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Previous Article | Next Article 
Molecular and Cellular Biology, November 2005, p. 9608-9620, Vol. 25, No. 21
0270-7306/05/$08.00+0 doi:10.1128/MCB.25.21.9608-9620.2005
Copyright © 2005, American Society for Microbiology. All Rights Reserved.
Radiobiology Division, National Cancer Center Research Institute, Tokyo 104-0045, and CREST and SORST, Japan Science and Technology Agency, Tokyo, Japan,1 David and Inez Myers Laboratory for Genetic Research, Department of Human Genetics and Molecular Medicine, Sackler School of Medicine, Tel Aviv University, Tel Aviv 69978, Israel,2 Department of Molecular and Cell Biology, Leiden University Medical Center, 2300 RA Leiden, The Netherlands,3 Department of Biological Sciences, Columbia University, New York, New York 10027,4 Molecular Oncology Division, National Cancer Center Research Institute, Tokyo 104-0045, Japan,5 Laboratory of Molecular Cancer Biology, Flanders Interuniversity Institute for Biotechnology, B-9052 Ghent, Belgium6
Received 17 February 2005/ Returned for modification 15 April 2005/ Accepted 14 August 2005
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ABSTRACT |
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INTRODUCTION |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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p53 is maintained at low levels in nonstressed cells to allow normal growth. Once cells are exposed to various forms of stresses, p53 is stabilized and activated as a sequence-specific transcription factor (20). Subsequently, activated p53 turns on multiple target genes, which induce a variety of biological outcomes such as cell cycle arrest or apoptosis (17). It is likely that induction of these target genes collectively protects organisms from developing cancer. Therefore, accurate regulation of p53 activity is crucial to maintain normal growth under nonstressed conditions and to prevent cells from undergoing oncogenic transformation.
A critical regulator of p53 is Mdm2. Mdm2 is the main protein responsible for maintaining p53 activity at a low level in nonstressed cells (15, 19, 36). Mdm2 inactivates p53 by promoting its degradation by functioning as an E3 ubiquitin ligase, stimulating its nuclear export, and blocking its transcriptional activity (22, 30). Interestingly, the mdm2 gene itself is a direct transcriptional target of p53, thus forming a negative feedback loop involving Mdm2 and p53 (5, 56). Mdm2 is overexpressed in a variety of human cancers, and most of these cancers retain wild-type p53. Therefore, the mdm2 gene is regarded as an oncogene that inactivates p53 by its overexpression (30).
Upon activation of p53 by external or internal stimuli, inactivation of Mdm2 plays an important role. Internal stimuli such as activated oncogenes activate p53 via induction of the p14ARF tumor suppressor, and it was shown that p14ARF induces p53 activity by inactivating Mdm2 (44). External stress, such as DNA damage, activates p53 by phosphorylating Mdm2 and inhibiting its activity as well as by directly inducing multiple posttranslational modifications of p53 itself (24, 26, 45, 49). Thus, Mdm2 is responsible for sensing a variety of cellular stresses and delicately modulating p53 activity.
The Mdm2-related protein Mdmx is another key negative regulator of p53 function. The importance of Mdmx on negative regulation of p53 is underscored by the fact that the embryonic lethal phenotype manifested by mdmx-null mice is rescued by p53 deficiency (10, 29, 33). Similar to Mdm2, Mdmx is overexpressed in a wide spectrum of human tumors that retain wild-type p53 (7, 37, 38). Thus, accumulating data indicate that mdmx is another oncogene that inactivates p53 upon overexpression.
Mdmx is related to Mdm2 in its structure and, like Mdm2, can inhibit transcriptional activity of p53 via direct binding at the N-terminal domain of p53 (46). In contrast to Mdm2, the mechanism by which Mdmx inhibits p53 activity is not well understood. Mdmx does not show robust E3 ubiquitin ligase activity toward p53 and is unable to target p53 for ubiquitin-dependent proteolytic degradation (14, 47). It was reported that Mdmx reduces p53 acetylation (7, 39), which may contribute to p53 inhibition by Mdmx.
It was demonstrated that Mdmx regulates Mdm2 as well as p53; Mdmx stabilizes Mdm2 and p53 (12, 14, 43, 47) and augments the ubiquitinase activity of Mdm2 toward p53 (3, 23, 47). On the other hand, a number of reports indicate that Mdmx in turn is regulated by Mdm2 and p53. Activated p53 stimulates Mdmx cleavage by caspase-3 (11), and Mdm2 targets Mdmx for ubiquitination and degradation (8, 16, 32). In addition, Mdm2 and p53 induce nuclear import of Mdmx (12, 21, 28). Thus, intricate feedback loops exist between p53, Mdm2, and Mdmx (15).
In contrast to Mdm2, it is not clear if inactivation of Mdmx is involved in p53 accumulation in response to various stimuli. It was shown that DNA damage induces Mdmx nuclear translocation (21) and Mdm2-dependent degradation of Mdmx (16). However, it remains unclear if nuclear transport or degradation of Mdmx impacts on p53 activity.
In order to gain further insight into the mechanisms of Mdmx regulation, we searched for a novel protein(s) that physically interacts with Mdmx. We found that several isoforms of 14-3-3 proteins bind to Mdmx and that binding of 14-3-3 is regulated by Mdmx phosphorylation at serine 367 (S367). S367 phosphorylation facilitates its degradation by Mdm2, while mutating S367 to alanine enhances the ability of Mdmx to inhibit transcriptional activity of p53 and promotes cell growth of normal fibroblasts. Furthermore, we demonstrate that DNA damage induces S367 phosphorylation and that the induction of the phosphorylation is associated with increased binding of Mdmx to 14-3-3 and shortening of the half-life of Mdmx. We discuss how DNA damage-induced phosphorylation of Mdmx at S367 can contribute to p53 activation.
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MATERIALS AND METHODS |
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To create pCMV-Myc-Hdm2, full-length human mdm2 cDNA was amplified by PCR with primers (5'-ATAGAATTCTGGTGAGGAGCAGGCAA-3' and 5'-TATCTCGAGCTAGGGGAAATAAGTTAGCA-3'), digested with EcoRI and XhoI, and inserted in frame into the corresponding sites of pCMV-Myc (Clontech). To create pCMV-HA-14-3-3
, full-length human 14-3-3 cDNA was amplified by PCR with primers 5'-ATAGAATTCTGGATGATCGAGAGGATC and 5'-TATCTCGAGTCACTGATTTTCGTCTTCC-3', digested with EcoRI and XhoI, and inserted in frame into the corresponding sites of pCMV-HA (Clontech). To create pBabe-hygro-Flag-Mdmx-wt and pBabe- hygro-Flag-Mdmx-S367, Flag-tagged full-length Mdmx or its S367A mutant was amplified by PCR with primers (5'-TATGGATCCGCCGCCACCATGGACT-3' and 5'-TATGTCGACTTATGCTATAAAAACCTTAATAA-3') using Flag-Mdmx and Flag-S367 as a template, respectively. Subsequently amplified DNA was digested with BamHI and SalI, and ligated into the corresponding sites of pBabe-hygro.
Antibodies.
The anti-Flag antibody (M2) conjugated with agarose and anti-Actin antibody were purchased from Sigma. Anti-14-3-3
antibody was purchased from Calbiochem. Anti-HA antibody was purchased from Covance. Anti-Flag (M2), anti-Myc tag (9E10), anti-14-3-3, anti-14-3-3
, anti-14-3-3 (K-19), and anti-Mdmx antibody (D-19) were purchased from Santa Cruz. Monoclonal anti-Mdmx antibodies 6B1A, 11F4D, and 12G11G were previously described (48). Monoclonal antibodies 3G12 and 7C8 were raised against purified glutathione S-transferase (GST)-Mdmx fusion proteins (K. Okamoto, unpublished data). A mixture of 6B1A, 11F4D, 12G11G, 3G12, and 7C8 was used for Western blot analysis described for Fig. 3B. Anti-LacZ antibody was purchased from Abcam. The anti-phospho-S367 polyclonal antibody was raised against a phosphopeptide corresponding to the sequences that span serine 367 (RTISAPVVRPC [phosphorylated serine is underlined]). The anti-phospho-S367 polyclonal antibody was further purified as described before (51).
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DNA transfection. In DNA transfection experiments using H1299, COS-1, CV-1 and MEF cells, 1 µg of DNA, and 3 µl of Fugene6 reagent (Roche) were introduced per 1.0 x 105 cells. Cells were then incubated for 48 h (COS-1 and CV-1) or 24 h (H1299 and MEFs) before harvest.
Retrovirus-mediated gene transfer. pBabe-hygro, pBabe-hygro-Flag-Mdmx-wt, or pBabe-hygro-Flag-Mdmx-S367 was used for preparation of amphotropic retroviruses as previously described (25). WI-38 or BJ cells were infected with retroviruses as described before (42), and hygromycin-resistant cells were selected with medium containing 150 µg/ml hygromycin for 4 days. Selected cells were then used for growth assays under the 3T3 protocol.
Purification of Mdmx-binding proteins. Flag-Mdmx was introduced into COS-1 cells by DNA transfection. For transfection in a large scale, 300 µg of DNA and 900 µl of fugene6 reagent (Roche) were introduced per 3.0 x 107 cells; 48 h after transfection, cells were lysed in MBP buffer (50 mM Tris, pH 7.5, 200 mM NaCl, 0.5% Tween 20, 10% glycerol, and 1 mM EDTA) supplemented with protease inhibitor cocktail (10 µg/ml antipain, 10 µg/ml leupeptin, 10 µg/ml pepstatin, 10 µg/ml chymostatin, 10 µg/ml E64, 10 µg/ml phenylmethylsulfonyl fluoride) and phosphatase inhibitor cocktail (PhI) (0.1 mM Na3VO4, 10 mM NaF) for 10 min. Lysates were sonicated, centrifuged twice at 20,000 x g for 10 min, and supernatant were agarose conjugated with anti-Flag antibody for 90 min. Anti-Flag immunoprecipitates were then washed two times with MBP buffer supplemented with protease inhibitor, PhI and 0.8 M NaCl, and four times with MBP buffer supplemented with protease inhibitor and PhI. Subsequently, Flag-Mdmx was eluted with Flag peptide (Sigma), and the eluent were concentrated by acetone precipitation. Flag-tagged proteins and copurified proteins were then separated by sodium dodecyl sulfate (SDS)-polyacrylamide gel electrophoresis (PAGE) and visualized by Coomassie staining. Proteins that were bound to Flag-Mdmx were eluted from the gel and used to determine their peptide sequences by mass spectrometry.
Immunoprecipitation and Western blot analysis. For immunoprecipitation of cell lysates, cells were washed in phosphate-buffered saline and lysed in 200-NP buffer (50 mM Tris-HCl, pH 7.5, 200 mM NaCl, 0.5% Nonidet P-40, 10% glycerol, 1 mM EDTA, 1 mM dithiothreitol) supplemented with protease inhibitor cocktail and PhI cocktail. In addition, the buffer was supplemented with 1 mg/ml N-methylmaleimide (Sigma), except for experiments described for Fig. 1B and 2B. Lysates were then centrifuged at 20,000 x g for 10 min, and supernatants were incubated with appropriate antibodies in the presence of protein G-Sepharose (Pharmacia) for 2 h. Immunoprecipitates were then washed four times with 200-NP buffer.
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In vivo ubiquitination assay. At 24 h after transfection, cells were treated with 50 µM MG132 for 3 h. Lysis of the cells and the purification of His-tagged proteins were performed as described before (8). Purified proteins conjugated with (His)6-ubiquitin were analyzed by Western blot analyses.
In vitro GST pull-down assay. GST and different GST-14-3-3 fusion proteins were expressed in bacteria and purified on glutathione-Sepharose; 1 µg of GST fusion protein was incubated with lysates prepared from neocarzinostatin-treated or untreated MCF-7 cells. The mixture was rotated for 2 h at 4°C and washed three times with Giordano lysis buffer (27). Proteins copurified on the Sepharose were separated on SDS-PAGE gels and used for Western blot analyses.
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RESULTS |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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30 kDa) that were specifically bound to Mdmx (Fig. 1A).
After large-scale copurification of Mdmx binding proteins, the identity of these polypeptides was determined by mass spectrometry. Analyses of oligopeptides derived from these endogenous proteins revealed that all of these polypeptides belong to a family of 14-3-3 proteins. The 14-3-3 family is composed of seven isoforms in mammals (ß, , , 
, 
, , and 
), and each member is involved in unique yet overlapping functions in cells (9, 52). The polypeptide that migrated more slowly than the others corresponds to 14-3-3, while the other two polypeptides that migrated faster as a doublet correspond to 14-3-3 and 14-3-3 (Fig. 1A). Binding of these 14-3-3 proteins to Mdmx was further confirmed by Western blot analyses (Fig. 1B).
Inspection of the amino acid sequences of human and mouse Mdmx revealed that they both harbor consensus motifs for binding of 14-3-3 (9, 52) that spans from amino acids 363 to 369 (Fig. 2A). In contrast, Mdm2 does not harbor a 14-3-3 consensus sequence, and failed to bind 14-3-3 proteins (Fig. 1A and 1B).
When we performed Western blot analyses under the same conditions as described for Fig. 1B, we also detected association of Mdmx with 14-3-3ß, 14-3-3, and 14-3-3 (data not shown). 14-3-3 expression was barely detectable, and association of Mdmx with 14-3-3 was not determined (data not shown). Thus, Mdmx associates with many isoforms of the 14-3-3 family.
Alanine substitution at serine 367 abolishes binding of Mdmx to 14-3-3. It is well documented that, in many cases, the conserved serine residue of the 14-3-3-binding consensus sequence (Fig. 2A) is phosphorylated in vivo, and that 14-3-3 binds preferentially to target proteins that are phosphorylated at this serine residue (9, 52). Thus, serine phosphorylation at the 14-3-3 binding site regulates functions of the target proteins by facilitating association between 14-3-3 and its targets.
In order to determine if binding of 14-3-3 to Mdmx is dependent on integrity of the conserved serine residue (S367) at the 14-3-3 binding consensus site, we created a mutant form of Mdmx in which S367 is substituted by alanine (S367A) (Fig. 2A). We transfected either wild-type Flag-Mdmx or its S367A mutant alone or together with HA-tagged 14-3-3 (HA-14-3-3) into cells and determined if the S367A mutation inhibits interaction between Mdmx and 14-3-3 by Western blot analyses. As expected, the S367A mutation abolished binding of Flag-Mdmx to HA-14-3-3 (Fig. 2B). Next we transfected either wild-type Flag-Mdmx or the S367A mutant into COS-1 cells, and examined if the the S367A mutation affects the association between transfected Mdmx and endogenous 14-3-3 proteins. As already presented in Fig. 1A, silver staining of proteins copurified with Mdmx demonstrated that wild-type Mdmx was capable of binding to endogenous 14-3-3 proteins (Fig. 2C, lane 2). In contrast, the S367A mutant was defective in binding to these proteins (Fig. 2C, lane 3). These data indicate that the S367A mutation abolishes binding between Mdmx and 14-3-3 proteins.
S367 is phosphorylated in vivo. Abolishment of Mdmx-14-3-3 interaction by mutation of S367 strongly suggests that this residue is phosphorylated in vivo. Therefore, we raised an antibody that specifically reacts with phosphorylated S367 (anti-P-S367). We validated specificity of the antibody by its loss of reactivity with Mdmx by the S367A mutation (Fig. 3A) and after phosphatase treatment of immunoprecipitated Mdmx (see Fig. S1 in the supplemental material). Using anti-P-S367, we determined if S367 of Mdmx is phosphorylated by Western blot analyses. We found that, after retrovirus-mediated transfer of wild-type Flag-Mdmx into WI-38 cells, the ectopically expressed Mdmx was phosphorylated at S367 and bound to 14-3-3 (Fig. 3A, lane 2). In contrast, neither S367 phosphorylation nor interaction with 14-3-3 was observed after introduction of the S367A mutant (Fig. 3A, lane 3).
In addition to WI-38, we also used two different cell lines, COS-1 and CV-1, to examine whether S367 is phosphorylated after introduction of Mdmx into cells by DNA transfection. In both cell lines, we found that wild-type Mdmx was phosphorylated on S367, and that the S367A mutation abolished both S367 phosphorylation and binding to 14-3-3 (data not shown). Thus, in three different cells, S367 is phosphorylated after exogenous introduction of Mdmx, and the S367A mutation abolishes both S367 phosphorylation and binding of Mdmx to 14-3-3. These data indicate that, like other 14-3-3 binding proteins, serine phosphorylation at the binding consensus sequence induces binding of 14-3-3 to Mdmx. Of note, aspartate mutation at S367 (S367D), as well as S367A, abolished binding of Mdmx to 14-3-3 (see Fig. S2 in the supplemental material). Presumably conformational change rather than a mere increase of negative charge at the 367 residue is necessary for binding of 14-3-3 to Mdmx phosphorylated at S367.
In order to determine if endogenous Mdmx is phosphorylated at S367 in vivo, we examined S367 phosphorylation in MCF-7 cells, which express high levels of endogenous Mdmx (7). Western blot analyses of anti-Mdmx immunoprecipitates indicated that S367 of endogenous Mdmx was phosphorylated in MCF-7 (Fig. 3B). Therefore, at least a fraction of S367 is phosphorylated at S367 under normal growth conditions.
The S367A mutation of Mdmx augments cooperative repression of p53-dependent transcriptional activation by Mdm2 and Mdmx. It was reported that Mdmx inhibits transcriptional activation by p53 (14, 46). In order to evaluate the potential effects of Mdmx S367 phosphorylation on transcriptional activation by p53, we determined the effect of either wild-type Mdmx or the S367A mutant on transactivation of the p53-responsive promoters (Fig. 4). Because it was reported that Mdm2 cooperates with Mdmx to inhibit transcriptional activity of p53 (12), we initially performed the transfection experiments both in the presence and the absence of Mdm2 in p53-deficient cells (H1299).
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In the presence of cotransfected Mdm2, we observed moderate reduction of luciferase activity from two p53-responsive promoters (the aip1 and the bax promoters) by wild-type Mdmx in H1299 cells. Notably, inhibition of luciferase activity by Mdmx was enhanced approximately by twofold when the S367A mutation was introduced (Fig. 4B and D), indicating that the S367A mutation augments the ability of Mdmx to repress transactivation by p53.
In contrast, in the absence of cotransfected Mdm2, we did not observe a significant reduction of luciferase activity from the aip1 or the bax promoter either by wild-type Mdmx or the S367A mutant under the same experimental conditions (Fig. 4A and C). These data indicate that Mdm2 and Mdmx cooperatively repress transcriptional activity of p53, and that the S367A mutation augments such cooperative repression of p53.
Next, we examined the effect of the S367A mutation in cells that are deficient in Mdmx or Mdm2. After cotransfection under conditions similar to those described for Fig. 4A and B, we measured luciferase activity from the aip1 promoter in p53–/–/mdmx–/– MEFs or p53–/–/mdm2–/– fibroblasts. Again we observed that the S367A mutation enhanced functional cooperation between Mdmx and Mdm2 to repress transactivation by p53 in p53–/–/mdmx–/– MEFs (Fig. 4E and F) and p53–/–/mdm2–/– fibroblasts (data not shown). Thus, enhancement of Mdmx function by the S367A mutation is not mediated by augmenting the activity of endogenous wild-type Mdmx or endogenous Mdm2, and the S367A mutant per se possesses higher activity to repress p53 function.
S367A mutant is resistant to Mdm2-dependent degradation of Mdmx. Enhanced repression of p53 by the S367A mutant prompted us to investigate its biochemical mechanism. In order to determine if the S367A mutation affects levels of introduced p53, Mdm2, or Mdmx, we first performed DNA transfection under the experimental conditions described for Fig. 4B and 4D in which the effect of S367 mutation on p53 was clearly observed, and determined levels of these proteins in H1299 cells.
In agreement with published data, levels of introduced Mdm2 increased after introduction of wild-type Mdmx (Fig. 5A, lanes 1 and 2). However, the S367A mutation did not cause a further increase the levels of Mdm2 (Fig. 5A, lanes 2 and 3). Likewise, the S367 mutation did not affect p53 levels (Fig. 5A, lanes 2 and 3). Therefore, it is not likely that enhanced activity of Mdmx by the S367A mutation depends on changes in the levels of Mdm2 or p53.
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The RING finger domain of Mdmx is responsible for its binding to Mdm2 (43, 50) and for its ubiquitination and degradation by Mdm2 (8, 23, 32). We examined if integrity of this domain is necessary for Mdm2-dependent inhibition of Mdmx in our experimental conditions. Mutation at C463, in which cysteine is substituted by alanine (C463A), compromises the integrity of the RING finger domain of Mdmx (23). Upon testing the mutant Mdmx (C463A), we found that it markedly reduced the affinity of Mdmx for Mdm2 (Fig. 5A, lane 4), and completely neutralized the ability of the S367A mutant to cooperate with Mdm2 to inhibit transcriptional activity of p53 (Fig. 5B). We also found that the C463A mutant was resistant to Mdm2-dependent inhibition (Fig. 6A, lanes 5 and 6), Thus, an intact Mdmx RING finger domain, which is needed for the Mdmx/Mdm2 interaction, is required for Mdm2-dependent inhibition of Mdmx.
S367A mutant is resistant to Mdm2-mediated proteasomal degradation. It was previously demonstrated that Mdm2 promotes Mdmx ubiquitination and targets it for proteasomal degradation (8, 16, 32). In order to determine if the reduction of levels of wild-type Mdmx by Mdm2 presented in Fig. 6A is mediated via proteasomal degradation, we introduced wild-type Mdmx alone or together with Mdm2 in either the absence or the presence of proteasome inhibitors. As already demonstrated in Fig. 6A, Mdm2 showed reduced levels of wild-type Mdmx in the absence of proteasome inhibitors (Fig. 6B, lanes 3 and 4). In contrast, reduction of wild-type Mdmx by Mdm2 was blocked in their presence (Fig. 6B, lanes 1 and 2), indicating that inhibition of wild-type Mdmx by Mdm2 is mediated by proteasome-mediated degradation.
It was previously shown that the half-life of wild-type Mdmx is markedly decreased in the presence of Mdm2 (8). In order to confirm that Mdm2 promotes degradation of wild-type Mdmx, the stability of introduced Mdmx was determined by a cycloheximide chase assay in the presence of Mdm2 (Fig. 6C). Either wild-type Flag-Mdmx or the S367A mutant was transfected into H1299 cells together with Mdm2 and lacZ, and transfected cells were further incubated with cycloheximide for 0 to 6 h. Subsequently, levels of Flag-Mdmx and LacZ in transfected cells before and after treatment with cycloheximide were determined by Western blot analyses to evaluate the stability of Flag-Mdmx and LacZ (8).
The results indicate clearly that the levels of wild-type Mdmx decreased more rapidly than those of the S367A mutant, while the stability of LacZ (Fig. 6C) as well as Mdm2 (data not shown) was similar in these transfections. Combined with the results described in Fig. 6A and 6B, these results indicate that the S367A mutation protects Mdmx from Mdm2-dependent proteasomal degradation.
Mdmx phosphorylated at S367 is preferentially degraded by Mdm2. The resistance of the S367A mutant to Mdm2-dependent degradation suggests that S367 phosphorylation facilitates degradation of Mdmx by Mdm2. In order to examine if Mdm2 preferentially targets Mdmx phosphorylated at S367 for degradation, we introduced wild-type Mdmx alone or together with Mdm2 into H1299 cells, and determined if the fraction of Mdmx phosphorylated at S367 relatively decreased in the presence of Mdm2 (Fig. 7A). Approximately equal amounts of immunoprecipitated Flag-Mdmx were used to compare the extent of S367 phosphorylation. Concomitantly with degradation of Mdmx by Mdm2 (Fig. 6A and 6B), the fraction of Mdmx phosphorylated at S367 decreased markedly (Fig. 7A, lanes 2 and 3). Furthermore, proteasome inhibitors blocked Mdm2-dependent reduction of a fraction of Mdmx phosphorylated at S367 (Fig. 7A, lanes 1 and 3). These results indicate that Mdmx phosphorylated at S367 is a preferred target for Mdm2-dependent proteasomal degradation. Taken together, our data demonstrate that S367 phosphorylation promotes Mdm2-dependent degradation of Mdmx.
S367A Mdmx mutant is resistant to Mdm2-dependent ubiquitination. Next, we attempted to determine whether the S367A mutation inhibits Mdm2-dependent degradation of Mdmx by blocking Mdmx ubiquitination by Mdm2. Either wild-type or the S367A mutant versions of Flag-tagged Mdmx were introduced into H1299 cells together with Myc-Mdm2, and the extent of Mdmx ubiquitination was determined by Western blot analyses. In order to facilitate detection of ubiquitinated Mdmx, (His)6-tagged ubiquitin was cotransfected. Subsequently we purified His-ubiquitin from lysates prepared from transfected cells and subjected them to Western blot analyses, probing with anti-Flag antibodies (Fig. 7B, upper panel). In the presence of transfected Mdm2, we observed polyubiquitination of wild-type Mdmx that was detected as slower-migrating forms of Mdmx (Fig. 7B, lane 3). In contrast, we did not observe significant polyubiquitination of the S367 mutant under the same conditions (Fig. 7B, lane 4). In the absence of transfected Mdm2, neither wild-type Mdmx nor the S367A mutant was ubiquitinated (Fig. 7B, lanes 1 and 2). We also observed the inhibition of polyubiquitination of Mdmx by S367 mutation if we examined anti-Flag immunoprecipitates after the cotransfection of Flag-Mdmx, Myc-Mdm2, and His-ubiquitin (see Fig. S4 in the supplemental material). Thus, the S367 mutation blocks Mdm2-mediated ubiquitination of Mdm2. Note that ubiquitination of Mdm2 itself was not significantly affected by the S367A mutation, as revealed by Western blotting of Myc-Mdm2 conjugated with His-ubiquitin (Fig. 7B, lower panel).
Taken together, our results show that S367 phosphorylation facilitates Mdm2-dependent ubiquitination and degradation of Mdmx.
S367 phosphorylation is induced by DNA damage. The stimulating effect of the S367A mutation on Mdmx-dependent inhibition of p53 activity strongly suggests that S367 phosphorylation may function to activate p53. The major stress known to induce p53 activity in cells is DNA damage. Of note, it was recently demonstrated that DNA damage profoundly affects the stability and subcellular localization of Mdmx (16, 21). Therefore, we examined if treatment of cells with DNA damaging agents can induce S367 phosphorylation in MCF-7 cells, which express high levels of endogenous Mdmx. Since our data indicate that Mdmx phosphorylated at S367 is targeted for proteasomal degradation, MCF-7 cells were pretreated with MG132 to block potential degradation of the phosphorylated Mdmx. Subsequently the treated cells were exposed to a variety of DNA-damaging agents, and lysates prepared from exposed cells were used to determine if S367 phosphorylation was induced.
Treatment of cells with gamma irradiation or etoposide caused rapid and drastic induction of S367 phosphorylation (Fig. 8B; see also Fig. S5 in the supplemental material). Treatment with adriamycin or UV also induced S367 phosphorylation, although the induction was weaker and slower than that caused by gamma irradiation or etoposide (Fig. 8B; see also Fig. S5 in the supplemental material). Thus, a variety of DNA lesions induce S367 phosphorylation of endogenous Mdmx.
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Induction of S367 phosphorylation after DNA damage is associated with shortening of the half-life of Mdmx. The results described in Fig. 6 and 7 indicate that S367 phosphorylation triggers Mdm2-dependent proteasomal degradation of Mdmx. Therefore, we next attempted to determine whether induction of S367 phosphorylation seen after DNA damage is associated with enhanced degradation of Mdmx. Remarkably, treatment of MCF-7 cells with adriamycin or etoposide reduced levels of Mdmx in the absence of MG132, while the proteasome inhibitor blocked such reduction (Fig. 8A). It is likely that reduction of Mdmx levels after etoposide treatment was caused by enhanced degradation of Mdmx, since etoposide treatment reduced stability of Mdmx (see Fig. S7 in the supplemental material).
Taken together, treatment of cells with DNA damage induces S367 phosphorylation, binding 14-3-3 to Mdmx, and degradation of Mdmx with a similar kinetics. Our data support the model that induced S367 phosphorylation triggers Mdmx degradation via facilitation of binding of 14-3-3 to Mdmx (see Fig. 10).
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DISCUSSION |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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, , and ) bind Mdmx, and that their association with Mdmx is dependent on Mdmx phosphorylation at S367. Through analyses of S367 phosphorylation, several new findings on Mdmx regulation are presented in this paper. First, S367 phosphorylation facilitates Mdm2-dependent ubiquitination and degradation of Mdmx. Second, the S367A mutation enhances the ability of Mdmx to cooperate with Mdm2 to repress transcriptional activity of p53. Third, S367 phosphorylation is induced after DNA damage. Finally, introduction of the S367A mutant into normal fibroblasts causes enhanced cell growth. Based on these data, we propose a model for the mechanism by which S367 phosphorylation of Mdmx regulates the trans-activating function of p53 (Fig. 10).
Our model depicts how a complicated network formed between Mdm2, Mdmx, and p53 is regulated by S367 phosphorylation. When Mdmx is not phosphorylated at S367, Mdm2 is not capable of targeting it for ubiquitination and degradation. This allows Mdmx to stably exist in cells and, in collaboration with Mdm2, to suppress p53 function. Once S367 is phosphorylated after DNA damage, Mdmx becomes a substrate for Mdm2-mediated ubiquitination and degradation. Thus, p53 is released from suppression by Mdmx and activated.
Mdm2 targets both Mdmx and p53 for degradation. Interestingly, efficient targeting of both substrates by Mdm2 is controlled by phosphorylation of its substrates. Ubiquitination and degradation of p53 by Mdm2 are inhibited by phosphorylation at the N-terminal domain of p53 (1, 36), while Mdm2-dependent ubiquitination and degradation of Mdmx are facilitated by S367 phosphorylation of Mdmx, as presented in this paper. Thus, in both cases, phosphorylation of the substrates of Mdm2 leads to p53 activation. p53 phosphorylation at the N-terminal domain is induced by DNA damage via activation of ATM/ATR kinases and Chk1/Chk2 kinases (6, 13, 40). Interestingly, S367 phosphorylation induced after DNA damage is blocked by caffeine, an inhibitor of ATM/ATR kinases (41) (see Fig. S8 in the supplemental material). Of note, Pereg et al. recently demonstrated that, after DNA damage, phosphorylation of Mdmx is induced at multiple sites, including S367 (S342, S367, and S403), and that one of the phosphorylation sites, S403, is a direct target of ATM kinase (34). Therefore, it is possible that the ATM/ATR kinase pathway plays a major role in phosphorylation of the N-terminal domain of both p53 and Mdmx at S367.
At this moment, the molecular mechanism of how S367 phosphorylation facilitates Mdm2-mediated ubiquitination is not clear. We observed that wild-type Mdmx and the S367 mutant showed a similar affinity for Mdm2 in transfected cells in the presence of MG132 (data not shown). Therefore, it is not likely that the resistance of the S367A mutant to Mdm2-mediated ubiquitination is due to reduced interaction between Mdm2 and the S367A mutant.
Because a direct outcome of S367 phosphorylation is likely to be binding of 14-3-3 proteins to Mdmx, it is likely that such binding facilitates Mdmx ubiquitination by Mdm2. 14-3-3 proteins bind a multitude of functionally diverse signaling proteins, and play critical roles in signal transduction pathways and cell cycle progression (53). One of the many functions attributed to 14-3-3 is shuttling of its target proteins between the cytoplasm and nucleus (9, 52, 53). In fact, it was demonstrated that Mdmx shuttles between these cellular compartments, and that Mdm2 can recruit Mdmx into the nucleus (12, 21, 28). Therefore, it may be possible that degradation of Mdmx is regulated through its translocation between the cytoplasm and the nucleus.
Recently it was demonstrated that Mdmx can be cleaved by caspase between amino acids 358 and 361, and it was proposed that this cleavage plays a functional role in p53 regulation (11). Since the caspase cleavage site is located in the vicinity of S367, we examined if caspase cleavage of Mdmx is regulated by S367 phosphorylation. The D361A mutation, which renders Mdmx resistant to caspase cleavage (11), did not inhibit the ability of the S367A mutant to enhance Mdmx-dependent inhibition of p53 (Fig. 5B). This is in agreement with the previous report that the D361A mutation does not affect Mdm2-dependent degradation of Mdmx (8). Thus, it is not likely that caspase cleavage of Mdmx is involved in regulation of Mdmx degradation by Mdm2.
It was reported that p14ARF stimulates Mdm2-dependent Mdmx ubiquitination and degradation by the proteasome (32). Interestingly, a splicing variant of Mdmx which lacks the Mdmx central domain shows increased sensitivity toward Mdm2- mediated ubiquitination and degradation (8). Thus, stimulation of Mdm2-dependent ubiquitination and degradation of Mdmx are caused by either S367 phosphorylation, binding of p14ARF, or deletion of the central domain. It may be possible that these effectors share the same molecular basis in facilitating Mdmx ubiquitination. Given that 14-3-3 functions as an adapter molecule (53) and S367 phosphorylation is required for interaction between Mdmx and 14-3-3, 14-3-3 binding may also regulate association between Mdmx and p14ARF or a protein(s) that interacts with the central domain of Mdmx. Detailed analyses of these observations may shed light on the mechanisms by which S367 phosphorylation and 14-3-3 binding facilitate Mdm2-dependent ubiquitination and degradation ofMdmx.
In line with our finding that the S367A mutation enhances the ability of Mdmx to suppress p53, we showed that S367A causes enhanced growth of normal cells in culture. Interestingly, the effect of the mutant is more striking in presenescent BJ fibroblasts that show retarded cell growth (Fig. 9B). It was reported that increased activity of p53 is associated with cell senescence (2, 18). Therefore, it may be possible that p53 is more active in presenescent BJ cells, and the potential effect of the S367A mutant to inhibit p53 becomes more pronounced as cells enter the presenescent stage and show higher levels of p53 activity. In fact, the S367A mutation decreases levels of p21, a p53 transcriptional target that plays a crucial role in cell cycle progression (Fig. 9B). Thus, the S367A mutation may affect Mdmx function by modulating transcriptional activity of p53 in BJ cells.
In summary, our data strongly suggest that Mdmx phosphorylation at S367 induced after DNA damage plays an important role in p53 activation. In future it will be very interesting to determine the precise mechanism for regulation of S367 phosphorylation in response to a variety of cellular stresses that are known to activate p53.
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ACKNOWLEDGMENTS |
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This work is supported by a Grant-in-Aid for Scientific Research from the Ministry of Education, Culture, Sports, Science and Technology of Japan (Y.T and K.O.), a Grant-in-Aid for Third Term Comprehensive Control Research for Cancer from the Ministry of Health, Labor and Welfare, Japan (Y.T.), a Grant-in-Aid from the Tokyo Biochemical Research Foundation (Y.T.), Research Grants from the Princess Takamatsu Cancer Research Fund and Takeda Science Foundation (Y.T.), and the Program for Promotion of Fundamental Studies in Health Sciences of Organization for Pharmaceutical Safety and Research of Japan (Y.T.). The work was also supported by NCI grant 87497 (to C.P). Work in the laboratory of Y.S. is supported by the A-T Children's Project, the A-T Medical Research Foundation, and the National Institute of Neurological Disorders and Stroke (NS31763).
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FOOTNOTES |
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Supplemental material for this article may be found at http://mcb.asm.org.
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