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J Biol Chem, Vol. 274, Issue 26, 18675-18685, June 25, 1999


M3 Muscarinic Acetylcholine Receptors Regulate Cytoplasmic Myosin by a Process Involving RhoA and Requiring Conventional Protein Kinase C Isoforms*

Derek StrassheimDagger , Lisa G. May§, Kimberly A. Varker, Henry L. Puhl§, Scott H. PhelpsDagger , Rebecca A. PorterDagger , Robert S. Aronstam§, John D. Notiparallel , and Carol L. WilliamsDagger **

From the Laboratories of Dagger  Molecular Pharmacology, § Neurobiology, and parallel  Molecular Biology, Guthrie Research Institute, and  Department of Surgery, Guthrie Clinic, Sayre, Pennsylvania 18840

    ABSTRACT
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES

Although muscarinic acetylcholine receptors (mAChR) regulate the activity of smooth muscle myosin, the effects of mAChR activation on cytoplasmic myosin have not been characterized. We found that activation of transfected human M3 mAChR induces the phosphorylation of myosin light chains (MLC) and the formation of myosin-containing stress fibers in Chinese hamster ovary (CHO-m3) cells. Direct activation of protein kinase C (PKC) with phorbol 12-myristate 13-acetate (PMA) also induces myosin light chain phosphorylation and myosin reorganization in CHO-m3 cells. Conventional (alpha ), novel (delta ), and atypical (iota ) PKC isoforms are activated by mAChR stimulation or PMA treatment in CHO-m3 cells, as indicated by PKC translocation or degradation. mAChR-mediated myosin reorganization is abolished by inhibiting conventional PKC isoforms with Go6976 (IC50 = 0.4 µM), calphostin C (IC50 = 2.4 µM), or chelerythrine (IC50 = 8.0 µM). Stable expression of dominant negative RhoAAsn-19 diminishes, but does not abolish, mAChR-mediated myosin reorganization in the CHO-m3 cells. Similarly, mAChR-mediated myosin reorganization is diminished, but not abolished, in CHO-m3 cells which are multi-nucleate due to inactivation of Rho with C3 exoenzyme. Expression of dominant negative RhoAAsn-19 or inactivation of RhoA with C3 exoenzyme does not affect PMA-induced myosin reorganization. These findings indicate that the PKC-mediated pathway of myosin reorganization (induced either by M3 mAChR activation or PMA treatment) can continue to operate even when RhoA activity is diminished in CHO-m3 cells. Conventional PKC isoforms and RhoA may participate in separate but parallel pathways induced by M3 mAChR activation to regulate cytoplasmic myosin. Changes in cytoplasmic myosin elicited by M3 mAChR activation may contribute to the unique ability of these receptors to regulate cell morphology, adhesion, and proliferation.

    INTRODUCTION
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES

Muscarinic acetylcholine receptors (mAChR)1 are heterotrimeric G protein-coupled receptors that regulate contraction of smooth muscle. Multiple subtypes of mAChR that transduce different intracellular signals are often co-expressed in smooth muscle tissues (reviewed in Ref. 1). The M1, M3, and M5 mAChR subtypes activate protein kinase C (PKC) by elevating intracellular Ca2+ and diacylglycerol. In contrast, the M2 and M4 mAChR subtypes inhibit protein kinase A (PKA) by diminishing adenylyl cyclase activity (reviewed in Refs. 2 and 3). Pharmacological studies indicate that M3 mAChR activation induces smooth muscle contraction, although activation of other co-expressed mAChR subtypes may modulate this response (reviewed in Ref. 1). Dissection of the biochemical pathways involved in M3 mAChR-mediated contraction is complicated by the co-expression of multiple mAChR subtypes in many smooth muscle tissues.

Contractile processes in non-muscle cells mimic those occurring in smooth muscle tissues, indicating the value of using non-muscle cells to investigate the biochemical pathways that regulate contraction (4-8). Phosphorylation of myosin light chains (MLC) in non-muscle cells causes the formation of myosin-containing stress fibers, which are contractile bundles of actin filaments associated with myosin II (4-8). Phosphorylation of MLC similarly increases actin-myosin interactions in smooth muscle cells, resulting in smooth muscle contraction (reviewed in Refs. 9-12). In addition to smooth muscle contraction, many fundamental cellular processes such as adhesion, migration, and division depend upon the interaction of myosin with actin in contractile filaments (reviewed in Ref. 12). Activation of mAChR may affect these fundamental processes by altering myosin activity in non-muscle cells as it does in smooth muscle. Although mAChR activation induces MLC phosphorylation and subsequent contraction in smooth muscle cells (13-17), the ability of mAChR to regulate MLC phosphorylation and myosin organization in non-muscle cells has not been reported.

We investigated the ability of transfected human mAChR subtypes to regulate myosin organization in Chinese hamster ovary (CHO) cells. Activation of transfected M3 mAChR induces MLC phosphorylation and causes myosin-containing stress fibers to form in CHO cells. The involvement of PKC in these events is indicated by our findings that 1) direct activation of PKC with phorbol esters induces MLC phosphorylation and myosin reorganization in CHO cells, 2) specific PKC antagonists inhibit M3 mAChR-mediated myosin reorganization, and 3) activation of transfected M1 but not M2 mAChR subtypes also induces the formation of myosin-containing stress fibers, demonstrating that only mAChR subtypes that stimulate PKC activity induce myosin reorganization. The participation of myosin light chain kinase (MLCK) and RhoA in mAChR-mediated myosin reorganization was also investigated, since these proteins regulate contractile processes in other systems (reviewed in Refs. 9-12). We found that MLCK antagonists inhibit mAChR-mediated myosin reorganization but only at antagonist concentrations that may affect PKC. Stable expression of dominant negative RhoAAsn-19 or inactivation of Rho with C3 exoenzyme lessens mAChR-mediated myosin reorganization but does not abolish it.

This study demonstrates that M3 mAChR activation significantly affects myosin organization in non-muscle cells. Our findings indicate that M3 mAChR activation induces cytoplasmic myosin reorganization by both PKC- and Rho-dependent mechanisms. These receptor-mediated changes in cytoplasmic myosin may contribute to the unique ability of M3 mAChR to regulate the adhesion (18-20) and morphology (21, 22) of non-muscle cells.

    EXPERIMENTAL PROCEDURES
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES

Reagents-- The SA-2 human IgM monoclonal autoantibody that reacts specifically with myosin heavy chains was obtained from cultures of a thymic B lymphocyte clone transformed with Epstein-Barr virus, as described previously (23, 24). Mouse monoclonal antibody to hemagglutinin (HA) was purchased from Babco (Berkeley, CA), and mouse monoclonal antibodies to PKC isoforms were purchased from Transduction Laboratories (Lexington, KY). Fluorescein-labeled goat anti-human IgM was obtained from Fisher. Horseradish peroxidase-labeled antibody to mouse immunoglobulins and enhanced chemiluminescence (ECL) reagents were obtained from Amersham Pharmacia Biotech. Reagents for LipofectAMINE-mediated transfection were purchased from Life Technologies, Inc. Carbachol and phorbol 12-myristate 13-acetate (PMA) were purchased from Sigma. The kinase inhibitors calphostin C, Go6976, chelerythrine, KT5926, ML-7, and ML-9 were obtained from Calbiochem, and KN-62 was bought from Research Biochemicals, Inc. (Natick, MA). Ham's F-12 medium was purchased from Mediatech (Herndon, VA); fetal calf serum (FCS) was obtained from Biofluids (Rockville, MD), and zeocin was bought from Invitrogen (Carlsbad, CA). Other reagents were obtained from Sigma or from sources listed in the text.

Cell Lines-- CHO-K1 sublines stably transfected with the M1, M2, or M3 subtypes of human mAChR are referred to as CHO-m1, CHO-m2, and CHO-m3, respectively. These sublines, as well as untransfected CHO-K1 cells, were generously provided by Dr. Mark Brann (University of Vermont). Cells were cultured in complete medium consisting of Ham's F-12 medium, heat-inactivated FCS (5%), glutamine (0.3 mg/ml), penicillin (20 units/ml), and streptomycin sulfate (20 µg/ml). Cells were maintained at 37 °C in a humidified atmosphere of 5% CO2, 95% air at densities that promoted exponential proliferation.

Establishment and Characterization of CHO-m3 Cell Lines Stably Expressing Wild-type or Mutant RhoA-- The pEF-BOS-HA-RhoA and pEF-BOS-HA-RhoAVal-14 plasmids coding for hemagglutinin (HA)-tagged wild-type RhoA or constitutively active RhoAVal-14, respectively, were a generous gift from Dr. Shinya Kuroda (Nara Institute of Science and Technology, Nara, Japan). The pEF-BOS-HA-RhoAAsn-19 plasmid coding for HA-tagged dominant negative RhoAAsn-19 was generated by site-directed mutagenesis of the pEF-BOS-HA-RhoA construct using the GeneEditor system from Promega (Madison, WI). Sequencing of the pEF-BOS-HA-RhoAAsn-19 plasmid indicated that the threonine at codon 19 of wild-type RhoA was successfully mutated to asparagine, with no other mutations. CHO-m3 cells were transfected with the pEF-BOS-HA-RhoA, pEF-BOS-HA-RhoAVal-14, or pEF-BOS-HA-RhoAAsn-19 plasmid and simultaneously co-transfected with the pZeoSV2 plasmid coding for zeocin resistance (Invitrogen, Carlsbad, CA), using LipofectAMINE according to the manufacturer's instructions (Life Technologies, Inc.). After transfection, the cells were cultured in complete medium for 3 days and then passaged every 3 days in complete medium containing zeocin (500 µg/ml). Cell lines expressing HA-tagged wild-type or mutant RhoA were detected by ECL Western blotting using HA antibody and cloned by limiting dilution. Clonal lines were considered to be stably transfected if they demonstrated expression of HA-tagged wild-type or mutant RhoA in three independent ECL Western blots conducted over a period of more than 1 month. The stably transfected clonal lines were subjected to DNA sequencing to ensure that the cells expressed the appropriate HA-tagged wild-type or mutant RhoA with the correct DNA sequence. The levels of M3 mAChR expressed by the cells were determined by measuring the binding of [3H]N-methylscopolamine on the surface of live cells and in total cell lysates, as described previously (25, 26). Carbachol-induced Ca2+ mobilization in the cells was determined by previously described methods using the fluorescent Ca2+-binding reagent, Fura-2AM (27).

Measurement of Myosin-containing Stress Fiber Formation-- The SA-2 human monoclonal autoantibody to the myosin heavy chain was used as described previously to determine the intracellular distribution of myosin (24). Cells were cultured on glass coverslips for 2 days in complete medium and then incubated in complete medium in the presence or absence of kinase inhibitors for 30 min before exposure to carbachol, PMA, or no drug. After incubation for the designated times, the cells were fixed by immersion in ice-cold acetone and incubated (30 min, 24 °C) in phosphate-buffered saline (PBS) containing 1% bovine serum albumin (BSA) to block nonspecific antibody-binding sites. The fixed cells were incubated (1 h, 24 °C) with the SA-2 antibody, washed in PBS, and incubated (1 h, 24 °C) with fluorescein-labeled anti-human IgM antibody diluted 1:100 in PBS, 1% BSA. In some assays, nuclei were fluorescently labeled by propidium iodide (5 µg/ml) that was present during the incubation with the secondary antibody. After washing, the cells were mounted in PBS containing 90% glycerol and 0.1% p-phenylenediamine and examined by fluorescence microscopy using a Nikon Optiphot fluorescence microscope.

The samples were scored for the presence of stress fibers by two investigators without knowledge of the identity nor treatment of the cell lines being examined. The investigators independently assigned scores to the cells in 10 different microscope fields in each sample, using the following values based on the presence of stress fibers in the cells: 0 = no detectable stress fibers, 1 = few, moderately defined stress fibers, 2 = well defined stress fibers, and 3 = abundant, strongly defined stress fibers. The calculated mean of the scores was used as a measurement of myosin-containing stress fiber formation.

Immunofluorescent Localization of PKC Isoforms-- Cells cultured on glass coverslips in complete medium were incubated in the absence or presence of drugs for the indicated times and fixed by incubating for 10 min in 3.7% formaldehyde diluted in PBS containing 0.2% Triton X-100. After nonspecific antibody-binding sites were blocked as described above, the cells were incubated (1 h, 24 °C) with mouse monoclonal antibodies to PKC isoforms diluted in PBS, 1% BSA. The cells were washed and incubated (1 h, 24 °C) with fluorescein-labeled anti-mouse IgG antibody diluted in PBS, 1% BSA. After washing, the cells were mounted and examined by fluorescence microscopy as described above.

ECL Western Blotting-- Cells were lysed by periodic agitation for 15 min in ice-cold lysis buffer (50 mM Tris-HCl, 120 mM NaCl, 2.5 mM EDTA, 1 mM dithiothreitol, 0.5% Nonidet P-40, pH 7.4) containing protease inhibitors (200 µM phenylmethylsulfonyl fluoride and 5 µg/ml leupeptin). The lysate was centrifuged (16,000 × g, 10 min, 4 °C), and the resulting supernatant was boiled 5 min with sample buffer and subjected to SDS-polyacrylamide gel electrophoresis using a 5% stacking gel and 10% separating gel. Proteins in the gels were electrophoretically transferred to PVDF membranes. The PVDF membranes were incubated overnight in blocking buffer (10 mM Tris, 150 mM NaCl, 0.1% Tween 20, 10% dried milk powder, pH 7.6), placed in a 25-channel miniblotter (Immunetics Inc., Cambridge, MA), and incubated (1.5 h, 4 °C) with antibodies diluted in blocking buffer. After washing twice in wash buffer (10 mM Tris, 150 mM NaCl, 0.1% Tween 20, pH 7.6), the PVDF membranes were incubated (1 h, 4 °C) with horseradish peroxidase-labeled anti-mouse immunoglobulins diluted 1:4000 in wash buffer. The PVDF membranes were washed three times in wash buffer, and bound antibody was visualized by ECL.

Measurement of MLC Phosphorylation-- The phosphorylation of MLC in Triton X-100-insoluble lysates was determined as described previously (28). Briefly, CHO-m3 cells were incubated for 16 h with 5 µCi/ml inorganic 32P in phosphate-free Dulbecco's modified Eagle's medium containing 1% heat-inactivated FCS. After incubating with drugs for the appropriate times, the cells were lysed in Triton X-100 lysis buffer (50 mM Tris-HCl, pH 7.4, 1% Triton X-100, 200 µM phenylmethylsulfonyl fluoride, 5 µg/ml leupeptin, 10 mM sodium fluoride, 1 mM sodium orthovanadate, 0.2 mM sodium PPi, and 10 mM beta -glycerophosphate). The resulting insoluble cytoskeletal pellets were washed twice with Triton X-100 lysis buffer and dissolved by boiling in sample buffer for 30 min. The samples were subjected to ECL Western blotting using a mouse monoclonal antibody to the 20-kDa myosin light chain (Sigma), followed by autoradiography. Densitometry was performed using a Storm PhosphorImager (Molecular Dynamics, Inc., Sunnyvale, CA).

Preparation and Use of Recombinant C3 Exoenzyme-- Recombinant C3 exoenzyme was purified from bacteria transformed with the pGEX2T-C3 exoenzyme expression vector, as described previously (29). CHO-m3 cells were electroporated in the presence or absence of recombinant C3 exoenzyme (15 µg/ml) by subjecting them to three electric pulses (capacitance, 0.25 microfarads; voltage, 0.5 kV; duration, 100 µs) using a Bio-Rad Gene Pulser. Electroporated cells were cultured in complete medium for 2 days before being used in the different assays. Measurements of [32P]ADP-ribosylation of endogenous Rho by recombinant C3 exoenzyme were performed as described previously (29). Briefly, lysates from cells electroporated in the presence or absence of recombinant C3 exoenzyme were incubated (30 min, 37 °C) with ribosylation buffer (100 mM Tris-HCl, pH 8.0, 20 mM nicotinamide, 10 mM thymidine, 10 mM dithiothreitol, 10 µM [32P]NAD, 5 mM MgCl2, 5 ng of recombinant C3 exoenzyme). The samples were mixed with 100 µl of 2× sample buffer (125 mM Tris, 4% SDS, 20% glycerol, 10% 2-mercaptoethanol, 0.01% bromphenol blue, pH 6.8), boiled for 5 min, and subjected to SDS-polyacrylamide gel electrophoresis using a 5% stacking gel and 15% separating gel. The proteins were electrophoretically transferred to PVDF membranes and subjected to ECL Western blotting and autoradiography.

    RESULTS
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES

Myosin Reorganizes into Stress Fibers upon Activation of M1 or M3 mAChR-- We tested the ability of transfected M3 mAChR to regulate myosin organization in CHO cells. Treatment with carbachol, which is an agonist for all mAChR subtypes, induces myosin reorganization in the CHO-m3 subline transfected with human M3 mAChR (Fig. 1). Myosin is diffusely distributed in untreated CHO-m3 cells (Fig. 1, panel A) and becomes peripherally localized within 15 min of carbachol exposure (Fig. 1, panel B). The close proximity of the cells to one another after treatment with carbachol for 15 min reflects cell-cell adhesion induced by mAChR activation (20). Myosin-containing stress fibers appear within 30 min of mAChR activation and remain prominent for several hours in the presence of carbachol (Fig. 1, panel C). The carbachol-treated cells initially exhibit increased cell spreading but become elongated with less detectable myosin-containing stress fibers after prolonged exposure to the agonist (Fig. 1, panel D). These findings indicate that M3 mAChR activation profoundly affects myosin organization.


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  		Fig. 1.   Activation of M3 mAChR induces myosin reorganization in CHO-m3 cells. CHO-m3 cells were incubated in the absence (A) or presence of 10 µM carbachol for 15 min (B), 90 min (C), or 24 h (D) and were immunofluorescently labeled with the SA-2 antibody to myosin. Bar represents 15 µm.

Carbachol also induces myosin reorganization in CHO-m1 cells transfected with human M1 mAChR but does not alter myosin organization in untransfected CHO cells nor in CHO-m2 cells transfected with the human M2 mAChR subtype (Fig. 2). These results indicate that only mAChR subtypes which activate PKC induce myosin reorganization. Direct activation of PKC with PMA induces myosin reorganization in all CHO sublines (Fig. 2), indicating that PKC activation reorganizes myosin. Stimulation of M1 or M3 mAChR induces the formation of myosin-containing stress fibers to a greater extent than does treatment with PMA (Fig. 2).


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  		Fig. 2.   Myosin reorganization is induced by carbachol in CHO-m1 and CHO-m3 cells and by PMA in all CHO sublines. a, untransfected CHO cells (A-C), and CHO-m1 (D-F), CHO-m2 (G-I), and CHO-m3 (J-L) cells were examined. The cells were incubated with no drug (A, D, G, and J), 10 µM carbachol (B, E, H, and K), or 10 nM PMA (C, F, I, and L) for 90 min and immunofluorescently labeled with the SA-2 myosin antibody. Bar represents 15 µm. b, the indicated CHO sublines were incubated with 10 µM carbachol, 10 nM PMA, or no drug for 90 min and immunofluorescently labeled with the SA-2 myosin antibody. The presence of myosin-containing stress fibers in the cells was scored by two independent investigators without knowledge of the identity nor treatment of the cells. Results are the means ± 1 S.E. calculated from three independent experiments.

Phosphorylation of MLC alters myosin organization in a variety of cell types (4-8,13-17). MLC phosphorylation also occurs in CHO-m3 cells incubated with carbachol or PMA (Fig. 3). Densitometry analysis indicates that MLC phosphorylation is increased by 319 ± 80% in carbachol-treated cells and 199 ± 57% in PMA-treated cells, compared with untreated cells (p < 0.05, n = 3). MLC phosphorylation is more effectively induced by carbachol than by PMA in CHO-m3 cells (Fig. 3), consistent with greater stress fiber formation induced by carbachol than by PMA (Fig. 2).


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  		Fig. 3.   Phosphorylation of MLC is enhanced by treatment with carbachol or PMA. CHO-m3 cells labeled with inorganic 32P were incubated with 10 µM carbachol, 10 nM PMA, or no drug for 60 min and lysed in 1% Triton X-100. The phosphorylated 20-kDa MLC in the Triton X-100-insoluble pellet from cells treated with no drug (lane 1), carbachol (lane 2), or PMA (lane 3) was identified by anti-MLC antibody in Western blots (a) and by autoradiography (b). The Western blot has smaller lane widths than the autoradiograph because the channels in which the antibodies were applied in the Western blot were a smaller width than the wells in which proteins were applied to the polyacrylamide gel. Results shown are representative of three independent experiments which produced similar results.

Conventional PKC Isoforms Are Activated by M3 mAChR Stimulation and Are Required for mAChR-mediated Myosin Reorganization-- CHO-m3 cells were immunofluorescently stained with antibodies to different PKC isoforms to determine whether mAChR agonists or PMA induce PKC translocation, which indicates PKC activation (30). Immunofluorescent staining of PKC-beta , -gamma , -epsilon , and -iota in CHO-m3 cells was undetectable, and immunofluorescent staining of PKC-delta and -µ produced a diffuse cytosolic pattern that was not detectably altered by PMA or carbachol treatment (data not shown). In contrast, PKC-alpha is diffusely distributed in the cytosol of untreated CHO-m3 cells (Fig. 4a, panel A), and localizes to cell-cell junctions within 15 min of exposure to carbachol (Fig. 4a, panel B). PKC-alpha remains at cell-cell junctions for over 24 h in the continuous presence of carbachol (Fig. 4a, panel D). Treatment with PMA increases PKC-alpha at cell-cell junctions and at regions of membrane ruffling (Fig. 4a, panel E). However, PKC-alpha is undetectable at cell-cell junctions or membrane ruffles after 24 h of PMA treatment (Fig. 4a, panel F).


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  		Fig. 4.   Translocation and degradation of PKC isoforms occurs in CHO-m3 cells treated with carbachol or PMA. a, CHO-m3 cells were untreated (A) or incubated with 10 µM carbachol for 15 min (B), 45 min (C), or 24 h (D) or incubated with 10 nM PMA for 15 min (E) or 24 h (F). All cells were immunofluorescently labeled with an antibody to PKC-alpha . Bar represents 15 µm. b, CHO-m3 cells were untreated, or incubated with 1 mM carbachol or 1 µM PMA for 24 h and lysed. The lysates were probed by ECL Western blotting using PKC isoform-specific antibodies. Densitometry of the ECL Western blots was performed to determine the percent of PKC isoform levels remaining in the drug-treated cells compared with untreated control cells. Results are the means ± 1 S.E. from three independent experiments. c, representative ECL Western blots from the experiments described in b.

Activation of PKC results in degradation of the enzyme; this effect is most evident when PKC is activated by phorbol esters (31, 32), but it can also occur when PKC is activated by Ca2+ and diacylglycerol (33). Degradation of PKC isoforms was measured to characterize further which isoforms are activated by PMA or M3 mAChR stimulation (Fig. 4, b and c). PKC-alpha , -delta , -iota , and -µ were detected by Western blotting of CHO-m3 cell lysates. Levels of PKC-alpha are significantly diminished by PMA but only minimally affected by carbachol (Fig. 4, b and c). This finding is consistent with the sustained presence of translocated PKC-alpha at cell membranes in carbachol-treated CHO-m3 cells (Fig. 4a, panel D) and the loss of translocated PKC-alpha in PMA-treated cells (Fig. 4a, panel F). Prolonged exposure to PMA or carbachol significantly diminishes the levels of PKC-delta and -iota but does not diminish PKC-µ (Fig. 4, b and c). These results indicate that conventional (alpha ), novel (delta ), and atypical (iota ) PKC isoforms are activated by PMA or carbachol in CHO-m3 cells.

The effects of specific PKC antagonists on myosin reorganization were investigated to determine the participation of different PKC isoforms in carbachol-induced cytoskeletal reorganization (Fig. 5). Previous in vitro studies using purified PKC isoforms indicate that conventional and novel PKC isoforms are inhibited by calphostin C (IC50 = 0.05 µM) and chelerythrine (IC50 = 0.66 µM) (34, 35), whereas only the conventional PKC isoforms are inhibited by Go6976 (IC50 = 0.006 µM) (36). These PKC antagonists also inhibit other purified kinases such as PKA when the antagonist concentrations exceed 50-170 µM (34-36). Carbachol-mediated stress fiber formation in CHO-m3 cells is inhibited by calphostin C (IC50 = 2.4 ± 0.3 µM), chelerythrine (IC50 = 8.0 ± 0.5 µM), and Go6976 (IC50 = 0.4 ± 0.02 µM) (Fig. 5). Calphostin C and chelerythrine inhibit both cell spreading and stress fiber formation (Fig. 5a, panels C and D), whereas Go6976 inhibits stress fiber formation but not cell spreading (Fig. 5a, panel E). The ability of Go6976 to inhibit mAChR-mediated stress fiber formation indicates that conventional PKC isoforms are required for mAChR-mediated stress fiber formation.


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  		Fig. 5.   Kinase antagonists inhibit the formation of myosin-containing stress fibers in CHO-m3 cells. a, CHO-m3 cells were untreated (A) or incubated with 10 µM carbachol (B-H) for 90 min. Before being exposed to carbachol, the cells were preincubated for 30 min with 4 µM calphostin C (C), 10 µM chelerythrine (D), 2 µM Go6976 (E), 2 µM KT5926 (F), 40 µM ML-7 (G), or 100 µM ML-7 (H). All cells were immunofluorescently labeled with the SA-2 antibody to myosin. Bar represents 15 µm. b, CHO-m3 cells were preincubated for 30 min with no antagonist (control cells) or with antagonists selective for PKC (A), CaMKII (B), or MLCK (C). The cells were then incubated with 10 µM carbachol for 90 min and immunofluorescently labeled with the SA-2 antibody to myosin. The presence of myosin-containing stress fibers in the cells was scored by two independent investigators without knowledge of the cell treatments. These scores were used to calculate the percent of carbachol-induced stress fiber formation in cells exposed to antagonist, compared with cells that were not exposed to antagonists. Results are the means ± 1 S.E. calculated from three to six independent experiments.

Intracellular Ca2+ mobilized by M3 mAChR stimulation may enhance activation of conventional PKC isoforms, which differ from other PKC isoforms by being sensitive to Ca2+ (reviewed in Ref. 30). Other Ca2+-dependent kinases, such as Ca2+/ calmodulin-dependent protein kinase II (CaMKII) or MLCK, may also participate in myosin reorganization. The role of CaMKII in mAChR-mediated stress fiber formation was tested using the antagonists KN-62 and KT5926. KN-62 specifically inhibits the in vitro activity of CaMKII (IC50 = 0.90 µM) (37), whereas KT5926 inhibits the in vitro activities of several kinases, including CaMKII (IC50 = 0.004 µM), MLCK (IC50 = 0.018 µM), and PKC (IC50 = 0.72 µM) (38, 39). Myosin reorganization induced by M3 mAChR activation is not affected by KN-62 at concentrations up to 20 µM, but it is inhibited by KT5926 (IC50 = 0.6 ± 0.04 µM) (Fig. 5). Interestingly, KT5926 induces the same morphological effects as the PKC antagonist Go6976; the cells are well spread but lack detectable stress fibers after M3 mAChR activation (Fig. 5a, panel F).

The effects of the MLCK antagonists ML-7 and ML-9 on mAChR-mediated stress fiber formation were also determined (Fig. 5). ML-7 and ML-9 were previously found to inhibit MLCK activity (IC50 = 0.3 and 3.8 µM, respectively) as well as PKC activity (IC50 = 42 and 54 µM, respectively) (40-42). We found that mAChR-mediated stress fiber formation is inhibited by ML-7 (IC50 = 75 ± 6.9 µM) and by ML-9 (IC50 = 82 ± 5.8 µM) (Fig. 5). Cells treated with 40 µM ML-7 continue to exhibit carbachol-induced stress fibers even though cell spreading is diminished (Fig. 5a, panel G). Carbachol-induced stress fibers are lost only when the cells are treated with high enough concentrations of ML-7 to cause the cells to detach from the substratum (Fig. 5a, panel H). Similar morphological effects were induced by comparable concentrations of the MLCK antagonist ML-9 (data not shown).

Inactivation of RhoA Diminishes but Does Not Abolish Stress Fiber Formation Induced by M3 mAChR Activation-- The involvement of RhoA in myosin organization was investigated using CHO-m3 cells stably transfected with HA-tagged wild-type or mutant RhoA. Two independent clonal CHO-m3 cell lines expressing HA-RhoA were generated and named m3WTRho-1 and m3WTRho-11. Two independent clonal CHO-m3 cell lines expressing constitutively active HA-RhoAVal-14 were named m3CARho-1 and m3CARho-4, and three independent clonal lines expressing dominant negative HA-RhoAAsn-19 were named m3DNRho-2, m3DNRho-4, and m3DNRho-6. These cell lines express similar levels of HA-tagged wild-type or mutant RhoA (Fig. 6a). Two independent clonal CHO-m3 cell lines stably transfected with only the pZeoSV2 plasmid, named m3Zeo-1 and m3Zeo-2, do not express HA (Fig. 6a). Similar levels of M3 mAChR are expressed by these cell lines and parental CHO-m3 cells, as indicated by [3H]N-methylscopolamine binding (data not shown). Proximal signal transduction by M3 mAChR is also similar in these cell lines, as indicated by carbachol-induced Ca2+ mobilization (Fig. 6b).


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  		Fig. 6.   Characterization of CHO-m3 cells stably expressing HA-tagged wild-type or mutant RhoA or electroporated with C3 exoenzyme. a, equal amounts of lysates from the indicated cell lines were probed with antibody to HA in ECL Western blots. A representative ECL Western blot is shown. Similar results were obtained in four other independent experiments. b, calcium mobilization induced by 10 µM carbachol (applied at 30 s) is similar in parental CHO-m3, m3Zeo-2, and m3DNRho-4 cells. Carbachol similarly mobilized Ca2+ in the other CHO-m3 sublines (data not shown). c, C3 exoenzyme ADP-ribosylates RhoA in CHO-m3 cells. Lysates were prepared from parental CHO-m3 cells cultured in vivo in the absence (lanes 1 and 3) or presence (lane 2) of C3 exoenzyme. The lysates were incubated in vitro with [32P]NAD in the absence (lane 3) or presence (lane 1 and 2) of C3 exoenzyme. The samples were probed with RhoA antibody (Western blot) and subjected to autoradiography (Autoradiograph). The striped and open rectangles indicate the positions of RhoA that migrated slower and faster, respectively.

Expression of constitutively active RhoAVal-14 induces the formation of myosin-containing stress fibers (Fig. 7a, panel D, and b). Carbachol increases stress fiber formation in all the sublines (Fig. 7). However, carbachol-induced stress fiber formation is diminished in cells expressing dominant negative RhoAAsn-19, compared with the other cell lines (Fig. 7a, panel G, and b).


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  		Fig. 7.   Stable expression of mutant RhoA alters myosin organization in the CHO-m3 sublines. a, m3Zeo-2 (A and E), m3WTRho-1 (B and F), m3DNRho-4 (C and G), and m3CARho-4 (D and H) cells were incubated in the absence (A-D) or presence (E-H) of carbachol (10 µM, 90 min). The cells were immunofluorescently labeled with the SA-2 myosin antibody. Bar represents 15 µm. b, control cell lines (solid bars) and cell lines expressing wild-type RhoA (open bars), constitutively active RhoAVal-14 (dotted bars), or dominant negative RhoAAsn-19 (striped bars) were incubated in the absence or presence of 10 µM carbachol for 90 min. The cells were immunofluorescently labeled with the SA-2 antibody to myosin. The presence of myosin-containing stress fibers in the cells was scored by two independent investigators without knowledge of the identity nor treatment of the cells. Results are the means ± 1 S.E. calculated from two to six independent experiments.

Since expression of dominant negative RhoAAsn-19 diminishes carbachol-induced stress fiber formation (Fig. 7), we investigated the effects of expressing dominant negative RhoAAsn-19 on PMA-induced stress fiber formation (Fig. 8). Interestingly, PMA treatment induces similar increases in stress fiber formation in cells expressing dominant negative RhoAAsn-19 and in the control cell lines (Fig. 8). These results indicate that expressing dominant negative RhoAAsn-19 does not alter PMA-induced stress fiber formation.


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  		Fig. 8.   Expression of dominant negative RhoAAsn-19 does not alter PMA-induced myosin reorganization. a, m3Zeo-2 (A and B) and m3DNRho-4 (C and D) cells were incubated in the absence (A and C) or presence (B and D) of PMA (10 nM, 90 min). The cells were immunofluorescently labeled with the SA-2 myosin antibody. Bar represents 15 µm. b, control cell lines (solid bars) and cell lines expressing dominant negative RhoAAsn-19 (striped bars) were incubated in the absence or presence of 10 nM PMA for 90 min and immunofluorescently labeled with the SA-2 myosin antibody. The presence of myosin-containing stress fibers in the cells was scored by two independent investigators without knowledge of the identity nor treatment of the cells. Results are the means ± 1 S.E. calculated from three independent experiments.

Some reports indicate that ADP-ribosylation of Rho by C3 exoenzyme more effectively produces an altered phenotype than expression of dominant negative RhoAAsn-19 (43, 44). CHO-m3 cells were electroporated with C3 exoenzyme to determine the effects of inactivating Rho by ADP-ribosylation. The ability of C3 exoenzyme to ribosylate Rho in CHO-m3 cells was tested in [32P]ADP-ribosylation assays (Fig. 6c). Ribosylation by C3 exoenzyme slows the migration of RhoA in Western blots (lanes 1 and 2, Western blot, Fig. 6c). Addition of C3 exoenzyme to lysates of untreated CHO-m3 cells causes [32P]ADP-ribosylation of a protein (lane 1, Autoradiograph, Fig. 6c) which co-migrates with the slower migrating form of RhoA (lane 1, Western blot, Fig. 6c). In contrast, [32P]ADP-ribosylation is greatly diminished if the cells are treated with C3 exoenzyme in vivo prior to adding C3 exoenzyme to the cell lysates (lane 2, Autoradiograph, Fig. 6c). These results indicate that RhoA in cells treated with C3 exoenzyme is ADP-ribosylated in situ and subsequently cannot be [32P]ADP-ribosylated by C3 exoenzyme in vitro.

Inactivation of Rho with C3 exoenzyme inhibits CHO-m3 cytokinesis, resulting in multinucleate cells (Fig. 9, panel B). Although these cells are abnormally spread and elongated, they exhibit a diffuse cytosolic distribution of myosin similar to cells electroporated in the absence of C3 exoenzyme (Fig. 9). Activation of M3 mAChR induces the formation of stress fibers in cells electroporated with C3 exoenzyme (Fig. 9, panel D), although stress fiber formation is somewhat diminished compared with untreated cells. These results indicate that myosin reorganization induced by M3 mAChR activation is reduced but not abolished by Rho inactivation.


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  		Fig. 9.   Rho inactivation with C3 exoenzyme causes CHO-m3 cells to become multi-nucleate, but does not abolish carbachol- or PMA-induced myosin reorganization. CHO-m3 cells were electroporated in the absence (A, C, and E) or presence (B, D, and F) of recombinant C3 exoenzyme (15 µg/ml) and cultured for 2 days. The cells were incubated for 90 min with no drug (A and B), 10 µM carbachol (C and D), or 10 nM PMA (E and F). Myosin was labeled with the SA-2 antibody, and nuclei were labeled with propidium iodide. The left side of each panel shows myosin and nuclei, and the right side of each panel shows only nuclei. Bar represents 15 µm.


    DISCUSSION
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
REFERENCES

This study demonstrates that M1 or M3 mAChR activation profoundly alters myosin organization in CHO cells. Conventional PKC isoforms and Rho proteins participate in the mAChR-mediated formation of myosin stress fibers, as depicted in the model shown in Fig. 10. Similar pathways of mAChR-mediated myosin reorganization occur in CHO cells and smooth muscle cells, although some differences exist. Comparing these pathways provides insight into the mAChR-mediated mechanisms controlling myosin organization.


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  		Fig. 10.   A model depicting the involvement of PKC and Rho in myosin reorganization induced by M3 mAChR activation. PKC and Rho may participate in independent but parallel pathways to induce myosin reorganization following M3 mAChR activation. We found that Rho inactivation diminishes but does not abolish mAChR-mediated myosin reorganization. This finding indicates that the PKC-mediated pathway of myosin reorganization can continue to operate when Rho is inactive. In contrast, PKC inactivation completely abolishes mAChR-mediated myosin reorganization. This result may occur because PKC activity is required for mAChR-mediated signaling to Rho. The depicted regulation of MLC phosphorylation by PKC and Rho and the effects of MLC phosphorylation on stress fiber formation are based on previous studies (reviewed in Refs. 9-12).

Role of PKC in mAChR-mediated Myosin Reorganization-- PKC participates in mAChR-mediated myosin reorganization in CHO cells. This conclusion is supported by our finding that M3 mAChR stimulation or PMA treatment activates several PKC isoforms and induces myosin stress fiber formation in these cells. Our finding that myosin reorganization is induced by the M1 but not the M2 mAChR subtype also supports this conclusion, since the M1 but not the M2 mAChR subtype activates PKC (2, 3).

The effects of the PKC antagonists Go6976, calphostin C, and chelerythrine provide compelling evidence that conventional PKC isoforms are required for myosin reorganization. Both mAChR-mediated stress fiber formation and cell spreading are inhibited by calphostin C or chelerythrine, which antagonize conventional and novel PKC isoforms (34, 35). In contrast, only mAChR-mediated myosin reorganization is inhibited by Go6976, which specifically antagonizes conventional PKC isoforms (36). It is generally believed that PKC activation is required for cell spreading, and other signals are required for cytoskeletal reorganization (45-51). Our findings suggest that while the novel PKC isoforms are needed for cell spreading, the conventional PKC isoforms are needed for myosin reorganization.

The concentrations of Go6976, calphostin C, or chelerythrine which inhibit myosin reorganization in CHO cells are approximately 10-70-fold higher than those that inhibit PKC in vitro (34-36). Higher concentrations of these drugs may be needed in vivo for the antagonists to cross the cell membrane and gain access to intracellular PKC, in contrast to in vitro studies in which the antagonists interact directly with purified PKC. Despite this requirement for higher drug concentrations in vivo, these antagonists still inhibit myosin reorganization more effectively in vivo than they inhibit other kinases such as PKA in vitro. This finding indicates that these antagonists inhibit myosin reorganization by inactivating PKC.

The ability of PKC to regulate myosin organization in CHO cells is consistent with the effects of PKC activation on smooth muscle myosin. Activation of PKC with phorbol esters enhances MLC phosphorylation in smooth muscle cells and induces sustained contraction of different smooth muscle tissues (reviewed in Ref. 10). Phosphorylation of MLC increases actin-myosin interactions by inducing the formation of bipolar myosin filaments and exposing actin-binding sites on myosin (reviewed in Refs. 9-12). PKC can directly phosphorylate MLC (52, 53) or enhance MLC phosphorylation by inhibiting MLC phosphatase (54). It is believed that smooth muscle contraction induced by phorbol esters involves the PKC-dependent inhibition of MLC phosphatase, rather than direct phosphorylation of MLC by PKC (reviewed in Refs. 9-11). PKC activation may similarly enhance MLC phosphorylation in CHO cells by inhibiting MLC dephosphorylation, as depicted in Fig. 10.

Although PKC is required for carbachol-induced myosin reorganization in CHO-m3 cells, the role of PKC in the mAChR-mediated regulation of smooth muscle myosin is less clear. PKC antagonists inhibit carbachol-induced contractions in some types of smooth muscle (55) but not in others (56). These variable responses may be due to the expression of different mAChR subtypes or PKC isoforms by different types of smooth muscle.

It was previously shown that PKC activation induces or enhances the formation of actin-containing stress fibers in some types of non-muscle cells (45, 47, 57) but not in others (58). These results indicate that PKC activation has cell type-specific effects on stress fiber formation. These specific effects may be due to altered PKC isoform expression or dissimilarities in PKC-mediated signaling pathways among different cell types.

Activation of M3 mAChR induces greater MLC phosphorylation and myosin reorganization than does treatment with PMA in CHO cells. We found that PKC-alpha remains at the junctions of carbachol-treated cells longer than it does in PMA-treated cells, indicating that mAChR stimulation and PMA treatment have different effects on PKC-alpha . These differences may contribute to the greater stress fiber formation induced by carbachol compared with PMA, as well as the sustained elongation of CHO-m3 cells which occurs during prolonged carbachol exposure (Fig. 1, panel D, and Fig. 4a, panel D) (21, 22).

Role of RhoA in mAChR-mediated Myosin Reorganization-- Increased stress fiber formation in cells expressing constitutively active RhoAVal-14 indicates that active RhoA contributes to myosin reorganization in CHO-m3 cells. However, active RhoA is not essential for mAChR-mediated myosin reorganization in CHO-m3 cells. This conclusion is supported by our finding that carbachol-induced stress fiber formation is diminished but not abolished in CHO-m3 cells expressing dominant negative RhoAAsn-19 or treated with C3 exoenzyme. Expression of dominant negative RhoAAsn-19 may specifically inhibit RhoA activity because dominant negative RhoAAsn-19 competitively interacts with RhoA regulatory proteins. In contrast, C3 exoenzyme can ADP-ribosylate several forms of Rho, including RhoA and RhoB (59), resulting in potentially greater Rho inactivation than that produced by expressing dominant negative RhoAAsn-19. Consistent with these possibilities, we found that the morphology of CHO-m3 cells is altered more drastically by C3 exoenzyme than by expression of dominant negative RhoAAsn-19.

Treatment with C3 exoenzyme causes CHO-m3 cells to become multi-nucleate, which is an indication of Rho inactivation (60-62). If Rho is inactive in dividing cells, the actomyosin contractile ring at the cleavage furrow does not function properly and cytokinesis is inhibited, resulting in multi-nucleate cells (61, 62). The ability of carbachol to induce stress fiber formation in multi-nucleate, C3 exoenzyme-treated CHO-m3 cells provides strong evidence that mAChR-mediated stress fiber formation still occurs even when Rho is inactive.

Although Rho is apparently not essential for stress fiber formation induced by mAChR activation, Rho may be required for stress fiber formation induced by other agonists. Rho must be active for bombesin or lysophosphatidic acid (LPA) to induce stress fiber formation in serum-starved Swiss 3T3 cells (58, 63). Bombesin- or LPA-dependent stress fiber formation is significantly diminished by 27 µM genistein and is completely abolished by 110 µM genistein, indicating that a tyrosine kinase is required for stress fiber formation induced by these agonists (58). In contrast, we found that genistein concentrations up to 180 µM do not alter mAChR-mediated stress fiber formation (data not shown). These findings indicate that different Rho-mediated signaling pathways leading to stress fiber formation are induced by bombesin or LPA in serum-starved Swiss 3T3 cells and by mAChR activation in exponentially proliferating CHO-m3 cells.

Rho inactivation diminishes the agonist-induced contraction of smooth muscle (17, 64-68). Carbachol-induced contraction of tracheal (66), ileal (68), and longitudinal intestinal (17, 67) smooth muscle strips is diminished by treatment with C3 exoenzyme. Phosphorylation of MLC induced by carbachol (17) or other agonists (reviewed in Ref. 10) is also diminished by inactivating Rho in smooth muscle. These and other findings support the model that Rho participates in contraction by enhancing MLC phosphorylation (reviewed in Refs. 10-12). Active Rho proteins can enhance MLC phosphorylation by inhibiting MLC phosphatase (69) or by activating Rho kinase, which directly phosphorylates MLC (70, 71). We are investigating the possibility that Rho proteins similarly regulate myosin organization in CHO cells by altering MLC phosphorylation, as depicted in Fig. 10. This possibility is supported by studies demonstrating that Rho inactivation diminishes MLC phosphorylation in non-muscle cells (8, 72).

Rho inactivation in CHO-m3 cells does not diminish PMA-induced myosin reorganization, even though it diminishes mAChR-mediated myosin reorganization. These findings are consistent with a report that Rho inactivation does not affect phorbol ester-induced contraction of cerebrovascular smooth muscle but inhibits serotonin-induced contraction of the same tissue (64). These results may occur because Rho and PKC participate in separate signaling pathways to regulate myosin organization, as depicted in Fig. 10. According to this model, PKC induces myosin reorganization independently of Rho. This model explains why Rho inactivation does not affect PMA-induced myosin reorganization but diminishes mAChR-mediated myosin reorganization. This model also explains why Rho inactivation does not completely abolish mAChR-mediated stress fiber formation; mAChR-mediated activation of PKC induces myosin reorganization even when Rho is inactive.

We found that PKC antagonists completely abolish mAChR-mediated stress fiber formation. This finding indicates that PKC inactivation inhibits both Rho- and PKC-dependent myosin reorganization induced by mAChR stimulation. This result may occur because PKC inactivation inhibits mAChR-mediated signaling to Rho. PKC may act in parallel with several other effectors to activate Rho following mAChR stimulation. If this possibility is correct, then PKC antagonists should inhibit mAChR-mediated activation of Rho and subsequent Rho-dependent myosin reorganization. This model does not predict that PKC activation can independently activate Rho, because other mAChR-mediated signals in addition to PKC activation may be needed to stimulate Rho activity.

Role of MLCK in mAChR-mediated Myosin Reorganization-- Many studies indicate that MLCK plays a central role in regulating myosin activity in muscle and non-muscle cells (reviewed in Refs. 9-12). Intracellular Ca2+ mobilized by M1 or M3 mAChR stimulation can activate MLCK, resulting in MLC phosphorylation and subsequent contraction of smooth muscle (13-16). Activation of MLCK in non-muscle cells similarly affects myosin activity (5, 6, 73). Thus, it is reasonable to assume that MLCK participates in mAChR-mediated myosin reorganization in CHO-m3 cells. However, the effects of the MLCK antagonists do not support the assumption that MLCK contributes to mAChR-mediated myosin reorganization in CHO-m3 cells. Very high concentrations of the MLCK antagonists ML-7 and ML-9 are needed to inhibit mAChR-mediated stress fiber formation in CHO-m3 cells. Carbachol-induced stress fiber formation in CHO-m3 cells is half-maximally inhibited by 75 µM ML-7 or 82 µM ML-9 and maximally inhibited by 100 µM ML-7 or 120 µM ML-9. These concentrations exceed those needed to inhibit MLCK, PKA, or PKC activity in vitro (40-42). The high antagonist concentrations needed to inhibit CHO-m3 microfilament formation do not simply reflect an inability of the drugs to enter the cells. Other studies demonstrated that concentrations as low as 3 µM ML-7 or 5 µM ML-9 can significantly affect in vivo processes (74). We found that 40 µM ML-7 diminishes mAChR-mediated cell spreading (Fig. 5a, panel G), indicating that effective intracellular concentrations of ML-7 and ML-9 accumulate in CHO-m3 cells even when the cells are exposed to relatively low antagonist concentrations. Thus, the higher ML-7 and ML-9 concentrations needed to inhibit mAChR-mediated stress fiber formation (100 and 120 µM, respectively) indicate that these MLCK antagonists may affect myosin organization by inactivating other kinases, such as PKC.

Incubation of CHO-m3 cells with 2 µM KT5926 abolishes mAChR-mediated stress fiber formation but not cell spreading (Fig. 5a, panel F). The effects of KT5926 are probably not mediated by CaMKII, since the CaMKII antagonist KN-62 does not affect mAChR-mediated myosin reorganization. Instead, KT5926 probably inhibits myosin reorganization by diminishing MLCK or PKC activity. Choi and colleagues (73) concluded that KT5926 inactivates both PKC and MLCK, based on their finding that 1 µM KT5926 inhibits both PKC-dependent and MLCK-dependent phosphorylation of MLC in rat basophilic RBL-2H3 cells. This result is consistent with our observation that KT5926 induces the same effects as the PKC antagonist Go6976 in CHO-m3 cells (Fig. 5a, panels E and F). Thus, the effects of KT5926 on mAChR-mediated myosin reorganization may involve inactivation of PKC.

Although MLCK can be activated by mAChR-mediated increases in intracellular Ca2+, it is possible that other kinases diminish MLCK activity following mAChR stimulation. CaMKII can phosphorylate MLCK and reduce the affinity of MLCK for Ca2+/calmodulin, diminishing MLCK activity (reviewed in Refs. 9-11). Thus, it is conceivable that mAChR stimulation does not significantly increase MLCK activity in CHO-m3 cells, due to concomitant mAChR-mediated activation of CaMKII. Previous studies demonstrated that mAChR or PKC stimulation can induce smooth muscle contraction in the absence of MLCK activity, indicating that MLCK activity is not absolutely required for mAChR- or PKC-dependent activation of myosin (75, 76).

The potential lack of MLCK participation in mAChR-mediated myosin reorganization may explain why myosin-containing stress fibers form in CHO-m3 cells only after prolonged exposure to carbachol. If mAChR stimulation does not activate MLCK, MLC phosphorylation may only slowly increase due to a PKC- and Rho-mediated inhibition of MLC phosphatase, resulting in a gradual increase in myosin-containing stress fibers. This possibility is consistent with reports that much slower smooth muscle contractions are induced by carbachol or PMA when MLCK is inactive, compared when MLCK is active (75, 76).

Conclusions-- This study provides the first evidence that M1 or M3 mAChR activation induces myosin reorganization in non-muscle cells. Both PKC and Rho participate in mAChR-mediated myosin reorganization in CHO-m3 cells. PKC and Rho also participate in the mAChR-mediated regulation of smooth muscle myosin. These findings indicate that mAChR regulate myosin activity by similar mechanisms in CHO cells and smooth muscle. The CHO sublines transfected with mAChR subtypes provide a useful system for elucidating receptor-mediated signals affecting myosin activity in both muscle and non-muscle cells.

The M1 and M3 mAChR subtypes have a unique ability to modulate the morphology (21, 22), adhesion (18-20), and proliferation (25, 77-80) of non-muscle cells. Changes in myosin activity also significantly alter the morphology, adhesion, and division of non-muscle cells (reviewed in Ref. 12). The ability of M1 or M3 mAChR to regulate non-muscle myosin suggests that some of the unique effects of activating these receptors may involve changes in cytoplasmic myosin activity.

    ACKNOWLEDGEMENTS

We thank Dr. Shinya Kuroda (Nara Institute of Science and Technology, Nara, Japan) for the generous gift of the pEF-BOS-HA-RhoA and pEF-BOS-HA-RhoAVal-14 plasmids and Jeff Mattison and Thomas Shay for excellent technical assistance.

    FOOTNOTES

* The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.

** To whom correspondence should be addressed: Molecular Pharmacology Laboratory, Guthrie Research Institute, Sayre, PA 18840. Tel.: 570-882-4650; Fax: 570-882-5151; E-mail: cwilliam{at}inet.guthrie.org.

    ABBREVIATIONS

The abbreviations used are: mAChR, muscarinic acetylcholine receptor; BSA, bovine serum albumin; CaMKII, Ca2+/calmodulin-dependent protein kinase II; CHO, Chinese hamster ovary; FCS, fetal calf serum; HA, hemagglutinin; LPA, lysophosphatidic acid; MLC, myosin light chain; MLCK, myosin light chain kinase; PKA, protein kinase A; PKC, protein kinase C; PMA, phorbol 12-myristate 13-acetate; PBS, phosphate-buffered saline; PVDF, polyvinylidene difluoride.

    REFERENCES
TOP
ABSTRACT
INTRODUCTION
EXPERIMENTAL PROCEDURES
RESULTS
DISCUSSION
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