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Hara et al. 1
Degradation of p27Kip1 at the G0-G1 transition mediated
by a Skp2-independent ubiquitination pathway
Taichi Hara,1,2 Takumi Kamura,1,2 Keiko Nakayama,2,3 Kiyotaka Oshikawa,2,3
Shigetsugu Hatakeyama,1,2 and Kei-Ichi Nakayama1,2,3,4
1Department of Molecular and Cellular Biology and 3Department of Molecular
Genetics, Medical Institute of Bioregulation, Kyushu University, 3-1-1
Maidashi, Higashi-ku, Fukuoka, Fukuoka 812-8582, Japan.
2CREST, Japan Science and Technology Corporation, 4-1-8 Honcho, Kawaguchi,
Saitama 332-0012, Japan.
4To whom correspondence should be addressed: Dr. Kei-Ichi Nakayama,
Department of Molecular and Cellular Biology, Medical Institute of
Bioregulation, Kyushu University, 3-1-1 Maidashi, Higashi-ku, Fukuoka,
Fukuoka 812-8582, Japan.
Tel.: +81-92-642-6815. Fax: +81-92-642-6819.
E-mail: [email protected]
Running title: Skp2-independent degradation of p27Kip1
Copyright 2001 by The American Society for Biochemistry and Molecular Biology, Inc.
JBC Papers in Press. Published on October 26, 2001 as Manuscript M107274200 by guest on July 4, 2020
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ABSTRACT
Targeting of the cyclin-dependent kinase inhibitor p27Kip1 for proteolysis has been
thought to be mediated by Skp2, the F-box protein component of an SCF
ubiquitin ligase complex. Degradation of p27Kip1 at the G0-G1 transition of the cell
cycle has now been shown to proceed normally in Skp2–/– lymphocytes, whereas
p27Kip1 proteolysis during S-G2 phases is impaired in these Skp2-deficient cells.
Degradation of p27Kip1 at the G0-G1 transition was blocked by lactacystin, a
specific proteasome inhibitor, suggesting that it is mediated by the ubiquitin-
proteasome pathway. The first cell cycle of stimulated Skp2–/– lymphocytes
appeared normal, but the second cycle was markedly inhibited, presumably as a
result of p27Kip1 accumulation during S-G2 phases of the first cell cycle.
Polyubiquitination of p27Kip1 in the nucleus is dependent on Skp2 and
phosphorylation of p27Kip1 on threonine-187. However, polyubiquitination activity
was also detected in the cytoplasm of Skp2–/– cells, even with a threonine-187 →
alanine mutant of p27Kip1 as substrate. These results suggest that a
polyubiquitination activity in the cytoplasm contributes to the early phase of
p27Kip1 degradation in a Skp2-independent manner, thereby promoting cell cycle
progression from G0 to G1.
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INTRODUCTION
Progression of the cell cycle in eukaryotic cells depends on the activity of a series
of protein complexes composed of cyclins and cyclin-dependent kinases (CDKs).1
The activity of cyclin-CDK complexes is regulated by various mechanisms,
including association of the kinase subunit with the regulatory cyclin subunit,
phosphorylation-dephosphorylation of the kinase subunit, and association of the
complex with a group of CDK inhibitors (CKIs) (1,2). The interaction of CKIs with
cyclin-CDK complexes is triggered by a variety of antimitogenic signals and
results in inhibition of the catalytic activity of the complexes and consequent
restraint of cell cycle progression (3,4).
A key question with regard to regulation of the cell cycle concerns the
mechanism by which cells undergo the transition from the resting state (G0) to
proliferation. The CKI p27Kip1 plays a pivotal role in the control of cell proliferation.
Transition from G0 phase to S phase of the cell cycle is promoted by complexes of
G1 cyclins with CDKs, and p27Kip1 inhibits the activity of these complexes directly
by binding to them (5). In normal cells, the amount of p27Kip1 is high during G0
phase, but it rapidly decreases on reentry into G1-S phases triggered by specific
mitogenic factors (6,7). Forced expression of p27Kip1 results in cell cycle arrest in
G1 phase (8,9); conversely, inhibition of p27Kip1 expression by antisense
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oligonucleotides increases the number of cells in S phase (10). Moreover, we and
others have demonstrated that mice homozygous for deletion of the p27Kip1 gene
are larger than normal mice, and that they exhibit multiple organ hyperplasia as
well as a predisposition to both spontaneous and radiation- or chemical-induced
tumors (11-14).
The ubiquitin-proteasome pathway plays an important role in the
degradation of short-lived regulatory proteins, including those that participate in
the cell cycle, cellular signaling in response to stress and to extracellular signals,
morphogenesis, the secretory pathway, DNA repair, and organelle biogenesis (15).
The concentration of p27Kip1 is thought to be regulated predominantly by this
proteolytic pathway (16-18). The ubiquitin-mediated proteolysis of many proteins
is regulated by phosphorylation of the target, which increases its susceptibility to
degradation (19-22). The proteolysis of p27Kip1 may also be regulated by such a
mechanism, given that degradation of the protein is promoted by its
phosphorylation on Thr187 by the cyclin E–CDK2 complex (23-25). Recent data
have also suggested that Skp2, an F-box protein that is thought to function as the
receptor component of an SCF ubiquitin ligase complex, binds to p27Kip1 in
conjunction with Cks1 only when Thr187 of p27Kip1 is phosphorylated; such binding
then results in the ubiquitination and degradation of p27Kip1 (26-30). These
biochemical observations are supported by genetic evidence that p27Kip1
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accumulates to high levels in the cells of mice that lack either Skp2 or Cks1 (29-
31).
We now show that, although the degradation of p27Kip1 during S and G2
phases of the cell cycle is markedly impaired in Skp2–/– cells, the degradation of
this protein at the G0-G1 transition occurs normally in these cells. Our data
suggest the existence of a second pathway of p27Kip1 degradation that is also
mediated by the ubiquitin-proteasome system. This second pathway may be
critical for regulation of cell cycle progression from the resting state to proliferation,
and may be important in mechanisms of carcinogenesis.
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EXPERIMENTAL PROCEDURES
Immunoblot analysis
Single-cell suspensions of lymphocytes were prepared from the lymph nodes of
4-month-old Skp2+/+ or Skp2–/– mice and were cultured (1.0 × 107 cells in 5 ml) for
the indicated times in RPMI 1640 medium supplemented with 10% fetal bovine
serum, 10 nM phorbol 12,13-dibutyrate (PDBu) (Sigma), and 300 nM ionomycin
(Sigma). In some experiments, 10 µM lactacystin (Kyowa Medics), 10 µM
MG132 (Peptide Institute), or vehicle (dimethyl sulfoxide) was added to the
culture medium. The cells were subsequently harvested and lysed in 50 µl of
RIPA buffer containing 0.4 mM Na3VO4, 0.4 mM EDTA, 10 mM NaF, 10 mM
sodium pyrophosphate, and antipain, pepstatin, chymostatin, leupeptin, and
phenylmethylsulfonyl fluoride each at a concentration of 10 µg/ml. The lysates
were incubated on ice for 15 min and then centrifuged at 20,000 × g. After
determination of its protein concentration with the Bradford assay (Bio-Rad), the
resulting supernatant (30 µg of protein) was subjected to SDS–polyacrylamide
gel electrophoresis (PAGE). The separated proteins were transferred to a
Hybond P membrane (Amersham Pharmacia Biotech) and subjected to
immunoblot analysis with antibodies (1 µg/ml) to p27Kip1 (Transduction
Laboratories), to cyclin D2 (Santa Cruz Biotechnology), to cyclin E (Santa Cruz
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Biotechnology), to Skp2 (Zymed), or to glycogen synthase kinase–3β (GSK-3β)
(Transduction Laboratories). Immune complexes were detected with appropriate
horseradish peroxidase–conjugated secondary antibodies and either
SuperSignal West Pico or SuperSignal West Dura chemiluminescence reagents
(Pierce).
Cell cycle analysis by flow cytometry
Single-cell suspensions of lymphocytes were cultured as described above. Cells
were exposed to 10 µM bromodeoxyuridine (BrdU) (Sigma) for 30 min before
harvesting, and were then subjected to fixation overnight in 70% ethanol at
–20°C followed by denaturation for 30 min at room temperature in 2 M HCl
containing 0.5% Triton X-100. After neutralization with borax buffer (pH 8.5), the
cells were subjected to dual-color staining with fluorescein isothiocyanate
(FITC)–conjugated antibodies to BrdU (Becton Dickinson) and propidium iodide
(5 µg/ml). The cells were then analyzed with a FACSCalibur flow cytometer and
Cell Quest software (Becton Dickinson).
RT-PCR analysis of immediate-early gene expression
Total RNA (1 µg) extracted from lymph node cells (2.0 × 107) with the use of
ISOGEN (Wako) was subjected to reverse transcription (RT) with ReverTra
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Dash (Toyobo) in a final volume of 20 µl. The resulting cDNA (1 µl) was amplified
by the polymerase chain reaction (PCR) in a final volume of 50 µl of PCR
reaction mix. The respective sequences of sense and antisense primers specific
for the target genes were as follows: c-Myc, 5'-AGT GCA TTG ATC CCT CAG
TGG TCT TTC CCT A-3' and 5'-CAG CTC GTT CCT CCT CTG ACG TTC CAA
GAC GTT-3'; c-Fos, 5'-GAG CTG ACA GAT ACA CTC CAA GCG-3' and 5'-CAG
TCT GCT GCA TAG AAG GAA CCG-3'; and c-Jun, 5'-GCA TGA GGA ACC
GCA TTG CCG CCT CCA AGT-3' and 5'-CGC AAA GTC TGC CGG CCA ATA
GGC CGC T-3'. The sense and antisense primers targeted to the gene for
glyceraldehyde-3-phosphate dehydrogenase (G3PDH), used as an internal
standard, were 5'-ACC ACA GTC CAT GCC ATC AC-3' and 5'-TCC ACC ACC
CTG TTG CTG TA-3', respectively. PCR products were separated by
electrophoresis on a 1.5% agarose gel and visualized by ethidium bromide
staining.
Production of recombinant proteins in bacteria
Glutathione S-transferase (GST) fusion proteins of mouse p27Kip1 and the T187A
mutant of p27Kip1 [each of which was tagged at its COOH-terminus with the
hexahistidine (His6) epitope] as well as a GST fusion protein of mouse Cks1
were expressed in Escherichia coli strain XL1-blue (Stratagene); the bacteria
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were cultured in the presence of 0.1 mM isopropyl-β-D-thiogalactopyranoside.
Bacterial cells were resuspended in phosphate-buffered saline (PBS) and lysed
by sonication, and cellular debris was removed by centrifugation for 20 min at
13,000 × g. Glutathione–Sepharose CL-4B beads (Amersham Pharmacia
Biotech) were added to the resulting supernatant, and the mixture was rotated
for 4 h at 4°C. The beads were washed with PBS, and the GST fusion proteins
attached to the beads were subjected to digestion for 4 h at 4°C with PreScission
protease (Amersham Pharmacia Biotech) in a solution containing 50 mM Tris-
HCl (pH 8.0), 150 mM NaCl, 1 mM EDTA, and 1 mM dithiothreitol (DTT). Only
the processed recombinant proteins (not the GST moiety nor the GST fusion
proteins) were released from the beads, as revealed by SDS-PAGE and
Coomassie blue staining (data not shown).
Human Ubc5a tagged at its NH2- and COOH-termini with the His6 and
Flag epitopes, respectively, human Ubc3 tagged at its NH2-terminus with the His6
epitope, Saccharomyces cerevisiae Uba1 tagged at its NH2- and COOH-termini
with the Myc and His6 epitopes, respectively, and a GST fusion protein of mouse
ubiquitin were expressed in E. coli strain BL21(DE3)pLysS (Novagen); the
bacteria were cultured in the presence of 0.1 mM isopropyl-β-D-
thiogalactopyranoside. The recombinant proteins were purified with the use of
ProBond resin (Invitrogen) or glutathione–Sepharose CL-4B. After dialysis
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against a solution containing 40 mM Hepes-NaOH (pH 7.6), 60 mM NaCl, 1 mM
DTT, and 10% glycerol, the proteins were stored at –80°C.
Baculovirus expression system
Baculoviruses were generated in Sf9 cells with the use of BacPAK6 virus DNA
and the pBacPAK9-GST vector (Clontech) containing either the cDNA for a GST
fusion protein of human cyclin E tagged at its NH2-terminus with the Myc epitope
or the cDNA for human CDK2 tagged at its NH2-terminus with the hemagglutinin
epitope. The GST-cyclin E–CDK2 recombinant protein complex was purified
(according to the protocol described above for purification of GST fusion proteins
expressed in bacteria) from a lysate of Sf9 cells coinfected with the two viruses.
Only the purified recombinant proteins were detected by electrophoresis and
Coomassie blue staining.
In vitro ubiquitination assay
Primary mouse embryonic fibroblasts (MEFs) were derived from 13.5-day-
postcoitum Skp2+/+ or Skp2–/– embryos and cultured as previously described (11).
In all experiments of this study, we used nonsenescent MEFs (no more than
passage 2). In some experiments, the cell cycle of MEFs was synchronized
either at G0-G1 by serum deprivation for 96 h in medium supplemented with 0.1%
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fetal bovine serum, or at S-G2 by arrest at the G1-S boundary induced by
incubation with aphidicolin (1 µg/ml) for 14 h followed by culture for 3 h in
aphidicolin-free medium. The cells (1.0 × 108) were washed with PBS and then
suspended in 500 µl of buffer A [40 mM Hepes-NaOH (pH 7.6), 1 mM DTT, and
protease inhibitor mixture (antipain, pepstatin, chymostatin, leupeptin, and
phenylmethylsulfonyl fluoride each at 10 µg/ml)] containing 60 mM NaCl. For
preparation of nuclear and cytoplasmic extracts, the cell suspension was frozen
and thawed, and then subjected to centrifugation at 2000 x g for 5 min at 4°C.
The resulting nuclear pellet was resuspended in 300 µl of ice-cold buffer
A containing 300 mM NaCl, rotated for 30 min at 4°C, and centrifuged at 100,000
x g for 4 h at 4°C. The new supernatant was dialyzed against buffer A containing
60 mM NaCl, centrifuged for 10 min at 20,000 x g to remove debris, and then
mixed with 800 µl of DE52 resin (Whatman) that had been equilibrated with
buffer A containing 60 mM NaCl. After incubation for 30 min at room temperature,
the slurry was transferred to a 2-cm-diameter column and washed with buffer A.
Proteins were eluted from the column in a stepwise manner with buffer A
containing 150 and 300 mM KCl, and 160-µl fractions were collected.
The cytoplasmic supernatant resulting from the centrifugation of the MEF
lysate at 2000 × g was subjected to further centrifugation at 100,000 × g for 4 h
at 4°C. The new supernatant was mixed with 800 µl of DE52 that had been
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equilibrated with buffer A containing 60 mM NaCl, and then subjected to column
chromatography as described above.
For preparation of whole-cell extracts, MEFs were suspended in buffer A
containing 300 mM KCl, frozen and thawed, rotated for 30 min at 4°C, and then
centrifuged at 100,000 × g for 4 h at 4°C. The resulting supernatant was dialyzed
against buffer A containing 60 mM NaCl, centrifuged for 10 min at 20,000 x g to
remove debris, and then mixed with 800 µl of DE52 that had been equilibrated
with buffer A containing 60 mM NaCl. Column chromatography was then
performed as described above.
DE52 column fractions (3 µl) were mixed with 50 ng of Uba1, 100 ng of
Ubc5a or Ubc3, 3 µg of GST-ubiquitin, and 50 ng of wild-type p27Kip1 or the
T187A mutant in a 10-µl reaction mixture containing 40 mM Hepes-NaOH (pH
7.6), 60 mM NaCl, 2 mM DTT, 5 mM MgCl2, 0.5 mM EDTA, 10% glycerol, and
1.5 mM ATP. In some experiments, 100 ng of GST-cyclin E–CDK2 complex or
100 ng of Cks1 were added to the reaction mixture. After incubation for 30 min at
26°C, the reaction mixtures were subjected to SDS-PAGE and immunoblot
analysis with a monoclonal antibody to p27Kip1.
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RESULTS
Normal degradation of p27Kip1 at the G0-G1 transition in Skp2–/– cells
Analysis of Skp2–/– mice revealed that phenotypic characteristics such as cellular
accumulation of p27Kip1 were less evident in lymphocytes than in liver, kidney,
and lung (31) (data not shown). With the use of immunoblot analysis, we
examined the mitogen-induced down-regulation of p27Kip1 in mature lymphocytes,
almost all of which reside in the G0 phase of the cell cycle in the absence of
stimulation (6). Mitogenic stimulation with the combination of PDBu and
ionomycin resulted in the almost complete disappearance of p27Kip1 from wild-
type lymphocytes within 12 h (Fig. 1A). Unexpectedly, Skp2–/– lymphocytes
exhibited similar kinetics of p27Kip1 down-regulation, suggesting that the
decrease in the abundance of p27Kip1 in the early phase (up to 12 h) of mitogenic
stimulation occurs independently of Skp2-mediated proteolysis. However, the
abundance of p27Kip1 increased again to substantial levels by 36 to 48 h in the
Skp2–/– cells, whereas the amount of this protein remained low in wild-type
lymphocytes (Fig. 1B).
The abundance of cyclin D, cyclin E, and Skp2 was also examined in
wild-type lymphocytes in the early (Fig. 1C) and late (Fig. 1D) phases of
mitogenic stimulation. Consistent with previous results (32), cyclin D1 was not
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detected in the lymphocytes (data not shown). Cyclin D2 was detected as early
as 3 h after stimulation, whereas the amount of cyclin E (which is expressed in
late G1 phase and degraded in S phase) increased 18 to 24 h after stimulation.
The expression of Skp2 was first evident 18 to 24 h after stimulation and was
maximal at 30 to 36 h.
The cell cycle profile did not differ substantially between Skp2+/+ and
Skp2–/– cells for up to 48 h after stimulation (Fig. 1E). In both instances, cells
began to enter S phase 18 to 24 h after stimulation and to enter G2 phase at 36 h.
Given that neither Skp2 nor cyclin E was expressed in the early phase (G0-G1) of
p27Kip1 degradation, and that the down-regulation of p27Kip1 occurred in Skp2–/–
cells, this process appears to require neither Skp2 nor cyclin E–mediated
phosphorylation of p27Kip1. In contrast, Skp2 is indispensable for the late phase
(S-G2) of p27Kip1 degradation.
Prevention of p27Kip1 degradation at G0-G1 by a proteasome inhibitor
We next examined whether the early phase of p27Kip1 degradation induced by
mitogenic stimulation is dependent on the ubiquitin-proteasome pathway. We
incubated wild-type lymphocytes in the presence of lactacystin, a specific
inhibitor of the proteasome, during mitogenic stimulation. The down-regulation of
p27Kip1 was markedly inhibited by lactacystin (Fig. 2A). Short-term inhibition of
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the proteasome by incubation of cells with the quick-acting compound MG132
for the last 2 h before cell harvest yielded similar results. MG132 thus markedly
inhibited the further degradation of p27Kip1 after its addition to the culture (Fig.
2B). To exclude the possibility that proteasome inhibition affects transduction of
the mitogenic signal, we also examined the expression of the immediate-early
genes c-Myc, c-Jun, and c-Fos by RT-PCR analysis (Fig. 3). The levels and
kinetics of expression of these genes were not substantially affected by
treatment of the wild-type cells with lactacystin, indicating that mitogenic
signaling was intact in lymphocytes exposed to this agent. These data suggest
that the early phase of degradation of p27Kip1 at the G0-G1 transition is mediated
by the ubiquitin-proteasome pathway.
Impairment of the second cell cycle in Skp2–/– cells
We previously demonstrated that the growth of Skp2–/– lymphocytes was slightly
reduced 4 days and substantially reduced 6 days after mitogenic stimulation
compared with the growth of wild-type lymphocytes (31). We thus examined the
cell cycle progression of Skp2–/– lymphocytes in greater detail (Fig. 4). Although
the cell cycle profile of Skp2–/– lymphocytes was similar to that of wild-type cells
for up to 2 days after stimulation, the proportion of cells in S phase after 3 days
was markedly lower for Skp2–/– lymphocytes (15%) than for the wild-type cells
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(40%). These results suggest that, although the G1-S transition of the first cell
cycle occurs normally in Skp2–/– cells (as a result of the degradation of p27Kip1
during the G0-G1 transition), the subsequent accumulation of p27Kip1 during S-G2
phases of the first cycle (caused by the absence of Skp2) results in G1 arrest
during the second cell cycle. The putative machinery responsible for p27Kip1
degradation at the G0-G1 transition of the first cell cycle thus does not appear to
function at the G1-S transition of subsequent cycles (see Fig. 8).
Skp2-dependent and -independent polyubiquitination of p27Kip1
We fractionated total extracts of Skp2+/+ and Skp2–/– MEFs by DE52 ion-
exchange column chromatography with stepwise elution with KCl. We then
examined the in vitro ubiquitination of p27Kip1 in the presence of the ubiquitin-
activating enzyme (E1) Uba1, the ubiquitin-conjugating enzyme (E2) Ubc5a, a
GST fusion protein of ubiquitin, and each column fraction (Fig. 5A). The Skp2+/+
cell extract yielded a pronounced peak of polyubiquitination activity
encompassing fractions 6 and 7, whereas the corresponding activity peak
derived from Skp2–/– cells spanned fractions 6 to 9. To determine whether
ubiquitination of p27Kip1 was dependent on phosphorylation of Thr187 at the
COOH-terminus of the protein, we subjected a p27Kip1 mutant in which Thr187 was
replaced by Ala (T187A) to the in vitro ubiquitination assay (Fig. 5B). A large
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peak of polyubiquitination activity was detected mostly in fractions 5 to 8 and a
smaller peak of activity was apparent in fractions 14 and 15 derived from both
Skp2+/+ and Skp2–/– cells. These data suggest that a mediator of p27Kip1
polyubiquitination is present in the Skp2–/– cells, and that the polyubiquitination
activity conferred by this factor is independent of phosphorylation of p27Kip1 on
Thr187.
We previously showed that Skp2 is predominantly localized to the
nucleus (33,34). We thus also subjected nuclear extracts prepared from Skp2+/+
and Skp2–/– MEFs to ion-exchange chromatography. Skp2 was detected mostly
in fractions 5 and 6 of the column eluate (Fig. 6A). Fraction 5 of the nuclear
extracts of Skp2+/+ and Skp2–/– cells was then included in the in vitro
ubiquitination assay with wild-type p27Kip1, E1, the E2s Ubc3 or Ubc5a, and
GST-ubiquitin (Fig. 6B). With the fraction from Skp2+/+ cells, polyubiquitination of
p27Kip1 was evident in the additional presence of cyclin E and CDK2 and was
further enhanced by Cks1. In contrast, polyubiquitinated species of p27Kip1 were
not detected with fraction 5 from Skp2–/– cells.
To confirm that the polyubiquitination of p27Kip1 mediated by Skp2 is
dependent on phosphorylation of p27Kip1 on Thr187, we subjected the T187A
mutant of p27Kip1 to the in vitro ubiquitination reaction in the presence of fraction
5 of the nuclear extracts of Skp2+/+ and Skp2–/– cells (Fig. 6C). In contrast to
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wild-type p27Kip1 (which underwent polyubiquitination in the presence of fraction
5 from wild-type cells), theT187A mutant did not undergo polyubiquitination in
the presence of fraction 5 from either Skp2+/+ or Skp2–/– cells. These data
suggest that polyubiquitination activity in the nucleus requires Skp2, and that
phosphorylation of p27Kip1 on Thr187 by the cyclin E–CDK2 complex is necessary
for Skp2-mediated polyubiquitination.
Given that p27Kip1 is translocated from the nucleus to the cytoplasm by
Jab1-mediated nuclear export (35), we next examined whether molecular
machinery for polyubiquitination of p27Kip1 is present in the cytoplasm.
Cytoplasmic extracts were prepared from Skp2+/+ and Skp2–/– cells and were
fractionated by ion-exchange chromatography. The resulting fractions 5 were
then included in the in vitro ubiquitination assay with wild-type p27Kip1 or the
T187A mutant as the substrate. Similar extents of polyubiquitination were
apparent with the fractions derived from Skp2+/+ and Skp2–/– cells as well as with
wild-type p27Kip1 and the T187A mutant (Fig. 6D). Thus, this cytoplasmic
polyubiquitination activity is independent both of Skp2 and of phosphorylation of
p27Kip1 on Thr187. The putative ubiquitin ligase responsible for this Skp2-
independent polyubiquitination appears to be located predominantly in the
cytoplasm, given that the corresponding fraction derived from nuclear extracts
did not contain such an activity. Together, our results suggest the existence of
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two pathways of p27Kip1 ubiquitination: a Skp2- and Thr187
phosphorylation–dependent pathway in the nucleus, and a Skp2- and Thr187
phosphorylation–independent pathway in the cytoplasm.
Finally, we examined the cell cycle dependence of the polyubiquitination
activities in the nucleus and cytoplasm. Nuclear and cytoplasmic extracts were
prepared from Skp2+/+ and Skp2–/– MEFs synchronized at G0 phase (Fig. 7A) or
at S-G2 phases (Fig. 7B), and were subjected to the in vitro ubiquitination assay.
The polyubiquitination activity in the nuclear extract of Skp2+/+ cells was greater
at S-G2 than at G0. In contrast, the activity in the cytoplasmic extracts of both
Skp2+/+ and Skp2–/– cells at G0 was similar to that at S-G2. Thus, the Skp2- and
Thr187 phosphorylation–dependent pathway of p27Kip1 polyubiquitination in the
nucleus is active when cells enter successive rounds of the cell cycle. In contrast,
the cytoplasmic polyubiquitination pathway is active at both G0 and S-G2 phases.
Given that signal-dependent nuclear export of p27Kip1 occurs at the G0-G1
transition,2 exported p27Kip1 may be polyubiquitinated by the constantly active
ubiquitination machinery in the cytoplasm.
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DISCUSSION
The amount of p27Kip1 is relatively high in quiescent (G0) cells, decreases on
entry of cells into the cell cycle, and is controlled predominantly by the rate of
p27Kip1 degradation (16,17). This CKI undergoes ubiquitination and is degraded
in a proteasome-dependent manner (5). Phosphorylation of p27Kip1 on Thr187 is
mediated by the cyclin E–CDK2 complex and has been shown to be required for
ubiquitination of p27Kip1 (23-25). Previous studies indicate that Skp2 specifically
interacts with the extreme COOH-terminus of p27Kip1 only when Thr187 is
phosphorylated by cyclin E–CDK2 (26-28). This association of Skp2 with p27Kip1
results in recruitment of the latter to the SCF core complex, thereby promoting its
ubiquitination and degradation. This ubiquitination process was recently shown
to be markedly enhanced by Cks1 associated with Skp2 (29,30).
In parallel with Skp2-mediated ubiquitination, p27Kip1 is exported from the
nucleus and degraded. This export step appears to be dependent on Jab1, a
component of the 450-kDa COP9 (signalosome) complex (35). Our unpublished
data indicate, however, that the Jab1-mediated export of p27Kip1 from the nucleus
at the G0-G1 transition occurs in a Skp2-independent manner.2 Furthermore,
given that Skp2 is localized predominantly to the nucleus, the ubiquitination of
p27Kip1 at this stage of the cell cycle is likely mediated by a ubiquitin ligase (other
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than SCFSkp2) that is located in the cytoplasm. We therefore propose that p27Kip1
is degraded by at least two distinct mechanisms, one of which is dependent on
Skp2 and one of which is not (Fig. 8). The Skp2-independent mechanism
operates in the cytoplasm and degrades p27Kip1 at the G0-G1 transition. Jab1-
mediated nuclear export of p27Kip1 may transfer this protein to the degradation
machinery in the cytoplasm. The Skp2-dependent mechanism, mediated by the
SCFSkp2 ubiquitin ligase, serves to degrade p27Kip1 that is phosphorylated on
Thr187 in the nucleus during S-G2 phases in successive rounds of the cell cycle.
In addition to Thr187, phosphorylation of other residues of p27Kip1 may be
important in the control of its stability. We recently showed that phosphorylation
of Ser10 accounted for ~70% of the total phosphorylation of p27Kip1, and that the
extent of phosphorylation at this site was ~75-fold greater than that at Thr187 (36).
The extent of Ser10 phosphorylation is markedly increased in cells in G0 phase of
the cell cycle compared with that apparent in cells in S or M phase. The stability
of p27Kip1 phosphorylated on Ser10 is also substantially greater than that of the
unphosphorylated form of the protein. These observations suggest that Ser10 is
the major site of phosphorylation of p27Kip1, and that phosphorylation at this site
(like that at Thr187) contributes to the regulation of p27Kip1 stability (36). The
increased stability of the Ser10-phosphorylated form of p27Kip1 suggests that
dephosphorylation of this residue might play an important role in progression of
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the cell cycle from G0 to G1. It is possible that phosphorylation of Ser10 may be a
determinant of the nuclear export of p27Kip1 or of the ubiquitination of this protein
in the cytoplasm.
The most obvious cellular phenotype of Skp2–/– mice is the presence of
markedly enlarged, polyploid nuclei and multiple centrosomes (31). However,
there is substantial tissue variability in the penetrance of this phenotype. It is
most prominent in liver, kidney, lung, and testis, whereas hematopoietic cells and
neurons appear normal. Although the reason for such tissue differences has
been unclear, they might result from variability in dependence on the two distinct
mechanisms of p27Kip1 degradation. Purification of the activity responsible for the
ubiquitination of p27Kip1 in the cytoplasm and molecular identification of the
corresponding putative ubiquitin ligase should provide insight into these issues.
Mutations in the p27Kip1 gene appear to be rare in human cancers.
However, a reduced abundance of p27Kip1 in a subset of colon and breast
cancers correlates well with poor prognosis (37-40). Furthermore, the loss of
p27Kip1 alleles in mice increases the sensitivity of these animals to cancer-
inducing agents (14). Identification of components of the protein degradation
machinery that determine the turnover rate of p27Kip1 may thus provide insight
into the altered expression of this protein in tumor cells as well as into whether
such altered expression is a cause or a consequence of cell transformation.
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Indeed, Skp2 is overexpressed in many human cancer cell lines (41), suggesting
that p27Kip1 degradation mediated by Skp2 may be related to carcinogenesis. It is
thus possible that the putative ubiquitin ligase responsible for the Skp2-
independent pathway of p27Kip1 degradation is also deregulated in cancer cells.
During revision of this manuscript, Malek et al. (42) demonstrated the
existence of two pathways of p27Kip1 degradation, one dependent on Thr187
phosphorylation and one not, with the use of a mouse "knock-in" model.
Although our present results are mostly consistent with those of Malek et al.,
these latter researchers suggested that the degradation of p27Kip1 at the G0-G1
transition is dependent on Skp2. This discrepancy might be attributable to a
difference in the number of passages of the MEFs studied. We have thus
observed that the Skp2-independent ubiquitination activity apparent at the G0-G1
transition is prominent in lymphocytes and in MEFs subjected to a small number
of passages, whereas senescent MEFs are prone to loss of this activity with
successive passages.2
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ACKNOWLEDGMENTS
We thank M. Matsumoto and N. Ishida for helpful discussion; R. Yasukochi, K.
Shimoharada, S. Matsushita, N. Nishimura, and other laboratory members for
technical assistance; and M. Kimura for help in preparing the manuscript. This
work was supported in part by a grant from the Ministry of Education, Science,
Sports, and Culture of Japan, by Nissan Science Foundation, and by a research
grant from the Human Frontier Science Program.
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FOOTNOTES
1Abbreviations: CDK, cyclin-dependent kinase; CKI, CDK inhibitor; PDBu,
phorbol 12,13-dibutyrate; PAGE, polyacrylamide gel electrophoresis; GSK-3β,
glycogen synthase kinase–3β; BrdU, bromodeoxyuridine; FITC, fluorescein
isothiocyanate; RT-PCR, reverse transcription–polymerase chain reaction;
G3PDH, glyceraldehyde-3-phosphate dehydrogenase; GST, glutathione S-
transferase; PBS, phosphate-buffered saline; DTT, dithiothreitol; MEF, mouse
embryonic fibroblast.
2Ishida, N., and Nakayama, K. I., in preparation.
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FIGURE LEGENDS
Fig. 1. Skp2-independent degradation of p27Kip1. (A and B) Lymphocytes derived
from Skp2+/+ and Skp2–/– mice were stimulated with the combination of 10 nM
PDBu and 300 nM ionomycin for 0 to 12 h (A) or 0 to 48 h (B). The intracellular
abundance of p27Kip1 was examined by immunoblot analysis of cell extracts with
a monoclonal antibody to p27Kip1. The same blots were also probed with
antibodies to GSK-3β as a control. (C and D) Skp2+/+ lymphocytes were
stimulated with 10 nM PDBu and 300 nM ionomycin for 0 to 12 h (C) or 0 to 48 h
(D), after which the abundance of p27Kip1, cyclins D2 and E, Skp2, and GSK-3β
(control) was examined by immunoblot analysis. (E) Skp2+/+ and Skp2–/–
lymphocytes were stimulated with PDBu and ionomycin for the indicated times,
labeled with 10 µM BrdU for 30 min before harvesting, stained with antibodies to
BrdU and propidium iodide, and analyzed by flow cytometry. The percentages of
cells in G0-G1, S, and G2-M phases of the cell cycle are shown.
Fig. 2. Effects of proteasome inhibitors on degradation of p27Kip1 at Go-G1 in
wild-type lymphocytes. (A) Cells were stimulated with 10 nM PDBu and 300 nM
ionomycin in the absence (–) or presence (+) of 10 µM lactacystin for the
indicated times, after which cell extracts were subjected to immunoblot analysis
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with antibodies to p27Kip1 or to GSK-3β (control). (B) Cells stimulated with 10 nM
PDBu and 300 nM ionomycin were treated with 10 µM MG132 (lower panels) or
vehicle (upper panels) for the last 2 h of the indicated times, after which cell
extracts were subjected to immunoblot analysis as in (A).
Fig. 3. Effect of lactacystin on the expression of immediate-early genes induced
by mitogenic stimulation in wild-type lymphocytes. Cells were stimulated with 10
nM PDBu and 300 nM ionomycin in the absence or presence of 10 µM
lactacystin for the indicated times, after which total RNA was isolated and
subjected to RT-PCR analysis with primers specific for c-Myc, c-Fos, or c-Jun as
well as with G3PDH-specific primers as a control. The PCR products were
separated by agarose gel electrophoresis and stained with ethidium bromide.
Fig. 4. Extended cell cycle profiles of lymphocytes derived from Skp2+/+ and
Skp2–/– mice. Cells stimulated with PDBu and ionomycin for the indicated times
were labeled with BrdU for 30 min before harvesting, stained with antibodies to
BrdU (and FITC-conjugated secondary antibodies) and propidium iodide, and
analyzed by flow cytometry. The percentages of cells in G0-G1, S, and G2-M
phase are shown below each panel.
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Fig. 5. In vitro ubiquitination of p27Kip1 in the presence of fractions derived from
total extracts of Skp2+/+ and Skp2–/– MEFs. Extracts were fractionated by
stepwise elution with KCl from a DE52 column, and portions of the resulting
fractions were assayed for the ability to mediate the ubiquitination of either wild-
type p27Kip1 (A) or the T187 mutant of this protein (B) in the presence of Uba1,
Ubc5a, and GST-ubiquitin. Reaction products were detected by immunoblot
analysis with antibodies to p27Kip1. The positions of the unmodified,
monoubiquitinated [(GST-Ub)1], and polyubiquitinated [(GST-Ub)n] p27 proteins
are indicated.
Fig. 6. Skp2-dependent and -independent ubiquitination of p27Kip1. (A) Nuclear
extracts prepared from Skp2+/+ and Skp2–/– MEFs were fractionated by stepwise
elution with KCl from a DE52 column. Portions of the resulting fractions were
subjected to immunoblot analysis with antibodies to Skp2. (B) Portions of
fraction 5 from the DE52 column eluate of the nuclear extracts were assayed for
their ability to mediate p27Kip1 ubiquitination in the absence or presence of cyclin
E–CDK2 or of Cks1. Reaction mixtures also included Uba1, Ubc3 (left panel) or
Ubc5a (right panel), and GST-ubiquitin. Reaction products were detected by
immunoblot analysis with antibodies to p27Kip1. (C) In vitro ubiquitination assays
were performed with wild-type p27Kip1 or the T187A mutant in the absence or
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presence of DE52 column fraction 5 from nuclear extract of Skp2+/+ or Skp2–/–
MEFs, Cks1, cyclin E–CDK2, and the combination (Reaction) of Uba1, Ubc5a,
and GST-ubiquitin, as indicated. (D) Cytoplasmic extracts from Skp2+/+ and
Skp2–/– MEFs were fractionated by stepwise elution with KCl from a DE52
column, and portions of the resulting fractions 5 were subjected to the in vitro
ubiquitination assay as in (C) in the absence of Cks1 and cyclin E–CDK2.
Fig. 7. Constant activity of the Skp2-independent p27Kip1 polyubiquitination
pathway in the cytoplasm. Nuclear and cytoplasmic extracts were prepared from
Skp2+/+ and Skp2–/– MEFs synchronized either at G0 phase (A) or at S-G2 phases
(B). The extracts were fractionated by stepwise elution with KCl from a DE52
column, and the resulting fractions were subjected to in vitro ubiquitination
assays with wild-type p27Kip1 or the T187A mutant in the presence of Cks1, cyclin
E–CDK2, and the combination (Reaction) of Uba1, Ubc5a, and GST-ubiquitin,
as indicated. Reaction products were detected by immunoblot analysis with
antibodies to p27Kip1.
Fig. 8. Model for cell cycle regulation through p27Kip1 degradation by two distinct
mechanisms. The degradation of p27Kip1 in the nucleus during successive
phases (G1-S-G2-M) of the cell cycle appears to be regulated by the SCFSkp2
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ubiquitin ligase, which targets p27Kip1 phosphorylated on Thr187 (T187-P). In
contrast, p27Kip1 appears to be ubiquitinated in the cytoplasm at the G0-G1
transition by an as-yet-unidentified ubiquitin ligase that functions independently
both of Skp2 and of phosphorylation of p27Kip1 on Thr187.
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B Time (h)
0 12 18 24 36 48
p27
Time (h)
0 3 6 9 12
A
30
Time (h)
0 12 18 24 36 48
Time (h)
0 3 6 9 12 30
GSK-3βGSK-3β
p27
C0 3 6 9 12
Time (h) Time (h)
Cyclin E
Cyclin D2
Skp2
p27
GSK-3β
D
0 12 18 24 30 4836
Cyclin E
Cyclin D2
Skp2
p27
GSK-3β
E Skp2+/+
Skp2-/-
Time (h)
G2-MS
1009080706050403020100
1009080706050403020100
0 12 24 36 48 0 12 24 36 48
G0-G1
Skp2+/+
Skp2+/+
Skp2-/-
Skp2+/+
Skp2-/-
Skp2-/-
Skp2+/+
Skp2-/-
Per
cen
tag
e o
f ce
lls in
eac
h p
has
e
Hara et al., Figure 1
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0 3 6 9 12
Time (h)
Lactacystin
(+)p27
( )
Time (h)
0 3 6 9 12Lactacystin
GSK-3β( )
(+)
Hara et al., Figure 2
0 3 5 7 9
Time (h)
p27
MG132 (+)
0 3 5 7 9
Time (h)
GSK-3β
MG132 (+)
A
B
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c-Fos
c-Jun
c-Myc
G3PDH
0 5 15 30 60 120 180 0 5 15 30 60 120 180
(+) Lactacystin( ) Lactacystin
Time (min):
Hara et al., Figure 3
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Skp2+/+
Skp2-/-
Time of stimulation (days)
Brd
U in
corp
ora
tio
n (
FIT
C)
DNA Content (Propidium Iodide)
0 1 2 3
0.1% 15.2%41.4%11.7%98.8%
1.1%
87.6%
0.4%
50.8%
6.8%
78.8%
4.9%
0.2%G0/G1
10.4% 45.4% 40.5%SG2/M
G0/G1S
G2/M
G0/G1S
G2/M
G0/G1S
G2/M
G0/G1S
G2/M
G0/G1S
G2/M
G0/G1S
G2/M
G0/G1S
G2/M
99.3%
0.5%
88.5%
0.8%
47.6%
6.1%
55.8%
3.4%
Hara et al., Figure 4
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p27-(GST-Ub)1
p27-(GST-Ub)1
p27-(GST-Ub)n
p27-(GST-Ub)n
p27 (T187A)
p27 (T187A)
p27-(GST-Ub)1
p27-(GST-Ub)1
p27-(GST-Ub)n
p27-(GST-Ub)n
p27
p27
B
Skp2+/+
Skp2-/-
Skp2+/+
Skp2-/-
0.15 M0.3 M
KCl
A
Fraction:
0.15 M
0.3 M
KCl
Fraction:4 5 6 7 8 9 10 11121314151617
43 5 6 7 8 9 1011121314151617
Hara et al., Figure 5
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4 5 6 7 8 9 10 11 12 13kDa62kDa51
kDa38
kDa62kDa51
kDa38
0.15 M0.3 M
Skp2
Skp2
A
B
Fraction:
KCl
--
--
Cks1:Cyclin E-CDK2: Cyclin E-CDK2:+
- ++
-- +
- ++
- + + + + + +Cks1: -
--- +
- ++
-- +
- ++
- + + + + + +
Ubc3 Ubc5a
p27 Fr:p27
Fraction 5: Fraction 5:
Skp2+/+
Skp2-/-
Skp2 +/+ Skp2
-/- Skp2 +/+ Skp2
-/-
p27-(GST-Ub)np27-(GST-Ub)n
Hara et al., Figure 6A, B
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C
Reaction: - --
Cks1:
Cyclin E-CDK2:
+ +
+
+++-
- +- ++
+ ++
++
- -- + +
+
+++-
- +- ++
+ ++
++Fraction 5:
p27
p27-(GST-Ub)1
Wild-type p27 Mutant p27 (T187A)
Mutant p27 (T187A)
Skp2 +/+Skp2 -/-Skp2 +/+ Skp2 -/-
Fraction 5:
Reaction: - -- + + - ---
+ ++ + + +- + + + +
Wild-type p27
Skp2 +/+Skp2 -/-Skp2 +/+ Skp2 -/-
p27-(GST-Ub)1
p27-(GST-Ub)n
p27-(GST-Ub)n
p27
D
Hara et al., Figure 6C, D
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Mutant p27 (T187A)Wild-type p27
Skp2 +/+Skp2 -/-Skp2 +/+ Skp2 -/-
Reaction: - -+ + - -+ +
Mutant p27 (T187A)Wild-type p27
Skp2 +/+Skp2 -/-Skp2 +/+ Skp2 -/-
- -+ + - -+ +
Mutant p27 (T187A)Wild-type p27
Skp2 +/+Skp2 -/-Skp2 +/+ Skp2 -/-
Reaction: - -+ + - -+ +
Mutant p27 (T187A)Wild-type p27
Skp2 +/+Skp2 -/-Skp2 +/+ Skp2 -/-
- -+ + - -+ +
Nucleus Cytoplasm
Nucleus Cytoplasm
p27-(GST-Ub)1
p27-(GST-Ub)n
p27
p27-(GST-Ub)1
p27-(GST-Ub)n
p27
A
B
Hara et al., Figure 7
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G1
S
G2
M G0
p27 P
p27
Skp2-independentT187-P-independentCytoplasm
Skp2-dependentT187-P-dependentNucleus
Hara et al., Figure 8
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Hatakeyama and Kei-Ichi NakayamaTaichi Hara, Takumi Kamura, Keiko Nakayama, Kiyotaka Oshikawa, Shigetsugu
ubiquitination pathwayDegradation of p27Kip1 at the G0-G1 transition mediated by a Skp2-independent
published online October 26, 2001J. Biol. Chem.
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