < 0.05) (Table 1). In addition, the expression profiles of XBP-1u and FoxO1 in this CRC cohort were positively and negatively correlated with p62 expression, respectively (P < 0.05) (Table 1). Importantly, we also found that high levels of XBP-1u or low levels of FoxO1 were significantly associated with the survival of CRC patients after surgery, as well as tumors in the lymph node and/or distant metastasis and a more advanced clinical stage (Supplementary information, Figure S7, Tables S1 and S2). These data further support the hypothesis that the correct balance of XBP-1u and FoxO1 activities is a critical factor that influences the development of cancer.
In this study, we provide evidence that autophagy induced by glutamine starvation is a dynamic process that is highly associated with the turnover of FoxO1 protein. XBP-1u binds to FoxO1 and recruits FoxO1 to the 20S proteasome for degradation. This interaction between XBP-1u and FoxO1 is greatly enhanced by ERK1/2, which specifically catalyzes the phosphorylation of XBP-1u at Ser61 and Ser176; this suggests that cellular signaling pathways regulate the autophagic process by influencing FoxO1 levels (Figure 7E).
Earlier studies have shown that macroautophagy is a constitutively activated process6,7,34,35. It was believed that macroautophagy was activated during the first hours of serum deprivation but then gradually returned to basal levels. If starvation continued beyond that time, the decrease in macroautophagy was concomitant with a progressive increase in chaperone-mediated autophagy (CMA), which benefitted cell survival35. In CMA-deficient cells, the high rates of sustained protein degradation in response to serum starvation were offset by upregulation of macroautophagy34. It is known that mTOR, an important autophagy repressor, is reactivated by the degradation of autolysosomal products in a dynamic manner7. Upon mTOR reactivation, tubules extend from autolysosomal membranes and give rise to vesicles that ultimately form functional lysosomes7. Consistent with previous reports, we also found that autophagy decreased after long-term glutamine starvation treatment (Figure 1), which suggests that even in cancer cells autophagy is a dynamic process. Furthermore, FoxO1 turnover may be an important factor used by cancer cells to control the autophagic process that occurs in response to glutamine starvation.
It has been reported that the degradation of FoxO family proteins is mediated by the ubiquitin-proteasome pathway32,33,36. It has also been demonstrated that XBP-1s targets FoxO1 for ubiquitin-dependent degradation in MEF cells24. In this study, however, we demonstrate that XBP-1u is also a key regulator that modulates FoxO1 degradation in response to glutamine starvation. We believe that the conflicting results uncovered by our group and others on the specific isoform of XBP-1 that is involved in the degradation of FoxO1 could be explained by the different cell lines used in the respective studies; cancer cell lines were used in our study, and MEFs were used in the other study. In addition, differences in treatment conditions might also cause cells to use alternative responses to induce FoxO1 degradation; for example, we exposed cells to glutamine-free medium, whereas the other group used normal medium. Nevertheless, we present several important pieces of evidence that XBP-1u is a true regulator of FoxO1 degradation. First, glutamine starvation induced a significant increase in XBP-1u mRNA levels but only slightly increased XBP-1s mRNA levels (Supplementary information, Figure S6). Second, it was found that FoxO1 degradation occurred only in the cytoplasm and that XBP-1u directly interacted with FoxO1 (Figures 2D, 2E, 3D and 3E); however, XBP-1s was found to be localized to nucleus, which would make it difficult to directly induce FoxO1 degradation in response to glutamine starvation. Third, we demonstrate that XBP-1u recruits FoxO1 into the 20S proteasome for ubiquitin-independent degradation (Figure 3G and 3H). Consistent with our data, XBP-1u has also been reported to play an important role in protein degradation in HeLa cells. XBP-1s (or ATF6) forms a complex with XBP-1u that is degraded by the proteasome; the degradation domain in the C-terminus of XBP-1u is critical for the interaction between XBP-1u and 20S proteasome37,38. Consistent with other studies, we found that overexpression of wild-type XBP-1u, but not XBP-1u lacking proteasome binding sites (1-204 aa), was sufficient to decrease FoxO1 protein levels (Figure 5G).
It has been reported that ERK directly phosphorylates FoxO3 and that phosphorylated FoxO3 can be degraded via the MDM2-mediated ubiquitin-proteasome pathway22. However, in this study, the phosphorylation of FoxO1 may not be the key modification for ERK1/2-mediated FoxO1 degradation (Figure 4C). For example, although FoxO1 is degraded by the 20S proteasome in vitro, it is fairly stable in vivo, suggesting that the FoxO1 protein may not be easily accessible to the 20S proteasome in cells. Therefore, the modification of other FoxO1-interacting proteins, such as XBP-1u, is likely to contribute to FoxO1 destabilization in response to glutamine starvation. It is possible that upon glutamine starvation, XBP-1u undergoes phosphorylation-induced conformational changes to facilitate the entry of FoxO1 into the channel of the 20S proteasome.
XBP-1s can be phosphorylated by p38 MAPK on Thr48 and Ser61, which results in the nuclear translocation and increased stability of XBP-1s39. Our results show that ERK is also an important regulator of XBP-1u localization. After phosphorylation on Ser61 and Ser176, XBP-1u is prone to localize to the cytoplasm and interact with the 20S proteasome, leading to degradation of XBP-1u and FoxO1. Substitution of Ser61 and Ser176 in XBP-1u with alanine (Ser61/176A) diminishes the capacity of XBP-1u to drive FoxO1 degradation (Figure 5G). These data support the notion that ERK-dependent phosphorylation of XBP-1u on Ser61 and Ser176 plays a significant role in enabling the rapid destabilization and inactivation of FoxO1.
A growing body of evidence suggests that the autophagy can protect cells against cell death as well as mediate autophagic cell death40,41,42. In response to starvation, autophagy appears to be a cytoprotective process, as cells degrade non-essential components in order to generate the essential nutrients to meet the cell's energetic demands and maintain biosynthetic reactions43,44. However, autophagy is also involved in cell death, which is caused by the progressive destruction of all cytoplasmic structures, including mitochondria45,46. Our study suggests that autophagy is a protective mechanism under starvation conditions, as long as the autophagic process is not persistently activated. Once autophagy becomes constitutively activated, it induces cell death, which is most likely the result of excessive degradation of essential cellular components. Consistently, we found that after glutamine starvation the maintenance of FoxO1 activity by knocking down XBP-1u was sufficient to decrease cell viability in an autophagy-dependent manner (Figure 7A and 7B). Interestingly, a recent study also shows that XBP-1 deficiency in mice led to increased expression of FoxO1 that may be related to an enhanced autophagy in neurons29, further supporting that XBP-1 level is negatively related to FoxO1 level and autophagy. Furthermore, the repression of XBP-1 expression has been shown to inhibit tumor development in animal models47 and human tumor tissues48. Consistent with this, we also found that XBP-1u is highly expressed in human colon cancer samples, whereas FoxO1 is weakly expressed (Figure 7C and 7D). Taken together, our data suggest that the relationship between XBP-1u and FoxO1 may have significant relevance to clinical research.
In conclusion, turnover of FoxO1 may be an important mechanism that allows cells to modulate the autophagic process. In response to glutamine starvation, phosphorylated XBP-1u binds to FoxO1 and induces FoxO1 degradation. Therefore, targeting XBP-1u may be a useful strategy for the development of novel cancer therapies in the future.
A549, HCT116 and H1299 cells were grown in DMEM supplemented with 10% fetal bovine serum (heat inactivated at 56 °C for 45 min) and the appropriate amount of penicillin/streptomycin in a 37 °C incubator with a humidified, 5% CO2 atmosphere.
Flag-XBP-1u and XBP-1u plasmids were kindly provided by Dr Ling Qi (Cornell University, USA). GST-XBP-1, GST-XBP-1 (1-101) and GST-XBP-1 (83-261) were kindly provided by Dr Qinong Ye (Beijing Institute of Biotechnology, China). FoxO1 (9A) was kindly provided by Dr Akiyoshi Fukamizu (University of Tsukuba, Japan).
Protein expression was detected by western blotting as previously described with minor modifications. Equal amounts of proteins (100 to 150 μg) were separated by 9% to 15% SDS-PAGE. The antibodies used are anti-XBP-1 (Santa Cruz), anti-FoxO1 (#9462, Cell Signaling), anti-20S proteasome (Santa Cruz), anti-LC3 (Cell Signaling), anti-actin (Santa Cruz), anti-Flag (sigma), p62 (MBL) and anti-GFP (Santa Cruz).
For immunoprecipitation, cells were harvested and then lysed in NP-40 buffer supplemented with a complete protease inhibitor cocktail (Roche). Whole-cell lysates were used for immunoprecipitation with the indicated antibodies. Generally, 1-4 μg of commercial antibody was added to 1 ml of cell lysate, which was incubated at 4 °C for 8-12 h. After addition of protein A/G agarose beads, the incubation was continued for 1 h. Immunoprecipitates were extensively washed with lysis buffer and eluted with SDS loading buffer by boiling for 5 min.
Primers for human XBP-1 were 5′-CCTGGTTGCTGAAGAGGAGG-3′ (forward) and 5′-CCATGGGGAGATGTTCTGGAG-3′ (reverse). Primers for human XBP-1u real-time PCR were 5′-ATGGATTCTGGCGGTATT-3′ and 5′-AAGGGAGGCTGGTAAGG-3′.
Cells were suspended in buffer A (10 mM Hepes, pH 7.9, 10 mM KCl, 0.1 mM EDTA, 0.1 mM EGTA, 1 mM DTT, 0.15% NP-40 and 1% cocktail), swollen for 10 min on ice, and centrifuged at 12 000× g for 30 s. Supernatant was collected as a cytoplasmic extract. The pellet was washed, resuspended in buffer B (20 mM Hepes, pH 7.9, 400 mM NaCl, 1 mM EDTA, 1 mM EGTA, 1 mM DTT, 0.5% NP-40 and 1% cocktail), and rocked for 15 min at 4 °C. The supernatant after centrifugation was used as nuclear extract.
Cells were cultured to ∼80% confluency using the Chamber Slide System. After stress treatment, cells were fixed with 4% paraformaldehyde and permeabilized with methanol. Chamber slides were incubated with blocking solution (2% BSA in PBS), treated with primary antibody (1:100 dilution for all of the antibodies) overnight at 4 °C. After washed 3 times with blocking buffer, sides were treated with FITC/TRITC as the secondary antibody. Microscopic observation was performed using an Olympus BX-51 Research Microscope.
GST or GST fusion proteins were expressed in E. coli BL21 (Tiangen Biotechnology, Beijing, China), induced with 0.1 mM isopropyl-1-thio-β-D-galactopyranoside for 12 h at 16 °C, and purified following the protocol from Amersham Biosciences. Equal amounts of GST or GST fusion proteins were incubated with glutathione-Sepharose 4B beads (Amersham Biosciences) by rocking at 4 °C for 1 h, and the beads were then washed three times with TEN buffer (20 mM Tris-HCl, pH 7.4, 0.1 mM EDTA and 100 mM NaCl). Total cell extracts from HCT116 cells were added to the beads and incubated by rocking at 4 °C overnight. The beads were washed three times with TENT buffer (0.5% NP-40, 20 mM Tris-HCl, pH 7.4, 0.1 mM EDTA and 300 mM NaCl), and then dissolved in 2× SDS loading buffer after centrifugation and boiled for 5 min at 100 °C. After centrifuging, the supernatant was extracted and analyzed by western blotting.
Cells were grown in a 12-well plate (1 ml DMEM with 10% FBS per well) 1 day prior to the experiment. Cells were washed, incubated with leucine-free medium (leucine-free DMEM + 10% FBS) for 1 h to exclude endogenous leucine, and 5 Ci/ml [3H]-leucine was added into the medium in the presence of 1 ml leucine-free DMEM with 10% dialyzed FBS for 48 h incubation. After washing three times with 1 ml of DMEM containing 2 mM unlabelled leucine, the cells were incubated in DMEM (containing 10% FBS and 2 mM unlabelled leucine) for 24 h to degrade short-lived proteins. After transfection and starvation, cell aliquots (100 μl) were taken to detect radioactivity (count per minute, cpm) at different time points. The medium was removed, and cells were lysed and placed into a vial to determine the total incorporated radioactivity. The protein degradation rate was calculated as cpm in the medium divided by the total incorporated cpm.
GST-FoxO1 and XBP-1u/XBP-1uNT were incubated at 37 °C in HEPES buffer (50 mM HEPES, pH 7.5, 1 mM DTT and 0.018% SDS) in the presence of 20S proteasomes for 1 h. Samples from reaction mixtures were subjected to immunoblot analysis.
In the Mn2+-Phos-tag-modified acrylamide gel, the phosphorylated proteins migrate slower than non-phosphorylated proteins by the interaction of phosphate groups with Mn2+-Phos-tag (NARD Institute, Ltd., Hyogo, Japan). GST-XBP-1u was incubated alone or with GST-ERK (MERCK) in the kinase buffer (40 mM Tris-HCl, pH 7.5, 80 mM NaCl, 8 mM MgCl2, 0.8 mM DDT and 50 μM ATP) in a total volume of 50 μl. Reaction mixtures were incubated at 30 °C for up to 60 min and were terminated by the addition of sample loading buffer. The mixtures were then subjected to the Mn2+-Phos-tag SDS-PAGE (12% polyacrylamide gel including 50 μm MnCl2 and Phos-tag acrylamide), and analyzed by western blotting using anti-XBP-1 antibody.
Post-treatment cell viability was determined by staining with propidium iodide (PI, 2 μg/ml) and flow cytometric analysis on a FACScan.
In this study, the paraffin-embedded pathologic specimens from 229 patients with CRC were obtained from the archives of Department of Pathology, Cancer Center, Sun Yat-Sen University and Guangdong Provincial People's Hospital, Guangzhou, China, between January 2000 and November 2006. The cases selected were based on distinctive pathologic diagnosis of CRC, undergoing primary and curative resection for CRC, availability of resection tissue and followup data, and had not received preoperative anticancer treatment. These CRC cases included 142 (62.0%) men and 87 (38.0%) women, with mean age of 57.3 years. Average followup time was 55.42 months (median, 60.0 months; range, 0.5-98 months). Patients whose cause of death remained unknown were excluded from our study. Clinicopathologic characteristics for these patients were summarized in Table 1. This study was approved by the medical ethics committee of our institutes.
TMAs were constructed in accordance with a previously described method49. Triplicate 0.6 mm diameter cylinders were punched from representative areas of an individual donor tissue block, and re-embedded into a recipient paraffin block in a defined position, using a tissue arraying instrument (Beecher Instruments, Silver Spring, MD, USA).
The TMA blocks were cut into 5-μm sections and processed for IHC. TMA slides were incubated with anti-XBP-1 (1:100), anti-FoxO1 (1:50) and anti-p62 (1:200), respectively, and stored overnight at 4 °C. Immunostaining was performed using the Envision System with diaminobenzidine (Dako, Glostrup, Denmark). A negative control was obtained by replacing the primary antibody with a normal rabbit IgG. For the case of non-informative TMA samples (i.e., samples with < 500 tumor cells per case and lost samples), IHC staining was performed by using whole-tissue slides.
Positive expressions of XBP-1, FoxO1 and p62 in CRC tissues were primarily cytoplasmic patterns with a few cells showing nuclear staining (Figure 7C and 7D). Thus, in this study, we assessed the cytoplasmic expressions of the 3 proteins in our cohort of 229 CRC tissues. A semi-quantitative scoring criterion for IHC of XBP-1, FoxO1 and p62 was used, in which both staining intensity and positive areas were recorded. A staining index (values 0-12), obtained as the intensity of XBP-1, FoxO1 and p62 positive staining (negative = 0, weak = 1, moderate = 2 or strong = 3 scores) and the proportion of immunostaining positive cells of interest (< 25% = 1, 25%-50% = 2, > 50% – < 75% = 3, ≥ 75% = 4 scores) were calculated. The mean staining index of XBP-1, FoxO1 and p62 in this CRC cohort was 5.2, 2.7 and 6.3. Thus, categories of high expressions of XBP-1, FoxO1 and p62 were defined as CRC cases with staining index of more than 5.2, 2.7 and 6.3, respectively. Two independent pathologists (M-Y Cai and D Xie) blinded to the clinic pathologic information performed the scorings. The inter-observer disagreements were reviewed a second time, followed by a conclusive judgment by both pathologists.
Statistical analysis was performed by using the SPSS statistical software package (standard version 13.0; SPSS Inc., Chicago, IL, USA). The correlations between molecular features detected with each other and the associations between expressions of XBP-1, FoxO1 and p62, and CRC patients' clinic pathological features were assessed by the Chi-square test. For univariate survival analysis, survival curves were obtained with the Kaplan-Meier method. The Cox proportional hazards regression model was used to identify the independent prognostic factors. P < 0.05 were considered statistically significant.
(Supplementary information is linked to the online version of the paper on the Cell Research website.)
This study was supported by the Ministry of Science and Technology of China (2011CB910100 to YZ; 2011CB504200 to WZ), Program for New Century Excellent Talents in University, the National Natural Science Foundation of China (81222028, 30900722, 31070691 and 30921062), and “111 project” from the Minister of Education of China.
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Localization of XBP-1u and XBP-1s.
Supplementary information, Figure S2
Coomassie blue staining of GST and GST fusion proteins.
Supplementary information, Figure S3
Activation of the ERK signaling pathway is involved in FoxO1 degradation.
Supplementary information, Figure S4
Phosphorylation of XBP-1u by ERK is critical for the increased interaction of XBP-1u and FoxO1.
Supplementary information, Figure S5
Downregulation of XBP-1u induces autophagy.
Supplementary information, Figure S6
mRNA expression of XBP-1u and XBP-1s.
Supplementary information, Figure S7
Survival analysis of 229 CRC patients with XBP1, FoxO1 and p62 expressions.
Supplementary information, Figure S8
Statistical analysis of western blot data.
Supplementary information, Table S1
Correlations between expression of XBP1, FoxO1 and p62 and clinic pathological features in 229 patients with colorectal carcinoma
Supplementary information, Table S2
Univariate and multivariate analysis of different prognostic parameters in 229 patients with colorectal carcinoma
Keywords: FoxO1, XBP-1u, ERK, autophagy, cancer.
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