Nuclear export regulation of COP1 by 14-3-3σ in response to DNA damage
© Su et al; licensee BioMed Central Ltd. 2010
Received: 28 June 2010
Accepted: 15 September 2010
Published: 15 September 2010
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© Su et al; licensee BioMed Central Ltd. 2010
Received: 28 June 2010
Accepted: 15 September 2010
Published: 15 September 2010
Mammalian constitutive photomorphogenic 1 (COP1) is a p53 E3 ubiquitin ligase involved in regulating p53 protein level. In plants, the dynamic cytoplasm/nucleus distribution of COP1 is important for its function in terms of catalyzing the degradation of target proteins. In mammalian cells, the biological consequence of cytoplasmic distribution of COP1 is not well characterized. Here, we show that DNA damage leads to the redistribution of COP1 to the cytoplasm and that 14-3-3σ, a p53 target gene product, controls COP1 subcellular localization. Investigation of the underlying mechanism suggests that COP1 S387 phosphorylation is required for COP1 to bind 14-3-3σ. Significantly, upon DNA damage, 14-3-3σ binds to phosphorylated COP1 at S387, resulting in COP1's accumulation in the cytoplasm. Cytoplasmic COP1 localization leads to its enhanced ubiquitination. We also show that N-terminal 14-3-3σ interacts with COP1 and promotes COP1 nuclear export through its NES sequence. Further, we show that COP1 is important in causing p53 nuclear exclusion. Finally, we demonstrate that 14-3-3σ targets COP1 for nuclear export, thereby preventing COP1-mediated p53 nuclear export. Together, these results define a novel, detailed mechanism for the subcellular localization and regulation of COP1 after DNA damage and provide a mechanistic explanation for the notion that 14-3-3σ's impact on the inhibition of p53 E3 ligases is an important step for p53 stabilization after DNA damage.
Mammalian constitutive photomorphogenic 1 (COP1) is an evolutionarily conserved E3 ubiquitin ligase containing a RING-finger, a coiled-coil and WD40-repeat domains. COP1 is a crucial mediator to block photomorphogenesis in the dark through the ubiquitinated proteasomal degradation of light-induced transcription factor HY5 . In mammalian cells, COP1 regulates various cellular functions, such as proliferation and survival, by facilitating the degradation of physiological substrates through ubiquitin-mediated protein degradation. The ubiquitinated targets of COP1 include stress-responsive transcription factors, p53 tumor suppressor , c-JUN [3–5], transducer of regulated CREB activity 2 (TORC2, a glucose metabolite regulator) , FOXO1  and nucleosome remodeling factor MTA1 . It has been shown that DNA damage leads to COP1 nuclear exclusion, [9, 10] however, there is a knowledge gap about how DNA damage regulates COP1's translocation from the nucleus to the cytoplasm.
The 14-3-3 proteins are a family of evolutionarily conserved regulatory chaperone molecules involved in many diverse physiological functions, including signal transduction, stress response, apoptosis and cell cycle checkpoint regulation [10, 11]. In mammals, the 14-3-3 family comprises seven isoforms: β, ε, γ, ζ, η, σ, and τ, which are widely expressed in various tissues and exert their biological functions by directly binding to phosphoproteins containing the consensus motif RX (Y/F) XpSXP or RSXpSXP. This binding alters the proteins stability and/or subcellular localization . 14-3-3σ was originally characterized as a human mammary epithelial-specific marker (HME1) , and was later found to be an essential regulator of apoptosis, cell migration, cell cycle and DNA damage response. In contrast to the other 14-3-3 family members (β, ε, γ, ζ, η, and τ), which are able to form both homo- and heterodimers with other members, 14-3-3σ can form only homodimers . This unique characteristic implies that 14-3-3σ has exclusive functions and behaviors. 14-3-3σ, but not other family members, has been found to be frequently lost or decreased in various human cancers  and functions as a potential tumor suppressor. 14-3-3σ negatively represses AKT-induced MDM2 activation by promoting the cytoplasmic translocation of MDM2 and triggering its degradation [10, 16, 17]. 14-3-3σ also directly inhibits AKT-mediated tumor progression through binding-mediated suppression of AKT kinase activity . 14-3-3σ also obstructs cell cycle progression and prevents tumor cell growth by inhibiting cyclin-CDK complex activity . In the DNA damage response, 14-3-3σ is known to be a p53 downstream target and may serve as a regulator to prevent oxidative and DNA-damaging stress-induced mitotic checkpoint dysfunction . Although 14-3-3σ may play an important role in protecting cells from DNA damage, the detailed mechanism by which 14-3-3σ modulates the DNA damage response is not well characterized.
In this study, we examined the role of 14-3-3σ in DNA damage-mediated COP1 sub-cellular localization. We found that DNA damage induced COP1 nuclear exclusion, and that this phenomenon was abrogated in 14-3-3σ-null or -knockdown cells. Further investigation revealed that 14-3-3σ physically interacted with COP1 through an ATM phosphorylation site, which is phosphorylated in response to DNA damage. Importantly, 14-3-3σ utilizes its NES to mediate COP1 nuclear export, which leads to enhanced COP1 ubiquitination. Furthermore, 14-3-3σ was shown to not only mediate COP1 nuclear export but also repress COP1-mediated p53 nuclear export. Thus, our studies of 14-3-3σ's impact on COP1-shuttling provide mechanistic insight into COP1 localization and p53 regulation during DNA damage.
Subcellular fractionation (Lamin B1 was used as the marker of nuclear (N) fraction, while α-tubulin was used as the marker for cytoplasmic fraction) followed by Western blot analysis confirmed that the proportion of COP1 in the cytoplasmic fraction increased in DNA damaged cells (treated with doxorubicin or IR) compared with untreated controls (Figure 1C). Given that 14-3-3σ can be induced by DNA damaging agents and that 14-3-3σ exerts its influence by regulating the subcellular localization of its targets [19, 21], we then sought to determine whether 14-3-3σ expression can affect the subcellular location of COP1. Time-lapse confocal microscopy demonstrated that RFP-COP1 is dynamically shuttled between the nucleus and the cytoplasm in RFP-COP1-overexpressing cells infected with Ad-βgal, but this dynamic shuttling of COP1 was compromised when cells were infected with adenovirus containing14-3-3σ (Ad-14-3-3σ; Figure 1D). Subcellular fractionation followed by Western blot analysis again confirmed that the proportion of COP1 in the cytoplasmic fraction increased in Ad-14-3-3σ infected cells compared with Ad-βgal infected controls (Figure 1D). Thus, 14-3-3σ inhibited the dynamic shuttling of COP1 into the nucleus, concurrent with the increase of COP1 cytoplasmic staining.
It has been shown that ATM-mediated COP1 serine 387 (S387) phosphorylation leads to IR-induced COP1 nuclear exclusion . To investigate whether 14-3-3σ is involved and whether facilitation of COP1 cytoplasmic translocation by 14-3-3σ is dependent on S387 phosphorylation, we constructed the S387A mutant of COP1. Figure 2C shows that the S387A mutation inhibits the increase of COP1 in the cytoplasm after Ad-14-3-3σ infection in response to DNA damage, suggesting that 14-3-3σ-mediated COP1 nuclear export is dependent on S387 phosphorylation of COP1. Next we used confocal microscopy to demonstrate that GFP-COP1 dynamic shuttling between the nucleus and the cytoplasm in cells cotransfected with 14-3-3σ is inhibited, with most GFP-COP1 accumulating in the cytoplasm (Figure 2D). On the contrary, the dynamic shuttling of GFP-COP1 (S378A) was resistant to the nuclear-export effect of 14-3-3σ expression, with most of the GFP-COP1 located in the nucleus (Figure 2D). Together, these results suggest that 14-3-3σ has an essential role in mediating IR-induced COP1 nuclear exclusion after COP1 phosphorylation at S387.
It has been shown that MDM2 can cause p53 nuclear export; therefore, it raises the question whether COP1-mediated p53 nuclear export is through uncharacterized activity on MDM2. To exclude the contribution of MDM2, we performed the experiments described above by cotransfecting RFP-COP1 with GFP-p53 into p53-/- MDM2-/- MEF cells. Our results show that RFP-COP1 expression still caused nuclear export of GFP-p53 in p53-/- MDM2-/- MEF cells (Figure 6B), suggesting that COP1's function is independent of MDM2. Further, COP1-mediated p53 nuclear export is again hindered by 14-3-3σ in such a context (Figure 6B). Together, these results show that 14-3-3σ's impact on COP1 nuclear export (Figure 1) is also translated into preventing COP1-mediated p53 nuclear export.
The dynamic cytoplasm/nucleus distribution of COP1 is important for its function. In plants, the major purpose of COP1's nuclear import is to function as a master regulator of nuclear transcription regulator HY5 [24, 25], a positive regulator of photomorphogenic development. In mammalian cells, one of COP1's nuclear targets is p53, but the biological consequence of cytoplasmic distribution of COP1 is not well characterized.
Here we are able to provide important insights. First, we have shown that IR induces cytoplasmic distribution of COP1 (Figure 1) and facilitates COP1 cytoplasmic ubiquitination (Figure 5D) and that 14-3-3σ is essential for increasing DNA damageinduced cytoplasmic ubiquitination of COP1 as this activity is compromised by 14-3-3σ deficiency (Figure 5D). This 14-3-3σ-COP1 link fits very well with the notion that the inhibition of p53 E3 ligases is an important step for p53 stabilization after DNA damage. Second, we have shown that the N-terminal portion of 14-3-3σ interacts with COP1 (Figure 3) and that 14-3-3σ causes the nuclear export of COP1 through its leucine-rich nuclear export signal sequence , since the 14-3-3σ NES mutant loses the ability to export COP1. This observation is reminiscent of 14-3-3σ's impact on nuclear export of Cdc2 and Cdk2 [19, 21]. It is important to point out that little is known about what signals or mediators control the subcellular localization of COP1. Our discovery of 14-3-3σ's role in mediating COP1 nuclear export has filled this gap in knowledge. Third, ATM-mediated phosphorylation of COP1 at S387 promotes COP1's binding to 14-3-3σ (Figure 4C). Significantly, the interaction of COP1 with 14-3-3σ is important for facilitating COP1 to stay in the cytoplasm since the COP1 (S387A) mutant, which also lost the characteristic to bind 14-3-3σ, is resistant to 14-3-3σ-mediated nuclear export (Figure 2D). Therefore, both ATM and 14-3-3σ are involved in regulating COP1 subcellular localization. Given that 14-3-3σ is also an important regulator for kinases [19, 21], whether 14-3-3σ synergize with ATM to reinforce the 14-3-3σ-COP1 interaction will be another interesting layer of regulation to explore in the future. Lastly, we demonstrate for the first time that COP1 is able to cause p53 nuclear export (Figure 6), and this process is MDM2-independent (Figure 6B). Further, COP1's mediation of p53 nuclear export can still be inhibited by the expression of 14-3-3σ (Figure 6B). Because the mechanism behind COP1- mediated p53 nuclear export remains unknown, it is not clear how the nuclear COP1 binds p53 to regulate p53 nuclear export in the presence of 14-3-3σ. It is possible that 14-3-3σ binds to COP1 in the nucleus, and this binding changes the conformation and thus masks COP1's capability to export p53. Further investigation will provide the insight into this regulation. Taken together, these data suggest that the COP1 axis is independent of the MDM2 axis in terms of regulating p53 nuclear export.
It is important to point out that 14-3-3σ regulates both the MDM2-p53 axis (our previous study)  and the COP1-p53 axis (this study). Although the detailed mechanisms of COP1-mediated p53 nuclear export remain to be characterized, these findings highlight the complexity of the p53 nuclear export process and demonstrate that 14-3-3σ exerts negative impact on two p53 ubiquitin ligases to stabilize p53.
Human 293T, H1299, AT22IJE-T/pEBS7 (ATM-/-), AT22IJE-T/YZ5 (ATM+/+) and (p53-/-, MDM2-/-) MEF cells were cultured in DMEM/F12 medium supplemented with 10% fetal bovine serum. AT22IJE-T cells [ataxia-telangiectasia mutated protein (ATM)-/- fibroblasts] and AT22IJE-TpEBS7-YZ5 cells (ATM+/+, ATM-/- fibroblasts complemented with ATM cDNA)  were gifts from Dr. Y. Shiloh (Tel Aviv University, Tel Aviv, Israel). HCT116 and U2OS cells were maintained in McCoy's 5A medium. For transient transfection, cells were transfected with DNA using either Lipofectamine 2000 (Invitrogen), or FuGENE HD (Roche) reagents.
N-terminal Flag-14-3-3σ (1-161), and C-terminal Flag-14-3-3σ (153-248) have been previously described . RFP-14-3-3σ or RFP-COP1 was cloned into pdsRed1-C1 vector. RFP-14-3-3σ (NES I205A, L208A) mutant , GFP-COP1 (S387A) or Flag- COP1 (S387A) was constructed by PCR cloning. Ad-14-3-3σ and Ad-β-gal viruses  were produced as previously described . GFP-p53 was kindly provided by Dr G. Wahl . GFP-MDM2 was a kind gift from Dr Sudha Shenoy. Antibodies were purchased from the indicated vendors: Flag (M2 monoclonal antibody, Sigma), tubulin (Sigma), COP1 (Bethyl Laboratories), 14-3-3σ RDI), Myc (mouse monoclonal 9E10, Santa Cruz Biotechnology; rabbit polyclonal, Sigma), HA (12CA5, Roche), His (Cell Signaling), ubiquitin (Zymed Laboratories, Inc.) and Lamin B1 (Abcam).
For generation of 14-3-3σ knockdown stable cell lines, HCT116 cells were infected with Mission lentiviral shRNA transduction particles (Sigma) containing either control shRNA, 14-3-3σ shRNA (1) (5'-CCGGC CGGGT CTTCT ACCTG AAGAT CTCGA GATCT TCAGG TAGAA GACCC GGTTT TTG) or 14-3-3σ shRNA (2) (5'-CCGGG ACGAC AAGAA GCGCA TCATT CTCGA GAATG ATGCG CTTCTT GTCGT CTTTT TG). After infection, cells were selected with 2 μg/mL puromycin for 2 weeks.
For generation of RFP-tagged-COP1 (RFP-COP1) overexpression stable transfectants, U2OS cells or NIH 3T3 cells were transfected with RFP vector or RFP-COP1 plasmids by electroporation (Amaxa). Forty-eight hours after transfection, cells were selected in a culture medium containing 500 μg/mL G418 for 4 weeks.
Cells were lysed in lysis buffer (10 mM Tris, pH 7.6, 10 mM MgCl2, 1 μM DTT, 0.5% NP-40, phosphatase inhibitors and protease inhibitors), incubated on ice for 30 min, and homogenized by 20 strokes in a glass homogenizer. The homogenate was centrifuged at 4000 rpm for 5 min to sediment the nuclei. The supernatant was then centrifuged at 13,200 rpm for 10 min, and the resulting supernatant was used as the cytosolic fraction. The nuclear pellet was washed three times and resuspended in regular lysis buffer to extract nuclear proteins. The extracted material was centrifuged at 16,100 g for 20 min, and the resulting supernatant was used as the nuclear fraction.
RFP-COP1-expressing cells were treated with DNA damaging agents, including 1 μg/mL doxorubicin and 10 Gy IR, or infected with Ad-β-gal (multiplicity of infection [MOI] = 100) or Ad-14-3-3σ (MOI = 100). Live images of cells stably expressing RFP-COP1 were captured with an Olympus FV300 microscope or Zeiss Axiovert 200 M microscope. DNA staining was performed with 0.04 μg/mL Hoechst 33342.
Total cell lysates were solubilized in lysis buffer and processed as previously described . Lysates were immunoprecipitated with indicated antibodies. Proteins were resolved by SDS-PAGE gels and proteins transferred to polyvinylidene difluoride membranes (Millipore). Membranes were washed and incubated with primary antibodies and peroxidase-conjugated secondary antibodies (Thermo Scientific). Chemiluminescent images of immunodetected bands were recorded on X-ray films using the enhanced chemiluminescence (ECL) system (Roche).
293T cells were transiently cotransfected with indicated plasmids to detect exogenous COP1 ubiquitination. HCT116 14-3-3σ-/-and 14-3-3σ+/+ cells were used to detect endogenous COP1 ubiquitination. Cells were treated with 5 μg/mL MG132 (Sigma) for 6 hrs before harvesting. Cells were harvested and lysed with lysis buffer described above. Ubiquitinated COP1 was immunoprecipitated with anti-Myc (9E10, Santa Cruz Biotechnology) or anti-COP1 (Bethyl Laboratories) and immunoblotted with anti-HA (Roche) or anti-ubiquitin (Zymed Laboratories).
We are grateful to Drs. Y.Y. Wen, E. Bianchi, and R. Pardi for material support. Also, we thank L. Pham, and J. Tseng for technical support. We thank Dr. Zhenbo Han and Bill Spohn for microscopy support. This work was supported by grants from the National Institutes of Health (NIH) (R01CA089266), Directed Medical Research Programs (DOD SIDA BC062166 to S.J.Y. and M.H.L.) and Susan G. Komen Breast Cancer Foundation (KG081048). This research was supported in part, by a cancer prevention fellowship for G.V.T. supported by the National Cancer Institute grant R25T CA57730, Shine Chang, Ph.D., PI". The University of Texas M. D. Anderson Cancer Center is supported by NIH core grant CA16672.
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