Protein methylation plays important roles in most, if not all, cellular processes. Lysine and arginine methyltransferases are known to regulate the function of histones and non-histone proteins through the methylation of specific sites. However, the role of the carboxyl-methyltransferase protein L-isoaspartyl methyltransferase (PIMT) in the regulation of protein functions is relatively less understood. Here we show that PIMT negatively regulates the tumour suppressor protein p53 by reducing p53 protein levels, thereby suppressing the p53-mediated transcription of target genes. In addition, PIMT depletion upregulates the proapoptotic and checkpoint activation functions of p53. Moreover, PIMT destabilizes p53 by enhancing the p53–HDM2 interaction. These PIMT effects on p53 stability and activity are attributed to the PIMT-mediated methylation of p53 at isoaspartate residues 29 and 30. Our study provides new insight into the molecular mechanisms by which PIMT suppresses the p53 activity through carboxyl methylation, and suggests a therapeutic target for cancers.
Protein l-isoaspartyl methyltransferase (PIMT), the 'protein repair enzyme', specifically methylates the isoaspartyl residue generated by the spontaneous deamidation of asparagine, and this methylation is an essential step for converting isoaspartate to aspartate1. Because asparagine deamidation, which is primarily found in aged proteins, impairs protein function2,3, most studies of PIMT focus on elucidating its role in protein repair1,4. However, recent studies have shown that asparagine deamidation regulates normal cellular processes, including synaptic transmission5, cellular matrix interactions6,7,8,9, lifespan10,11 and apoptosis12,13,14,15. Thus, the PIMT-mediated methylation of isoaspartate may also be involved in normal biological processes.
Research to date has suggested that PIMT is linked to apoptosis, which is an essential cellular process for cell death. These studies show that the induction of PIMT protects cells from apoptosis caused by H2O2 stress16 or Bax overexpression17, whereas the inhibition of PIMT increases apoptosis upon DNA damage18. In addition, the effect of PIMT on apoptosis is mediated through modulating the deamidation of Bcl-xL16,19. Although these results raise the possibility that PIMT could be a regulator of apoptosis, the precise molecular mechanisms of PIMT in apoptosis have yet to be defined.
p53 is a potent tumour suppressor and regulates several cellular processes, including metabolic homeostasis, DNA repair, growth arrest, senescence and apoptosis. p53 is involved in various signal pathways by interacting with cellular proteins, and its activity is regulated by different post-translational modifications, such as ubiquitination, phosphorylation, acetylation, ribosylation and glycosylation20. Recently, it was also found that the activity and cellular functions of p53 are regulated by lysine or arginine methylation of specific site in p5321,22,23,24,25,26. However, the role of carboxyl methylation in p53 regulation is still unrevealed.
Here we show that PIMT suppresses the activity of p53 through destabilizing p53 by enhancing the p53–HDM2 interaction, which leads to the inhibition of p53 target gene expression. We also find that PIMT methylates p53 at isoaspartate residues 29 and 30, which is required to negatively regulate the p53 activity. Collectively, we suggest carboxyl methylation as a post-translational modification of p53, providing an alternative function of PIMT in p53 regulation.
PIMT is associated with the p53 pathway
To examine the clinical relevance of PIMT, we dichotomized lung (n=442) and breast (n=404) cancer patients according to the expression levels of PIMT using publicly available gene expression data27,28,29. The survival of patients exhibiting higher expression of PIMT levels was significantly poorer than those with lower expression levels (Fig. 1a). These data suggest that the increased expression of PIMT might be a key genetic event during cancer development. On the basis of these findings and previous observations16,17,18,19, we hypothesized that PIMT could be involved in regulating the function of p53, which is a potent tumour suppressor and major regulator of apoptosis. To test this hypothesis, we examined the expression levels of PIMT and p53 in several cell lines. The level of p53 protein was generally anti-parallel with that of PIMT protein, particularly in the NTERA2 and NCCIT cells derived from poorly differentiated aggressive tumours (Fig. 1b). To gain insight into the influence of PIMT on the p53 pathway, we tested the effect of PIMT depletion using short interfering RNA (siRNA) and short hairpin RNA (shRNA), and found that reduction in the levels of PIMT increased the p53 protein levels in U2OS cell (Fig. 1c,d). The effects of PIMT depletion on the level of endogenous p53 protein were confirmed in other cancer cell lines (Fig. 1e). Conversely, the ectopic expression of PIMT decreased the p53 protein levels in a dose-dependent manner (Fig. 1f). In addition, the expression of PIMT in the PIMT-depleted cells suppressed the increase of p53 protein levels, suggesting that the effect of PIMT is specific (Fig. 1g). PIMT knockdown in U2OS cells did not affect the MEK and AKT signalling pathways that regulate the p53 protein levels (Supplementary Fig. S1a–c). Overall, these data demonstrate that PIMT negatively regulates p53 protein levels.
PIMT inhibits the activity of p53
To investigate the effects of PIMT on p53 function further, we examined whether PIMT regulates p53 target gene expression. Among the genes activated by p53, the depletion of PIMT resulted in the expression of p21, HDM2, PUMA and TSP1 (Fig. 2a,b), whereas PIMT knockdown reduced the expression of CD44, a gene that is normally repressed by p53 (Fig. 2b). However, upon the ectopic expression of PIMT, the expression levels of the p53 target genes were inversely proportional to those resulting from PIMT depletion (Supplementary Fig. S2a,b). These data indicate that PIMT represses the expression of p53 target genes. We then used H1299 cells, which lack endogenous p53, to examine whether the effect of PIMT on the target gene expression depended on p53. In the absence of p53, PIMT did not affect the expression of the p53 target genes, whereas PIMT negatively effected the expression of the p53 target genes in the H1299 cells transfected with p53 (Supplementary Fig. S3a,b). Moreover, the upregulation of p21 expression upon PIMT knockdown was eliminated by the co-knockdown of p53 (Fig. 2c and Supplementary Fig. S3c). These results indicate that PIMT represses the expression of the p53 target genes in a p53-dependent manner.
The effects of PIMT on p53 target gene expression suggested that PIMT might regulate p53-dependent transcriptional activity. Thus, we used a luciferase construct linked to a p21 or Bax promoter, which are well-characterized p53 target genes, to address this possibility and found that PIMT inhibited the p53-dependent transcription of both reporter genes (Supplementary Fig. S4a,b). Using a chromatin immunoprecipitation assay, we investigated whether PIMT could affect the p53 occupancy at the promoters of its target genes and observed that PIMT depletion induced p53 occupancy at the p21 and HDM2 promoters (Fig. 2d). These data indicate that PIMT negatively affects the transcriptional activity of p53. Because PIMT reduced p53 target gene expression and repressed the transcriptional activity of p53, we speculated that PIMT might inhibit the cellular functions of p53. To determine whether PIMT could suppress the response of p53 to DNA damage, we measured the expression of p53 target genes upon DNA damage. Under genotoxic stress, PIMT depletion induced the expression of p53 target genes, including p21, HDM2, TSP1, 14-3-3, PUMA and GADD45 (Supplementary Fig. S5a–c); however, the expression of CD44 and BIRC5, genes that are normally repressed by p53, was reduced by PIMT depletion (Supplementary Fig. S5c). In contrast, the expression of the p53 target genes was suppressed by the ectopic expression of PIMT (Supplementary Fig. S6a,b). These data indicate that PIMT inhibits p53 target gene expression upon DNA damage. We next addressed the role of PIMT in apoptosis and cell-cycle arrest. Using lentivirus-mediated PIMT shRNA, we generated three stable cell lines with different PIMT expression patterns that contrasted with the p53 expression patterns. Consistent with the induction of p53 in these cells, the expression of the p53 target genes was also upregulated. Furthermore, the active caspase-3 and poly-(ADP-ribose) polymerase cleavage levels, which are well-known apoptosis markers, were increased in the PIMT knockdown stable cell lines (Fig. 2e). Compared with the control, the growth rate of the PIMT knockdown stable cell lines was reduced and correlated with the reduction of PIMT expression (Fig. 2f and Supplementary Fig. S7a). In addition, the PIMT knockdown stable cell lines displayed a lower efficiency of colony formation in soft agar, a phenotype that is representative of cell transformation (Fig. 2g). Upon DNA damage, the PIMT knockdown rendered the cells more prone to apoptosis compared with the control cells (30.1% early apoptosis in the PIMT-depleted cells versus 19.5% for the control cells treated with 1 μg ml−1 adriamycin) (Fig. 2h). These data were also confirmed in the PIMT knockdown stable cell lines (Supplementary Fig. S7b). These results suggest that PIMT represses apoptosis and growth arrest through the negative regulation of the p53 activity.
The methylase activity of PIMT is required to regulate p53
We then sought to determine whether the methylase activity of PIMT was required for modulating the p53 activity. To this end, we mutated glycine 88 (G88) within motif I, a residue that is critical for the methylase activity of PIMT30,31. The overexpression of this PIMT mutant, if not all, failed to reduce the p53 transactivation activity and p53 target gene expression (Fig. 2i,j). These data were also confirmed in H1299 cells through the ectopic expression of p53 (Supplementary Fig. S8a,b). These results demonstrate that the methylase activity of PIMT is necessary for regulating p53 activity.
PIMT interacts with p53
To clarify the role of PIMT in p53 regulation, we confirmed that PIMT could interact with p53. p53 was found to co-immunoprecipitate with PIMT in H1299 cells co-expressing PIMT and p53 (Fig. 3a,b). Using MCF7 or U2OS cells, the reciprocal immunoprecipitation with PIMT demonstrated the interaction with endogenous p53, and this interaction was disrupted by adriamycin treatment (Fig. 3c,d). These data indicate that PIMT interacts with p53.
PIMT methylates asparagine residues 29 and 30 of p53
Because PIMT interacted with p53 and its methylase activity was necessary for regulating p53, we examined whether PIMT directly methylates p53. Using an in vitro methylation assay, we found that PIMT methylated p53, whereas the PIMT G88A mutant did not (Fig. 4a and Supplementary Fig. S9a). To determine the specific region of p53 methylation, we performed the in vitro methylation assay using truncated p53. The N terminus of p53 (amino acids 1–82) was methylated by PIMT, but not by the PIMT G88A mutant (Fig. 4b,c). Moreover, these methylations were removed upon alkaline treatment, confirming that the p53 methylations were specifically attributed to carboxyl methylation and not lysine or arginine methylation (Fig. 4d). We then generated several mutants in which selected asparagine or aspartate residues were replaced with alanine residues, and then performed in vitro methylation assays. The substitution of N29 or N30 with alanine (N29A or N30A) in the N terminal of p53 mostly abolished the PIMT-mediated methylation (Fig. 4e). To confirm that PIMT methylates p53 at isoaspartate residues 29 and 30, we synthesized peptides consisting of amino acids 22–40 of p53, in which asparagines 29 and 30 were replaced with isoaspartates (N29IsoD, N30IsoD and N29,30IsoD). Using in vitro methylation assay, we found that PIMT methylated N29IsoD, N30IsoD and N29,30IsoD, but not the wild-type p53 peptide (Fig. 4f and Supplementary Fig. S9b). We also observed a 14 Da mass shift for both N29IsoD and N30IsoD, but not for the p53 peptide containing asparagine residues 29 and 30 (Supplementary Fig. S9c). Furthermore, we identified 14 and 28 Da mass shifts for the p53 peptide, N29,30IsoD (Supplementary Fig. S9c). In consistent with this result, the substitution of N29 and N30 with alanine in the full-length p53 (N29,30A) resulted in the depletion of the PIMT-mediated methylation (Fig. 4g). Nano-flow liquid chromatography-coupled electro spray ionization tandem mass spectrometry (nano-LC-ESI-MS/MS) analysis also confirmed the methylations at IsoD29 and IsoD30 in the recombinant p53 (Supplementary Fig. S9d). These data indicate that asparagine 29 and 30 could be target sites for PIMT-mediated p53 methylation.
To test the stability of p53 methylation, we performed an in vitro methylation assay with purified GST-p53 and GST-PIMT, and incubated the methylated GST-p53 at 37 °C under different pH conditions. The methylation of p53 was stable at pH 6.4–8.4, a physiological pH range of cells (Fig. 4h). We also found that methylation of p53 peptide was maintained after incubation at 37 °C for 24 h (Fig. 4i).
PIMT only methylates isoaspartate, which is generated by the deamidation of asparagine residue. For this reason, we next determined whether or how fast asparagine residues 29 and 30 in the p53 peptide (amino acids 22–40) are deamidated (Fig. 5a). PIMT methylated the p53 peptide during a 30-min incubation period and the level of methylated peptide increased with increasing incubation time (Fig. 5b). Nano-LC-ESI-MS/MS analysis also identified the deamidation of asparagine residues 29 and 30 in incubated p53 peptides, indicating that asparagine residues 29 and 30 of p53 can be rapidly deamidated in vitro (Fig. 5c and Supplementary Fig. S10a–c).
Next, we determined whether PIMT methylates p53 under physiological conditions through nano-LC-ESI-MS/MS analysis of endogenous p53 purified from U2OS cells or ectopic-expressed p53 purified from H1299 cells under conditions in which the PIMT-catalyzed methylation of the isoaspartyl residues was stable enough for detection (Fig. 4h,i). We found that two asparagine residues, N29 and N30, were deamidated and methylated (Supplementary Fig. S11a–c); however, methyl+deamidated p53 was not detected in the PIMT knockdown U2OS cells (Supplementary Fig. S11d). These results confirm the PIMT-mediated methylation of endogenous p53.
In addition, there are two theoretical deamidation-susceptible sites in p53, asparagine residues 239 and 268. Although we found that only one site, asparagine 268, in the endogenous p53 immunoprecipitated from the U2OS cell extracts was deamidated, we could not detect the methylation of the deamidated asparagine 268 (Supplementary Fig. S12). Thus, the methylation of deamidated asparagine residues 29 and 30, but not 268, might play an important role in the regulation of p53 activity. Our sequence alignment analysis confirms that asparagine residues 29 and 30 are conserved in the nine upper vertebrate p53 proteins listed in GenBank (Supplementary Fig. S13a). Interestingly, the p53 proteins in Rattus norvegicus and Mus musculus do not contain conserved asparagine 29 and 30 residues. Moreover, the PIMT knockdown in three different mouse cell lines does not affect the level of p53 protein (Supplementary Fig. S13b).
PIMT influences the stability of p53
The N29 and N30 residues are located near the domain implicated in the regulation of HDM2 binding and p53 stability (Fig. 6a). Furthermore, PIMT depletion upregulated the p53 protein levels without increasing the p53 mRNA levels (Fig. 6b). These results suggest that PIMT regulates p53 levels by destabilizing the p53 protein. To test this possibility, we investigated the effects of PIMT on the major regulation mechanism for p53 stability, degradation and ubiquitination. PIMT depletion restrained p53 degradation (half-life of p53, 58.1 min in the PIMT-depleted cells versus 8.7 min in the control cells) and reduced the ubiquitination of p53 (Fig. 6c–e). Conversely, the ectopic expression of PIMT increased p53 ubiquitination (Fig. 6f). These results suggest that PIMT positively regulates the ubiquitination and destabilization of p53.
To investigate how these effects converged on p53 ubiquitination, we next determined whether PIMT affects the interaction of HDM2 and p53 and found that the interaction was impaired by PIMT depletion and enhanced by the ectopic expression of PIMT (Fig. 6g,h). In addition, the binding of the p53 mutants (N29A, N30A) to HDM2 was diminished and was accompanied with an increase in the p53 protein levels (Fig. 6i,j). These data were also confirmed using other p53 mutants in which glutamate (E) or glutamine (Q) residues were substituted for the asparagine residues (Fig. 6k,l). These results indicate that methylation at N29 and N30 are necessary for the destabilization of p53, most likely through ubiquitination by enhancing the interaction of p53 and HDM2.
Because deamidation of asparagine residues resulted in structural change of protein, it could affect the binding affinity of target proteins5,32. To test this, we performed surface plasmon resonance analysis using the N29,30IsoD peptide and revealed that N29,30IsoD peptide had a lower (KD=694 μM) HDM2 binding affinity than wild-type peptide (KD=141 μM) (Supplementary Fig. S14a–c). In addition, a competitive binding assay of N29,30IsoD and methylated N29,30IsoD peptides with HDM2 showed that the methylated N29,30IsoD peptide had a higher HDM2 binding affinity than the N29,30IsoD peptide (Supplementary Fig. S15a,b).
PIMT is a well-known carboxyl-methyltransferase that specifically methylates isoaspartyl residues. Although the enzymatic mechanism of PIMT is well established, the biological function of PIMT is controversial and far from being completely understood. Here, we reveal the critical roles of PIMT in p53 regulation. We show that PIMT suppresses p53 protein levels and target gene expression by reducing the transcriptional activity of p53. We also find that PIMT disrupts the response of p53 to DNA damage. Under genotoxic stress, PIMT inhibits the expression of damage-induced p53 target genes and protects cancer cells from apoptosis, which is the most important function of p53 in tumour suppression. Moreover, cell proliferation is impaired in the PIMT knockdown stable cell lines, as indicated by the increased p53 protein levels and target gene expression. We also demonstrate that the reduced survival rates of cancer patients are related to the increased expression of PIMT. We observe that PIMT expression is increased in several cancer cell lines, including the NTERA2 and NCCIT cells, derived from poorly differentiated aggressive tumours. Thus, we speculate that PIMT plays an important role in obstructing the tumour suppression function of p53 by modulating its activity; thus, PIMT is a potential oncogene. On the basis of our results, PIMT deserves further investigation to understand its full potential in cancer development and progression.
In this study, we also reveal that p53 protein is a novel substrate for PIMT. We show that asparagine residues 29 and 30 of p53 are methylated by PIMT in vivo and in vitro. We demonstrate that PIMT depletion hinders the interaction between p53 and HDM2, resulting in an augmentation of the p53 protein. We also observe that the protein levels of p53 mutants in which asparagine residues 29 and 30 are replaced with glutamines or alanines are increased, as indicated by the reduction of their binding to HDM2. These results suggest that PIMT and its methylation of p53 are required for p53 destabilization through the enhancement of the interaction between HDM2 and p53. Because the PIMT-mediated methylation of p53 could directly regulate the interaction between HDM2 and p53, PIMT might act as a regulator for the maintenance of p53 steady-state levels, and the interaction of p53 and HDM2 could be regulated through the PIMT-mediated methylation of isoaspartyl residues. The surface plasmon resonance analysis and a competitive binding assay demonstrate that p53 deamidation impairs the binding to HDM2, while methylation of deamidated p53 enhances it (Supplementary Figs S14a–c and S15a,b). These observations support the hypothesis that PIMT might act as a regulator for the maintenance of p53 steady-state levels by tagging p53 for degradation rather than by repairing the isoaspartyl residues to aspartates.
Although asparagine deamidation is a non-enzymatic and spontaneous reaction, it is now clear that the rate of asparagine deamidation primarily depends on the amino-acid residues near the asparagine in the peptide chain and the three-dimensional structure of the protein33,34,35. Several studies suggest that asparagine deamidation is not unregulated, but is genetically programmed and acts as an embedded clock that functions during the lifetime of a protein36,37. Thus, asparagine residues 29 and 30 of p53 might not be suitable for deamidation reaction because Asn–Asn–Val is an unusual deamidation-susceptible sequence36. However, we demonstrate that asparagine residues 29 and 30 in the p53 peptide could be rapidly deamidated in vitro, despite their unusual deamidation-susceptible sequence (Fig. 5b,c). Consistent with these observations, we also observe the deamidation of asparagine residues 29 and 30 in immunoprecipitated p53 in vivo (Supplementary Fig. S11a–d). Several studies demonstrate that the deamidation rate could also be regulated through signal-transduction pathways: the deamidation of Bcl-xL occurs in response to DNA damage12,13,14,15,16,19 and is suppressed by the Rb protein12, the p56lck kinase14, the BCR-ABL and mutant JAK2 proteins15. Thus, we speculate that there is a specific regulation mechanism for accelerating the asparagine deamidation of p53 in the intracellular environment, even though asparagine residues 29 and 30 of short-lived p53 are present in an unusual deamidation-susceptible sequence.
Our studies are the first to elucidate the function of PIMT in p53 regulation and to uncover p53 as a novel substrate of PIMT. These results provide a previously unrecognized link between the p53 pathway and carboxyl methylation, and show that PIMT is a key regulator of the p53 pathway. We anticipate that our results will improve the current understanding of how carboxyl methylation regulates cellular processes.
The DNA constructs were a generous gifts from Dr Danny Reinberg21 (pCDNA-HA-p53, pGEX-GST-p53, pGEX-GST-p53 (1–82), pGEX-GST (83–289), pGEX (290–393) and pET-His-p53) and Dr Ber Vogelstein38 (full-length human p21 promoter luciferase). The constructs for wild-type PIMT were generated using PCR and cloned into the backbone of pCMV (Clontech), pGEX (Clontech) and pET32 (Invitrogen). The mutant constructs for p53 and PIMT were generated using site-direct mutagenesis (p53 N7A, D21A, N29A, N30A, D41A, D42A, D48A, D49A, N29 30A, N29D, N30D, N29 30D, N29E, N30E, N29 30E, N29Q, N30Q and N29,30Q, as well as PIMT G88A). All of the constructs were confirmed via sequencing.
The anti-p53 clone DO-1 (Santa Cruz Biotechnology; SC-126, SC-126AC, SC-126HRP), anti-PIMT (SC-100977, SC-133894, 1:1,000 dilution), anti-PUMA (SC-28226, 1:250 dilution), anti-HDM2 (SC-965, SC-965HRP, SC-965AC, SC-812, 1:500 dilution), anti-Bax (SC-493, 1:1,000 dilution), anti-p21 (SC-756, 1:500 dilution), anti-tubulin (SC-32293, 1:2,000 dilution), anti-Flag (Santa Cruz Biotechnology, SC-807AC; Sigma, F-3165; Abcam, ab49763HRP) and anti-HA (SC-7392HRP, 1:4,000 dilution) antibodies were used in this study.
Generation of stable cell lines
The lentiviral shRNA set for PIMT (shRNA H3, 5′-GCGCTAGAACTTCTATTTGAT-3′; shRNA H2, 5′-CCAGGCGCTAATAGATCAGTT-3′; and shRNA H4, 5′-GATCACATTAAAGAGCTAGTA-3′) was purchased from Open Biosystems. The lentivirus was obtained from 293TF cells according to the manufacturer's protocol. The U2OS cells were seeded onto 100 mm plates and infected with lentivirus containing the shRNA for PIMT. Cells expressing PIMT shRNA were selected using puromycin (2 μg ml−1).
H1299 cells were plated at 1×105 cells per well in 12-well plates and transiently transfected using Lipofectamine 2000 (Invitrogen). The total amount of plasmid DNA added to each well was adjusted to 1 μg by adding the necessary amount of empty vector. After transfection, the luciferase activities of the cell lysates were measured according to the manufacturer's instructions (Promega). The relative luciferase activity was normalized to the protein content of the cell extract39.
Flow cytometry analysis
U2OS cells were transfected with PIMT siRNA or control siRNA. At 2 days after transfection, the U2OS cells were treated with adriamycin at the indicated dose, and one day after treatment, the apoptotic cells were determined using flow cytometry. The fluorescence-activated cell sorting (FACS) analysis was performed using a FACS Canto II machine (BD Biosciences). For each treatment, a minimum of 10,000 cells was analysed. The data analysis was conducted using the DB FACSDiva software. Raw data of FACS analysis are described in Supplementary Fig. S16.
Immunoblotting and immunoprecipitation
For immunoblotting, each sample was subjected to electrophoresis on 4–12% NuPAGE Bis–Tris gradient gels (Invitrogen), and the proteins were transferred to polyvinylidene difluoride membranes using semi-dry transfer (Bio-Rad). The membranes were incubated overnight with the indicated primary antibodies, followed by incubation for 1 h with the secondary antibody, which was conjugated to horseradish peroxidase (Abcam). The signals were detected using chemiluminescence reagents (Intron). For immunoprecipitation, the cells were harvested and lysed in IP lysis buffer (40 mM HEPES (pH 7.4), 120 mM NaCl, 1 mM EDTA, 50 mM NaF, 1.5 mM Na3VO4, 10 mM β-glycerophosphate, 0.30% CHAPSO and protease inhibitors)40. The lysates were centrifuged for 20 min at 10,000 g at 4 °C. The specific antibodies conjugated to agarose (for FLAG, HA and p53, purchased from Santa Cruz Biotechnology) were added to the supernatants for overnight incubation at 4 °C. Subsequently, the beads were pelleted for 1 min at 7,000 r.p.m. and washed two times with IP lysis buffer. The proteins were eluted in 2× Laemmli buffer (Bio-Rad) or 4× LDS sample buffer (Invitrogen) by boiling for 5 min. The immunoprecipitated proteins were subjected to immunoblotting using horseradish peroxidase-conjugated primary antibodies. Raw data of the important protein blot are described in Supplementary Fig. S16.
Escherichia coli BL21 harbouring pGEX-GST-p53, pGEX-GST-PIMT, pET-His-p53 or pET-His-PIMT was cultured overnight at 37 °C in the LB medium containing ampicillin. Approximately 1 ml of seed culture was inoculated into 100 ml LB and cultured at 37 °C. When the culture reached OD 600, isopropyl-b-D-thiogalactopyranoside was added to 0.2–1 mM and incubated at 30 °C for 4 h. The cell pellet was lysed using a sonicator fixed with a 2-mm probe for 3 min in lysis buffer (50 mM NaH2PO4 (pH 8.0), 300 mM NaCl, 1 mM dithiothreitol, 0.1 mM phenylmethyl sulphonyl fluoride and 10 μg ml−1 aprotinin) and centrifuged at 8,000 g for 20 min. A 50% Ni2+-NTA or glutathione S-transferase bead slurry was added to the supernatant and incubated at 4 °C for 1 h. The beads were washed three times with wash buffer. After centrifugation, the proteins were eluted with elution buffer for 30 min at 4 °C.
In vitro methylation assay
Purified p53 protein or p53 peptides were used for the in vitro methylation assays. Each protein was incubated in citrate-phosphate buffer (0.25 M citric acid, 0.5 M Na2HPO4, 0.02 M EDTA (pH 6.0), and 7.19 pM S-adenosyl-L-[methyl-3H]methionine (specific activity of 76.4 Ci mmol−1)) at 30 °C for 30 min. The reaction was terminated upon the addition of sample buffer and subjected to electrophoresis on 4–12% NuPAGE Bis–Tris gradient gels (Invitrogen) using MES running buffer. The gels were stained with Coomassie blue R-150 to visualize the protein bands and then subjected to fluorography for 72 h at −70 °C using sensitized AGFA 100 NIF film (Agfa) or analyzed using a liquid scintillation counter (GE Healthcare).
For the p53 protein identification, trypsin, chymotrypsin or endoproteinase Asp-N peptides were separated using a biocompatible Ultimate 3000 nano-LC system (Dionex) equipped with a PepMap100 C-18 trap column (300 μm i.d.×5-mm-long cartridge, from Dionex) and PepMap100 C-18 analytic column (75 μm i.d.×150-mm-long cartridge, from Dionex). The gradient consisted of (A) 0.1% formic acid in water and (B) 0.08% formic acid in ACN: 4–30% B from 0 to 105 min, 80% B from 105 to 110 min and 4% B from 110 to 125 min. The flow rate was 300 nl min−1 from 0 to 12 min, 75 nl min−1 from 12 to 105 min and 300 nl min−1 from 105 to 125 min. An HCT ultra-PTM discovery system (Bruker Daltonics) was used to record the peptide spectra over the mass range of m/z 350–1,500 and the MS/MS spectra using information-dependent data acquisition over the mass range of m/z 100–2,800. Repeatedly, the MS spectra were recorded, followed by four data-dependent collision-induced dissociation MS/MS spectra and four electron transfer dissociations. The MS/MS spectra were generated from the four highest intensity precursor ions using the following parameters: an absolute threshold limit of 30,000 and a 25% relative threshold. The voltage between the ion spray tip and spray shield was set to 1,550 V. The drying nitrogen gas was heated to 170 °C, and the flow rate was 10 l min−1. The collision energy was set automatically according to the mass and charge state of the peptides chosen for fragmentation. Two 3-charged peptides were chosen for the MS/MS experiments because of their good fragmentation characteristics. The MS/MS spectra were interpreted, and the peak lists were generated using DataAnalysis 4.0 (Bruker Daltonics), with the parameters set to an absolute threshold limit of 5,000 and a 0.1% relative threshold. The searches were performed using MASCOT v2.2 (Matrix Science) against the UniProtKB/Swiss-prot database (version 57.14) for protein identification. The following MASCOT searching parameters were set: enzyme selected as trypsin or Asp-N, with three maximum missing cleavage sites; species limited to human; a mass tolerance of 0.2 Da for peptide tolerance; 0.2 Da for MS/MS tolerance; ion score cutoffs lower than 20; fixed modification of carbamidomethyl (C) and variable modification of oxidation (M), deamidation (N, Q), methylation (D, E) and methyl+deamidation (N). The positive protein identifications were based on significant molecular weight search scores. After the protein identification, an error-tolerant search with set parameters was performed to detect unspecific cleavages, amino-acid substitutions and unassigned modifications41.
Quantitative real-time PCR
Total RNA was isolated using Easy-Blue (Intron). The reverse transcriptase PCR was performed using the Access RT–PCR system (Promega). The quantitative real-time PCR was performed using the KAPA™ SYBR FAST qPCR Kit (Kapabiosystems) and a CFX96™ or Chromo4™ real-time PCR detector (Bio-Rad). The relative mRNA levels were normalized to the values of GAPDH mRNA for each reaction. The primer sequences are listed in Supplementary Table S1.
Chromatin immunoprecipitation assay
The chromatin immunoprecipitation assay was performed according to the manufacturer's protocol (Upstate Biotechnology). A small portion of the crosslinked, sheared chromatin solution was saved as the input DNA, and the remainder was employed for the immunoprecipitation using a p53 antibody conjugated to agarose (Santa Cruz Biotechnology). The immunoprecipitated DNAs were purified by phenol–chloroform extraction and ethanol precipitation; the DNA was re-suspended in 20 μl TE buffer. The immunoprecipitated and input DNA were analyzed using quantitative real-time PCR.
Statistical significance was analyzed using the Student's t-test and expressed as a P-value.
How to cite this article: Lee, J.C. et al. Protein L-isoaspartyl methyltransferase regulates p53 activity. Nat. Comm. 3:927 doi: 10.1038/ncomms1933 (2012).
Clarke, S. Aging as war between chemical and biochemical processes: protein methylation and the recognition of age-damaged proteins for repair. Ageing Res. Rev. 2, 263–285 (2003).
Weintraub, S. J. & Deverman, B. E. Chronoregulation by asparagine deamidation. Sci. STKE 409, re7 (2007).
Reissner, K. J. & Aswad, D. W. Deamidation and isoaspartate formation in proteins: unwanted alterations or surreptitious signals? Cell. Mol. Life Sci. 60, 1281–1295 (2003).
Desrosiers, R. R. & Fanélus, I. Damaged proteins bearing L-isoaspartyl residues and aging: a dynamic equilibrium between generation of isomerized forms and repair by PIMT. Curr. Aging Sci. 1, 8–18 (2011).
Bidinosti, M. et al. Postnatal deamidation of 4E-BP2 in brain enhances its association with raptor and alters kinetics of excitatory synaptic transmission. Mol. Cell 37, 797–808 (2010).
Curnis, F. et al. Spontaneous formation of L-isoaspartate and gain of function in fibronectin. J. Biol. Chem. 281, 36466–36476 (2006).
Curnis, F. et al. Isoaspartate–glycine–arginine: a new tumor vasculature-targeting motif. Cancer Res. 68, 7073–7082 (2008).
Curnis, F. et al. Critical role of flanking residues in NGR-to-isoDGR transition and CD13/integrin receptor switching. J. Biol. Chem. 285, 9114–9123 (2010).
Corti, A. & Curnis, F. Isoaspartate-dependent molecular switches for integrin-ligand recognition. J. Cell Sci. 124, 515–522 (2011).
Chavous, D. A., Jackson, F. R. & O'Connor, C. M. Extension of the Drosophila lifespan by overexpression of a protein repair methyltransferase. Proc. Natl. Acad. Sci. USA 98, 14814–14818 (2001).
Khare, S., Linster, C. L. & Clarke, S. G. The interplay between protein L-isoaspartyl methyltransferase activity and insulin-like signaling to extend lifespan in Caenorhabditis elegans. PLoS One 6, e20850 (2011).
Deverman, B. E. et al. Bcl-xL deamidation is a critical switch in the regulation of the response to DNA damage. Cell 111, 51–62 (2002).
Zhao, R. et al. DNA damage-induced Bcl-xL deamidation is mediated by NHE-1 antiport regulated intracellular pH. PLoS Biol. 5, e1 (2007).
Zhao, R., Yang, F. T. & Alexander, D. R. An oncogenic tyrosine kinase inhibits DNA repair and DNA-damage-induced Bcl-xL deamidation in T cell transformation. Cancer Cell 5, 37–49 (2004).
Zhao, R. et al. Inhibition of the Bcl-xL deamidation pathway in myeloproliferative disorders. N. Engl. J. Med. 359, 2778–2789 (2008).
Cimmino, A. et al. Protein isoaspartate methyltransferase prevents apoptosis induced by oxidative stress in endothelial cells: role of Bcl-Xl deamidation and methylation. PLoS One 3, e3258 (2008).
Huebscher, K. J. et al. Protein isoaspartyl methyltransferase protects from Bax-induced apoptosis. Gene 240, 333–341 (1999).
Lee, S. H. & Cho, Y. D. Induction of apoptosis in leukemia U937 cells by 5′-deoxy-5′-methylthioadenosine, a potent inhibitor of protein carboxyl-methyltransferase. Exp. Cell Res. 240, 282–292 (1998).
Sambri, I. et al. The microRNA 15a/16-1 cluster down-regulates protein repair isoaspartyl methyltransferase in hepatoma cells: implications for apoptosis regulation. J. Biol. Chem. 286, 43690–43700 (2011).
Meek, D. W. & Anderson, C. W. Posttranslational modification of p53: cooperative integrators of function. Cold Spring Harb. Perspect. Biol. 1, a000950 (2009).
Chuikov, S. et al. Regulation of p53 activity through lysine methylation. Nature 432, 353–360 (2004).
Huang, J. et al. Repression of p53 activity by Smyd2-mediated methylation. Nature 444, 629–632 (2006).
Shi, X. et al. Modulation of p53 function by SET8-mediated methylation at lysine 382. Mol. Cell 27, 636–646 (2007).
Huang, J. et al. p53 is regulated by the lysine demethylase LSD1. Nature 449, 105–108 (2007).
Jansson, M. et al. Arginine methylation regulates the p53 response. Nat. Cell Biol. 10, 1431–1439 (2008).
Huang, J. et al. G9a and Glp methylate lysine 373 in the tumor suppressor p53. J. Biol. Chem. 285, 9636–9641 (2010).
Director's Challenge Consortium for the Molecular Classification of Lung Adenocarcinoma et al. Gene expression-based survival prediction in lung adenocarcinoma: a multi-site, blinded validation study. Nat. Med. 14, 822–827 (2008).
Miller, L. D. et al. An expression signature for p53 status in human breast cancer predicts mutation status, transcriptional effects, and patient survival. Proc. Natl. Acad. Sci. USA 102, 13550–13555 (2005).
Ivshina, A. V. et al. Genetic reclassification of histologic grade delineates new clinical subtypes of breast cancer. Cancer Res. 66, 10292–10301 (2006).
Ingrosso, D., Fowler, A. V., Bleibaum, J. & Clarke, S. Sequence of the D-aspartyl/L-isoaspartyl protein methyltransferase from human erythrocytes. Common sequence motifs for protein, DNA, RNA, and small molecule S-adenosylmethionine-dependent methyltransferases. J. Biol. Chem. 264, 20131–20139 (1989).
Kagan, R. M. & Clarke, S. Widespread occurrence of three sequence motifs in diverse S-adenosylmethionine-dependent methyltransferases suggests a common structure for these enzymes. Arch. Biochem. Biophys. 310, 417–427 (1994).
Corti, A. & Curnis, F. Isoaspartate-dependent molecular switches for integrin-ligand recognition. J. Cell. Sci. 124, 515–522 (2011).
Geiger, T. & Clarke, S. Deamidation, isomerization, and racemization at asparaginyl and aspartyl residues in peptides. Succinimide-linked reactions that contribute to protein degradation. J. Biol. Chem. 262, 785–794 (1987).
Ota, I. M. & Clarke, S. Enzymatic methylation of L-isoaspartyl residues derived from aspartyl residues in affinity-purified calmodulin. The role of conformational flexibility in spontaneous isoaspartyl formation. J. Biol. Chem. 264, 54–60 (1989).
Robinson, N. A. & Robinson, A. B. Deamidation of human proteins. Proc. Natl. Acad. Sci. USA 98, 12409–12413 (2001).
Robinson, N. E. Protein deamidation. Proc. Natl. Acad. Sci. USA 99, 5283–5288 (2002).
Robinson, N. E. & Robinson, A. B. Amide molecular clocks in drosophila proteins: potential regulators of aging and other processes. Mech. Ageing Dev. 125, 259–267 (2004).
el-Deiry, W. S. et al. WAF1, a potential mediator of p53 tumor suppression. Cell 75, 817–825 (1993).
Kim, Y. K. et al. Activation of NF-kappaB by HDAC inhibitor apicidin through Sp1-dependent de novo protein synthesis: its implication for resistance to apoptosis. Cell Death Differ. 13, 2033–2041 (2006).
Vander Haar, E. et al. Insulin signalling to mTOR mediated by the Akt/PKB substrate PRAS40. Nat. Cell Biol. 9, 316–323 (2007).
Kang, S. U., Heo, S. & Lubec, G. Mass spectrometric analysis of GABAA receptor subtypes and phosphorylations from mouse hippocampus. Proteomics 11, 2171–2181 (2011).
We thank K.Y. Chung, W.S. Choi, , Y.K. Kim, D.W. Seo, J.K. Kang, H.Y. Lee, G.U. Bea and J.S. Kang for comments; D. Reinberg, B. Vogelstein and H.D. Youn for constructs; E.K. Shin (Woojung BSC, inc.) for data analysis of Surface Plasmon Resonance; M.S. Kim and J Zhong (Laboratory of A. Pandey in Johns Hopkins school of Medicine) for further validation of mass spectrometric results during revising the manuscripts. This research was supported by Basic Science Research Program through the National Research Foundation of Korea(NRF) funded by the Ministry of Education, Science and Technology (2011-0028282, 2011-0028283, 2011-0028284), and by a grant from the National R&D Program for Cancer Control, Ministry of Health and Welfare, Republic of Korea (0720140).
The authors declare no competing financial interests.
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Lee, JC., Kang, SU., Jeon, Y. et al. Protein L-isoaspartyl methyltransferase regulates p53 activity. Nat Commun 3, 927 (2012). https://doi.org/10.1038/ncomms1933
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