|Home | About | Journals | Submit | Contact Us | Français|
We report here a novel role for Jun dimerization protein-2 (JDP2) as a regulator of the progression of normal cells through the cell cycle. To determine the role of JDP2 in vivo, we generated Jdp2-knockout (Jdp2KO) mice by targeting exon-1 to disrupt the site of initiation of transcription. The epidermal thickening of skin from the Jdp2KO mice after treatment with 12-O-tetradecanoylphorbol 13-acetate (TPA) proceeded more rapidly than that of control mice, and more proliferating cells were found at the epidermis. Fibroblasts derived from embryos of Jdp2KO mice proliferated faster and formed more colonies than fibroblasts from wild-type mice. JDP2 was recruited to the promoter of the gene for cyclin-A2 (ccna2) at the AP-1 site. Cells lacking Jdp2 had elevated levels of cyclin-A2 mRNA. Furthermore, reintroduction of JDP2 resulted in the repression of transcription of ccna2 and of cell-cycle progression. Thus, transcription of the gene for cyclin-A2 appears to be a direct target of JDP2 in the suppression of cell proliferation.
Progression of the cell cycle in mammalian cells is regulated by the interplay of protein kinase complexes, known as cyclin-dependent kinases (CDKs). CDKs are controlled by the levels of expression of their respective cyclin partners, which act as positive coactivators or as negative regulators in the case of the so-called CDK inhibitors (Grana and Reddy, 1995; Sherr and Roberts, 1999; Malumbres and Barbacid, 2009; Satyanarayana and Kaldis, 2009; Caldon and Musgrove, 2010). Although cyclin-D–cdk4/6 and cyclin-E–cdk2 control progression through the G1 phase and cyclin-B–cdc2 appears to be necessary for entry into mitosis (Furuno et al., 1999), cyclin-A is a rate-limiting component required for the initiation of DNA synthesis and entry into mitosis (Pagano et al., 1992; Chaudhry et al., 2004). There are two subtypes of cyclin-A: cyclin-A2, which is expressed almost ubiquitously, and cyclin-A1, the expression of which is restricted to the testis (Sweeney et al., 1996). In conditional cyclin-A-knockout mice, the functions of cyclin-A are essential for progression of hematopoietic cells and embryonic stem cells through the cell cycle; however, cyclin-A and cyclin-E have redundant roles in cell proliferation in fibroblasts (Kalaszczynska et al., 2009).
Jun dimerization protein-2 (JDP2), a member of the activation protein-1 (AP-1) family, forms homodimers, as well as heterodimers, with other members of the AP-1 family, such as c-Jun, JunB, JunD and ATF2, and with a member of the C/EBP family, C/EBPγ (Aronheim et al., 1997; Broder et al., 1998; Jin et al., 2001). Assays involving ectopic expression of JDP2 indicate that it can block transformation of NIH3T3 cells and of prostate cancer cell lines (Heinrich et al., 2004). JDP2 also induces the partial transformation of chick embryonic fibroblasts (Blazek et al., 2003) and functions as a cell-survival protein in several cell lines (Piu et al., 2001; Lerdrup et al., 2005). JDP2 inhibits the differentiation of embryonal carcinoma F9 cells (Jin et al., 2002) and adipocytes (Nakade et al., 2007), and even promotes the differentiation of osteoclasts (Kawaide et al., 2003), C2 myoblasts and rhabdomyosarcoma cells (Ostrovsky et al., 2002).
JDP2 most likely participates in the repression of transcription through multiple mechanisms, which include DNA-binding competition and inactivation of the formation of heterodimers with other members of the AP-1 family (Aronheim et al., 1997), recruitment of HDAC-3 (Jin et al., 2002), inhibition of histone acetylation and direct regulation of chromatin assembly (Jin et al., 2006). However, the details of the physiological role of JDP2 in cell fate remain unknown, and the mechanisms by which JDP2 acts as a regulator of the proliferation or transformation of cells are yet to be clarified. Recently, we generated Jdp2-deficient mice with a deletion in the promoter and non-coding exon-1 region of the Jdp2 locus (Jdp2KO mice) and reported that ‘knockout' of Jdp2 affects adipocyte differentiation (Nakade et al., 2007) and resistance to replicative senescence (Nakade et al., 2009).
Although our Jdp2KO mice did not show any apparent abnormalities under standard breeding conditions, we report here that loss of JDP2 results in accelerated cell cycling by mouse embryonic fibroblasts (MEFs) and enhances the expressions of cyclin-A2. Increased expression of cyclin-A2 occurred through loss of direct binding to the promoter of cyclin-A2 gene at the AP-1 site. We also observed accelerated cell growth, which resulted in epidermal thickening in adult Jdp2KO mice after treatment with 12-O-tetradecanoylphorbol 13-acetate (TPA). Our data indicate that the gene for cyclin-A2 is one of the targets of JDP2 in the repression of cell proliferation by JDP2.
To investigate the functional effect of loss of expression of the JDP2 gene in vivo, we used the epidermal thickness assay to compare the back skins from TPA-treated hairless skins of wild-type (WT) or Jdp2KO mice. Both WT and Jdp2KO mice have a thin back epidermis of only 2–3 cells thick (Figure 1). However, the epidermal thickness of the hairless skins from Jdp2KO mice increased by 1.4-fold compared with that of WT mice four days after treatment with TPA (Figures 1A and B). The expression of proliferation cell nuclear antigen (PCNA) in the epidermis from Jdp2KO mice was 1.3-fold higher than that in the epidermis of WT mice (Figures 1B and C). The results of wound-healing assay in vivo also indicated the higher healing potential in Jdp2KO mice (Supplementary Figure S1).
We prepared MEFs from Jdp2KO embryos on day 12.5 post coitus. Northern blotting and western blotting of embryos and MEFs from Jdp2KO mice failed to show any signals of JDP2 mRNA or protein (Figures 2a and b). We next examined the proliferation of MEFs using three different assays, namely, Trypan blue dye exclusion, Alamar Blue assay and colony formation. Jdp2KO MEFs proliferated more rapidly than WT MEFs when plated at 5 × 105 cells per 10-cm dish in Dulbecco's modified Eagle's medium (DMEM) plus 10% fetal calf serum (FCS) (Trypan blue dye exclusion; Figure 2c). The results of the cell growth assay with Alamar Blue dye and colony formation assay also supported this conclusion (Figures 2d and e). These results indicated that JDP2 has a crucial role in growth control in vitro and in vivo.
We found that UV-irradiated MEFs underwent apoptosis in a dose-dependent manner at doses of UVC from 20 to 60J/m2; however, we did not detect any obvious differences between WT and Jdp2KO MEFs in subsequent Trypan blue dye exclusion assays and assays of the activities of caspases 3 and 7 (Supplementary Figures S2A and B). When MEFs were exposed to UVC at 60 and 600J/m2, for 2 and 8h, the level of expression of JDP2 fell significantly (Supplementary Figure S2D). The size of the sub-G1 population of UV-irradiated MEFs from Jdp2KO mice was identical to that of MEFs from WT mice (Supplementary Figure S2C). All reagents of apoptosis inducers increased the activities of caspases 3 and 7 in a dose-dependent manner (data not shown); however, no significant differences in respective activities were found between WT and Jdp2KO MEFs (Supplementary Figure S3) except after application of cycloheximide. These data suggested that JDP2 has no significant effect on the apoptotic responses to UV and inducers of cell death in normal MEFs.
We next performed a cell-cycle re-entry assay, counting propidium iodide-stained MEFs by flow cytometry. A representative experiment after 18-h serum stimulation showed that 28% of Jdp2KO MEFs were in the S-phase, whereas only 20% of WT MEFs were in the S-phase (Figure 3a). The number of MEFs derived from Jdp2KO mice in the S-phase was considerably higher than that of WT MEFs (1.5-fold; Figure 3b). Proliferation of Jdp2KO MEFs was accelerated by the enhanced progression of cells from the G1- or the G0-phase to the S-phase, and not because of differential activity related to cell death.
We also examined the incorporation of bromodeoxyuridine (BrdU) into MEFs. The percentages of BrdU-positive cells in the six chambers showed that Jdp2KO MEFs moved more frequently from a quiescent state to a proliferative state than did WT MEFs (3.5-fold; Figures 3c and d).
To examine the role of JDP2 in the cell cycle, we analyzed the expression of individual cell-cycle-related genes. MEFs were arrested at the G0/G1-phase by deprivation of serum for 48h and then re-entry into the cell cycle was triggered by re-plating in DMEM plus 15% FCS. No notable differences in protein levels, such as cyclin D1, cyclin D3, cyclin-dependent kinase-4 (cdk4), cdk6 and Rb were detected between WT and Jdp2KO MEFs (Figure 4a). However, p53 and p21 levels in Jdp2KO MEFs were lower than those in WT MEFs after induction by serum, suggesting JDP2 might affect the p53-p21 cascade, which is further discussed in the section Discussion (Vousden and Prives, 2009).
We next examined global gene expression in Jdp2KO MEFs using an oligo DNA microarray known as ‘Mouse' (Agilent Technologies Inc., Santa Clara, CA, USA) (Supplementary Table 1; the entire data set from the microarray analysis is available at the Center for Information Biology Gene Expression Database (CIBEX; DDBJ, Mishima, Japan; CIBEX accession, CBX101)). Higher levels of expression of genes for cyclin-A2 and cyclin-E2 were detected in Jdp2KO MEFs as compared with WT MEFs. Conversely, genes for the CDK inhibitors p21, p16 and p15, but not p27, were expressed at lower levels in Jdp2KO MEFs than in WT MEFs. However, the mRNA levels of p53, p107 and RB were not altered. The expression of genes from families of apoptosis-related genes and genes for other AP-1 and C/EBPs did not show any remarkable differences between Jdp2KO and WT MEFs, except for JDP2 and C/EBPδ. The expression of 21 known genes, including the Wnt/transforming growth factor-β (TGFβ) regulators Wisp2, Sfrp2 and Ltbp1, was enhanced in Jdp2KO MEFs as compared with WT MEFs, and the expression of another 20 known genes, including the Wnt target gene Lef1 and cAMP/Ca2+ regulators Cap-1 and Penk-1, was depressed in Jdp2KO MEFs as compared with WT MEFs (Supplementary Table 1).
As shown in Figure 4b, the correlation coefficient with respect to the relative change in levels of mRNAs between the two assays was higher than 0.8, indicating that the data from the microarrays were valid. We examined the levels of the transcripts of representative genes by real-time PCR and found that the results were consistent with those in the microarray assay (Figures 4c and d).
We examined the levels of cyclin-A2 mRNA by real-time PCR after re-stimulation of MEF by serum. The expression of cyclin-A2 was enhanced by the addition of FCS in both WT and Jdp2KO MEF lines (Figure 5a). However, a more significant increase in the expression of cyclin-A2 was noted in Jdp2KO MEFs than in WT MEFs after stimulation (>1.8-fold; 12h after serum re-stimulation). In parallel, we also measured the kinetics of changes in the levels of mRNA for JDP2 and c-fos. The expression of JDP2 mRNA decreased slightly after serum stimulation in WT MEFs. By contrast, expression of c-fos mRNA rose rapidly but transiently within 4h after the start of stimulation, without any significant difference between the two lines of MEFs. As shown in Figure 5b, expression of mRNAs for cyclin-A2 and cyclin-E2 started earlier and were significantly higher and expressions of both genes started earlier in Jdp2KO MEFs than in WT MEFs after re-addition of serum. By contrast, expression of p16Ink4a decreased significantly for the first 6h after the start of stimulation with serum in Jdp2KO MEFs.
Chromatin immunoprecipitation (ChIP) assay showed that PCR product that corresponded to the promoter regions of the genes for cyclin-A2 and p16Ink4a were detected in sonicated chromatin derived from WT MEFs but not in that from Jdp2KO MEFs (Figure 5c). In the case of cyclin-E2, no specific band was detected. Our data indicate that the genes for cyclin-A2 and p16Ink4a are the most likely targets of JDP2 in the progression of the cell cycle, even though they showed opposite responses upon serum stimulation of serum-starved cells.
We cloned an 1101-bp fragment of DNA from the promoter region of the mouse gene for cyclin-A2 and constructed a series of promoter deletion-luciferase genes (Figure 6a). We detected 2.5–4.5-fold higher luciferase activity in Jdp2KO MEFs than in WT MEFs when we tested this series of deletion constructs (Figures 6b and d). A point mutation at the AP-1 site of this SacI–XhoI region enhanced luciferase activity in WT MEFs but not in Jdp2KO MEFs (Figure 6c).
To determine whether JDP2 represses the expression of the gene for cyclin-A by exploiting its histone modification activity, as described previously (Jin et al., 2006), we performed ChIP assays and found that the level of acetylation of histone-H4 in Jdp2KO MEFs was clearly higher than that in WT MEFs (Supplementary Figure S4).
We performed electrophoretic mobility-shift assays to verify the DNA-binding activity of JDP2 using DNA probes that corresponded to the AP-1, the CRE and the AP-1-like sites (lanes 2–5 in Figure 7). The AP-1 and CRE probes but not the AP-1-like probe generated DNA–protein complexes with nuclear extracts (NEs) from either WT MEFs or Jdp2KO MEFs. The corresponding competitor AP-1 released [32P]-AP-1 oligodeoxynucleotide from the DNA–protein complexes but the mutant competitor mAP-1 did not (lanes 9, 10, 11, 14, 15 versus lanes 12, 13, 16 in Figure 7a). When we added an antibody specific for JDP2 to the reaction mixture with the AP-1 probe, we detected super-shifted bands in the case of NEs from WT MEFs but not from Jdp2KO MEFs (lanes 2 and 6 versus lanes 4 and 8 in Figure 7b). Furthermore, the band in serum-stimulated WT MEFs was less intense than that from serum-starved WT MEFs, indicating that addition of serum suppressed the formation of a protein–DNA complex that included JDP2 under these conditions. In the case of the NEs from WT MEFs, the antibodies against JDP2 and JunD affected the migration and density of the protein–DNA complexes (lanes 5 and 9 in Figure 7c); however, antibodies against JunD and c-Jun shifted the DNA–protein complexes in the NEs from Jdp2KO MEFs (lanes 12 and 14 in Figure 7c). By contrast, the CRE probe–protein complex was shifted by the addition of antibodies specific for JunD but not by antibodies specific for JDP2 (lane 9 in Figure 7d), indicating that the CRE site ‘preferred' members of the AP-1 family other than JDP2. These data strongly suggest that JDP2 binds to the AP-1 site of the cyclin-A2 gene promoter.
The level of cyclin-A2 was fourfold higher in Jdp2KO MEFs than in WT MEFs at 8h after stimulation with serum (Figure 8a). We also found that no significant increases of cyclin-E2, cdk1 and cyclin-B1 proteins (Figure 8a, data not shown). We immunoprecipitated cdk2 from equal amounts of cell lysates prepared from WT and Jdp2KO MEFs 0, 8, 16 and 20h after re-addition of FCS (Figure 8b). Immunoblotting of the immuprecipitates and/or cell lysates with antibodies specific for cyclin-A2, cyclin-E2, cdk2 and β-actin as a loading control showed that the amounts of cdk2-associated cyclin-A and of cdk2-associated cyclin-E2 were increased by serum stimulation (two- and fivefold, and six- and twofold, at 16 and 20h, respectively), even though the level of cdk2 was almost constant.
In an attempt to measure the levels of cyclin-associated kinases, we prepared lysates from WT and Jdp2KO MEFs and subjected them to immunoprecipitation with antibodies against cyclin-A2 and cyclin-E2. We found that immunoprecipitates of cyclin-A2 and cyclin-E2 from Jdp2KO MEFs had 8- and 3-fold higher kinase activity, respectively, than those from WT MEFs (on the basis of radioactivity; Figure 8c). The increased kinase activity of cyclin-E2 was found 12 and 24h after serum stimulation, and that of cyclin-A2 was detected 24h after serum stimulation.
We examined the effects of JDP2 on the proliferation of MEFs by overexpressing JDP2 in WT MEFs and re-expressing JDP2 in Jdp2KO MEFs. First, we introduced a pJDP2 vector into WT and Jdp2KO MEFs (two- to threefold increase of JDP2 mRNA than that of WT MEFs). Introduction of pJDP2 suppressed cell growth in both lines of MEFs (Figure 9a). We used the cyclin-A2 promoter–reporter construct pA2M and its AP-1 mutant pA2mAP-1 to examine the effect of re-expression of JDP2 in Jdp2KO MEFs. Transfection with pJDP2 significantly reduced the reporter luciferase activity in pA2M, but not in the mutant reporter pA2mAP1 (Figure 9b). These data suggested, yet again, that JDP2 represses the activity of the cyclin-A2 promoter, in a manner dependent specifically on the AP-1 site.
The infection with adenovirus JDP2 (Ad-JDP2) significantly suppressed cell growth in both WT and Jdp2KO MEFs, acting in a dose-dependent manner, even at a multiplicity of infection of 1 (Ad-JDP2 increased the expression of JDP2 by 50–100-fold; Nakade et al., 2009). Infection with the JDP2-expressing virus almost halved the number of WT and Jdp2KO MEFs by day 5 (Figure 9c). However, expression of cyclin-A2 was depressed in Jdp2KO MEFs (Figure 9d). In WT MEFs, two different JDP2–siRNA constructs reduced the expression level of JDP2 by as much as 50% (Figure 9f). These small interfering RNAs (siRNAs) accelerated the proliferation of WT MEFs but not of Jdp2KO MEFs (Figure 9e). Furthermore, treatment of WT MEFs with JDP2–siRNA increased the level of cyclin-A2 mRNA but reduced the level of cyclin-A2 mRNA in Jdp2KO MEFs (Figure 9f). These data strongly suggest that JDP2 represses the progression of the cell cycle through expression of cyclin-A2, thereby inhibiting the proliferation of MEFs at least partially.
In this study, we show that loss of JDP2 accelerates cell-cycle progression with higher cyclin-associated cdk kinase activities in MEFs and cyclin-A2 is one of the molecular targets of JDP2. Thickening of epidermis after treatment with TPA showed the proliferation inhibition of JDP2 in mice skin derived from Jdp2KO and WT mice in vivo. Other assays in vitro, including population doubling, cell cycle and BrdU-incorporation, showed the elevated proliferative potential of Jdp2KO MEFs as compared with WT MEFs.
To identify the molecular targets of JDP2 on cell proliferation, we performed a microarray-quantitative PCR analysis and found genes encoding cyclin-A2, p16Ink4a and cyclin-E2 are the potential targets of JDP2. So far, only five JDP2 targets were identified, namely c-Jun, ATF-2, C/EBPδ, ATF3 and CHOP10 (Aronheim et al., 1997; Jin et al., 2001; Nakade et al., 2007; Cherasse et al., 2008; Weidenfeld-Baranboim et al., 2009). Here we found that JDP2 was recruited to the promoter of the gene for cyclin-A2 at the AP-1 site. A gel-shift assay and site-directed mutagenesis of the promoter also showed that the AP-1 site is crucial for JDP2-mediated repression of the cyclin-A2 promoter, suggesting that JDP2 is the major component in the regulation of the cyclin-A2 promoter. However, the endogenous partner with JDP2 to form heterodimer in vivo has not been identified yet.
A number of studies suggest that JDP2 has a dual role with pro- or anti-oncogenic properties in malignant transformation. JDP2 was found to inhibit cell-cycle progression (Ostrovsky et al., 2002), Ras-dependent cell transformation and tumor formation in xenografts (Heinrich et al., 2004). Conversely, overexpression of JDP2 in chicken embryo fibroblasts imparts a partial oncogenic phenotype (Blazek et al., 2003). Furthermore, viral integration sites were identified within the genome of JDP2 resulting in T-cell lymphoma (Hwang et al., 2002; Rasmussen et al., 2005, 2009; Stewart et al., 2007). Recent publication showed that JDP2 potentiates the chemical carcinogenesis of liver cancer (Bitton-Worms et al., 2010). JDP2 acts at the promotion stage in which full blown inflammation is evident. Furthermore, multiple members of the bZIP family are highly expressed at this stage, including CHOP10. Heterodimerization between CHOP10 with either ATF3 or overexpressed JDP2 transgene may result in the transcriptional activation (Weidenfeld-Baranboim et al., 2008) of otherwise suppressed JDP2 target genes involved in cell-cycle progression such as cyclin-A2, cyclin-E2 or p16Ink4a, which were identified in this report. These data indicate that JDP2 acts as a transcriptional activator or a repressor depending on the bZIP protein at each stage of cancer progression with which it is associated. However, the role of JDP2 in cancer progression mediated through regulation of cyclin-A2 transcription has not been determined yet; further investigations are necessary to clarify the JDP2 partner to regulate cell-cycle progression in response to various signals.
We show here that transcriptional regulation is the major mechanism of the JDP2-mediated expression of the cyclin-A2 promoter. Other possible regulations described below cannot be ruled out. First JDP2-mediated inhibitions of histone acetylation at H3 and H4 (Jin et al., 2006; Nakade et al., 2007) and histone methylation at H3K27 at p16Ink4a locus (Nakade et al., 2009) are possible. Second, the stability of cyclin-A2 might be controlled by JDP2 (Mateo et al., 2009; data not shown). In fact, we found that JDP2 colocalized with cyclin-A in the nucleus (Supplementary Figure S6).
In the case of cyclin-E2 the mRNA and protein levels after serum induction were not coincident each other and, however, the cdk2–cyclin-E2 complex showed slightly higher cyclin-associated cdk kinase activity in Jdp2KO MEFs as compared with that in WT MEFs. The specific recruitment of JDP2 to the promoter of cyclin-E2 was not detected and no AP-1/CRE elements were found in the promoter of the cyclin-E2 gene. Thus, regulation of cyclin-E2 by JDP2 might not be direct transcriptional regulation by JDP2. Another indirect regulation like JDP2-induced p16Ink4a-Rb-E2F regulation of cyclin-E2 gene might be possible (Nakade et al., 2009; Polager and Ginsberg, 2009).
The increase in the protein levels of p53 and p21 proteins was less significant in Jdp2KO MEFs after stimulation by serum as compared with that in WT MEFs. We generated p53-knockdown MEFs by using a short-hairpin RNA against p53 (shp53) and introduced lentivirus vector-encoded JDP2 (Supplementary Figure S5A). In MEFs in which p53 was downregulated completely, JDP2 still inhibited cell proliferation significantly (>P=0.0075; Supplementary Figures S5B and S5C). In addition, expression of p53 mRNA was increased by introducing JDP2 the level of which is comparable with the results in Figure 4a. These observations indicate that JDP2 may inhibit cell proliferation in p53-dependent and p53-independent manners, in the latter case, at least partially, by suppression of cyclin-A2 gene.
In summary, our data indicate that JDP2 has a crucial role in the suppression of cyclin-A2 expression, with subsequent inhibition of cyclin-associated cdk kinase activity, and in the suppression of cell proliferation. This hypothesis is also supported by overexpression of JDP2 encoded by a recombinant adenovirus and by gene suppression experiments with siRNA. The expression of cyclin-A2 is controlled at the transcription level by JDP2. It is clear that JDP2 interferes with progression of the cell cycle at least partially by downregulation of cyclin-A2 but not apoptosis. The control of cell cycle by JDP2 may then lead to the commitments of cell differentiation, cellular senescence or cell fate determination possibly through the signal cascades of RB-E2F or p53-p21 or Wnt/TGFβ as indicated by the results of microarray and qPCR.
MEFs were prepared from embryos at embryonic day 12.5 (E12.5) with a mixed genetic background of B6 and 129 as described previously (Nakade et al., 2007). For serum starvation experiments, MEFs were incubated in DMEM containing 0.1% FCS for 48h, at confluence; then they were re-plated in DMEM that contained 15% FCS.
The assay for epidermal thickening was measured as described previously with a slight modification (Nakamura et al., 1998). Briefly, the dorsal skin of each mouse (six pairs of WT and Jdp2KO) was shaved before treatment with TPA. TPA or acetone as solvent control was administered four times to each animal at an interval of 24h (8.1nmol in 100μl acetone; Sigma-Aldrich Co., St Louis, MO, USA). Mouse skin was obtained 1h after the fourth application of TPA or acetone. Tissues were frozen and sectioned at 5ìm thickness. The epidermal thickness of the skin was measured at 10 randomly selected sites using an Olympus microscope (Olympus, Tokyo, Japan). The vertical thickness of the epidermis was defined as the distance from the stratum basal to the stratum corneum. After incubation overnight at room temperature with or without mouse monoclonal antibody against PCNA (PC10; Abcom, Cambridge, MA, USA), slides were incubated with goat anti-mouse IgG 1h at room temperature. PCNA labeling index was calculated by immunoreactive nuclei per total nuclei in epidermis.
Cyclin-A2 promoter-reporter DNAs were transfected into WT and Jdp2KO MEFs with or without pcDNA3-JDP2 or pcDNA3 empty vector as 1μg of total DNA per well of a 24-well plate (5 × 104 cells/well) using 2μl of Lipofectamine-2000 reagent (Invitrogen, Paisley, UK). A series of JDP2 promoter-reporters were transfected as described elsewhere (Jin et al., 2002; Nakade et al., 2007).
We immunoprecipitated total cellular proteins with antibodies against cyclins as indicated and using protein-A- and protein-G-Sepharose beads. Beads with bound immune complexes were mixed with [32P]-ATP and histone H1 peptide substrate (cat. no. 14–155; Upstate Biotechnology Inc., Charlottesville, VA, USA) in a kinase assay buffer (50m HEPES (pH 7.0), 10m MgCl2, and 1m dithiothreitol) for 30min at 30°C. Reaction products were resolved by sodium dodecyl sulfate-PAGE (12% polyacrylamide) and phosphorylated histone H1 peptide was detected by autoradiography.
Results are expressed as the means±s.d. of the results for each set of replicates. Statistical comparison of single parameters between two groups was performed by paired Student's t-test. P-values less than 0.05 or 0.01 were considered significant.
Plasmid constructions, generation and characterization of JDP2-deficient mice, skin wound healing, cell cycle, isolation of RNA, microarrays and real-time quantitative reverse transcription–PCR, recombinant virus infection and siRNA transfection, cell proliferation and apoptosis, electrophoretic mobility-shift assays, immunoprecipitation-western blotting, ChIP assay and immunofluorescence are described in the Supplementary Information.
We thank S Itohara, C Jin, R Chiu, K Itakura, T Kondo, S Takahashi, P Kourilsky and G Gachelin for discussion, and L-H Lee, M Hirose and K Inabe for technical support. This work was supported by grants from the RIKEN Bioresource Project (to AY, YO and KKY), the Ministry of Education, Culture, Sports, Science and Technology of Japan (to KN, NY and KKY) and Kaohsiung Medical University, Taiwan (KMU-EM-99-3, to KKY, C-HL and ET).
The authors declare no conflict of interest.
Supplementary Information accompanies the paper on the Oncogene website (http://www.nature.com/onc)