Cell cycle G2/M arrest through an S phase-dependent mechanism by HIV-1 viral protein R
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Cell cycle G2 arrest induced by HIV-1 Vpr is thought to benefit viral proliferation by providing an optimized cellular environment for viral replication and by skipping host immune responses. Even though Vpr-induced G2 arrest has been studied extensively, how Vpr triggers G2 arrest remains elusive.
To examine this initiation event, we measured the Vpr effect over a single cell cycle. We found that even though Vpr stops the cell cycle at the G2/M phase, but the initiation event actually occurs in the S phase of the cell cycle. Specifically, Vpr triggers activation of Chk1 through Ser345 phosphorylation in an S phase-dependent manner. The S phase-dependent requirement of Chk1-Ser345 phosphorylation by Vpr was confirmed by siRNA gene silencing and site-directed mutagenesis. Moreover, downregulation of DNA replication licensing factors Cdt1 by siRNA significantly reduced Vpr-induced Chk1-Ser345 phosphorylation and G2 arrest. Even though hydroxyurea (HU) and ultraviolet light (UV) also induce Chk1-Ser345 phosphorylation in S phase under the same conditions, neither HU nor UV-treated cells were able to pass through S phase, whereas vpr-expressing cells completed S phase and stopped at the G2/M boundary. Furthermore, unlike HU/UV, Vpr promotes Chk1- and proteasome-mediated protein degradations of Cdc25B/C for G2 induction; in contrast, Vpr had little or no effect on Cdc25A protein degradation normally mediated by HU/UV.
These data suggest that Vpr induces cell cycle G2 arrest through a unique molecular mechanism that regulates host cell cycle regulation in an S-phase dependent fashion.
KeywordsCell Cycle Profile Double Thymidine Block Double Thymidine Cdc25A Protein Checkpoint Control Gene
Human immunodeficiency virus type 1 (HIV-1) viral protein R (Vpr) is a virion-associated accessory protein with an average length of 96 amino acids and a calculated molecular weight of 12.7 kDa . Increasing evidence suggests that Vpr plays an important role in the viral pathogenesis of HIV-1. For example, infections with Vpr-defective viruses in rhesus monkeys, chimpanzees or human subjects seem to correlate with low viral load and slow disease progression [2, 3, 4], and some of the vpr point mutants could revert back to the wild type phenotype in the viral genome, which further supports the importance of Vpr in viral survival [5, 6, 7].
Vpr displays several distinct activities in host cells. These include cytoplasm-nuclear shuttling [4, 8], induction of cell cycle G2 arrest , and cell killing . The cell cycle G2 arrest induced by Vpr is thought to suppress human immune function by preventing T-cell clone expansion  and to provide an optimized cellular environment for maximal levels of viral replication . Therefore, further understanding of Vpr-induced cell cycle G2 arrest could provide additional insights into the molecular actions of Vpr in augmenting viral replication and modulation of host immune response.
Progression of cell cycle from G2 phase to mitosis requires activation of the cyclin-dependent kinase 1 (Cdk1), which determines onset of mitosis in all eukaryotes [12, 13, 14]. Cdk1 is typically phosphorylated on Tyr15 by Wee1 kinase in late G2 [13, 15], and it is rapidly dephosphorylated at the same amino acid residue by the Cdc25 tyrosine phosphatases to trigger entry into mitosis . Thus it is the balance between the Wee1 kinase and Cdc25 phosphatases activities that determines cellular entry of mitosis. In human cells, there are three Cdc25 homologues, Cdc25A, Cdc25B and Cdc25C . Cdc25A plays general roles in regulating cell-cycle transition, especially in G1/S transition and the exit of mitosis . The activity of Cdc25A is tightly regulated at the protein level, being periodically synthesized and degraded via ubiquitin-mediated proteolysis . Cdc25A is rapidly degraded in response to DNA damage or stalled replication and is known to be a crucial substrate in the mitotic DNA checkpoint response [20, 21]. Ultraviolet light (UV) or hydroxyurea (HU) treatments are known to rapidly activate the ATR-Chk1 pathway, leading to phosphorylation of Cdc25A and triggering the signal for its degradation by proteasome leading to S-phase arrest . On the other hand, Cdc25B and Cdc25C have a more restricted role in promoting progression from G2 phase to mitosis . Despite the seemingly similarity in functions, however, Cdc25B and Cdc25C have distinct roles temporally in cell proliferation with Cdc25B activity peaking before Cdc25C [22, 23]. Cdc25B may acts as a 'starter phosphatase', promoting the initial activation Cdk1-cyclinB, which in turn initiates mitosis through the up-regulation of Cdc25C . Deletion of all Cdc25 genes is lethal. Depletion of any one of these two phosphatases will result in significant delay of mitotic entry; however, this will not lead to cell cycle G2 arrest due to the functional redundancy of the Cdc25 phosphatases [25, 26]. In response to DNA damage such as double strand DNA breaks (DSBs), Cdc25C is phosphorylated on Ser216 via a Chk1/Chk2-mediated pathway then is bound to 14-3-3, leading to the translocation of Cdc25C from the nucleus to the cytoplasm for final proteasome-mediated protein degradation, leading to cell cycle G2/M arrest [27, 28]. Previous studies demonstrated that Vpr induces cell cycle G2 arrest through the promotion of hyper-phosphorylation of Cdk1 [9, 29, 30], which is achieved through inhibition of the Cdc25 phosphatase [31, 32, 33, 34] and the activation of the Wee1 kinase [32, 33].
Eukaryotic cells have an elaborate network of checkpoints to monitor the successful completion of every cell cycle step and to respond to cellular abnormalities such as DNA damage and replication inhibition as they arise during cell proliferation. Among many of the checkpoint control regulations, ATR or ATM and Chk1 or Chk2 are essential kinases of cell cycle checkpoint controls [35, 36]. For example, treatment of cells with UV or HU causes single strand break (SSB) or disruption of DNA replication respectively, which triggers DNA replication checkpoint through activation of the sensor kinase ATR. Activated ATR in turn results in the specific phosphorylation and activation of the effector kinase Chk1 at the Ser345 residue leading to the S-phase arrest. Similarly, when severe DNA damage such as DSBs is induced by ionizing radiation (IR), DSB signals mostly activate the sensor kinase ATM, which in turn activates the effector Chk2 kinase leading to cell cycle G2 arrest [31, 37, 38, 39]. However, both Chk1 and Chk2 can phosphorylate three Cdc25 homologues to induce cell cycle S or G2 arrest under different circumstances [40, 41].
Given that the DNA damage checkpoint and Vpr both induce G2 arrest through inhibitory phosphorylation of Cdk1, Vpr might induce G2 arrest through the DNA damage checkpoint pathway. Indeed, Tachiwana et al. showed Vpr induces DNA DSBs, which supports the idea that Vpr induces G2 arrest through DNA damage checkpoint . However, a different report showed that Vpr does not induce DNA DSBs . Moreover, the ATR kinase instead of the ATM kinase was found to play a major role in Vpr-induced G2 arrest through the phosphorylation and activation of Chk1 [44, 45]. These studies suggested that Vpr-induced G2 arrest may in fact resemble more the activation of DNA replication checkpoint than the DNA damage checkpoint control. Further studies have shown numerous similarities between the ATR pathway activated by Vpr and that by HU/UV. These similarities include the requirement for Rad17 and Hus1, the induction of phosphorylation on Chk1 and the formation of nuclear foci by RPA, 53BP1, BRCA1 and γH2AX [43, 44, 45]. However, these conclusions remain controversial based on the fact that expression of vpr does not change the radiosensitivity of the checkpoint defective mutants  and/or increase gene mutation frequency , which argues against the possibility that Vpr actually causes DNA damage for G2 induction. Furthermore, activation of DNA replication checkpoint generally leads to S phase arrest, but not G2 arrest. In another study, by using siRNA, a special isoform of PP2A was shown to play an essential role in the G2 arrest induced by Vpr in human cells. Unlike UV/HU-induced Chk1-Ser345 phosphorylation, the phosphorylation of Chk1-Ser345 induced by Vpr required the existence of this PP2A, but was independent of γH2AX activation . This finding suggests that Vpr-induced G2 arrest may be different to a certain extent from the DNA damage and replication checkpoint controls.
Even though Vpr-induced cell cycle G2 arrest has been extensively studied, what triggers the cell cycle G2 arrest by Vpr is at present unknown. One of the technical difficulties to examine this molecular event is that most of the early studies on Vpr-induced G2 arrest measured the Vpr effect 48-72 hours after the introduction of Vpr into asynchronized cell populations. To facilitate this study, measurement of the initiating event(s) for Vpr-induced G2 arrest would benefit from a system that uses synchronized cells and minimizes the time between initiation of Vpr expression and the measurement of the G2 arrest. For this reason, we have adapted an approach that allows us to monitor the cellular signaling for Vpr-induced G2 arrest within a single cell cycle. By using this single cell cycle assay, we have now uncovered that the G2-initiating signal(s) induced by Vpr is actually generated in the S phase of the cell cycle through induction of Chk1-Ser345 phosphorylation. To the best of our knowledge, the Vpr effect described here is unique and may represent a novel viral action for modulating host cell cycle regulation.
Vpr-induced Chk1 Activation Occurs in the S Phase of the Cell Cycle
Since previous studies showed that the Chk1-S345 phosphorylation is required for Vpr-induced G2 arrest [44, 48], potential Chk1-S345 phosphorylation was measured as a marker for Vpr-induced G2 arrest by Western blot analysis. Consistent with the idea that Chk1 activation, as indicated by Chk1-Ser345 phosphorylation, triggers G2 induction [44, 48], the Chk1-Ser345 phosphorylation appeared as early as 5 hours (in S-phase) after Adv-Vpr transduction (Figure 1A-b, second row). In contrast, no Chk1-Ser345 phosphorylation was observed in the Adv transduction control. To further verify this finding and test whether the activation of Chk1 induced by Vpr indeed starts in S phase, HeLa cells were synchronized in the M phase (Figure 1B) by treatment with 100 ng/mL of Nocodazole . Cell cycle profiles and Chk1-Ser345 phosphorylation were then detected. If Vpr-induced Chk1 activation is S-phase independent, Chk1-Ser345 phosphorylation would be observed within 5 hours after viral transduction regardless of the cell cycle stages. In contrast, if Vpr-induced Chk1 activation is S-phase dependent, Chk1-Ser345 phosphorylation would not be observed until the transduced cells have entered the next S phase. As shown in Figure 1B-b, first row, no Chk1-Ser345 phosphorylation was detected until 11 hours after Adv-Vpr viral transduction when cells entered the S phase, which precedes the G2 arrest. Consistently, no G2 cell accumulation was observed prior to Chk1-Ser345 phosphorylation. However, after the cells passed through the S phase at 15 hours, the cells stopped at the next G2 phase at 20 hours, whereas the Adv-transduced control cells continued into the G1 phase (Figure 1B-a). Together, these data suggest that Vpr triggers the activation of Chk1, as shown by Chk1-Ser345 phosphorylation, in the S-phase of the cell cycle.
Chk1-Ser345 Phosphorylation Is Exclusively Required for Vpr-induced G2 Arrest
Chk1-Ser345 Is Activated by HU, UV and Vpr with Different Cell Cycle Outcomes
HU/UV Promotes Proteasome-mediated Protein Degradation of Cdc25A
To ascertain the observed differences in the Cdc25A protein levels are indeed due to Chk1 activation, Chk1 was depleted by specific siRNA against Chk1, or by control siRNA. As shown in Figure 4C, depletion of Chk1 completely abolished HU-mediated Cdc25A degradation (Figure 4C, lanes 4 vs.3). In contrast, depletion of Chk1 had no obvious effect on Cdc25A protein level in vpr-expressing cells (Figure 4C, lanes 2 vs. 1). Note that the Cdc25A protein bands migrated a little faster in Chk1-depleted cells than that in control cells (Figure 4C, lanes 2 vs. 1; lanes 4 vs. 3). This difference in protein size could potentially be due to the lack of Cdc25A phosphorylation by Chk1 as previously described [20, 21]. Together, these data suggest that, in contrast to Vpr, HU/UV promotes protein degradation of Cdc25A through Chk1.
Vpr Promotes Proteasome-mediated Protein Degradations of Cdc25C and Cdc25B
There were also overall small but appreciable decreases of Cdc25B in vpr-expressing cells at all three time points as soon as cells were released from the DT block (Figure 5A-a, first row, lanes 8-10 vs. lane 1). This was in contrast to the normal and HU-treated cellular profile of Cdc25B, where a small increase of Cdc25B was seen instead (Figure 5A-a, first row, lanes 8-10 vs. lanes 2-4); while HU-treated cells remained constant (lanes 5-7). Like Cdc25C, the treatment of vpr-expressing cells with MG132 restored normal level of Cdc25B, suggesting that the observed reduction of Cdc25B was indeed due to degradation by the proteasome (Figure 5C, lanes 4-6). Moreover, Vpr-induced reduction of Cdc25B is likely mediated through Chk1 since the depletion of Chk1 by siRNA also restored the protein level back to the normal level (Figure 5C, lanes 7-9). Altogether, these results support the idea that Vpr promotes proteasome-mediated protein degradation of Cdc25C and possibly Cdc25B through Chk1.
Vpr Promotes Chk1-Ser345 Phosphorylation and G2 Arrest Possibly through Signaling of DNA Re-replication via Cdt1
To further examine whether we could actually observe the accumulation of DNA polyploidy over time, DNA content in the Adv-control and Adv-Vpr transduced cells was measured by flow cytometric analysis over a period of 55 hours. As we have shown in Figure 3B, most of the synchronized HeLa cells returned back to G1 stage (2N) by 11 hours after the DT release, with a minor amount of cells being in G2/M (4N) (Figure 6A-b). The % of G2 cells gradually increased over time from 33 to 55 hours. In contrast, nearly 100% of the vpr-expressing cells were arrested in the G2 phase by 11 hours after the DT release with no visible G1 cells (Figure 6A-b). A small hump of 8N cells was seen at 11 hours. This 8N population appeared to increase over time as the 4N cell population decreased (Figure 6A-b). All together, these findings indicate that Vpr promotes DNA re-replication, but at a relatively low level.
To further test whether Vpr could potentially affect the Cdt1 or Cdc6 activity leading to Chk1-Ser345 phosphorylation, either one or both proteins were depleted using specific siRNA against Cdt1 and/or Cdc6. As shown in Figure 6B-a, untreated HeLa cells showed basal level phosphorylation of Chk1-Ser345. Consistently, cells transduced with Adv-Vpr showed strong phosphorylation of Chk1-Ser345 even with pretreatment of control siRNA (Figure 6B-a, lane 2). While depletion of Cdt1 or Cdc6 had no obvious effect on Chk1-Ser345 phosphorylation (Figure 6B-a, lanes 3 and 5), interestingly, the depletion of Cdt1 significantly reduced Chk1-Ser345 phosphorylation induced by Vpr (Figure 6B-a, lane 6). Reduced Chk1-Ser345 phosphorylation was also seen in the vpr-expressing and Cdc6-depleted cells, but the latter showed less reduction than that from Cdt1 depletion (Figure 6B-a, lane 4 vs. 6). Double depletion of Cdt1 and Cdc6 showed no additional reduction on the Vpr effect (data not shown). The successful depletion of Cdt1 or Cdc6 protein by siRNAs was confirmed by Western blotting with antibody against Cdt1 or Cdc6 (Figure 6B-b).
To evaluate whether the effect of Vpr on Cdt1 or Cdc6 contributes to Vpr-induced G2 arrest, we tested the same Cdt1 or Cdc6 depletion effect on Vpr-induced G2 arrest using the single cell cycle assay 11 hours after the DT release and Adv-Vpr transduction. Consistent with cell cycle profiles shown in Figure 1A, about 65% of the synchronized cells returned back to the G1 phase by 11 hours; in contrast, about 98% of Adv-Vpr transduced cells arrested at the G2/M phase (Figure 6C, top panel). Significantly, a strong reduction of G2 cells (from 98% to 41%) was observed in the Cdt1-depleted cells; a relative small reduction (from 98% to 72%) was also observed in the Cdc6-depleted cells. Noticeably, depletion of either Cdc6 or Cdt1 alone slightly increased the G2 cell populations. However, such a G2 increase would only underestimate the reduction of Vpr-induced G2 arrest in the Cdt1- or Cdc6-depleted cells. Together, these data suggest that Vpr promotes low level of DNA re-replication through Cdt1 and with a lesser extent through Cdc6, which triggers Chk1-Ser345 phosphorylation possibly leading to cell cycle G2 arrest.
In this report, by using a single cell cycle assay, we demonstrated that Vpr induces cell cycle G2 arrest through a rather unusual molecular mechanism. Vpr causes cell cycle G2/M arrest, but the triggering event occurs in the S phase of the cell cycle. Specifically we showed that the expression of HIV-1 vpr elicits activation of Chk1 through Ser345 phosphorylation, which coincides with the hyperphosphorylation of Cdk1-Tyr15, a hallmark of G2/M arrest. The S phase-specific activation of Chk1 by Vpr was verified by testing the Vpr effect in different phases of the cell cycle (Figure 1) and by siRNA-mediated depletion of Chk1 (Figure 2). The exclusive requirement of Chk1-Ser345 phosphorylation for Vpr-induced G2 arrest was further confirmed by site-directed mutagenesis (Figure 2). Subsequent mechanistic analysis revealed that Vpr-induced Chk1-Ser345 phosphorylation and G2 arrest are likely triggered during the onset of DNA replication, since the depletion of Cdt1 by specific siRNA significantly reduced Chk1-Ser345 phosphorylation and G2 arrest induced by Vpr (Figures 6 and 7). To the best of our knowledge, the Vpr effect described here is unique in that it may represent a novel viral action for modulating host cell cycle regulation.
Even though Vpr-induced G2 arrest has been studied quite extensively (for reviews, see [65, 66, 67, 68]), how the expression of vpr triggers cell cycle G2 arrest is not fully understood. Early reports suggested that Vpr triggers the activation of the cellular DNA damage or replication checkpoint controls for the G2 induction, because some of the classic checkpoint control genes such as ATR, Chk1, Hus1, Rad17 and γH2AX-Ser139 phosphorylation are elevated upon Vpr production [44, 45]. Indeed, one of the key resemblances of the Vpr effect to the HU/UV effect is the ATR-mediated Chk1 activation through Chk1-Ser345 phosphorylation. Careful examination of this effect among these inducing agents revealed, however, some subtle differences. For instance, a specific isoform of PP2A is required for Vpr-induced Chk1-Ser345 phosphorylation and G2 arrest, whereas the same PP2A is not needed for HU/UV-mediated Chk1-Ser345 phosphorylation . Moreover, under the same experimental conditions, neither HU nor UV-treated cells were able to pass through S phase in contrast to Vpr-expressing cells (Figure 3B). Consequently, HU/UV-treated cells stopped at the G1/S boundary while vpr-expressing cells went through S phase and arrested at the G2/M boundary. Thus even though Vpr and HU/UV all induce Chk1-Ser345 phosphorylation, the cell cycle outcomes are quite different. These observations are strengthened by the additional findings that Vpr preferentially targets Cdc25C and possibly Cdc25B for Chk1-mediated inhibitory degradation by proteolysis (Figure 5). In contrast, HU/UV primarily promotes proteasome-mediated degradation of Cdc25A, instead of Cdc25C/B (Figure 4). Thus although Vpr and HU/UV all cause Chk1-Ser345 phosphorylation, Vpr-induced Chk1-Ser345 phosphorylation might be unique in that it is mediated through a PP2A-dependent process , which could further lead cells into the G2 phase of the cell cycle where Cdc25B and Cdc25C are primarily active and thereby being more affected relative to Cdc25A.
Unlike what we described here, prior studies including ours have shown that both UV and Vpr induce γH2AX-Ser139 phosphorylation, a classic sign of DNA damage and the activation of DNA damage checkpoints [45, 48]. γH2AX-Ser139 phosphorylation was typically observed 48 hours after vpr gene expression. These observations suggest that the observed γH2AX-Ser139 phosphorylation is more likely a late event induced by the vpr gene expression rather than the cause of Vpr-induced G2 arrest. This notion is supported by our new observation showing that no γH2AX-Ser139 phosphorylation was found beyond the background level in cells transduced by Adv-Vpr in the first round of cell cycle; whereas low dose UV induces strong γH2AX-Ser139 phosphorylation during the same time period (Figure 3A, row 2). Even though this observation does not exclude the possibility that Vpr may still induce a low level of DNA damage leading to G2 arrest, it nevertheless supports one of our earlier studies showing that a special isoform of PP2A, which is required for Chk1-S345 phosphorylation and Vpr-induced G2 arrest, is not required for γH2AX-Ser139 phosphorylation. Furthermore, depletion of γH2AX has no effect on Vpr-induced Chk1-S345 phosphorylation and Vpr-induced G2 arrest .
The potential differences between the Vpr effect and activation of DNA checkpoint controls were also implicated by early studies from the fission yeast model showing that Vpr is still able to induce G2 arrest when those checkpoint control genes such as Rad3 (ATR/ATM) or Chk1 were depleted [46, 69, 70]. Since DNA checkpoint control genes are highly conserved among eukaryotes, those observations in fission yeast reinforce the idea that Vpr may induce G2 arrest through a molecular mechanism that is somehow different from activation of the classic checkpoint controls (for reviews, see [68, 71]). Therefore, combining some of the early observations with the new findings described here, we conclude that Vpr induces cell cycle G2 arrest through a unique mechanism that is most likely different from the activation of DNA damage or replication checkpoint controls.
One of the most unique findings described here for Vpr-induced G2 arrest is that although Vpr arrests cells in G2 phase of the cell cycle, but the initiation event actually occurs in the S phase of the cell cycle. Mechanistically, we now show that this S phase-dependent initiation of cell cycle G2 arrest is likely triggered by cellular signaling of DNA re-replication through the DNA licensing factor Cdt1 and possibly Cdc6 (Figures 6 and 7). The replication licensing factors Cdt1 and Cdc6 are essential cellular proteins for ensuring DNA replicates only once per cell cycle in all eukaryotes [56, 57]. In particular, Cdc6 functions in conjunction with Cdt1 to promote the loading of minichromosome maintenance (MCM) complex for initiation of DNA replication . In fact, Cdt1 and Cdc6 are mutually dependent upon each other for MCM loading and initiation of DNA replication through direct protein-protein interaction . No DNA replication licensing will be initiated if Cdc6 failed to bind Cdt1 . Conversely, abnormal elevation of Cdt1 and Cdc6 will lead to DNA re-replication [57, 63], which causes Chk1-Ser345 phosphorylation . Interestingly, however, overexpression of either Cdt1 or Cdc6 alone does not induce detectable re-replication , further confirming the synergistic relationship between these two proteins. Thus, Cdt1 and Cdc6 are normally tightly regulated during the cell cycle and are rapidly inhibited or degraded upon onset of DNA replication by various mechanisms to prevent re-replication (for a recent review, see ).
Our data described here suggest that Cdt1 might be one of the primary contributing factors with the possible contribution of Cdc6 to Vpr-induced Chk1-Ser345 phosphorylation and G2 arrest. This notion is certainly supported by our observations that depletion of Cdt1 and/or Cdc6 by siRNA significantly reduced Vpr-induced Chk1-Ser345 phosphorylation (Figure 6B, Figure 7B) and cell cycle G2 arrest (Figure 6C, Figure 7C). Moreover, depletion of both Cdt1 and Cdc6 at the same time showed no additional reduction of Chk1-Ser345 phosphorylation (data not shown) indicating that Cdt1 and Cdc6 are indeed working in the same pathway for the Chk1 activation. It is unclear for the moment why depletion of Cdc6 gave rise to less reduction of Vpr-induced Chk1-Ser345 phosphorylation (Figure 6B-a, lane 4 vs. 6; Figure 7B) and G2 arrest (Figure 6C, Figure 7C). One possibility is that the Cdt1 activity is regulated, besides Cdc6, by additional mechanisms including the inhibitory binding of geminin and Cul4-DDB1-Cdt2-mediated protein degradation (for a review, see ). It is thus likely that Cdc6 participates only partially in regulating Cdt1 for Vpr-induced DNA re-replication. Consistent with the involvement of Cdt1 and Cdc6 in the Vpr effect, Vpr induces the accumulation of increasing DNA ploidy over time [[54, 55]; (Figure 6A-b, Figure 7A)] implicating DNA re-replication. Noticeably, however, only a relatively low level of 8N DNA accumulation was observed. Since a small increase of Cdt1 activity could induce DNA re-replication [57, 63] leading to Chk1-Ser345 phosphorylation , and since the depletion of Cdt1 diminishes Vpr-induced Chk1-Ser345 phosphorylation (Figure 6B, Figure 7B), it is conceivable that the low level of DNA re-replication triggered by Vpr is probably sufficient to induce Chk1-Ser345 phosphorylation and cell cycle G2 arrest. Verification of this possibility is certainly warranted in future studies. It should be mentioned that the effects of Vpr on Chk1-Ser345 phosphorylation and Cdt1 or Cdc6 were shown here in two different cell types (HeLa and CEM-SS), which suggest a general effect of Vpr on these cells. Noticeably, however, a much reduced impact of Vpr was seen in the CEM-SS cells than in HeLa cells. This discrepancy is probably due to the fact that Cdt1 or Cdc6 was only partially reduced in CEM-SS cells; whereas nearly complete depletion of these two proteins was obtained in HeLa cells. In addition, these effects were tested in synchronized HeLa cells, which could show cell cycle-specific effect; while when asynchronized CEM-SS cells were used Vpr may have little or no effect in other cell cycle phases except the S-G2 phases. Our future investigation will attempt to resolve these differences. Intriguingly, a recent paper  reported that a HBV viral protein X (pX) also induces partial polyploidy and DNA re-replication; but it promotes Cdt1 activity through increase the Cdt1-to-germini ratio. Even though HBV pX and HIV Vpr do not otherwise share the same molecular mechanism of actions, the fact that two distinct viral proteins are both affecting the same cellular target as Cdt1 may imply some potential underlying similarities between these two viruses during host-pathogen interactions.
In summary, we have shown in this study that Vpr interferes with host cell cycle regulation through a very distinctive molecular mechanism that could be characteristically different from the cell cycle DNA checkpoint controls. Even though the biologic and virologic significance of this unique viral action in HIV-1 infected cells is not fully understood, in-depth study of the molecular mechanism underlying Cdt1/Cdc6-mediated induction of cell cycle G2 arrest by Vpr through an S-mediated cellular event(s) could have broad impact toward our understanding of the basic host cell cycle regulation and HIV biology.
Cell Line, Cell Cycle Synchronization and Adenoviral Transduction
HeLa cells were grown in Dulbecco's modified Eagle's medium (DMEM) (Cellgro) and CEM-SS cells were grown in RPMI 1640 medium supplemented with 10% heat-inactivated fetal calf serum (FCS, Invitrogen) and 100 unit/ml of penicillin/streptomycin. HeLa cells were synchronized to the G1/S boundary of the cell cycle using a previously described double thymidine (DT) block method . Synchronized mitotic cells were obtained following treatment with Nocodazole for 20 hrs (100ng/ml, Sigma) . To induce DNA checkpoints, cells were treated either with HU (10mM) or UV (10 sec at the dose rate of 3 J/m2) immediately after cell release from the DT block. Similarly, synchronized cells were also transduced immediately after release of the DT block with the adenoviral vector control (Adv) or with Vpr (Adv-Vpr) by using MOI of 1.0 as we described previously [74, 75]. The Adv and Adv-Vpr vectors were provided by Dr. Ling-Jun Zhao (St. Louis University, St. Louis, MO) and have been described previously [74, 75, 76]. Cells were harvested at the indicated time for further analysis.
Plasmids and Site-directed Mutagenesis
A mammalian expression plasmid pEGFP-Chk1 that expresses wild type (WT) Chk1  was used as a template to construct the siRNA-resistant WT Chk1 (siR-Chk1) and its mutant derivatives. Specifically, two rounds of PCR were used to construct the siR-Chk1, i.e., the modified Chk1 gene transcripts produce the same WT Chk1 proteins, but they cannot be depleted by the siRNA normally used to deplete endogenous Chk1 (Cat. No. 1024702, Qiagen). Briefly, the pEGFP-Chk1 WT was used as a template in the first round PCR with forward primers 5'-CAT GGT CCT GCT GGA GTT CGT G-3' (P1) and reverse primers 5'-CTT AAT ATT TTC GGG GCA ATC CAC TGC TCT TTT CAT ATC TAC AAT CTT CAC-3' (P2) to generate left side of the WT Chk1 sequence, and with forward primers 5'-GTG AAG ATT CTA CAT ATG AAA AGA GCA GTG GAT TGC CCC GAA AAT ATT AAG-3' (P3) and reverse primers 5'-ACT GCA GAA TTC GAA GCT TGA GCT CGA ACG GG-3' (P4) to generate the right side of the WT Chk1 sequence with 51 base pairs overlapping. After isolating each of the PCR products using agarose gel elution kit, the second round of PCR was conducted with each of first round PCR product and the P1 and P4 primers. The PCR product was isolated and digested with XhoI/EcoRI restriction enzymes. The digested products were then sub-cloned at the same restriction sites into the parental plasmid pEGFP-C1. Site-directed mutagenesis of the siRNA-resistant Chk1-S345 phosphorylation-site was carried out by the using same procedure as described above with specific nucleotide mutant built in the primers. In this case, the serine residue at position 345 was changed to alanine by using the siR-Chk1-carrying plasmid as template, which results in siRNA-resistant mutant Chk1-S345A (siR-Chk1-S345A). All mutant constructs were confirmed by nucleotide sequencing.
Cell Cycle Analysis
At the indicated time, cells were collected by trypsinization. Cells were then washed twice with 2 ml of 5 mM EDTA/PBS and centrifuged at 1,500 rpm. After resuspension in 1 ml 5 mM EDTA/PBS, cells were fixed with 2.5 ml of 95-100% cold ethanol and kept at 4°C overnight. After centrifugation, fixed cells were washed twice with 2 ml of 5 mM EDTA/PBS and centrifuged at 1,500 rpm. After resuspension in 0.5 ml PBS, cells were incubated with RNase A (50 μg/ml) at 37°C for 30 minutes and then at 0°C with addition of propidium iodine (PI, 10 μg/ml) for 1 hour. Cells were then filtered prior to analysis of DNA content by FACScan flow cytometry (Becton Dickinson). The cell cycle profiles were modeled by use of the ModFit software (Verity Software House, Inc.).
Specific siRNA duplex against endogenous Chk1 "Chk1 siRNA" (Cat. No. 1024720), the FlexiTube siRNA against Cdt1 (Cat. No. SI04159477 and SI04142250) and the control non-silencing siRNA (Cat. No. 1022083) were purchased from Qiagen (Valencia, CA). The siGenome Smartpool siRNA against Cdc6 (Cat. No. M-003233-02) was purchased from Dharmacon (Chicago, IL). The siRNA mixtures were transfected at a concentration of 10 nM into approximately 5 × 105 dividing HeLa or CEM-SS cells by using 8 μl of Lipofectamine RNAiMAX following manufacturer's instructions (Invitrogen). Measurement of transfection efficiency of siRNAs by using Rhodamine labeled siRNA indicated >90% transfection efficiency.
One of the technical challenges for Cdt1 depletion by siRNA is that we cannot test prolonged depletion effect of Cdt1 because it causes cell death [[78, 79]; our unpublished data]. However, an early study showed that depletion of Cdt1 after first few rounds of DNA replication does not affect cell viability and ongoing cell cycle profile . Thus Cdt1 or Cdc6 was depleted and tested in our experiments as follows. Briefly, HeLa cells were treated with 2 mM thymidine for 18 hrs (first thymidine block) then thymidine was removed by washing with PBS three times. Specific siRNA against Cdt1, Cdc6 or control siRNA was then added with fresh media for 8 hrs. The HeLa cells were further synchronized to G1/S boundary with the second thymidine block for 16 hours. The Cdt1 or Cdc6 depletion effect was measured at 5 or 11 hours after the DT release and transduction with Adv-Vpr. For CEM-SS cells, asynchronized CEM-SS cells were pretreated with Cdt1, Cdc6 or Ctr siRNA, and then were transduced with Adv or Adv-Vpr 24 hours after addition of siRNAs. Cells were then harvested 48 hours post-transduction for further analyses.
Rabbit monoclonal anti-phospho-Chk1-Ser345 (133D3) antibody was purchased from Cell Signaling Technology, Inc (Danvers, MA). Mouse monoclonal anti-Chk1 (G-4), mouse monoclonal anti-Cdc25A (F-6) and rabbit polyclonal anti-Cdt1 antibodies were purchased from Santa Cruz Biotechnology, Inc (Santa Cruz, CA). Mouse monoclonal anti-Cdc25B (DCS.162.2) antibody was from EMD Chemicals, Inc (Gibbstown, NJ). Mouse monoclonal anti-Cdc25C (TC-15) antibody and mouse monoclonal anti-phospho-Histone γ-H2AX (Ser139) were from Upstate, Inc (Lake Placid, NY). Mouse monoclonal anti- Cdc6 (DCS-180) and mouse monoclonal anti-β-actin (AC-15) antibodies were from Sigma-Aldrich, Inc. Goat anti-mouse IgG (H+L) HRP conjugate and goat anti-rabbit IgG (H+L) HRP conjugate secondary antibodies from BioRad, Laboratories (Hercules, CA), and rabbit polyclonal anti-Vpr serum was custom generated through the Proteintech Group, Inc (Chicago, IL).
Cells were lysed with lysis buffer (50 mM Tris, pH7.5, 150 mM NaCl, 2 mM EDTA, 1% Triton X-100) on ice for 30 minutes, and the debris was removed by centrifugation at 13,000 rpm for 1 minute. The protein concentrations of supernatants were measured by BCA protein assay kit (Pierce). After boiling, 50 μg of protein were loaded on Criterion Precast Gels (BioRad) for electrophoretic separation. Proteins were transferred to the Trans-blot® Nitrocellulose membranes and blocked with 5% skim milk in TBST buffer (10 mM Tris, pH 8.0, 150 mM NaCl, 0.1% Tween 20) for 1 hour at room temperature. Primary antibodies were then applied overnight at 4°C. After washing 3 times in TBST for 10 minutes each time, the membranes were incubated with secondary antibody for 1 hour at room temperature. Membranes were washed again, and proteins were detected with Supersignal® West Dura Chemiluminescent Substrate (Pierce, Rockford, IL).
To quantify the intensity of protein of interest, densitometry was used to quantify the protein band and compared to either the protein loading control such as β-actin or the same protein at the baseline.
We are grateful to Dr. Ling-Jun Zhao (St. Louis University, St. Louis, MO) for providing the Adv and Adv-Vpr vectors and Dr. Helen Piwnica-Worms (Washington University, St. Louis, MO) for the pEGFP-Chk1-WT plasmid. This study was support in part by National Institute of Health Grants AI40891 and GM63080 (to R.Y.Z).
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