Abstract
E2F transcription factors control the oscillating expression pattern of multiple target genes during the cell cycle. Activator E2Fs, E2F1–3, induce an upswing of E2F targets, which is essential for the G1‐to‐S phase transition, whereas atypical E2Fs, E2F7 and E2F8, mediate a downswing of the same targets during late S, G2, and M phases. Expression of atypical E2Fs is induced by E2F1–3, but it is unknown how atypical E2Fs are inactivated in a timely manner. Here, we demonstrate that E2F7 and E2F8 are substrates of the anaphase‐promoting complex/cyclosome (APC/C). Removal of CDH1, or mutating the CDH1‐interacting KEN boxes, stabilized E2F7/8 from anaphase onwards and during G1. Expressing KEN mutant E2F7 during G1 impairs S phase entry and eventually results in cell death. Furthermore, we show that E2F8, but not E2F7, interacts also with APC/CC dc20. Importantly, atypical E2Fs can activate APC/CC dh1 by repressing its inhibitors cyclin A, cyclin E, and Emi1. In conclusion, we discovered a feedback loop between atypical E2Fs and APC/CC dh1, which ensures balanced expression of cell cycle genes and normal cell cycle progression.
Keywords: anaphase‐promoting complex, CDH1, cell cycle, DNA replication, E2F
Subject Categories: Cell Cycle
Introduction
Eukaryotic cell division is tightly controlled by transcriptional and posttranslational regulation of genes that drive progression through the different phases of the cell cycle. The decision to enter S phase is of critical importance, because unscheduled entry leads to replication stress, which may result in mutations through errors during DNA synthesis, and eventually could lead to genetic instability and cancer 1, 2. The activity of E2F transcription factors plays a central role in the ability of cells to enter S phase. Vertebrate species have no less than eight different E2F family members (E2F1–8), three dimerization partners (DP1–3), and 3 pocket proteins (RB, P107, P130), whose interplay determines transcription of hundreds of target genes in mammalian cells.
Dissecting the specific and unique functions of the E2F family members in various cellular processes, including S phase entry, has proven a difficult task 3. For instance, E2Fs 1–3 switch from activators to repressors during differentiation of intestinal progenitor cells, depending on pocket protein binding 4. However, the actions of the atypical E2F family members, E2F7 and E2F8, seem almost exclusively repressive, as they lack transactivation domains and are not regulated by pocket proteins 5, 6, 7, 8. After the start of S phase, E2F7 represses many genes that drive the G1/S transition, via occupation of E2F motifs on proximal promoters 8. Based on their high extent of homology and redundant functions in vivo, E2F8 is expected to act in the same manner 9. In addition, E2F7/8 drive the switch from mitotic cell cycles to endocycles in placenta and liver, and can suppress apoptosis during embryonic development, demonstrating their central role in cell cycle regulation 9, 10, 11.
Expression of atypical E2Fs is comparatively high in tissues with high rates of cell division 5, 6. Thus, given that E2F7 and E2F8 are potent cell cycle regulators, their activities must be tightly controlled. During late G1, a feed‐forward loop is triggered through activation of E2F1–3 resulting in a rise of cyclin‐dependent kinase (Cdk) activity and rapid transcriptional activation of E2F target genes, including cyclins and E2Fs themselves 12. Since E2F7 and E2F8 are also E2F target genes, we proposed the requirement for additional control mechanisms to inhibit their preliminary activation in late G1.
Another important mechanism that coordinates progression from G1 to S phase is the inactivation of the anaphase‐promoting complex/cyclosome APC/CCdh1. This permits accumulation of proteins that are required to progress through a single round of S phase properly, such as cyclin A, geminin, and CDC6 13, 14. Inactivation of APC/CCdh1 also relies on rising Cdk activity, leading to inactivation of CDH1, as well as E2F‐mediated transcription of Emi1, a direct APC/CCdh1 inhibitor 15, 16, 17. APC/CCdh1 maintains a necessary time window in G1 to prepare the cell for replication, illustrated by the fact that loss of CDH1 can lead to premature S phase entry, and induces replication stress and the accumulation of DNA damage 18, 19, 20.
Here, we show that E2F7 and E2F8 are targeted for ubiquitin‐mediated proteasomal degradation via APC/CCdh1 during the late stages of mitosis and G1 phase. Remarkably, E2F7 and E2F8 in turn can activate the APC/CCdh1 via repression of Emi1 and cyclins A and E, which are all known to inhibit APC/C activity. Thus, during the course of G1 phase, APC/CCdh1 eventually stimulates its own inactivation: Targeting E2F7 and E2F8 for destruction permits accumulation of Emi1, and cyclins A and E. Collectively these data show that atypical E2Fs and APC/CCdh1 are engaged in a feedback loop that tightly coordinates S phase entry and proper DNA replication. Importantly, we show that blocking the APC/CCdh1‐mediated destruction of ectopically expressed E2F7 and to a lesser extent E2F8 prohibits S phase and results in cell death.
Results
E2F7 and E2F8 are targeted for proteasomal degradation during G1
We first explored whether atypical E2Fs are subjected to posttranslational regulation. We treated the hTERT‐immortalized retinal pigment epithelium cell line RPE1‐TERT (RPE) with the protein translation inhibitor cycloheximide (CHX) and found a robust decrease in E2F7/8 protein levels within 1 h of treatment (Fig 1A and B). The disappearance of E2F7 and E2F8 was inhibited by co‐treatment with the proteasome inhibitor MG132. Then, we arrested RPE1 cells in G1 with the selective CDK4/6 inhibitor PD0332991 (PD). Protein expression of E2F7 and E2F8 was markedly reduced after 16 h of treatment (Fig 1C). U2OS osteosarcoma cells with intact RB function 21 also showed a reduction in E2F7/8 protein levels after 16 h of PD treatment. Arresting these cells in G2 phase with the CDK2 inhibitor NU6140 did not decrease E2F7/8 expression, suggesting that this effect is cell cycle phase‐specific (Fig 1C). We found that the disappearance E2F7/8 by PD0332991 treatment could be rescued by adding the proteasome inhibitor MG132 2 h prior to harvesting (Fig 1D). Together, these results strongly point toward a high turnover of E2F7 and E2F8 via proteasomal degradation, particularly during the G1 phase of the cell cycle.
One likely candidate to mediate proteasomal degradation early in G1 phase is APC/CCdh1. Using the ELM protein sequence analysis resource (http://elm.eu.org), we found that atypical E2Fs contain evolutionary conserved KEN domains, which are the canonical substrate recognition motifs for APC/CCdh1 (Fig 1E) 22. Furthermore, observations in a cell free system suggested that atypical E2Fs may be substrates of the APC/C 23. We then took advantage of the Fluorescent Ubiquitination‐based Cell Cycle Indicator (FUCCI) system, which is based on the activities of APC/CCdh1 and SCFSkp2 24. Using FACS sorting, we isolated cell populations in different phases of the cell cycle as indicated to determine protein and mRNA levels of atypical E2Fs (Fig 1F). From the onset of anaphase until the next S phase the APC/C is active, and Azami green‐tagged geminin1‐110 is absent. Notably, E2F7 and E2F8 proteins were nearly undetectable in these G1 cells (Fig 1G). The protein levels of E2F1 and cyclin B1, which are also APC/C substrates 25, 26, 27, showed expression patterns consistent with APC/C activity (Fig 1G). Interestingly, CCNB1 transcript levels were not decreased in cells labeled as telophase‐to‐early G1, confirming that this sharp drop in cyclin B1 protein was entirely caused by APC/C‐mediated proteasomal degradation (Fig 1H). Although protein and transcript levels of E2F7 and E2F8 in sorted cells showed a similar trend, transcripts were only mildly regulated in the cell cycle, while protein levels fluctuated considerably (Fig 1H). This confirms the important contribution of posttranslational regulation mechanisms. Collectively, these data show that E2F7 and E2F8 are relatively unstable proteins during G1 phase and that their degradation coincides with high APC/C activity.
E2F7 and E2F8 are APC/CCdh1 substrates
To determine whether E2F7 and E2F8 are bona fide APC/CCdh1 substrates in human cells, we transfected 293T cells with Flag‐tagged CDH1. We observed a robust reduction of endogenous E2F7/8 proteins after overexpression of CDH1 similar to the known APC/CCdh1 substrates CDC6 and aurora kinase A (Fig 2A and B). To rule out an indirect transcriptional effect of CDH1 overexpression on E2F7/8, we then expressed EGFP‐tagged E2F7 or E2F8 (transcriptionally controlled by a CMV promoter) in combination with CDH1. We observed a near‐complete reduction in exogenous E2F7/8 by CDH1 overexpression (Fig 2C). Reciprocally, depleting CDH1 in cells with stable doxycycline‐inducible expression of E2F7 or E2F8 using RNAi, stabilized exogenous E2F7 and E2F8 proteins (Fig 2D). We then performed co‐immunoprecipitation experiments and found that E2F7/8 and CDH1 physically interacted with each other (Fig 2E).
Next, we followed the levels of E2F7 and E2F8 when cells progressed through mitosis and G1 phase. We used time‐lapse microscopy experiments in HeLa cell lines with stable inducible overexpression of EGFP‐tagged E2F7 and E2F8. These experiments revealed that both proteins are degraded during telophase and the subsequent G1 phase, coinciding with APC/CCdh1 activation (Figs 2F and EV1A). Importantly, we could completely prevent the degradation of E2F7 by treating cells with siRNA oligos targeting CDH1. CDH1 RNAi also caused a marked, but incomplete stabilization of E2F8, indicating that additional E3 ligase activity, such as CDC20, could be partially responsible for E2F8 degradation (Fig 2F). To evaluate the contribution of CDC20 in degrading atypical E2Fs and to verify that the APC/C targets endogenous E2F7 and E2F8 proteins, we transfected RPE cells with CDC20 or CDH1 RNAi and measured protein levels during mitosis. The RNAi‐treated cells were synchronized in prophase with nocodazole and then released by washing out the drug and forced into mitotic exit with the CDK1 inhibitor RO3306 and the MPS1 inhibitor reversine (Fig EV1B). E2F7 was almost completely degraded within 1 h after release, and CDH1 RNAi completely prevented this degradation (Fig 2G), demonstrating that endogenous E2F7 protein levels are regulated by CDH1. Surprisingly, CDC20 RNAi also prevented degradation of E2F7, as well as CDC6 and aurora kinase A, which were previously shown to be regulated by CDH1, but not by CDC20 28, 29. Most likely, CDH1 activity was indirectly compromised by CDC20 RNAi. This is illustrated by incomplete dephosphorylation of the APC/C subunit APC3, which is heavily phosphorylated during the prophase arrest and rapidly dephosphorylated after the release (Fig 2G). In contrast, cells treated with CDH1 RNAi showed complete degradation of the APC/CCdc20 substrate cyclin B1, demonstrating that CDC20 is highly active under CDH1 RNAi conditions. Nevertheless, E2F7 as well as CDC6 and aurora kinase A were completely stabilized, making it highly unlikely that E2F7 is targeted by CDC20. We could not detect major differences in the expression levels of endogenous E2F8 protein levels after release from the mitotic arrest or under CDC20 RNAi or CDH1 RNAi conditions. Since the protein expression of E2F8 was very low during nocodazole treatment, we used HeLa cells with inducible overexpression of E2F8‐EGFP to further evaluate the effects of CDC20 RNAi. Consistent with the time‐lapse imaging, CDH1 RNAi resulted in a partial stabilization of E2F8‐EGFP during mitotic exit (Fig 2H). Remarkably, this stabilization was more pronounced in cells treated with CDC20 RNAi, suggesting that CDC20 can target E2F8 for degradation.
These results show that E2F7 and E2F8 are targeted for degradation by APC/CCdh1 during mitotic exit. Furthermore, E2F7 appears to be more tightly regulated by APC/CCdh1 than E2F8. APC/CCdc20 and most likely a yet‐unidentified additional E3 ligase activity account for additional E2F8 degradation.
Mutation of KEN domains in E2F7 and E2F8 prevent their APC/CCdh1‐mediated destruction
To evaluate whether the KEN domains on E2F7 and E2F8 are indeed true APC/CCdh1‐interacting sites, we performed site‐directed mutagenesis experiments. E2F7 contains a conserved KEN domain at amino acid positions 31–33. E2F8 has two conserved KEN motifs, located at amino acids 5–7 and 374–376, respectively. The KEN motifs were replaced with three consecutive alanine residues (Fig EV2A). For E2F8 we created single‐ as well as double‐mutant plasmids (E2F8KEN5mut and E2F8KEN374mut, and E2F8K/K, respectively). We co‐transfected 293T cells with equal amounts of these constructs in combination with CDH1‐Flag or empty vector. Notably, protein levels of KEN mutant versions of E2F7 and E2F8 were clearly higher than their wild‐type counterparts, particularly in the presence of CDH1‐Flag (Fig 3A). Because both KEN mutations in E2F8 had a similar effect, we concluded that both domains are functional and decided to perform all subsequent experiments with the double mutant (E2F8K/K). We then performed stable transfection of these constructs in HeLa cells expressing the Tet repressor. We confirmed that the KEN mutants are not misfolded or otherwise dysfunctional, by showing repression of the known E2F target genes CDC6 and cyclin A2 after 16 h of doxycycline treatment (Fig 3B). In fact, cell lines expressing KEN mutants showed stronger repression, notwithstanding comparable overall expression levels. Using FACS analysis to plot levels of E2F7/8 (EGFP) against DNA content (propidium iodide) we noted that stable cell lines expressing the wild‐type versions of E2F7/8 contain only few EGFP‐positive cells with 2C DNA content (G1 phase, Fig 3C). However, induction of E2F7/8KEN showed a much higher percentage of EGFP‐positive cells with 2C DNA content (Figs 3C and EV2B). Importantly, CDH1 RNAi during doxycycline induction caused a massive increase in the number of strongly EGFP‐positive E2F7WT‐ or E2F8WT‐expressing cells with 2C DNA content, comparable to the effect of KEN mutation, confirming CDH1‐dependent degradation of E2F7/8 during G1 (Figs 3C and EV2B).
Time‐lapse imaging showed that E2F7KEN and E2F8K/K degradation after anaphase is blocked, in sharp contrast to their wild‐type counterparts (Figs 3D and EV2C). We found that E2F8K/Kmut degradation was not completely prevented, unlike E2F7KEN. In line with this, co‐immunoprecipitations showed a robust KEN‐domain‐dependent interaction between E2F7 and endogenous CDH1, but a much weaker interaction with E2F8, which was not affected by KEN mutation (Fig EV3A). The residual degradation of KEN mutant E2F8 may be explained by APC/C binding via CDC20. Indeed, we found three putative D‐boxes in E2F8 (Fig EV3B). Accordingly, we found that both wild‐type and KEN mutant E2F8 co‐immunoprecipitated with CDC20‐Flag (Fig EV3C and D). In contrast, CDC20 did not co‐immunoprecipitate with E2F7, again suggesting that E2F7 is only targeted by CDH1 (Fig EV3D). These data show that E2F7 and E2F8 have functional KEN domains, and mutation of these domains results in stabilization of E2F7 and E2F8 during mitotic exit and G1.
Stabilization of E2F7/8 during G1 inhibits cell proliferation by reduced S phase entry and increased cell death
We previously showed that inducible E2F7WT overexpression inhibits proliferation by delaying S phase progression, while not affecting S phase entry 8. This could indicate that during unperturbed cell cycles, cells very efficiently degrade E2F7/8 for normal progression through G1 phase. We therefore hypothesized that stabilization of E2F7 or E2F8 in G1 by preventing its APC/CCdh1‐mediated degradation would prevent cells from starting S phase. To test this hypothesis, we quantified incorporation of the thymidine‐analog BrdU in cells with stable inducible expression of KEN mutant and wild‐type E2F7/8. Both E2F7WT‐ and E2F8WT‐expressing cells continued to incorporate BrdU at high levels after 24 and even 48 h of doxycycline treatment (Figs 4A and EV4A). Nevertheless, proliferation was inhibited by induced overexpression of the wild‐type versions of E2F7 and E2F8 (Fig 4B). However, induction of E2F7KEN severely reduced BrdU incorporation, indicating that interfering with APC/C‐mediated degradation of E2F7 in G1 negatively impacts S phase entry. The overexpression of E2F8K/K also demonstrated a significant reduction in BrdU incorporation, although the effect was less pronounced than that of E2F7KEN (Fig 4A). To further investigate whether cells overexpressing KEN mutant E2F7 arrest in G1, we performed a time‐course experiments by releasing cells from a mitotic arrest. The control cells showed a very steep induction of classic target genes, such as E2F1 and CCNE1, at 8 h and 12 h after release indicating S phase entry, but this induction was completely blocked by E2F7KEN expression (Fig 4C). Remarkably, the cell line expressing E2F8K/K only showed a minor inhibition of target gene expression. The difference between E2F8 and E2F7 could be potentially explained by differences in the percentages of cells expressing detectable levels of the constructs. To correct for this, we traced cell cycle fates at the individual cell level. We quantified S phase entry using PCNA‐mCherry as a marker and followed its subcellular distribution with time‐lapse imaging (Fig 4D, Movie EV1). The onset of S phase is characterized by formation of PCNA dots, known as replication factories 30. Whereas the bulk of cells without expression of KEN mutant E2F7 and E2F8 (EGFP‐negative) entered S phase during the 40 h of imaging, only very few cells expressing E2F7KEN did so (Figs 4E and G, and EV4B). E2F8K/K‐expressing cells also showed a reduced percentage of cells entering S phase, but again the effect was less pronounced. Instead of entering S phase, 50% of the E2F7KEN‐expressing cells died within 40 h of live cell imaging, as detected by leakage of PCNA into the cytoplasm, followed by cell blebbing (Figs 4F and EV4B, Movie EV2). Most of these cells died during G1 defined by observation of a normal mitosis, but no evidence of PCNA nuclear dot formation prior to cell death (Fig 4G).
The KEN mutations in E2F8 caused a much less severe S phase entry defect than in E2F7, and while many E2F7KEN cells died during imaging, E2F8K/K were mostly still alive at the end of analysis (Figs 4F and G, and EV4B). To verify this, we stained cells with annexin V and again found that only the E2F7KEN‐expressing cells showed a robust increase of apoptosis (Fig EV5A). We then asked whether the E2F8K/K‐expressing cells were able progress through S phase normally. To this end, we released E2F8‐expressing cells from a HU arrest and quantified cell cycle progression of doxycycline‐treated cells and their vehicle‐treated counterparts (Fig 4H). Although the percentages of positive cells and average EGFP intensity were very similar between E2F8WT and E2F8K/K, we gated out EGFP‐negative cells to avoid bias (Fig EV5B and C). We observed a marked delay in S phase progression of cells expressing E2F8K/K compared to E2F8WT‐expressing cells, suggesting that unscheduled expression of E2F8 in G1 causes problems during the subsequent S phase (Figs 4I and EV5D).
Next, we tested whether depletion of CDH1 would also impair S phase entry in E2F7/8WT‐expressing cells, using BrdU incorporation and live PCNA imaging. Treatment with CDH1 RNAi slightly reduced the percentage of BrdU‐positive E2F7/8WT‐expressing cells (Fig 5A). An explanation for this modest effect is that CDH1 depletion causes the accumulation of cyclin A and other proteins that drive S phase entry, which could in part override the effect of E2F7/8 stabilization 19. However, despite modest effects on BrdU incorporation, time‐lapse microscopy of individual cells showed that CDH1 RNAi completely prevented normal PCNA dot formation in the E2F7WT‐ or E2F8WT‐EGFP‐expressing cells (Fig 5B). Instead, almost all cells with combined CDH1 depletion and overexpression of E2F7/8 underwent cell death, as seen by leakage of PCNA‐mCherry into the cytosol followed by cell blebbing (Figs 5B and C, and EV4B). Notably, CDH1 RNAi did not cause a discernible effect on S phase entry or cell death in EGFP‐negative control cells, except for a minor delay in S phase entry of EGFP‐negative cells in the E2F8WT cell line. These data demonstrate that APC/CCdh1‐dependent degradation of ectopic E2F7 or E2F8 during G1 is required for the initiation and progression of DNA replication.
A feedback loop between E2F7/8 and APC/CCdh1
During late G1, APC/CCdh1 is inhibited by two mechanisms. First, phosphorylation of CDH1 by cyclin A/CDK2 or cyclin E/CDK2 prevents its interaction with APC/C, and second, the endogenous APC/C inhibitor Emi1 starts to be expressed 31, 32. Both mechanisms are at least in part dependent on E2F activity, although the role of E2F7/8 has not been explored yet 16, 33. We found that doxycycline‐induced expression of E2F7 and E2F8 caused a severe reduction in Emi1 protein levels (Fig 6A). This reduction was stronger with KEN mutants, particularly in the case of E2F8. To show that this is a direct effect, we then performed quantitative PCR on FACS‐sorted, HU‐synchronized cells (Fig EV6A and B). Quantitative PCR showed that 8 h of doxycycline treatment was sufficient to cause a marked repression of FBXO5, the gene encoding Emi1 in cells expressing E2F7WT or E2F8WT (Fig 6B). Cyclin E1 and A2, two other APC/C inhibitors, were also transcriptionally repressed by E2F7/8 (Fig 6B). Aurora kinase A was not repressed at the transcriptional level, but proteins levels were reduced upon overexpression of E2F7/8 (Fig 6A and B). These findings suggest that E2F7/8‐mediated repression of the APC/C inhibitors Emi1, cyclin E, and cyclin A results in enhanced APC/C activity as observed by the enhanced degradation of the APC/C substrate aurora kinase A.
To test whether endogenous E2F7/8 repress Emi1, we transfected HeLa cells with RNAi directed against E2F7 and E2F8. We harvested the cells in late S phase, 6 h after HU release, where E2F7 and E2F8 are expected to be highly expressed. Because E2F7 and E2F8 can transcriptionally repress each other, and can compensate for each other's function, we analyzed target gene expression in cells where both atypical E2Fs were knocked down (Fig 6C and D). We found a significant increase in FBXO5 transcript and Emi1 protein levels upon inactivation of atypical E2Fs, demonstrating that atypical E2Fs functions as transcriptional repressors of APC/C inhibitors (Fig 6C and D).
Next, we tested how APC/C impacts endogenous E2F7/8 expression during G1 and S phase. We transfected RPE cells with CDH1 RNAi, arrested them in G1 with the CDK4/6 inhibitor PD0332991, and released them by removing the drug (Fig EV6C). We verified that this synchronization approach was successful by FACS analysis of propidium iodide/BrdU‐stained cells (Fig 6E). We found no discernible effect of CDH1 RNAi on cell cycle progression under these experimental conditions, although it was previously reported that G1 is shortened after CDH1 depletion after nocodazole release 34, 35. However, knockdown of CDH1 resulted in enhanced protein expression of E2F7 during PD0332991 treatment and after release, as well as the APC/CCdh1 substrates CDC6 and aurora kinase A (Fig 6F). Importantly, 8 h after release, when Emi1 expression became clearly detectable, CDH1 RNAi caused a reduction in Emi1 levels, consistent with unscheduled E2F7 expression. E2F8 expression was again very low during G1 and surprisingly not enhanced after CDH1 RNAi. In fact E2F8 was further reduced, following a pattern similar to Emi1 expression (Fig 6F). To more conclusively study the effects of APC/C activity on endogenous E2F8, we performed an inverse experiment. Emi1 is critical for inactivation of the APC/C during S phase; therefore, we reasoned that Emi1 RNAi would result in decreased E2F7/8 expression. We arrested cells in S phase using HU, and indeed E2F7 and E2F8, as well as CDC6 and aurora kinase A, were partially degraded (Fig 6G). Because CDK2 can also inhibit APC/CCdh1, we also added the CDK2 inhibitor NU6140. This approach resulted in a near‐complete degradation of E2F7/8 as well as the other substrates after Emi1 RNAi, providing further support for a direct feedback loop between E2F7/8 and APC/C activity.
We noticed that many APC/C substrates are also target genes of E2F7/8. CDC6 and cyclin A2 are prominent examples, but in fact 27% of the genes from a published curated list of APC/C substrates 36, 37 are E2F7 and E2F8 target genes we have previously identified 8, 10 (Fig 6H). Based on this observation and the data presented here, we propose a model where the interplay between atypical E2Fs and APC/C controls the levels of important cell cycle genes on the transcriptional and posttranslational level (Fig 6I).
Discussion
Using a combination of time‐lapse fluorescence imaging experiments, in which we followed cells as they progress through the cell cycle, we found that E2F7 and E2F8 are degraded during late mitosis via APC/CCdh1. Furthermore, we demonstrate that APC/CCdh1 plays an important role in keeping E2F7/8 levels low throughout G1, because mutations in the KEN boxes or knockdown of CDH1 stabilized atypical E2Fs during this phase of the cell cycle. Combining E2F7/8 overexpression levels with ablation of CDH1 or expressing atypical E2F‐KEN mutants resulted in severely impaired S phase entry. These findings suggest that degradation of E2F7/8 is required for cells to enter S phase. Since atypical E2Fs function as transcriptional repressors of genes involved in DNA replication, inactivation of atypical E2F activity would allow the initiation of the DNA synthesis machinery 5, 6, 7, 8. The activator E2F1, E2F2, and E2F3 are required for transcriptional activation of S phase genes, and RB needs to be phosphorylated by cyclin/CDK complexes to release its inhibitory effect on the activator E2Fs. Similar to RB, atypical E2Fs can repress transcription of activator E2Fs as well, and we now provide a potential mechanism for keeping E2F7/8 levels low during G1 through APC/CCdh1‐mediated degradation to allow an upswing of E2F activator activity and transcription of S phase genes.
In many cellular contexts, the activator E2Fs and atypical E2Fs counterbalance each other: first, common target genes can be regulated in opposite manner, and secondly, E2F1–3 can directly activate E2F7/8, whereas E2F7/8 can also repress E2F1–3 9, 10, 11, 38. Thus, it seems counterintuitive that both classes of E2Fs would be regulated in the same manner at the posttranslational level. Nevertheless, activator E2Fs were found to be targeted for destruction by the APC/C under specific conditions. E2F3 degradation via APC/CCdh1 was linked to cell cycle exit and differentiation 39. E2F1 is degraded via APC/CCdc20 in prometaphase, but also by APC/CCdh1 26, 27. Interestingly the interaction with the dimerization partner DP protects E2F1 from destruction via the APC/C 26. Thus, a significant pool of E2F1 could be insensitive to degradation in G1 cells. In contrast, E2F7/8 do not interact with DP, and thus cannot be protected against degradation in this manner 5, 6, 7, 40. Also, the substrate binding by CDC20 and CDH1 appeared to occur via non‐canonical recognition motifs in E2F1, and E2F3, because the mutation of putative D‐boxes in E2F1 and E2F3 did not affect their degradation 26, 39. This indicates that their degradation follows different kinetics than the degradation of E2F7/8. Thus, APC/C activity can control the balance between activator and atypical E2F activity.
We provide evidence that E2F8, but not E2F7 is targeted for degradation by APC/CCdc20. However, the physiological relevance is yet unknown, because our time‐lapse imaging experiments showed that cells expressing stable, KEN mutant E2F8 did not have any apparent mitosis defects. We also observed that E2F8 levels already decrease during G2 and prophase (nocodazole), to rather low levels; furthermore, E2F8 was extremely low during G1, and contrary to E2F7, CDH1 depletion did not enhance its expression. Thus, it is highly likely that additional, yet‐unidentified E3 ligases can mediate E2F8 degradation. This could possibly be SKP1‐CUL1‐F‐box‐protein (SCF) complex, given its important role in cell cycle regulation 31 and its role in regulating activator E2F expression 41.
We noted a substantial overlap between activator E2Fs, atypical E2Fs, and APC/CCdh1 in regulating the expression of cell cycle genes (Fig 6I). Whereas E2F1–3 function as transcriptional activators and E2F7/8 as transcriptional repressors, APC/CCdh1 induces the degradation of a common set of E2F targets. The majority of the E2F target genes are essential for cell cycle progression, suggesting that the interaction between E2Fs and APC/CCdh1 coordinates the transcription and degradation of these cell cycle genes to allow proper cell cycle progression. Moreover, inactivation of the inhibitors of these cell cycle genes, the atypical E2Fs and APC/CCdh1, resulted in similar in vivo phenotypes. For example in mice, deletion of the CDH1‐encoding gene Fzr1, or E2f7/8 loss, both cause defects in trophoblast giant cell polyploidization 11, 19. In contrast, inactivation of the activators E2F1, E2F2, and E2F3, resulted in an enhanced trophoblast giant cell polyploidization 11. These findings provide further support that E2F‐ APC/CCdh1 interaction is critical for regulating common cell cycle genes.
Many of these common E2F target genes display an oscillating expression pattern during the cell cycle, characterized by low expression during M/G1, an upswing in expression during G1/S and downswing during G2/M 42. The orchestration of this oscillating pattern is partially mediated through the high APC/CCdh1 activity during the M and G1 phases, the induction of activator E2F1–3 during G1/S, and the increase of E2F7/8 during S/G2. Since APC/CCdh1 can degrade E2Fs as well as E2F targets, its activity needs to be downregulated during S/G2. Previous studies have demonstrated that Emi1 and CDK2 are the main inhibitors of APC/CCdh1 15, 16. Importantly, we show here that all these APC/CCdh1 inhibitors are directly repressed by the atypical E2Fs, providing strong evidence for a novel feedback loop between APC/CCdh1 and E2F7/8. Thus, E2F7/8 can activate its own degradation as well as the degradation of some of its targets by transcriptionally repressing the APC/CCdh1 inhibitors Emi1 and cyclin A/E‐CDK2. This regulatory mechanism is most likely important during late S, G2, and M phases to coordinate the downregulation of E2F target genes. In addition, it might be also relevant during DNA damage, because previous studies have shown that E2F7/8 expression increases during DNA damage 43, 44, 45 and APC/CCdh1 activity becomes reactivated in G2 cells with DNA damage 46, 47. Further support for an APC/CCdh1‐E2F feedback loop is provided by the fact that the Emi1‐encoding gene FBXO5 and the CDK2‐activating genes CCNA2 and CCNE1/2 are known target genes of the activator E2F1–3 33, 48, 49. Since E2F1–3 are induced during the G1/S phase transition, the transcriptional activation of Emi1 and CDK2‐activating cyclins most likely mediates the inhibition of APC/CCdh1 activity, which is crucial for S and G2 phase progression and mitotic entry 16, 50, 51.
In summary, we show a novel and important role for atypical E2Fs in determining the balance between synthesis and repression of E2F target genes, and balancing APC/C activity.
Materials and Methods
Generation of cell lines and cell culture
Mouse E2F8 cDNA (Reference sequence: NM_001013368.5) was amplified with primers that introduced a NotI site at the 5′ and a XhoI site at the 3′ end, using Pfu polymerase (New England Biolabs). The cDNA was then cloned into the pEGFP‐N3 plasmid (Invitrogen) using a double digestion with these two enzymes, followed by ligation with T4 ligase (New England Biolabs), in such a way that a C‐terminal E2F8‐EGFP fusion protein is transcribed. Subsequently, E2F8‐EGFP was digested from the pEGFP plasmid by an enzymatic digestion with NotI and subsequently ligated into the pcDNA4/TO plasmid (Invitrogen) using T4 ligase. Correct orientation of E2F8‐EGFP in the plasmid was verified by running XhoI‐digested plasmids in an agarose gel. Plasmids containing E2F7 were generated as described before 8.
Site‐directed mutagenesis against sequences encoding KEN domains was performed by PCR amplification with Pfu polymerase of the E2F7/8 plasmids with primers encoding the required mutations. To ensure complete inhibition of these motifs, the KEN sequences were replaced by three consecutive alanines. Successful cloning and mutagenesis were confirmed with Sanger sequencing (Macrogen).
Tet repressor‐expressing HeLa cells (T‐REx HeLa; Invitrogen) were transfected with these constructs, and stable clones were established by Zeocin selection (Invitrogen, 300 μg/ml). The cells were cultured in DMEM containing 10% Tet System Approved fetal bovine serum (Clontech). Overexpression was induced by adding 0.2 μg/ml doxycycline (Sigma) to the cell culture medium. Cells were synchronized by adding 2 mM hydroxyurea (Sigma‐Aldrich) to the medium for 16 h, or 2.5 mM thymidine to arrest cells at the onset of S phase. Cells were released from the block by washing three times with PBS and adding fresh medium containing 10% FBS. Other drugs used were as follows: MPS1 inhibitor reversine (50 nm, Cayman Chemicals 10004412), CDK1 inhibitor RO‐3306 (10 μM, Calbiochem #217699), Cdk4/6 inhibitor PD0332991 (0.5 μM, Selleck S116), nocodazole (830 nM Sigma‐Aldrich M1404), and CDK2 inhibitor NU6140 (10 μM, Tocris 3301).
Flow cytometry and FACS sorting
For measurement of DNA contents, cells were trypsinized, washed with PBS, fixed with 70% ethanol, and stored at 4°C up to 1 week. Cells were washed twice with TBS and then reconstituted in PBS containing 20 μg/ml propidium iodide, 250 μg/ml RNase A, and 0.1% bovine serum albumin (BSA).
DNA synthesis was measured by adding 100 μM 5‐bromo‐2′‐deoxyuridine (BrdU; Sigma) to the culture medium for 2 h prior to harvesting. Ethanol‐fixed samples were washed once with PBS, cells were incubated with 0.1 N HCl/0.5 mg/ml pepsin for 20 min. After washing with TBS/0.5% Tween/0.1% BSA, 2 N HCl was added for 12 min, followed by pH neutralization with sodium tetraborate buffer (pH 8.5). After washing twice with TBS‐0.1% Tween, cells were incubated for 1 h with a FITC‐conjugated antibody against BrdU (Becton Dickinson 347583). Cells were washed with TBS, and labeled with propidium iodide as indicated above. All samples were measured on a BD FACSCanto II (BD Biosciences) and further analyzed using FlowJo software.
Two‐way FACS sorting based on FUCCI markers was performed on a BD Influx system by a senior operator. Cells were collected in cold PBS and briefly centrifuged at 800 g. After removing the PBS, lysis buffer was added to the cell pellet. For RNA isolation, 50,000 cells were collected, and for protein 300,000 cells.
Transfections
HEK293T cells were seeded at a density of 3 million in 10‐cm petri dishes. The next morning cells were transfected with 10 μg of E2F7/8 plasmid and/or 2 μg of CDH1‐Flag using the calcium phosphate method. After 48 h, transfected cells were harvested. For co‐immunoprecipitation experiments, 10 μM of MG132 (Cayman Chemicals) was added to the culture medium 5 h prior to harvesting.
For siRNA experiments, RPE or HeLa cells were plated in 6‐well dishes and transfected with 10 nM of CDC20, CDH1, Emi1, E2F7, E2F8, or scrambled siRNA (all SmartPool; Dharmacon) using RNAiMAX or Lipofectamine according to the manufacturer's instructions, with the modification that transfection complexes were added to the cells for 6 h in basic medium containing no serum or antibiotics. Afterward, cells were washed and fresh medium containing 10% FBS and pen/strep was added.
To create inducible E2F7/8‐EGFP cell lines co‐expressing Cherry‐PCNA, cells were infected with the viral plasmid pLIB‐Cherry‐PCNA as described before 14. Virus carrying Cherry‐PCNA was created by calcium phosphate transfection of HEK293T cells, and double infection of target cells in the presence of polybrene.
Time‐lapse fluorescence microscopy
Acquisition of differential interference contrast (DIC) and fluorescence images started 24 h after transfection on a microscope (Axio Observer Z1; Carl Zeiss) in a heated culture chamber (5% CO2 at 37°C) using DMEM with 8% FCS and antibiotics. The microscope was equipped with an LD 0.55 condenser and 40× NA 1.40 Plan Apochromat oil DIC objective and CFP/YFP and GFP/HcRed filter blocks (Carl Zeiss) to select specific fluorescence. Images were taken using ZEN 2012 acquisition software (Carl Zeiss) with a charge‐coupled device camera [ORCA R2 Black and White CCD (Hamamatsu Photonics)] at 50‐ms exposure time for EGFP excitation and 200‐ to 300‐ms exposure time for mCherry excitation at 30% LED intensity. For quantitative analysis of degradation, ImageJ (National Institutes of Health) and Excel (Microsoft) were used. Captured images were processed using Photoshop and Illustrator software (Adobe). Plots were created by GraphPad Prism version 6.0f, for Mac OS X (GraphPad Software).
Quantitative PCR
Isolation of RNA, cDNA synthesis, and qPCR were performed as previously described 8. Gene expression was calculated using a ΔΔC t method adapted for multiple‐reference gene correction 52. All samples were corrected for the two reference genes β‐actin and GAPDH. Primer sequences are provided in Table EV1.
Co‐IP and immunoblotting
Cells were harvested by washing twice with PBS, and scraped in a lysis buffer containing 50 mM Tris–HCl, 1 mM EDTA, 150 mM NaCl, 0.25% deoxycholic acid, 1% Nonidet P‐40, 1 mM NaF, 1 mM NaV3O4, and protease inhibitor cocktail (Roche). Cells were lysed on ice for 20 min, and centrifuged for 10 min at 12,000 g. The supernatants were then immunoblotted with standard SDS–PAGE techniques. Antibodies used throughout this paper are listed in Table EV2. Visualization was done by ECL (GE Healthcare RPN2106) and exposure to a film (GE Healthcare). All blot photos are representative examples of three independent experiments, unless stated otherwise.
Co‐immunoprecipitations were performed as follows: cells in one near‐confluent 10‐cm dish were harvested in 1 ml of protein lysis buffer as described above. Then, BSA‐blocked prot G beads (Fastflow; Millipore) were added and incubated for 30 min at 4°C to preclear the lysates. One 1% of the total input was kept separately, and immunoprecipitation was done by rotating samples at 4°C for 1 h in the presence of 2 μg of anti‐Flag and BSA‐blocked prot G beads. EGFP‐tagged fusion proteins were immunoprecipitated with GFP‐Trap (Chromotek). After washing the beads with lysis buffer, protein was eluted using Laemmli loading buffer and immunoblots were performed as described above.
Data analysis
All immunoblots, co‐immunoprecipitations, FACS data, and qPCR results were replicated three times, unless stated otherwise in the figure legends. Statistical analysis on qPCR and FACS data was performed by ANOVA followed by Holm‐Sidak post hoc individual group comparisons. Individual curves for S phase entry and cell death were compared as pairs by log‐rank (Mantel–Cox) test.
Author contributions
MB, RY, APW, HAS, EAvL, NA, IJ, and BW performed experiments. MB, RMFW, AdB, and BW conceived experiments, analyzed and interpreted the data, and wrote the manuscript.
Conflict of interest
The authors declare that they have no conflict of interest.
Supporting information
Acknowledgements
We thank Dr. Daniele Guardavaccaro (Hubrecht Institute, Utrecht, NL) for kindly providing CDH1 and CDC20 constructs and helpful discussion. The stable RPE‐FUCCI cell lines were provided by Prof. Rene Medema (Netherlands Cancer Institute, NL). Ger Arkesteijn (Utrecht University, NL) provided expert assistance with FACS sorting experiments. This work was financially supported by a Dutch Cancer Society grant (KWF: UU2013‐5777) to BW and AdB, Netherlands Organization for Scientific Research (NWO: ALW‐IN11‐28) to AdB, and a HFSP project grant to MB and RMFW (RGP0053/2010).
EMBO Reports (2016) 17: 414–427
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