a novel role for gqα in α-thrombin-mediated mitogenic signalling pathways
TRANSCRIPT
A novel role for Gqa in a-thrombin-mediated mitogenic
signalling pathways
Alice Gardnera, Polly J. Phillips-Masonb, Daniel M. Rabenc, Joseph J. Baldassarea,*aDepartment of Pharmacological and Physiological Sciences, St. Louis University Medical School,
1402 South Grand Boulevard, St. Louis, MO 63104, USAbDepartment of Molecular Biology and Microbiology, Case Western Reserve University, Cleveland, OH 44106, USA
cDepartment of Physiology, The Johns Hopkins University School of Medicine, Baltimore, MD 21205, USA
Received 31 August 2001; accepted 13 November 2001
Abstract
a-Thrombin activates several G-proteins including members of the Gq, Gi, and G12/13 families, although the physiological importance of
these proteins is still not completely understood. We specifically investigated the role of Gqa in modulating a-thrombin-induced
mitogenesis. In Gqa1 cells, a stable cell line expressing reduced amounts of Gqa, concentrations of a-thrombin (1 NIH unit/ml), which
induce cell cycle reentry and progression into S phase in wild-type IIC9 cells, do not stimulate phosphatidylinositol (PI) hydrolysis, the rapid
early phase of ERK activity, and transit through G1 into S phase as quantified by cyclin-dependent kinase (CDK)4–cyclin D activity and
[3H]thymidine incorporation. Interestingly, high concentrations of a-thrombin restore these activities and cell cycle progression into S phase.
While, it is well documented that a-thrombin-induced sustained ERK activity mediates important responses for transit through G1 into S
phase, the importance of the rapid, Gq-dependent phase as a prerequisite for a-thrombin-mediated mitogenesis has not been appreciated.
D 2002 Elsevier Science Inc. All rights reserved.
Keywords: PAR, Protease-activated receptor; ERK, Extracellular-regulated kinase; CDK, Cyclin-dependent kinase; GPCRs, G-protein-coupled receptors
1. Introduction
It is well established that a-thrombin is a potent mitogen
in various cell types such as fibroblasts [1], vascular smooth
muscle cells [2], and astrocytes cells [3]. a-Thrombin
induces cell growth in these cells by the activation of
protein-coupled protease-activated receptors (PARs) [4].
Four PARs, PAR1, PAR2, PAR3, and PAR4, have been
cloned and found to be expressed in a variety of tissues [4].
In the case of PAR1, PAR3, and PAR4, these are activated
when a-thrombin clips the amino-terminus domain of the
receptor to unmask a new amino-terminus, which functions
as a tethered ligand. The prototypical thrombin receptor
known as PAR1 has been cloned from human platelets and
hamster fibroblasts [5,6]. Recently, the PAR1 receptor has
been shown to mediate a-thrombin’s ability to induce
mitogenesis [7], as CCL39 fibroblasts from tr � /� knockout
mice, which are missing this receptor, did not reenter the
cell cycle in response to thrombin.
Depending on the cell type, a-thrombin selectively
couples to distinct G-proteins to potentiate growth-factor-
stimulated mitogenesis [8]. For example, in 1321N astrocy-
toma cells, the pertussis toxin-insensitive G12 protein medi-
ates thrombin-induced mitogenesis via a Shc/Ras-dependent
pathway [9]. Conversely, microinjection of Gia2 antibodies
to quiescent Balb3 fibroblasts inhibited thrombin-induced
mitogenesis, indicating that the pertussis toxin-sensitive Gi
family mediated this process in these cells. Furthermore,
dual coupling of the thrombin receptor to pertussis toxin-
insensitive Gq and pertussis toxin-sensitive Gi/o has been
shown to regulate cell growth in the mouse lung fibroblast
CCL39 cell line [10].
a-Thrombin is known to induce the PLC-mediated
hydrolysis of cellular phosphatidylinositol (PI) hydrolysis,
leading to the production of 1,4,5-triphosphate (IP3) and
diacylglycerol (DA) [11,12]. The PAR1 receptor stimulates
PI hydrolysis in a number of cell types [13–15]. For
0898-6568/01/$ – see front matter D 2002 Elsevier Science Inc. All rights reserved.
PII: S0898 -6568 (01 )00279 -0
* Corresponding author. Tel.: +1-324-577-8543; fax: +1-324-577-
8233.
E-mail address: [email protected] (J.J. Baldassare).
www.elsevier.com/locate/cellsig
Cellular Signalling 14 (2002) 499–507
example, in IIC9 cells, a-thrombin-induced PI hydrolysis is
mediated through PAR1 [14]. Evidence indicates that ago-
nist-induced hydrolysis of cellular PI via PI–PLC has an
important role in signal transduction pathways that mediate
mitogenesis [12,16]. In a rat hepatoma cell stably transfected
with antisense PLC constructs, profound effects on cell
growth are observed, namely, a two- to threefold increase
in doubling time and suppressed DNA synthesis [16].
The signalling properties of the thrombin receptor(s) are
mediated in part by coupling to a variety of G-proteins. The
pertussis toxin-insensitive G12 and G13 interact with the
activated thrombin receptor in astrocytoma cells [17]. In
contrast, the thrombin receptor couples to the Gq/11 and the
Gi/o family of G-proteins in neuroblastoma SH-EP cells and
fibroblasts [8,18]. Studies of prototypical G-proteins dem-
onstrate that activation of the thrombin-activated PAR1
receptor and subsequent PI hydrolysis is via coupling to a
specific G-protein, namely Gq [19]. In COS-7 cells, a
chimeric receptor carrying the thrombin receptor’s second
cytoplasmic loop-activated PI hydrolysis in response to a
nonthrombin agonist by coupling directly to Gq [19].
The mitogen-activated protein kinases (MAPKs) are
activated by a variety of growth factors in the process of
mitogenesis [20–22]. MAPKs are activated by sequential
phosphorylation of a three-kinase module. This cascade
comprises a MAPK (e.g. ERK1/2), a MAPK kinase (e.g.
MEK1), and a MAPK kinase kinase, such as Raf-1 [23].
During mitogenesis, the extracellular-regulated kinase
(ERK) pathway is activated by receptor tyrosine kinases
and G-protein-coupled receptors (GPCRs) [24]. a-Throm-
bin-induced activation of ERK is known to be essential for
its mitogenic action [25]. However, the specific role of the
G-proteins coupling a-thrombin to the ERK cascade have
presently not been delineated.
Balancing the growth-stimulatory and -inhibitory signals
that a cell receives regulates the transition between prolifera-
tion and quiescence. Cell cycle G1 progression and entry into
S phase are controlled by a series of sequential regulatory
events mediated by the cyclin/cyclin D-dependent kinase
complexes [26–29]. The cyclin-dependent kinases (CDKs)
CDK4 and CDK6 are activated by the D-type cyclins [26,30].
Early events in the cell cycle show that expression levels of
D-type cyclins are stimulated by growth factors and their
signal transduction cascades [30,31]. Specifically, the ERK
pathway has been shown to regulate expression of cyclin D
[32]. In addition to cyclin binding, CDK activity is regulated
by the binding of CDK inhibitors and posttranslational
modifications [33,34]. Cyclin D–CDK4 plays a crucial role
in reversing the inhibitory action of the retinoblastoma (Rb)
family of proteins by phosphorylation [35,36]. During early
to mid-G1 phase, the phosphorylation of Rb by CDK4–
cyclin D releases histone deacetylation inhibition [37,38] and
induces cyclin E expression [60,61].
In this paper, we show that reduction of the amounts of
Gqa in IIC9 cells stably transfected with antisense cDNA
for Gqa results in the inability of a-thrombin to stimulate
cell growth. Furthermore, the Gqa mutant (Gqa1) exhibits
altered inositol phosphate levels, CDK activity, and altered
activation of the rapid phase of ERK. The data in this work
is the first to show that the a-thrombin-stimulated acute
phase of ERK activation, mediated by Gqa, appears to be
important for mitogenesis.
2. Materials and methods
2.1. Cells and cell culture
IIC9 cells, a subculture of Chinese hamster embryo
fibroblasts, were grown and maintained in Dulbeco’s modi-
fied Eagle’s medium (DMEM) (Life Technologies, Grand
Island, NY) containing 10% (v/v) foetal calf serum and
2 mM L-glutamine (Sigma, St. Louis, MO) and 100 U
penicillin/ml 100 mg streptomycin/ml. All chemicals were
purchased from Sigma, unless specified otherwise. Subcon-
fluent cultures were growth-arrested by washing twice with
serum-free DMEM (Life Technologies) and incubated for
two days in serum free DMEM containing 1 mg/ml bovine
serum albumin plus 20 mM HEPES, pH 7.4 (basal media).
Growth-arrested cells were washed twice and equilibrated in
basal media for 30 min prior to addition of agonist.
a-Thrombin was added to growth-arrested cells at 1 U/ml
in all experiments.
2.2. Generation of Gqa-deficient cells
Gqa antisense transfectants were generated and main-
tained as described previously [39]. Briefly, 5 mg of
pcDNA3 containing Gqa cDNA (a generous gift from Dr.
R. Reed) in an antisense orientation to the cytomegalovirus,
as shown in Fig. 4, was transfected into subconfluent IIC9
cells using Lipofectamine (Life Technologies) according to
the manufacturer’s protocol. As a control, pcDNA3 without
an insert was used. The transfected cells were incubated for
16–18 h in Opti-MEM (Life Technologies) mixture at 37 �C.The media was replaced with DMEM plus 10% serum,
and cells were grown for 48 h to allow expression of the
neomycin-resistant gene. The transfected cells were subcul-
tured into 100-mm culture dishes and were grown for
several weeks in selection media containing 500 mg/ml
G418 (Boehringer Mannheim, Indianapolis, IN). G418-
resistant clones were isolated with cloning rings, and the
transfected clones were maintained in DMEM containing
10% serum plus 250 mg/ml G418.
2.3. Western blot analysis
Individual colonies from the stable transfections were
screened for the expression of appropriate proteins by
immunoblotting with Gqa polyclonal antibody (Calbio-
chem, La Jolla, CA) and tested against the parental cell line
IIC9 without insert (positive control). Expression of Gi2a,
A. Gardner et al. / Cellular Signalling 14 (2002) 499–507500
Gi3a, and Gqa antisense cDNAs were immunoblotted with
HA-12CA5 monoclonal antibody (Boehringer Mannheim)
or Ga polyclonal antibodies (Calbiochem), respectively.
Serum-deprived cell cultures were stimulated in the absence
or presence of a-thrombin or EGF, washed in cold 1�PBS, lysed, on ice, in 30 ml of solubilization buffer (25 mM
HEPES, 300 mM NaCl, 2 mM ethylenediaminetetraacetic
acid (EDTA), 1.5 mM MgCl2, 1% Triton X-100, 0.5 mM
phenylmethylsulfonylfluoride, 0.1 mM Na3VO4, 10 mg/ml
leupeptin, 10 mg/ml aprotinin, and 10 mg/ml pepstatin), and
then subjected to brief sonication. Following centrifugation
(Eppendorf 5415C, 14,000 rpm, 4 �C), an equal volume of
Laemmli loading buffer was added. Protein concentrations
of lysates were determined by Bio-Rad Protein Assay (Bio-
Rad), as recommended by the manufacturer. Protein lysates
(10–15 mg) were resolved by 10% SDS–polyacrylamide
gel electrophoresis, and separated proteins were transferred
to polyvinylidine (PVDF) membranes (Immobilon, Bed-
ford, MA). The blot was incubated overnight, at 4 �C, inwash buffer (20 mM Tris, pH 8.0, 150 mM Na Cl, 0.01%
Tween 20) containing 10% dry milk (w/v) and was then
washed. The membranes were probed with the appropriate
antibody, and after washing, they incubated with a second-
ary antibody (HRP-conjugated goat antimouse IgG or anti-
rabbit, Bio-Rad). Immunoreactive bands were visualized by
enhanced chemiluminescence (ECL) Western blotting sys-
tem (Amersham), as recommended by the manufacturer.
2.4. Phosphoinositide hydrolysis assay
Phosphoinositide hydrolysis was determined essentially
as described by Hung et al. [40]. IIC9 cells were seeded into
six-well plates (Corning) at a density of approximately 105
cells/well and were grown to subconfluence (approximately
50%). Cells were washed twice with basal media and were
then incubated for 24–48 h with basal media containing no
myoinositol plus 1–2 mCi/ml [3H]Myoinositol (DuPont/
NEN, Boston, MA, USA) for 24 h at 37 �C. LiCl (20
mM) was added to the cells 1 min prior to addition of a-thrombin, and cells were incubated at 37 �C. After 15 min,
the cells were rinsed once in cold PBS, and total inositol
phosphates were extracted in 600 ml of cold 4% HClO4 (v/v)
for 30 min at 4 �C. To each supernatant, 50 ml of phenol red/60 mM HEPES was added, neutralized with NH4OH, and
then centrifuged. The supernatants were applied to a 0.5-ml
column of Dowex AGIX8 (200–400 mesh size), formate
form (Bio-Rad). Columns were washed with 3 ml water
(� 3), followed by 3 ml 0.05 M ammonium formate/0.005
M borax (� 3). [3H]Inositol phosphates were eluted with
3 ml of 0.1 M formic acid/1.8 M ammonium formate, and
1 ml quantified by scintillation counting.
2.5. Immune-complex kinase ERK assay
Subconfluent (80%), growth-arrested IIC9 cells were
stimulated with a-thrombin (1 U/ml) for 5 min at 37 �C.
The medium was removed, and cells were washed twice in
cold PBS and scraped into 150 ml of ice-cold ERK lysis
buffer (20 mM Tris–HCl, pH8, 10% glycerol, 1% Triton
X-100, 1 mM NaF, 1 mM sodium vanadate, 50 mM
b-glycerolphosphate, 10 mg/ml aprotinin, 10 mg/ml pepstatin,
and 10 mg/ml leupeptin). The lysates were briefly sonicated,
and insoluble material was pelleted by centrifugation at
14,000� g at 4 �C for 5 min. Protein concentrations were
determined using the Bio-Rad Protein Assay, according to
the manufacturer’s specifications. For the immunoprecipita-
tions, 2 mg of either ERK1 polyclonal antibody (Santa Cruz
Biotechnology, Santa Cruz, CA) or monoclonal antibody
12CA5, raised to a peptide from influenza HA1 protein
(Boehringer Mannheim), was added to the supernatants and
incubated with gentle rocking at 4 �C for 4 h. The complexes
were then incubated for 2–3 h with either protein A-Sepha-
rose for polyclonal antibodies, or protein G-Sepharose for
monoclonal antibodies. ERK1 immune complexes were
washed twice with 1 ml of cold lysis buffer, twice with
1 ml of cold LiCl buffer (0.5 M LiCl, 100 mM Tris–HCl,
pH 7.6), and once with 1 ml of cold assay buffer (20 mM
Tris–HCl, pH 7.5, 50 mM b-glycerolphosphate, 1.5 mM
ethyleneglycol-bis{b-aminoethylether}N,N,N00,N00-tetra-
acetic acid (EGTA), 1 mM dithiothreitol). ERK1 immune
complexes were pelleted for 2 min at 14,000� g and
resuspended in 20 ml of reaction buffer per sample (20 mM
Tris–HCl, pH 7.3, 10 mM MgCl2, 50 mM ATP), 10 mgmyelin basic protein (MBP) per sample, and 2.5–5.0 mCi of[g32P]ATP. The samples were incubated for 45 min at 30 �C,and the reaction terminated by the addition of 5 ml of
4�Laemmli sample buffer. They were then boiled for
5 min and subjected to SDS–PAGE. The gels were dried,
and ERK activity was quantified by PhosphoImager analysis
(Molecular Dynamics).
2.6. [3H]Thymidine incorporation
Wild-type IIC9 or Gqa cells were plated in 12-well plates
at 2.5� 104 cells/well in DMEM (Life Technologies) with
10% foetal calf serum (Sigma). After 24 h, cells were
washed twice in DMEM and incubated for 48 h in DMEM
containing 1 mg/ml bovine serum albumin (Sigma, radio-
immunoassay grade), 2 mM L-glutamine (Sigma), 100 U
penicillin, 100 mg streptomycin/ml, and 20 mM Na HEPES,
pH 7.4 (Washington University Tissue Culture Facility,
MO). Following 20 h of incubation with either serum
(10%, v/v) or a-thrombin (1 U/ml), or EGF (100 ng/ml),
1 mCi/ml [3H]thymidine (DuPont/NEN) was added, and the
incubation was continued for an additional 3 h. Cells were
washed twice with cold PBS, and [3H]thymidine incorpora-
tion was determined as trichloroacetic acid (TCA)-insoluble
radioactivity by liquid scintillation counting as previously
described [32]. Briefly, DNAwas precipitated by incubating
the cells for 30 min with 1 ml of cold 5% (v/v) TCA. The
TCA-precipitated DNA was washed twice with cold 5%
TCA and solubilized with 500 ml of 2% (w/v) sodium
A. Gardner et al. / Cellular Signalling 14 (2002) 499–507 501
bicarbonate/0.1 M NaOH. Cells were scraped, and the lysate
was neutralized with 100 ml of 5% TCA. The TCA-pre-
cipitated [3H]DNA was quantified by scintillation counting.
3. Results
3.1. Reduced amounts of Gqa result in apparent growth
A number of studies implicate a critical role that Gqaplays in the regulation of cell growth [41–43]. To invest-
igate the importance of Gqa in cell growth, we isolated a
clonal cell line in which a full-length Gqa cDNA construct
in the antisense orientation is expressed (Fig. 1A). Western
blot analysis with antibodies directed against Gqa show a
60% reduction in the amounts of Gqa in the Gqa-reducedclones, Gqa1 (Fig 1B) and Gqa2, as well as four independ-
ently isolated Gqa-reduced clones (data not shown). In
contrast to Gqa, no change in the amounts of the other
Ga subunits, expressed in IIC9 and Gqa1 cells, is detected
(Fig. 1C). In the presence of 10% serum IIC9, cells double
within 24 h. Interestingly, the Gqa1 cells show a marked
increase in the time to transit the cell cycle with a doubling
time of approximately 36–40 h (Fig. 2). To investigate
the ability of the Gqa1 cells to enter into the cell cycle
and progress into S phase, we determined the effect of
a-thrombin on [3H]thymidine incorporation in Gqa1 cells
20 h after a-thrombin addition. In IIC9 cells, addition of low
mitogenic concentrations of a-thrombin (1 NIH unit/ml)
stimulates a four- to sixfold increase in [3H]thymidine
incorporation as compared with unstimulated IIC9 cells
(Fig. 3). Interestingly, a-thrombin fails to stimulate a
significant increase in [3H]thymidine incorporation in
Gqa1 cells (Fig. 3). The Gqa1 cells, however, have not lost
the ability to reenter the cell cycle and transit through G1, as
serum (10%) induces a similar increase in [3H]thymidine
incorporation in the Gqa1 cells as compared to IIC9 cells.
3.2. IP levels in Gqa1 cells are abolished using mitogenic
concentrations of a-thrombin
Previous studies in IIC9 cells demonstrate that a-throm-
bin induces rapid activation of phospholipase C (PI–PLC)-
mediated phosphoinositide hydrolysis, presumably via Gqa.We reasoned that if PI–PLC activity is dependent on
activation of Gqa, then a-thrombin-induced PI hydrolysis
should be markedly reduced in Gqa1 cells (Fig. 4). In wild-
type IIC9 cells, mitogenic concentrations of a-thrombin (1
NIH unit/ml) induce a fourfold increase in phosphoinositide
amounts above basal levels (Fig. 4). However, this level of
a-thrombin is ineffective in the Gqa1 cells (Fig. 4). We next
examined whether increased concentrations of a-thrombin
can induce PI hydrolysis. Addition of 10 NIH units/ml
results in increases in the Gqa1 cells that are similar to
those seen in IIC9 cells with only 1 NIH unit/ml a-thrombin
(Fig. 4). A dose–response analysis clearly demonstrates that
the reduction of Gqa results in a marked decrease in the
potency without any decrease in efficacy (Fig. 4), indicating
that the increasing amounts of a-thrombin can compensate
for the loss of Gqa.Our data clearly demonstrate that a reduction in amounts
of Gqa results in the failure of low doses of a-thrombin to
Fig. 1. Western blot analysis of Gqa antisense ablation. (A) Schematic
representation of the Gqa antisense construct. EcoRI fragment of Gqa from
pGEM-2/Gqawas subcloned into a vector plasmid, pcDNA3, in an antisense
orientation. The 30 end of the Gqa cDNA was immediately adjacent to the
cytomegalovirus promoter under which control the antisense was tran-
scribed. (B and C) Membrane proteins were separated on SDS–PAGE gel
(12.5%), and membranes were probed with an antibody against Gqa, Gi2a,Gi3a Gsa Goa, and G13a at 1:1000 dilution, for 1 h, as described in the
Materials and Methods. G-protein bands were detected by ECL.
Fig. 2. Gqa1 cells display a marked increase in cell cycle transit time. IIC9
cells were plated at approximately 20,000 cells/well in six-well dishes in
DMEM media containing 10% FCS. On the following day, cells were
washed with calcium- and magnesium-free PBS and fed with DMEM plus
a-thrombin (1 U/ml). Media were changed daily. To evaluate growth, cells
were trypsinized, resuspended, and counted with a Coulter counter. All
growth curves are representative of at least two separate experiments.
A. Gardner et al. / Cellular Signalling 14 (2002) 499–507502
induce cell cycle reentry and progression through G1.
Because high doses of a-thrombin (10 NIH units/ml) restore
PI hydrolysis, we reasoned that high doses would rescue
a-thrombin’s ability to stimulate growth. In support of this
idea, addition of 10 NIH units/ml stimulates cell cycle entry
and progression through G1 as determined by [3H]thymi-
dine incorporation (Fig. 5). Interestingly, high concentra-
tions of a-thrombin (10 NIH units/ml) induce amounts of
[3H]thymidine incorporation comparable to that seen in IIC9
cells when activated by low doses (1 NIH unit/ml) of
a-thrombin (Fig. 5). In agreement with the previous data,
the dose–response analysis for a-thrombin-induced thymi-
dine incorporation clearly demonstrates that the reduction of
Gqa results in a marked decrease in the potency without any
decrease in efficacy, indicating that increasing amounts of
a-thrombin can compensate for the loss of Gqa.
3.3. Gqa1 cells exhibit altered activation of the rapid phase
of ERK activity
To understand the mechanism for the growth-deficient
phenotype of the Gqa1 cells, we examined whether these
cells have altered signalling pathways known to be import-
ant for growth. Previous studies in a number of fibroblast
Fig. 3. Gqa1 cells display aberrant DNA sythesis. Quiescent Gqal cells were stimulated with or without a-thrombin (2 U/ml, 20 h) or serum (20 h). Following
removal of the mitogen, [3H]thymidine (1 mCi/ml) added for 3 h. The effects of Gqa ablation on thymidine incorporation were analyzed, as described in the
Materials and Methods. Means ± S.D. of three independent experiments performed in triplicate are presented.
Fig. 4. Inositol phosphate levels are aberrant in antisene-ablated Gqa1
cells. Wild-type IIC9 and Gqa1 cells were labeled with myo-[3H] inositol
(1 mCi/ml) for 24 h and then incubated in serum-free media supplemented
with 20 mM LiCl in the absence or presence of 0.01, 0.1, 0.5, 1.0, 2.0, 5.0,
or 10.0 U/ml thrombin for 15 min at 37 �C. IP3 levels were quantified as
described in the Materials and Methods. Triplicate samples were
performed on each set of experiments, which yielded the means ± S.D.
of three independent experiments.
Fig. 5. DNA synthesis in Gqa1 cells is rescued by high mitogenic
concentrations of thrombin. Quiescent Gqa1 cells were stimulated with or
without a-thrombin (0.01, 0.1, 0.5, 1.0, 2.0, 5.0, or 10.0 U/ml) for 20 h.
Following removal of the mitogen, [3H]thymidine (1 mCi/ml) was added for
3 h. The effects of Gqa ablation on thymidine incorporation were analyzed,
as described in the Materials and Methods. Triplicates were performed on
each set of experiments, which yielded the means ± S.D. of three
independent experiments.
A. Gardner et al. / Cellular Signalling 14 (2002) 499–507 503
cell lines [22,44,45] found that ERK activation is critical for
cell entry and progression through G1. Furthermore, studies
from our laboratory demonstrate that inhibition of a-throm-
bin-stimulated ERK activation blocks G1 progression in
IIC9 cells (unpublished observations). To ascertain whether
the reduced amounts of Gqa expressed in Gqa1 cells results
in inhibition of ERK activity, we examined the effect of low
mitogenic concentrations of a-thrombin on endogenous
ERK activity, as evidenced by the degree of phosphoryla-
tion of MBP (Fig. 6). As shown in Fig. 6, addition of 1 NIH
unit/ml of a-thrombin to IIC9 cells induces a rapid fivefold
increase in ERK activity, as indicated by the robust degree
of phosphorylation of MBP, followed by a lower, sustained
increase. We and others have shown, in a variety of cells,
that a-thrombin-stimulated ERK activation is biphasic,
with a rapid, initial phase within the first few minutes
of activation, followed by a late sustained phase of
ERK activity lasting for at least 4 h [8,39,44,63]. In agree-
ment with previous data, the rapid peak of ERK activity
in IIC9 wild-type cells is observed within 5–10 min after
a-thrombin addition (Fig. 6). However, in the Gqa1 cells, 1
NIH unit/ml a-thrombin stimulates only a two- to threefold
increase above basal levels, approximately 50% of that seenin IIC9 cells (Fig. 6). Interestingly, sustained ERK activity
is similar to the sustained activity reported in IIC9 cells
(Fig. 6). These data suggest that the rapid increase in ERK
activity is dependent in part on Gqa. Because high concen-
trations of a-thrombin restore PI hydrolysis, we reasoned
that high concentrations of a-thrombin could also restore
the rapid phase of ERK activity in the Gqa1 cells to the level
found in IIC9 cells (Fig. 7). Consistent with this reasoning,
high doses of a-thrombin stimulate a four- to fivefold
increase in ERK activity measured 5 min after a-thrombin
addition (Fig. 7). These results clearly suggest that the rapid
increase in a-thrombin-induced ERK activation is depend-
ent on Gqa, while sustained activation is unaffected.
3.4. Gqa1 cells exhibit altered CDK activity
Previous results show that a-thrombin, and PDGF,
induce cyclin D1 protein expression and CDK4–cyclin
D1 activity in IIC9 cells [44,46]. Furthermore, our labor-
atory, and others, also found that inhibition of mitogen-
induced ERK activation prevents the expression of cyclin
D1, CDK4–cyclin D1 activity, and G1 progression [44,46].
To identify a potential downstream cell cycle target in
the Gqa1 cells, we quantified the levels of cyclin D1.
As determined by Western blot analysis, low doses of
a-hrombin stimulate similar amounts of cyclin D1 protein
expression in IIC9 and Gqa1 cells (Fig. 8A). Our observa-
tions indicate that reduction of the amounts of Gqa does not
affect cyclin D1 expression. We next examined whether the
CDK4–cyclin D1 activity is altered in these cells. While
addition of low amounts of a-thrombin increases CDK4–
cyclin D1 levels within 4 h in IIC9 cells, only after 8 h is a
comparable increase seen in the Gqa1 cells (Fig. 8B).
Fig. 6. ERK-1 activation is aberrant in Gqa-antisene-deficient Gqa1 cells.
Quiescent IIC9 and Gqa1 cells, serum deprived for 48 h, were stimulated
with thrombin (1 U/ml, 5 min for the initial peak or 4 h for the sustained
peak) and ERK activity determined as described in the Materials and
Methods. ERK1 complexes were immunoprecipitated from lysates
containing equal protein, and kinase activity was tested by its ability to
phosphorylate MBP in vitro as described in the Materials and Methods.
ERK1 activity was quantitated using a Molecular Dynamics Phosphor-
Imager. Data are represented as fold increase relative to basal (normalized
to one). Duplicates were performed on each set of experiments, which
yielded the means ± S.D. for three independent experiments.
Fig. 7. ERK-1 activation in Gqa1 cells is rescued by high mitogenic
concentrations of thrombin. Quiescent IIC9 and Gqa1 cells, serum deprived
for 48 h, were stimulated (0.01, 0.1, 0.5, 1.0, 2.0, 5.0, or 10.0 U/ml) for 5
min, and ERK activity was determined as described in the Materials and
Methods. ERK1 was immunoprecipitated, and kinase activity was tested by
its ability to phosphorylate MBP. Data are represented as fold increase
relative to basal (normalized to one). Duplicates were performed on each
set of experiments, which yielded the means ± S.D. for three independ-
ent experiments.
A. Gardner et al. / Cellular Signalling 14 (2002) 499–507504
Interestingly, high concentrations of a-thrombin result in
an increase in CDK4–cyclin D1 activity within 4 h, similar
to IIC9 cells (Fig. 8B). These data show that the rapid
increase in ERK activation is important for CDK4–cyclin
D1 expression.
4. Discussion
a-Thrombin is a potent inducer of a variety of cellular
responses including phosphoinositide hydrolysis [14], ERK
activation [8], and DNA synthesis [47,48] in a variety of cell
types. Studies from several laboratories [40,49,50] dem-
onstrate that a-thrombin activates several G-proteins includ-
ing members of the Gq, Gi, and G12/13, although the
physiological importance of these proteins is still not
completely understood. We specifically investigated the role
of Gqa in modulating a-thrombin-induced mitogenesis. We
show in Gqa1 cells, a stable cell line expressing reduced
amounts of Gqa, that concentrations of a-thrombin (1 NIH
unit/ml), which induce cell cycle reentry and progression
into S phase in wild-type IIC9 cells, do not stimulate PI
hydrolysis, the rapid early phase of ERK activity, and transit
through G1 into S phase as quantified by CDK4–cyclin D
activity and [3H]thymidine incorporation. Interestingly, high
concentrations of a-thrombin (10 NIH units/ml) restore
these activities and cell cycle progression into S phase.
While it is well documented that a-thrombin-induced sus-
tained ERK activity mediates important responses important
for transit through G1 into S phase, the importance of the
rapid, Gq-dependent phase has not been appreciated.
A question naturally arises as to whether the same PAR-
type receptor mediates a-thrombin signalling events in IIC9
cells, or whether these cells utilize two distinct thrombin
receptors. PAR1, PAR3, and PAR4 thrombin receptors are
all activated by a-thrombin [4]. Non-PAR1-blocking anti-
bodies block platelet activation by low, but not high,
concentrations of a-thrombin [51]. Similar results are found
in transgenic mice in which PAR1 is knocked out [7]. These
data suggest the presence of an additional thrombin receptor
distinct from the PAR1 type. Indeed, further work indicated
that a low-affinity PAR4 receptor was present in mouse
platelets that mediated responses at higher concentrations of
a-thrombin [7]. However, a-thrombin’s effects in IIC9 cells
appear to be mediated by PAR1. Enterokinase treatment of
IIC9 cells expressing a mutant PAR1 receptor, which con-
tains an enterokinase site in place of the a-thrombin site,
stimulates PI hydrolysis [52], ERK activation, and G1
transit (Baldassare JJ, Chen J, Raben DM, unpublished
observation), suggesting that a-thrombin mediates mito-
genesis through activation of PAR1. Furthermore, Northern
blot analysis of IIC9 cells, using low-stringency hybridiza-
tion conditions, indicated that only one species of thrombin
receptor is expressed [52]. Consistent with these data that
PAR1 is the only a-thrombin-responsive species in fibro-
blasts is the observation that the fibroblasts from PAR1-
deficient mice do not respond to a-thrombin, whereas
platelets from these mice do respond [7].
While a-thrombin induces a marked increase of phos-
phoinositide hydrolysis in wild-type mice, this activity is
completely lost in transgenic mice in which PAR1 is
knocked out [7]. Studies from a number of laboratories
indicate that a-thrombin-induced phosphoinositide release
is mediated specifically by Gqa [19]. We report that
reduction of Gqa results in a marked reduction of the
potency of a-thrombin but no loss in efficacy. Additionally,
loss of phosphoinositide hydrolysis correlates with partial
loss rapid ERK activation and deficient growth in these
cells. There is a precedence that agonists that regulate
cell growth also activate phosphoinositide metabolism
[12,16,43]. Evidence indicates that a-thrombin-stimulated
phosphoinositide release correlates with the induction of
immediate early genes and proliferation of pulmonary artery
smooth muscle cells [12]. Furthermore, work by Nebigil
demonstrated that suppression of PI-specific PLCb, by
expression of PLCb mRNA antisense, inhibited protein
kinase C (PKC), Ras, and ERK activity, as well as growth
in FTO-2B cells [16]. Additionally, in clones with sup-
pressed PLC activity, cellular levels of PIP2 were elevated
and correlated with growth inhibition in these cells [16].
Fig. 8. CDK4–cyclin D activity is rescued by high mitogenic concen-
trations of thrombin. (A) IIC9 cells or Gqa1 cells were stimulated with 1 U/
ml of thrombin for the times indicated. Membrane proteins from either IIC9
cells or Gqa1 cells were separated on SDS–PAGE gel (10.0%), and
membranes were probed with an antibody against cyclin D1 at 1:1000
dilution, for 1 h, as described in the Materials and Methods. Lanes 1, 3, and
5 are wild-type IIC9 cells, and lanes 2, 4, and 6 are Gqa1 cells data. G-
protein bands were detected by ECL. (B) Quiescent IIC9 and Gqa1 cells,
serum deprived for 48 h, were stimulated with thrombin (1 or 10 U/ml) for
5 min, and ERK activity was determined as described in the Materials and
Methods. CDK4–cyclin D activity was immunoprecipitated, and kinase
activity was tested. Results are represented as fold increase relative to basal
(normalized to one). Data are representative of at least three independ-
ent experiments.
A. Gardner et al. / Cellular Signalling 14 (2002) 499–507 505
These data further support our observations that Gq-coupled
phosphoinositide hydrolysis is a prerequisite for a-throm-
bin-stimulated mitogenesis.
ERK regulation by GPCRs is a common phenomenon
and is necessary and adequate for the regulation of prolif-
eration in cell systems [53]. ERK activation by receptors
linked to pertussis toxin-sensitive Gai proteins is mediated
by bg subunits [54] and preferentially coupled to activation
of Ras and PI3 kinase [55]. In the majority of cases, the
activation of ERK by pertussis toxin-sensitive Gia proteins
is PKC independent, which is indicative of a lack of
receptor-mediated PI hydrolysis [56,57]. Conversely, per-
tussis toxin-insensitive Gqa proteins are generally associ-
ated with the activation of ERK by a Raf–PKC-dependent
route. In mouse lung fibroblasts, the mechanism by which
a-thrombin activates the rapid phase of ERK has been
shown to be dependent on two pathways [8]. In one
pathway, the PAR1 thrombin receptor utilizes PKC and is
c-Raf dependent, and the second is Gia dependent and
c-Raf independent [8]. Our observations in IIC9 wild-type
cells indicate that the rapid phase of ERK activation by
a-thrombin is modulated by two pathways: one is Gqadependent (Baldassare JJ, Gardner A, unpublished observa-
tions), and the other is pertussis toxin sensitive and Ras
dependent and is mediated by bg subunits (Baldassare JJ,
Gardner A, unpublished observations). Importantly, our data
suggests that cooperative signalling of Gqa- and Gia-mediated pathways for the proficient activation of the
ERK cascade is a prerequisite for the efficient commence-
ment of the a-thrombin mitogenic cascade, as Gqa1 cells
were not fully proficient at mediating the activation of the
rapid phase of ERK and subsequent thymidine incorpora-
tion, even though the sustained phase of ERK was normal in
these cells. The notion that dually coupled GPCRs require
cooperation of pertussis toxin-sensitive and -insensitive
pathways in the efficient activation of mitogenic cascades
has recently been addressed [53]. Blaukat et al. [53]
demonstrated that the bradykinin B2 receptor required the
cooperative signalling of Gqa- and Gia-mediated pathways
for the proficient activation of the ERK cascade, indicating
that this concept is a potential mechanism by which GPCRs
regulate various cellular responses.
The indication that reduced levels of Gqa result in a
marked decrease of the a-thrombin mitogenic signalling
pathways suggests that the mitogenic potency of the path-
way is diminished. In support of this suggestion, high doses
of a-thrombin restored PI hydrolysis, as well as the activ-
ities of ERK and CDK4–cyclin D, and cell cycle progres-
sion into S phase. However, the mechanism resulting in this
phenomenon remains to be determined. An answer may lie
in the recent paper by DeFea et al. [62], who demonstrated
that agonist activation of the Gq-coupled PAR2 receptor
induces the formation of a multiprotein signalling complex
that is required for the appropriate intracellular targeting of
activated ERK and, therefore, its mitogenic potential. They
showed that b-arrestin-dependent endocytosis of the signal-
ling complex, containing internalised PAR2 receptor, raf-1,
and ERK, was required for ERK activation. Other GPCRs
have been found to have a similar mechanism for the
activation of ERK [58,59]. Therefore, in the case of Gqa1
cells, it is conceivable that a decreased quotient of internal-
ised receptor exists in the multiprotein signalling complex,
which leads to an overall decreased level of ERK activity
and growth potential. In contrast, when high levels of a-thrombin are utilized, a greater number of PAR1 receptors
are recruited to the multiprotein signalling complex, thus
normalizing the signalling mechanism, namely, the required
level of ERK activity and the consequent rescue of a-thrombin’s mitogenic potential.
Therefore, our observations suggest that decreased Gqalevels could result in decreased coupling efficiency to a
signal transduction pathway that functions as an early,
essential signal linked to the induction of cell proliferation.
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