• We are sorry, but NCBI web applications do not support your browser and may not function properly. More information
Logo of pnasPNASInfo for AuthorsSubscriptionsAboutThis Article
Proc Natl Acad Sci U S A. Sep 25, 2001; 98(20): 11211–11217.
Inaugural Article

Binding of cyclin-dependent kinases to ORC and Cdc6p regulates the chromosome replication cycle


Cdc6p and the origin recognition complex (ORC) are essential for assembly of a pre-replicative complex (preRC) at origins of replication, before the initiation of DNA synthesis. In the absence of Cdc6p, cells fail to initiate DNA replication and undergo a “reductional” mitosis, in which the unreplicated chromosomes are randomly segregated to the spindle poles. We show here that the cells harboring a mutation in the essential Cdc6p Walker A-box arrest in late mitosis, probably at anaphase. This cell cycle block requires either the three Cdc28p phosphorylation sites within the N terminus of Cdc6p or a short region (aa 8–17) that contains a Cy (Cyclin) interaction sequence. These same two Cdc6p mutants that allow a reductional mitosis are defective in binding Cdc28p kinase. In addition to Cdc6p, ORC also binds to cyclin-dependent kinases (CDKs). Interestingly, Sic1p, a CDK inhibitor protein, blocked the S phase-specific Cdc28p-Clb5p kinase from interacting with ORC, but did not prevent the G1-specific Cdc28p-Cln2p kinase–ORC interaction. We suggest that ORC, Cdc6p, and Sic1p bind to different CDKs in a cell cycle-dependent manner to temporally regulate events that (i) allow preRC formation after mitosis, (ii) prevent mitosis before DNA replication can occur, and (iii) promote initiation of DNA replication.

The initiation of DNA replication in Saccharomyces cerevisiae and other eukaryotes is a cell cycle-regulated process requiring the assembly of a pre-replicative complex (preRC) at origins of DNA replication during G1 phase (14). The preRC contains several conserved initiation proteins and assembles before DNA synthesis (4). PreRC proteins include the origin recognition complex (ORC) that binds to and marks replication origins throughout the entire cell cycle, the Cdc6 protein (Cdc18 in Schizosaccharomyces pombe; ref. 5), the minichromosome maintenance (MCM) helicase, and Cdt1 (6). Cdc6p is an unstable protein that interacts with ORC and promotes loading of the six-subunit MCM complex to origins in an ATP-dependent manner (715). Although not yet identified in budding yeast, Cdt1 is also required for MCM binding to chromatin (6). The preRC renders chromosomes competent for initiation of DNA replication, but initiation does not occur because cells have not yet committed to S phase. Both cyclin-dependent protein kinases (CDKs; Cdc28p-Clb5p and -Clb6p) and Cdc7p-Dbf4p are required for S phase commitment by activating origin firing and promoting loading of Cdc45p (16–29).

Yeast Cdc28p interacts with two types of cyclins, the Cln and Clb cyclins, to form an active CDK (30). The G1 cyclins, Cln1p and Cln2p, control bud formation, spindle pole body duplication, and one step in the initiation of DNA replication. The Cln-CDKs promote DNA replication by allowing expression and activation of the other type of CDK-cyclin, the B-type CDKs containing Clb5p or Clb6p cyclins (31, 32). In late G1, the Clns promote degradation of the B-type CDK inhibitor, Sic1p, and the initiation protein Cdc6p (3335). There are six CLB genes (CLB1-6) in budding yeast. Clb5p- and Clb6p-dependent kinases promote origin activation in a temporally controlled manner (36) and activation of origins by loading Cdc45p (23), whereas Clb1–4p kinases act later in the cell cycle, during G2 and M phase.

DNA replication is controlled by CDKs in at least two ways. First, preRC assembly can only occur when CDKs are inactive, thereby restricting preRC assembly to the period from mitotic exit to late G1 (3742). During this period, CDKs are kept inactive by a functioning anaphase-promoting complex (APC/cyclosome) and the presence of the CDK inhibitor Sic1p. The APC/cyclosome containing the adaptor Cdc20p promotes exit from mitosis by ubiquitinating the anaphase inhibitor Pds1 and Clb cyclins, such as Clb5p (43). The Cdc28p inhibitor Sic1p (p40) inhibits the kinase activity of any Cdc28p-Clb cyclin until late G1 (44). Later in the cell cycle, when CDK activity is high during S, G2, and early mitosis, assembly of the preRC cannot occur. However, CDKs provide a second function because they are required for origin activation in late G1 (3739, 45). CDK regulation of preRC assembly includes control of cell localization of MCM proteins and stability or availability of initiation regulatory proteins such as Sic1p and Cdc6p (34, 4042). After inhibition of APC and destruction of Sic1p, CDKs are activated and promote loading of Cdc45p and other proteins at each origin in a temporally regulated manner (23, 24, 46).

In addition to regulating the assembly of the preRC, cells also have checkpoint mechanisms to coordinate progression from one phase of the cell cycle to the next (4750). Checkpoints act to inhibit subsequent cell cycle events if there is a delay or error in a preceding stage. For instance, the S phase checkpoint acts to inhibit the metaphase to anaphase transition in budding yeast when DNA damage or incomplete DNA replication occurs during S phase. DNA damage or incomplete DNA replication is sensed and results in the activation of the Mec1p and Rad53p kinases that mediate repair and cell cycle arrest. Johnston and colleagues (51) have also described a G1–M phase checkpoint that operates in budding yeast to prevent mitosis in the absence of the initiation of DNA replication. This less well characterized pathway is independent of the Mec1p checkpoint kinase that mediates the inhibition of mitosis in response to incomplete DNA replication or damage. Furthermore, not all yeast strains have retained this checkpoint mechanism. The G1–M checkpoint is dominant in heterozygous diploids, suggesting that some standard yeast strains have mutations in this pathway.

Depletion of Cdc6p prevents replication initiation and results in a reductional mitosis in which cells randomly segregate their unreplicated chromosomes (8). Under these circumstances, the G1–M checkpoint is not operating. Paradoxically, we described a nonfunctional cdc6 mutant (in the same strain background) that prevented mitosis in the absence of DNA replication (12). Cdc6p is predicted to be an ATP binding protein and a mutant that changed a conserved lysine to glutamate (K114E) in the Walker A box was not able to initiate DNA replication or load the MCM proteins at the origin. So, in contrast to depletion of Cdc6p, cells expressing cdc6(K114E) (hereafter referred to as cdc6KE) did not pass through mitosis, suggesting that the inhibition of mitosis required Cdc6p itself. The inhibitory activity was mapped to the N-terminal 50 aa of Cdc6p, a region that is dispensable for its essential role in initiation (12).

Cdc18, the fission yeast homologue of Cdc6p, is required for the initiation of DNA replication (5) and also inhibits passage through mitosis when the protein is overproduced (52, 53). Like Cdc6p, Cdc18 is an unstable protein. Cdc18 contains six consensus CDK phosphorylation sites (five within the N terminus) that mediate its turnover, because mutation of these sites increases Cdc18p stability (54). Inhibition of B-type CDK activity also increased the stability of Cdc18. Like Cdc6p, which binds Cdc28 cyclin (55), Cdc18 interacts through its N terminus with the CDK subunit Cdc2 associated with the B-type cyclins (Cdc13 and Cig2; ref. 56). Increasing Cdc18 levels through overproduction leads to repeated rounds by DNA synthesis by promoting replication re-initiation. This may reflect an inhibition of mitotic CDK activity through direct binding and by promotion of new initiation events when Cdc18 is greatly overproduced.

Here we show that the ability to inhibit mitosis is abrogated by one of two separate mutations within the N terminus of Cdc6p. The first changes the three Cdc28 consensus phosphorylation sites at T7, T23, and S43 to alanine (TTS). The second, by deleting a 10-aa region (Δ8–17) containing a match to the Cy (Cyclin) motif. The Cy motif is found in other eukaryotic proteins and mediates binding to CDK-cyclins (5760). The ability of Cdc6p to inhibit mitosis is also correlated with binding to Cdc28p. A genetic analysis indicates that increasing B-type CDK activity can overcome the mitotic arrest of the cdc6KE mutant. The inhibition of mitosis is independent of RAD53, indicating that it is independent of the G1–S or S phase checkpoint pathways. These results suggest that the N terminus of Cdc6p has a function during mitosis and might be involved in the G1–M checkpoint pathway. We also suggest that Cdc6p, together with Sic1p and the APC/cyclosome, antagonizes CDK activity in late mitosis to early G1, perhaps directly at origins of replication. Finally, we demonstrate that Sic1p, in addition to regulating CDK activity, controls substrate accessibility.

Materials and Methods

Strains and Plasmids.

Genetic manipulation and transformation of yeast was done by standard techniques (61, 62). All S. cerevisiae strains were derivatives of W303 (63). Mutations in CDC6 were introduced by using site-directed mutagenesis of single-stranded uracil-containing phagemid DNA. After sequencing a restriction fragment containing the mutation, the mutations were transferred to pMW71 (pRS415-CDC6) for testing complementation and into pMW333 (pRS405-cdc6KE) for integration into the LEU2 locus as described (12). The plasmids pWS945 (pGAL-CLB5) and yCpG2 (pGAL-CLN1) were obtained from B. Futcher (Cold Spring Harbor Laboratory, Cold Spring Harbor, NY). pJA92 (RAD53 URA3) was from S. Elledge (Baylor College of Medicine, Houston). pMW479 (pGAL-CDC4) was constructed by cloning a BamHI-SacI PCR fragment using genomic DNA as template into the pGAL expression plasmid pVF1. CDC4 was entirely sequenced to verify that it was wild type. Galactose-dependent induction of Cdc4p was determined by Western blot using rabbit polyclonal antibodies against Cdc4p (from M. Goebl, Indiana University School of Medicine, Bloomington, IN).

Immunoprecipitation of HA-CDC6 and Associated Proteins.

Baculovirus transfer vectors were constructed in pAcSG2 (PharMingen) to encode HA-HIS6-CDC6 wild type (pMW44) and the TTS (pMW475) and Δ8–17 (pMW476) derivative mutants. An NcoI site was introduced at the N terminus of CDC6 and the epitope tag was inserted into this site. Recombinant viruses were constructed by using the BaculoGold system as described (7). The viruses were separately infected into 2 × 107 Sf9 cells on 10-cm plates and harvested after 40 h at 27°C. The multiplicity of infection was adjusted so that the HA-HIS6-Cdc6 proteins were produced equally. Sf9 cells were lysed in 1 ml Sf9 lysis buffer (10 mM Tris[center dot]HCl (pH 7.5)/0.2% Nonidet P-40/1 mM EDTA/1 mM EGTA) containing 150 mM NaCl and a mixture of protease and phosphatase inhibitors. After centrifugation at 14,000 rpm, the soluble fraction was taken and the NaCl concentration was adjusted to 0.5 M. Monoclonal antibody 12CA5 coupled to protein A Sepharose beads (10 μl bed volume) was added to the lysate and mixed at 4°C for 2 h. Antibody beads were collected and washed four times in the same buffer containing 500 mM NaCl and then once in same buffer containing 150 mM NaCl. W303 was grown to an OD600 = 0.5, harvested, washed once with water, and resuspended in 2 ml of yeast Nonidet P-40 lysis buffer (20 mM Tris[center dot]HCl (pH 7.5)/150 mM NaCl/1 mM EGTA/0.5% Nonidet P-40) containing a mixture of protease and phosphatase inhibitors. Bead-beated yeast cell extracts were made as described (25) and equal volumes of yeast extract (500 μl) were added to each of the Sf9 immunoprecipitates. After a further 2-h incubation at 4°C, the beads were washed four times in the same buffer, resuspended in protein sample buffer, and separated on SDS/12.5% PAGE gels. These gels were silver-stained to visualize Cdc6p or blotted and probed with rabbit polyclonal antibodies directed against Cdc28p (1:2000 from B. Futcher) to detect associated proteins. Control beads from wild-type Sf9 cell lysates (i.e., not charged with HA-HIS6-Cdc6p) did not immunoprecipitate Cdc28p (data not shown).

Other Methods.

Tubulin staining (64), fluorescence-activated cell sorter (FACS) analysis and chromatin binding experiments to look at Orc6p phosphorylation were carried out as described (65). Baculoviruses expressing ORC (66) and Cdc28p-Clb5p (67) have been described. The Sic1p baculovirus was obtained from Mike Tyers (University of Toronto), and the Cln2p baculovirus from Ray Deschaies (California Institute of Technology, Pasadena). Baculovirus transfer vectors to express Clb1p and Clb6p were constructed by cloning the HindIII-NheI CLB1 and CLB6 restriction fragments into pAcPK31 (7) to give pMW10 and pMW11, respectively. Baculoviruses were constructed by using the BaculoGold system (PharMingen). For the kinase assays in Fig. Fig.66C, the immunoprecipitates (IPs) were washed in 50 mM Tris[center dot]HCl/10 mM MgCl2 and then resuspended in 10 μl 50 mM Tris[center dot]HCl/10 mM MgCl2/1 mM ATP containing 1 μg histone H1 and 10 μCi (1 Ci = 37 GBq) [γ-32P]ATP. The reactions were incubated for 10 min at 30°C and then separated on SDS/12.5% PAGE gels.

Figure 6
Cdc28p kinase coimmunoprecipitates with ORC. (A) Sf9 insect cells were infected with baculoviruses expressing ORC, Cdc28p, Clb5p, and Sic1p in various combinations. The same amount of ORC was immunoprecipitated in each case by using monoclonal anti-ORC ...


Cells Expressing cdc6KE Arrest in G2/M in a RAD53-Independent Manner.

Depletion of Cdc6p resulted in a failure to initiate DNA replication and after a period, a “reductional” mitosis occurred in which unreplicated chromosomes formed spindle attachments and randomly segregated to the two spindle poles (8). Subsequent cytokinesis resulted in cell death because cells accumulated with fractional (0.5C) DNA contents. The cdc6KE Walker A mutant also failed to initiate DNA replication because it did not load the MCMs onto chromatin; however, these cells did not undergo a reductional mitosis, but arrested with a 1C DNA content (12).

To determine whether the cdc6KE mutation caused cells to arrest in G1 or G2/M, we compared the morphology of cells expressing this mutant form of Cdc6p with cells lacking any Cdc6p. Cells expressing cdc6KE from its natural promoter and wild-type CDC6 under control of the methionine repressible MET3 promoter were grown to early exponential phase. The wild-type Cdc6p had a half-life of ≈5 min and disappeared rapidly after the addition of methionine to the medium (8). Cells expressing only cdc6KE accumulated as large budded cells with a 1C DNA content and with long spindles (Fig. (Fig.11 AC), indicating that cells accumulated in mitosis, probably late anaphase, and not in G1.

Figure 1
Cells expressing cdc6KE arrest after entry into mitosis. (A) FACS profile of YB504 (MET3-CDC6 cdc6KE) showing accumulation of cells with 1C DNA content after repression of wild-type MET3-CDC6. (B) Budding index of K4055 (MET3-CDC6 Δcdc6) ...

A trivial explanation for the mitotic arrest phenotype seen with the cdc6KE mutant could be that this allele allowed initiation of replication at a very small subset of origins. Such limited initiation events could activate the RAD53-dependent G1/S or S phase checkpoint response pathway that prevents mitosis when DNA replication is blocked (4749). We thought that RAD53 was not likely to be involved in the CDC6-dependent mitotic arrest because in the absence of DNA replication, sister chromatid cohesion is not possible. It is thought that RAD53 inhibits the metaphase to anaphase transition by inhibiting cleavage of Pds1p and Scc1p, thereby preventing sister chromatid separation (68, 69). However, to test whether this arrest was RAD53-dependent, the rad53-1 mutation was introduced into the cdc6KE strain and DNA content was measured by FACS following shut off of the wild-type MET3-CDC6. Two rad53-1 segregants from the cross were analyzed. One of the cdc6KE rad53-1 strains (YB791) still arrested with a 1C DNA content, but unexpectedly, a second cdc6KE rad53-1 strain (YB792) underwent reductional mitosis (data not shown). Both cdc6KE rad53-1 strains were transformed with a wild-type copy of RAD53 on an ARS-CEN plasmid. RAD53 reversed the hydroxyurea (HU) sensitivity of both strains as expected; however, it had no effect on the reductional mitosis of the YB792 strain. Therefore, the mitotic block in the first cdc6KE strain was RAD53-independent. The reductional mitosis seen in the second strain was also RAD53-independent and must have been caused by an alteration at another locus, consistent with previous findings that not all S. cerevisiae strains have an intact G1–M checkpoint pathway (51).

One of the functions of a checkpoint response is to maintain cell viability by delaying the cell cycle until the error in cell division process is corrected. We tested whether the cdc6KE-dependent arrest maintained cell viability by comparing the number of viable cells over time following shut off of wild type MET3-CDC6 in the cdc6KE mutant strain to the strain containing no additional CDC6. Both strains lost viability at a similar rate to 5–10% after 5 h (Fig. (Fig.11D). This observation indicated that this arrest was not a true checkpoint, because the entry into mitosis with unreplicated chromosomes was a lethal event. The arrest more likely reflects some function (besides MCM loading) that wild-type Cdc6p promotes during mitosis, and this function is also required for the completion of mitosis under these circumstances.

Inhibition of Mitosis Requires One of Two Sequences in Cdc6p.

A structure-function analysis was used to determine which of the amino acids within the N terminus of Cdc6KEp were responsible for the mitotic arrest in the absence of DNA replication. A series of nested deletions beginning at the N terminus was created and after introduction into cells, DNA content was determined by sampling every hour for 5 h following shut-off of the wild-type CDC6 gene. Deletion of the first eight amino acids had no effect on the mitotic arrest, however, all subsequent deletions were unable to maintain an arrest and accumulated with 0.5C DNA content (summarized in Fig. Fig.2).2). Further deletions within this N-terminal region defined aa 8–17 as critical for this function. Deletion of 8–17 residues removed the sequence RRNL that matched the Cy box (zRxL) defined in higher eukaryotes as a sequence that mediates binding to the cyclin subunit of CDKs (5760). However, a smaller deletion comprising this sequence (Δ13–17, RRNLF) had no effect, indicating that the upstream sequence is required. All of the CDC6 N-terminal mutants (containing wild-type K114), including the point mutants (below), were able to efficiently complement a deletion of CDC6 when using a plasmid-based assay and had no discernable growth defects. This was expected, because the N-terminal 50 aa of Cdc6p are nonessential.

Figure 2
Summary of CDC6 mutational analysis. The sequence of the N-terminal 50 aa is shown at the top. Cells expressing cdc6KE containing the indicated N-terminal mutation were grown to early exponential phase. Then wild-type MET3-CDC6 was repressed by the ...

Cdc6p contains three consensus Cdc28p kinase phosphorylation sites within the N terminus at positions 7, 23, and 43. All three serine and threonine residues were changed to alanine. This triple mutant (TTS) was unable to arrest in mitosis and accumulated with fractional DNA content (Fig. (Fig.2).2). However, no single phosphorylation site was essential for this activity, because the individual point mutants still maintained the 1C DNA arrest. (The first deletion of residues 2–7 removes the first Cdc28p phosphorylation site, T7.) From an analysis of all possible double site mutants, the first residue was the most critical because the T7A T23A double mutant accumulated with fractional DNA content, the T7A S43A mutant did so partially, and the T23A S43A mutant still arrested with a 1C DNA content. Furthermore, the double mutant T7A Δ13–17 deletion still arrested in mitosis, again indicating that aa 8–12 were also critical for the arrest. These data suggest that mutation of two separate regions of Cdc6p can abrogate the mitotic arrest: the Cdc28p consensus phosphorylation sites and a short 10-aa sequence from residues 8–17. The sequences may function together to recruit a factor that mediates the arrest.

Increasing Cdc28p/Clb Kinase Levels Can Overcome the Mitotic Arrest Caused by cdc6KE.

Because the mutational analysis suggested that a CDK interaction at the N terminus might be important for the mitotic arrest, we next examined the effect of overproducing various factors that affect Cdc28p activity (Fig. (Fig.33A). Cells containing MET3-CDC6, cdc6KE, and various plasmids capable of overproducing CLN1, CDC4, or CLB5 and a vector control were grown in raffinose medium lacking methionine. At an early exponential phase of growth, methionine and galactose were added to the medium to both repress the wild-type copy of CDC6 and to induce expression of the respective genes. Time points were taken every 2 h for 8 h. Neither the vector control nor expression of CLN1 or CDC4 could overcome the mitotic arrest. We also tried Gal expression of CLN2; however, this in itself was lethal to the cells and greatly broadened the 1C and 2C DNA peaks by FACS. In contrast, Gal-induced expression of CLB5 overcame the mitotic arrest, indicating that increasing Cdc28p-Clb5p kinase levels reversed the inhibitory effect of Cdc6KEp on mitosis.

Figure 3
Increasing Cdc28p-Clb kinase activity abrogates the mitotic block. (A) YB504 (MET3-CDC6 cdc6KE) was transformed with vector (yCP50) or GAL expression plasmids for CLN1, CDC4, or CLB5 and grown to early exponential phase in minimal raffinose (2%) ...

Because Sic1p is an inhibitor of Cdc28p-Clb kinase but not Cdc28p-Cln kinase (33, 44), we constructed a strain containing sic1Δ MET3-CDC6 cdc6KE(YB777). When the wild-type CDC6 was shut off in these cells lacking SIC1, they also underwent a reductional mitosis (Fig. (Fig.33B). Transformation of an ARS CEN plasmid containing wild type SIC1 into the sic1Δ strain (YB777) restored the ability to block entry into mitosis and also the normal growth properties of the strain (data not shown). This observation further indicates that increasing Cdc28p-Clb kinase activity can overcome the mitotic arrest induced by cdc6KE cells that have failed to initiate DNA replication.

Mitotic Inhibition by Cdc6KEp Is Correlated with Binding to Cdc28p.

It has been reported that Cdc6p interacts with Cdc28p and inhibits its kinase activity (55). Furthermore, it was reported that this Cdc28p interaction is mediated by the N-terminal ≈50 aa of Cdc6p (55). Because the mutational analysis and genetic data suggested that Cdc6p might inhibit mitosis through an interaction with Cdc28p-Clb kinase, we tested whether wild-type Cdc6p and the two mutants that failed to arrest in mitosis could coimmunoprecipitate Cdc28p. It was difficult to detect binding to Cdc28p after immunoprecipitation of HA3-Cdc6p from yeast cells, but another experimental approach was informative. HA epitope-tagged versions of wild-type Cdc6p or the two mutants were produced in Sf9 insect cells by using recombinant baculoviruses. The HA-Cdc6p was immunoprecipitated under stringent salt conditions and the immunoprecipitates washed extensively. This efficient purification yielded very few contaminating insect cell proteins. The immunoprecipitates were then mixed with wild-type yeast whole cell extracts and, after a further 2-h incubation, the presence of Cdc28p was examined by immunoblotting (Fig. (Fig.4). 4).

Figure 4
Cdc28p is coimmunoprecipitated with wild-type Cdc6p, but not the two mutants (TTS and Δ8–17) that go through a reductional mitosis. (Upper) Cdc6p following immunoprecipitation by silver staining. (Lower) Western blot for Cdc28p. Experimental ...

Similar amounts of wild-type Cdc6p and the two mutants were recovered in the immunoprecipitates (Fig. (Fig.44 Upper). Fig. Fig.4 4 Lower shows a Western blot for Cdc28p. Although the wild-type Cdc6p protein coimmunoprecipitated Cdc28p, as reported (55), both of the mutants that fail to arrest in mitosis (TTS and Δ8–17) produced proteins that were defective in coimmunoprecipitating Cdc28p (Fig. (Fig.44 Lower). Together with the genetic data presented above, these results suggest that a Cdc6p–Cdc28p interaction is important in restraining mitosis in the absence of DNA replication initiation. This could be through Cdc6p phosphorylation, binding of the Cdc28p–cyclin, inhibition of Cdc28p–cyclin activity, or all three.

Cells Expressing cdc6KE Activate S Phase Cdc28-Clbs on Schedule During Passage Through G1.

Cells in G1 that do not have active Cdc28p-Clb kinase, but have activated Cdc28-Cln kinase, have a multibudded phenotype. In contrast, cells that have not activated Cdc28p-Cln kinase arrest as unbudded cells. Because cells expressing only cdc6KE arrested with a dumb-bell morphology, it is likely that they had activated Cdc28p-Clb5p during passage through G1, even though replication initiation had not occurred. We sought an independent confirmation that Cdc28p-Clb5p was activated normally and sought a marker for Cdc28p-Clb5p activation during G1. Orc6p was a good candidate because it is phosphorylated as cells initiate DNA synthesis, and dephosphorylated as cells exit mitosis and enter G1 (65). Furthermore, Orc6p phosphorylation required the ORC6 Cdc28p consensus phosphorylation sites (65), but it was not known whether Cdc28p-Cln or -Clb kinases were responsible.

To determine whether CLB5 or CLB6 was responsible for the Orc6p phosphorylation as cells entered S phase, the timing of Orc6p phosphorylation in wild-type and Δclb5 clb6 cells was compared after a synchronous release from an alpha factor-mediated G1 arrest. Cdc28p-Cln kinase is known to be activated on schedule in the Δclb5 clb6 cells; however, there is an ≈30-min delay in the initiation of DNA replication because of a failure to activate Cdc28p-Clb5p and -Clb6p kinases (31, 32). Under these circumstances, initiation is thought to be dependent on the later Cdc28p-Clb3p and -Clb4p kinases. At the alpha factor arrest, Orc6p was in the dephosphorylated form in the two strains (Fig. (Fig.55A). Orc3p was shown as a loading control. Orc6p was phosphorylated at 30 min after release in the wild-type strain, but was significantly delayed to 60 min in the Δclb5 clb6 mutant. FACS analysis indicated that the Δclb5 clb6 strain also delayed entry into S phase relative to the wild type by 30 min (data not shown), as reported (32). These results suggest that Clb5p and Clb6p were required for the phosphorylation of Orc6p before S phase. Cdc6p bound to chromatin 20 min after release from the alpha factor arrest and was removed by 30 min in both the wild-type and Δclb5 clb6 strains, indicating that Cdc28p-Clb5p and -Clb6p kinases were not required for either Cdc6p binding or removal from the chromatin.

Figure 5
Orc6p phosphorylation requires CLB5 CLB6 and Orc6p phosphorylation occurs on schedule in the cdc6KE mutant during passage through G1. (A) Cells (W303 MATa and W303 MATa Δclb5 clb6) arrested in G1 by using alpha factor were released into the ...

Using Orc6p phosphorylation as a marker, we then tested whether Clb5p and Clb6p were activated on schedule in cells that were transiting G1-expressing cdc6KE as compared with cells expressing wild-type Cdc6p. Cells were synchronized in late mitosis by using the dbf2-1 mutation. While arrested, the wild-type MET3-CDC6 gene was repressed by the addition of methionine for 30 min and the cells were allowed to enter G1 at the permissive temperature for dbf2-1, expressing either wild-type CDC6 or cdc6KE from the endogenous CDC6 promoter. Orc6p was dephosphorylated within 10 min of release and was rephosphorylated beginning at 30 min in both strains (Fig. (Fig.55B), thus the Cdc28p-Clb5p and -Clb6p were activated in both strains at the same time. The wild-type cells passed through mitosis and entered G1 phase again during the 105–120-min interval as evidenced by the dephosphorylation of Orc6p (Fig. (Fig.55B). However, the cdc6KE cells arrested with a 1C DNA content by FACS (data not shown) and Orc6p remained phosphorylated. These results demonstrated that Cdc28p-Clb5p and -Clb6p kinases were activated in the cdc6KE mutant during passage through G1, consistent with the large-budded arrest phenotype of this strain. Furthermore, cells actually exited mitosis from the dbf2-1 arrest point after shutting off wild-type CDC6 and expressing only cdc6KE, suggesting that the Cdc6KEp mitotic block occurred earlier than the DBF2 execution point.

Sic1p Regulates Cdc28–Cyclin Interaction with ORC.

Because Orc1p, Orc2p, and Orc6p contain Cdc28p phosphorylation sites and are phosphorylated in vitro by purified Cdc28p-Clb5p kinase (data not shown and Fig. Fig.66C), we tested whether ORC could also physically interact with Cdc28p kinase. Baculovirus expressing ORC and either Cdc28p alone or Cdc28p together with Cln2p, Clb1p, Clb5p, or Clb6p were co-infected into Sf9 cells. Soluble Sf9 extracts were made as described (7) and ORC protein was immunoprecipitated by using a mixture of monoclonal antibodies against the ORC subunits. The IP was separated on SDS/PAGE gels and then tested for coimmunoprecipitation of Cdc28p by Western blotting. Cdc28p was coimmunoprecipitated with ORC no matter what cyclin subunit was coexpressed and even in the absence of any cyclin subunit (Fig. (Fig.66B, lanes 1, 3, and 5, and data not shown). Cdc28–cyclin was not immunoprecipitated in the absence of ORC protein (Fig. (Fig.66A, lane 6). We additionally verified that each cyclin subunit was being coimmunoprecipitated together with Cdc28p by making S35-labeled Cdc28p–cyclin Sf9 extracts as described (7). S35-labeled extracts were mixed with (nonlabeled) Sf9 extract expressing ORC, ORC was immunoprecipitated, and after separation on SDS/PAGE gels, Cdc28–cyclin coimmunoprecipitated only when ORC protein was also present in the extract (data not shown).

We then tested whether the CDK inhibitor Sic1p could either interact with ORC or prevent interaction of various Cdc28–cyclin pairs with ORC. Sic1p could not be coimmunoprecipitated with ORC (Fig. (Fig.66A, lanes 9 and 10). However, coexpression of Sic1p with ORC and Cdc28–cyclin prevented the interaction of Cdc28p-Clb5p with ORC (Fig. (Fig.66A, lanes 7 and 8, and B, lanes 1 and 2), but not the interaction of Cdc28p-Cln2p (Fig. (Fig.66B, lanes 3 and 4) or Cdc28 (Fig. (Fig.66B, lanes 5 and 6) with ORC. This observation is consistent with the observation that Sic1p interacts with and inhibits Cdc28p-Clb, but not Cdc28p-Cln kinases.

We tested whether the Cdc28p kinase in the ORC immunoprecipitates was active. ORC was immunoprecipitated from baculovirus-infected Sf9 cells expressing ORC alone, ORC plus Cdc28p, or ORC plus Cdc28p-Clb5p. After extensive washing, histone H1 kinase activity was measured. Fig. Fig.66C shows that although no H1 kinase activity was present in the ORC alone IP or when Cdc28p was also expressed, a very active H1 kinase is present in the ORC IP when Cdc28p-Clb5p were coexpressed. In addition, the Orc1p, Orc2p, and Orc6p subunits were phosphorylated by Cdc28-Clb5p in the IP. There was also weak phosphorylation of these ORC subunits in the ORC alone and ORC-Cdc28p IP (Fig. (Fig.66C, lanes 1 and 2), probably reflecting the association of an insect cell kinase. Only these three ORC subunits contain consensus Cdc28p phosphorylation sites. Orc1p has one site, Orc2p has six sites, and Orc6p has four sites. Finally, an ORC–Cdc28p interaction likely also occurs in yeast. Following immunoprecipitation of ORC from exponentially growing yeast, we detected a CDC28-dependent ORC and H1 kinase activity, because the ORC-associated kinase activity was seen in wild-type cells but not in cdc28-4 cells (data not shown).


We have described mutations within the N-terminal nonessential domain of Cdc6p that define regions required for the inhibition of mitosis in the absence of DNA replication initiation. One mutation deleted a motif that matches the Cy box consensus present in higher eukaryotic organisms shown to mediate binding to cdk2-cyclinA (5760). This Cdc6p deletion mutant also failed to coimmunoprecipitate Cdc28p, consistent with it acting as a Cdc28–cyclin interaction domain. We have noticed that the CDK inhibitor Sic1p also contained a match to the Cy motif near the C terminus at positions 260 to 263 (KRRL). A C-terminal deletion analysis of SIC1 found that the 26 C-terminal aa were required for growth arrest caused by overproduction of a nondegradable form of Sic1p (M.W. and B.S., unpublished data). One essential sequence within these 26 aa was the Cy motif and similar findings to ours have been published (70). This data supports the hypothesis that the Cy motif is also present in budding yeast and mediates interaction with the B-type Cdc28p complexes, the inhibitory target of Sic1p. Our data, shown in Fig. Fig.6,6, also demonstrate that Sic1p has an additional function to block Clb-CDKs from interacting with ORC. Interestingly, the Cdc28p-Cln2p kinase could still bind ORC in the presence of Sic1p. We suggest that Sic1p not only ensures a temporal pattern of CDK activation, but also regulates access of specific CDKs to their key substrates.

The second mutation that abrogated the mitotic block was a triple alanine substitution of the three N-terminal Cdc28p phosphorylation sites in Cdc6p. The corresponding protein was also defective in coimmunoprecipitating Cdc28p. Because we were able to overcome the mitotic arrest phenotype by increasing the amount of Cdc28p-Clb activity, either by overproducing Clb5p or deleting the Cdc28p-Clb inhibitor SIC1, together this data suggests that, like Sic1p, Cdc6p plays a role in passage through mitosis by interaction with Cdc28-Clb kinases.

The CDC6 homologues share a conserved core region shown by the recently solved crystal structure of an archaeal Cdc6 orthologue to encode a two-domain, ATP-binding module of the AAA+ family, and a C-terminal winged-helix that may interact with DNA or other proteins (71). An alignment of human, Xenopus, S. pombe, and S. cerevisiae CDC6 homologues indicates very little sequence conservation in their N-terminal regions, and in fact the N termini have very different lengths. So it was surprising to find that the alignment showed sequence conservation just covering the ten amino acids from positions 8–17 in the budding yeast protein. Furthermore, all of the Cdc6 proteins had CDK consensus phosphorylation sites in their N termini. Perhaps the mitotic function of this N-terminal domain is conserved in the various Cdc6 proteins.

Cdc6p may be one component of the previously described G1–M phase checkpoint that blocks mitosis in the absence of replication initiation; however, the CDC6-dependent arrest could be a separate phenomenon. The mitotic arrest seen in the cdc6KE mutant was RAD53-independent and our data indicated that another locus in addition to CDC6 was also involved.

An apparent discrepancy with our finding of a mitotic inhibitory role for the Cdc6p N terminus is the report that depletion of Cdc45p also resulted in a reductional mitosis in the absence of initiation of DNA replication (28). There are several explanations for this finding. One is that not all S. cerevisiae strains retain the ability to block mitosis in the absence of initiation and this pathway may be defective in the particular strain used. Alternatively, the nonfunctional K114E mutation in Cdc6p might be required to reveal the mitotic arrest, because this mutant is unable to load the Mcm proteins during late mitosis. The absence of the preRC may be required for the mitotic block.

Recent studies in Xenopus have suggested that binding of cyclinE-cdk2 to preRCs is necessary for the initiation of DNA replication (72). Also, many tumor cells overexpress cyclin E, and it is known that this circumstance can lead to genetic instability and inappropriate regulation of S phase (73). It is therefore likely that inappropriate temporal regulation of CDKs will disrupt the events that lead to accurate inheritance of the genome. In this paper we have uncovered additional mechanisms to ensure that cyclin-dependent kinases are precisely coordinated with the events necessary to lead to initiation of DNA replication. As cells exit mitosis and proceed through G1 phase, Clb-cyclin kinases are kept inactive by the combination of an active APC and the presence of CDK inhibitor Sic1p. We suggest that the Cdc6p on chromatin during the G1 phase of the cell cycle (12) may also act to inhibit Clb-cyclin kinase activity as cells exit mitosis, and therefore provide an opportunity for preRCs to be formed. Paradoxically, Clb-like CDKs are required in late G1 phase to activate S phase and initiation of DNA replication at each origin. Cdc6 is located at each origin because it binds directly to ORC (14). Thus, Cdc6 could potentially create a local environment in which CDKs would be prevented from prematurely activating preRCs. We have also demonstrated that Cln-CDKs can bind to ORC in the presence of Sic1p, but that Clb-CDKs cannot. Cln-CDKs trigger the destruction of Cdc6p and Sic1p, thereby removing Cdc6p from origins. In the absence of Sic1p, the Clb-CDKs then act on preRCs to initiate DNA replication. Thus, Sic1p acts as a molecular chaperone to orchestrate temporal-specific CDK function at replication origins. The presence of Cdc6 at origins during G1 phase also ensures that cells do not enter into mitosis without having replicated DNA, but it is clear that additional mechanisms must be operating to ensure the dependence of mitosis on DNA replication.


We thank J. Duffy for preparation of figures, J. Diffley for the Cdc6 antibody, and P. Wendel and M. Russo for technical help. This work was supported by a grant from the National Institutes of Health (GM45436 to B.S.). M.W. was a Special Fellow of the Leukemia Society.


origin recognition complex
pre-replicative complex
minichromosome maintenance
fluorescence-activated cell sorter
cyclin-dependent kinase
anaphase-promoting complex

Note Added in Proof.

Note Added in Proof.

Similar conclusions have recently been published (74). “Cdc6 cooperates with Sic1 and Hct1 to inactivate mitotic cyclin-dependent kinases.”


This contribution is part of the special series of Inaugural Articles by members of the National Academy of Sciences elected on May 2, 2000.


1. Diffley J F X. Genes Dev. 1996;10:2819–2830. [PubMed]
2. Stillman B. Science. 1996;274:1659–1663. [PubMed]
3. Dutta A, Bell S P. Annu Rev Cell Dev Biol. 1997;13:293–332. [PubMed]
4. Lei M, Tye B K. J Cell Sci. 2001;114:1447–1454. [PubMed]
5. Kelly T J, Martin G S, Forsburg S L, Stephen R J, Russo A, Nurse P. Cell. 1993;74:371–382. [PubMed]
6. Lygerou Z, Nurse P. Science. 2000;290:2271–2273. [PubMed]
7. Liang C, Weinreich M, Stillman B. Cell. 1995;81:667–676. [PubMed]
8. Piatti S, Lengauer C, Nasmyth K. EMBO J. 1995;14:3788–3799. [PMC free article] [PubMed]
9. Coleman T R, Carpenter P B, Dunphy W G. Cell. 1996;87:53–63. [PubMed]
10. Donovan S, Harwood J, Drury L S, Diffley J F X. Proc Natl Acad Sci USA. 1997;94:5611–5616. [PMC free article] [PubMed]
11. Perkins G, Diffley J F X. Mol Cell. 1998;2:23–32. [PubMed]
12. Weinreich M, Liang C, Stillman B. Proc Natl Acad Sci USA. 1999;96:441–446. [PMC free article] [PubMed]
13. Neuwald A F, Aravind L, Spouge J L, Koonin E V. Genome Res. 1999;9:27–43. [PubMed]
14. Mizushima T, Takahashi N, Stillman B. Genes Dev. 2000;14:1631–1641. [PMC free article] [PubMed]
15. Seki T, Diffley J F. Proc Natl Acad Sci USA. 2000;97:14115–14120. [PMC free article] [PubMed]
16. Aparicio O M, Weinstein D M, Bell S P. Cell. 1997;91:59–69. [PubMed]
17. Hardy C F, Dryga O, Seematter S, Pahl P M, Sclafani R A. Proc Natl Acad Sci USA. 1997;94:3151–3155. [PMC free article] [PubMed]
18. Lei M, Kawasaki Y, Young M R, Kihara M, Sugino A, Tye B K. Genes Dev. 1997;11:3365–3374. [PMC free article] [PubMed]
19. Owens J C, Detweiler C S, Li J J. Proc Natl Acad Sci USA. 1997;94:12521–12526. [PMC free article] [PubMed]
20. Bousset K, Diffley J F X. Genes Dev. 1998;12:480–490. [PMC free article] [PubMed]
21. Donaldson A D, Fangman W L, Brewer B J. Genes Dev. 1998;12:491–501. [PMC free article] [PubMed]
22. Mimura S, Takisawa H. EMBO J. 1998;17:5699–5707. [PMC free article] [PubMed]
23. Zou L, Stillman B. Science. 1998;280:593–596. [PubMed]
24. Aparicio O M, Stout A M, Bell S P. Proc Natl Acad Sci USA. 1999;96:9130–9135. [PMC free article] [PubMed]
25. Weinreich M, Stillman B. EMBO J. 1999;18:5334–5346. [PMC free article] [PubMed]
26. Jares P, Blow J J. Genes Dev. 2000;14:1528–1540. [PMC free article] [PubMed]
27. Nougarede R, Della Seta F, Zarzov P, Schwob E. Mol Cell Biol. 2000;20:3795–3806. [PMC free article] [PubMed]
28. Tercero J A, Labib K, Diffley J F. EMBO J. 2000;19:2082–2093. [PMC free article] [PubMed]
29. Zou L, Stillman B. Mol Cell Biol. 2000;20:3086–3096. [PMC free article] [PubMed]
30. Futcher B. Yeast. 1996;12:1635–1646. [PubMed]
31. Kuhne C, Linder P. EMBO J. 1993;12:3437–3447. [PMC free article] [PubMed]
32. Schwob E, Nasmyth K. Genes Dev. 1993;7:1160–1175. [PubMed]
33. Schwob E, Bohm T, Mendenhall M D, Nasmyth K. Cell. 1994;79:233–244. [PubMed]
34. Verma R, Annan R S, Huddleston M J, Carr S A, Reynard G, Deshaies R J. Science. 1997;278:455–460. [PubMed]
35. Drury L S, Perkins G, Diffley J F. Curr Biol. 2000;10:231–240. [PubMed]
36. Donaldson A D, Raghuraman M K, Friedman K L, Cross F R, Brewer B J, Fangman W L. Mol Cell. 1998;2:173–182. [PubMed]
37. Correa-Bordes J, Nurse P. Cell. 1995;83:1001–1009. [PubMed]
38. Dahmann C, Diffley J F X, Nasmyth K A. Curr Biol. 1995;5:1257–1269. [PubMed]
39. Piatti S, Bohm T, Cocker J H, Diffley J F X, Nasmyth K. Genes Dev. 1996;10:1516–1531. [PubMed]
40. Labib K, Diffley J F, Kearsey S E. Nat Cell Biol. 1999;1:415–422. [PubMed]
41. Nguyen V Q, Co C, Irie K, Li J J. Curr Biol. 2000;10:195–205. [PubMed]
42. Noton E, Diffley J F. Mol Cell. 2000;5:85–95. [PubMed]
43. Shirayama M, Toth A, Galova M, Nasmyth K. Nature (London) 1999;402:203–207. [PubMed]
44. Mendenhall M D, al-Jumaily W, Nugroho T T. Prog Cell Cycle Res. 1995;1:173–185. [PubMed]
45. Wuarin J, Nurse P. Cell. 1996;85:785–787. [PubMed]
46. Tanaka T, Nasmyth K. EMBO J. 1998;17:5182–5191. [PMC free article] [PubMed]
47. Elledge S J. Science. 1996;274:1664–1672. [PubMed]
48. Longhese M P, Foiani M, Muzi-Falconi M, Lucchini G, Plevani P. EMBO J. 1998;17:5525–5528. [PMC free article] [PubMed]
49. Weinert T. Cell. 1998;94:555–558. [PubMed]
50. Rhind N, Russell P. J Cell Sci. 2000;113:3889–3896. [PMC free article] [PubMed]
51. Toyn J H, Johnson A L, Johnston L H. Mol Cell Biol. 1995;15:5312–5321. [PMC free article] [PubMed]
52. Nishitani H, Nurse P. Cell. 1995;83:397–405. [PubMed]
53. Jallepalli P V, Kelly T J. Genes Dev. 1996;10:541–552. [PubMed]
54. Jallepalli P V, Brown G W, Muzi-Falconi M, Tien D, Kelly T J. Genes Dev. 1997;11:2767–2779. [PMC free article] [PubMed]
55. Elsasser S, Lou F, Wang B, Campbell J L, Jong A. Mol Biol Cell. 1996;7:1723–1735. [PMC free article] [PubMed]
56. Brown G W, Jallepalli P V, Huneycutt B J, Kelly T J. Proc Natl Acad Sci USA. 1997;94:6142–6147. [PMC free article] [PubMed]
57. Zhu L, Harlow E, Dynlacht B D. Genes Dev. 1995;9:1740–1752. [PubMed]
58. Adams P D, Sellers W R, Sharma S K, Wu A D, Nalin C M, Kaelin W G. Mol Cell Biol. 1996;16:6623–6633. [PMC free article] [PubMed]
59. Chen J, Saha P, Kornbluth S, Dynlacht B D, Dutta A. Mol Cell Biol. 1996;16:4673–4682. [PMC free article] [PubMed]
60. Russo A A, Jeffrey P D, Patten A K, Massague J, Pavletich N P. Nature (London) 1996;382:325–331. [PubMed]
61. Rose M, Winston F, Hieter P. Methods in Yeast Genetics: A Laboratory Course Manual. Plainview, NY: Cold Spring Harbor Lab. Press; 1990.
62. Guthrie C, Fink G R. Methods Enzymol. 1991. 194.
63. Thomas B J, Rothstein R. Cell. 1989;56:619–630. [PubMed]
64. Lee L, Klee S K, Evangelista M, Boone C, Pellman D. J Cell Biol. 1999;144:947–961. [PMC free article] [PubMed]
65. Liang C, Stillman B. Genes Dev. 1997;11:3375–3386. [PMC free article] [PubMed]
66. Bell S P, Mitchell J, Leber J, Kobayashi R, Stillman B. Cell. 1995;83:563–568. [PubMed]
67. Duncker B P, Pasero P, Braguglia D, Heun P, Weinreich M, Gasser S M. Mol Cell Biol. 1999;19:1226–1241. [PMC free article] [PubMed]
68. Sanchez Y, Bachant J, Wang H, Hu F, Liu D, Tetzlaff M, Elledge S J. Science. 1999;286:1166–1171. [PubMed]
69. Uhlmann F, Wernic D, Poupart M A, Koonin E V, Nasmyth K. Cell. 2000;103:375–386. [PubMed]
70. Hodge A, Mendenhall M. Mol Gen Genet. 1999;262:55–64. [PubMed]
71. Liu J, Smith C L, DeRyckere D, DeAngelis K, Martin G S, Berger J M. Mol Cell. 2000;6:637–648. [PubMed]
72. Furstenthal L, Kaiser B K, Swanson C, Jackson P K. J Cell Biol. 2001;152:1267–1278. [PMC free article] [PubMed]
73. Spruck C H, Won K A, Reed S I. Nature (London) 1999;401:297–300. [PubMed]
74. Calzada A, Sacristan M, Sanchez E, Bueno A. Nature (London) 2001;412:355–358. [PubMed]

Articles from Proceedings of the National Academy of Sciences of the United States of America are provided here courtesy of National Academy of Sciences
PubReader format: click here to try


Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...


Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...