Serotonin or 5-hydroxytryptamine (5-HT) influences numerous functions in the gastrointestinal tract. We previously demonstrated that 5-HT treatment of Caco-2 cells inhibited Na+/H+ exchangers (NHE) and Cl−/OH− exchange activities via distinct signaling mechanisms. Since regulation of several ion transporters such as NHE3 is influenced by intact cytoskeleton, we hypothesized that 5-HT modifies actin cytoskeleton and/or brush-border membrane architecture via involvement of signaling pathways. Ultrastructural analysis showed that 5-HT (0.1 μM, 1 h) treatment of Caco-2 cells caused the apical membrane to assume a convex dome shape that was associated with shortening of microvilli. To examine whether these cellular architecture changes are cytoskeleton driven, we analyzed actin cytoskeleton by fluorescence microscopy. 5-HT induced basal stress fibers with prominent cortical actin filaments via 5-HT3 and 5-HT4 receptor subtypes. This induction was partially attenuated by chelation of intracellular Ca2+ and PKCα inhibition (Go6976). In vitro assays revealed that PKCα interacted with actin and this association was increased by 5-HT. Our data provide novel evidence that 5-HT-induced signaling via 5-HT3/4 receptor subtypes to cause Ca2+ and PKCα-dependent regulation of actin cytoskeleton may play an important role in modulation of ion transporters that contribute to pathophysiology of diarrheal conditions associated with elevated levels of 5-HT.
- serotonin and actin
- 5-HT and curvature
- stress fibers
- ion transporter
serotonin (5-HT) is an important hormone and neurotransmitter that influences diverse functions in the gastrointestinal tract. High levels of 5-HT have been implicated in several diarrheal conditions associated with inflammatory bowel diseases or carcinoid syndrome (3, 5, 23, 37). We have previously shown that 5-HT inhibits Na+/H+ exchange (NHE) and Cl−/OH− exchange activities in human intestinal epithelial cells via 5-HT4 and 5-HT3/4 receptor subtypes, respectively (16, 31). The 5-HT-mediated inhibition in NHE2 and NHE3 activity occurred via a signal transduction pathway involving sequential activation of c-Src kinases, PLCγ1 and Ca2+-dependent PKCα (16). In contrast, 5-HT inhibited Cl−/OH− exchange activity via a Ca2+-independent pathway involving Src-kinase induced activation of PKCδ (31). Furthermore, recent studies have shown that 5-HT causes cytoskeletal reorganization via 5-HT4 receptors to induce pulmonary artery smooth muscle cell migration (10). However, nothing is known regarding the regulation of major cytoskeletal elements such as actin by 5-HT in intestinal epithelial cells.
A number of ion transporters such as members of NHE gene family have been shown to interact with the cytoskeleton (40). Microfilaments have been suggested to maintain basal activity of NHE3 and have also been implicated in transducing regulatory signals from receptors or hormones. For example, binding of NHE3 to the cytoskeletal binding proteins is an important factor for its inhibition by cAMP/protein kinase A-, Ca2+-, or cGMP/PKG-mediated pathways (4, 22, 24, 36, 39). Increasing evidence suggests that distinct signaling molecules interact with cytoskeleton to mediate physiological functions (14). In addition, a role for the actin cytoskeleton has emerged during clathrin- and caveolin-mediated endocytosis and exocytosis (29, 34). Our previous studies suggested that 5-HT induced inhibition of NHE activity involved Vmax changes indicating the involvement of membrane trafficking events (16). Hence, elucidating the role of 5-HT in cytoskeleton modification and/or cellular architecture warrants further investigations.
In light of 5-HT being an important signaling molecule, the aim of the present studies was to assess whether 5-HT causes modification in brush-border membrane architecture and cellular cytoskeletal proteins in the human intestinal epithelial cells. Our studies showed for the first time that 5-HT treatment of human intestinal epithelial monolayers altered the apical membrane curvature and induced prominent actin cytoskeletal reorganization. The underlying mechanisms of 5-HT-induced actin cytoskeletal reorganization required 5-HT3/4 receptor subtypes as well as Ca2+- and PKCα-dependent pathways. Additionally, PKCα was shown to interact with F-actin, and this association was significantly increased by 5-HT treatment. These studies have potential significance in increasing our understanding of 5-HT-mediated effects on intestinal ion transport processes in general and NHE3 in particular. Furthermore, identifying distinct mechanisms by which 5-HT modulates cytoskeleton or cellular architecture is crucial for defining various effects of 5-HT such as modulation of intestinal electrolyte absorption, secretion or motility.
MATERIALS AND METHODS
5-HT was obtained as creatinine sulfate complex from Sigma Chemical (St. Louis, MO). Caco-2 cells were obtained from ATCC (American Type Culture Collection, Manassas, VA). Bisindolylmaleimide (BIM), Go6976, BAPTA-AM, and rottlerin were obtained from Biomol (Plymouth Meeting, PA). 5-HT4 agonist 2-[1-(4-pieronyl)piperazinyl] benzothiazole and 5-HT3 agonist (m-chlorophenylbiguanide) were procured from Tocris (Ellisville, MO). PKC isoform antibodies were obtained from Santa Cruz (Santa Cruz, CA). Anti-actin antibody was from Sigma Chemical. All other chemicals were of at least reagent grade and were obtained from Sigma Chemical or Fisher Scientific (Pittsburgh, PA), etc.
Caco-2 cells were grown routinely in 75-cm2 plastic flasks at 37°C in a 5% CO2-95% air environment. The culture medium consisted of DMEM, 20% FBS, 100 IU/ml penicillin, and 100 μg/ml streptomycin. Cells reached confluence after 4–5 days in culture and were used for these studies between passages 25 and 55. Caco-2 cells were plated on Transwell inserts (Costar, Corning, NY) at a density of 4 × 104 cells/Transwell and used 12–14 days postplating. Cells were treated with 5-HT (0.1 μM) from either the apical side or the basolateral side for 60 min. In separate set of experiments, Caco-2 cells were pretreated with different inhibitors of PKC, Ca2+ (BAPTA-AM), in the Caco-2 medium for 1 h before the addition of 5-HT and then coincubated along with 5-HT for another 1 h as indicated in various figure legends.
Quantitative analysis of phalloidin binding.
Quantitative analysis of phalloidin binding was used to determine F-actin content as previously described (33). Cell monolayers were fixed with 3% paraformaldehyde in Hanks’ buffered saline solution (HBSS) at indicated times after 5-HT treatment. After fixation, the cell monolayer were washed twice with HBSS, permeabilized for 15 min in HBSS with 0.5% saponin (wt/vol), and incubated with 0.5 mM Alexa Fluor 488-conjugated phalloidin (Invitrogen) for 1 h at room temperature. Unbound phalloidin was removed by five washes in HBSS. Bound Alexa Fluor 488-conjugated phalloidin was then extracted quantitatively by incubation for 18 h at 4°C (in the dark) in 100% methanol. The fluorescent intensity of the extracted Alexa Fluor 488-conjugated phalloidin was measured on an Ultrospec 3300 fluorescent plate reader (Molecular Dynamics, Sunnyvale, CA).
Caco-2 cells were grown in 35-mm tissue culture dishes, washed with phosphate-buffered saline and initially fixed with 2.5% glutaraldehyde in 0.1 M sodium cacodylate (pH 7.4) buffer. The cells were postfixed with 1% osmium tetroxide and dehydrated in a series of ethanol solutions. After embedding in epoxy resin Lx112, cells were remounted on aluminum stubs for proper orientation of cutting plane (cross section and whole face). Ultramicrotome thick sections of 1 μm were stained with toluidine blue. Thin sections 87 nm were placed on 200 mesh copper grids and stained with 2% uranyl acetate and Reynolds lead citrate. The sections were examined utilizing a JEOL 1220 transmission electron JEM-1220 electron microscope (JEOL USA, Peabody, MA). Digital micrographs were taken with a Gatan micrograph charge-coupled device camera (Digital Micrograph 2.5 CCD Digital Camera/Software Gatan, Pleasanton, CA).
For staining of actin, Caco2 cells grown on Transwell inserts were washed twice in 1 × PBS containing 1 mM CaCl2, pH 7.4, and then fixed with 2% paraformaldehyde. Cells were then permeabilized with 0.08% saponin, washed and blocked in 5% normal goat serum for 30 min to 2 h at 25°C. Cells were then stained with rhodamine-phalloidin (Molecular Probes) diluted 1:60 and Hoechst 33342 (Invitrogen) for 60 min. For staining of PKCα, Caco-2 cells grown on Transwell inserts were treated with 5-HT (0.1 μM, 1 h) from either the apical or basolateral side and then incubated with anti-PKCα antibody followed by incubation with Alexa 488-conjugated goat anti-rabbit IgG, Alexa 568-conjugated phalloidin, and Hoechst 33342 for 60 min. Microscopy was performed with a Carl Zeiss LSM 510 laser scanning confocal microscope equipped with a ×63 water-immersion objective. Beams of 488 and 534 nm from an Ag-Kr laser and 361 nm from a UV laser were used for excitation. Green and red fluorescence emissions were detected through LP505 and 585 filters, respectively. The two different fluorochromes were scanned sequentially by using the multitracking function to avoid any bleedthrough among these fluorescent dyes. Series sections were taken at the z direction and orthogonal sections were made in a Z stack.
Image processing and analysis.
Images were processed postacquisition with Autodeblur 9 (AutoQuant Imaging, Watervliet, NY). For presentation of 3D projections, deconvolved stacks were imported into AutoVisualize 9 (AutoQuant Imaging) and 3D hardware-generated maximum volume projections were created by using matched settings for corresponding images. Well-oriented electron micrographs were used to quantify brush-border membrane curvature (33). To trace the shape of the brush-border membrane, the curved path between the most apical cell-cell contact sites within same cell was drawn by placing hinges at the base of each microvillus. The length ratio between the curved path and the distance between the two ends of the path were calculated. Forty segments were measured for each condition examined.
Actin spin-down assay.
Interaction of PKCα with actin was investigated utilizing commercially available actin spin-down assay kit from Cytoskeleton. Briefly, 50 μg of recombinant PKCα (rPKCα) reconstituted in 50 μl of actin compatible buffer (100 mM KCl, pH 7.0) was used for F-actin binding reactions as per instructions in the kit (Cytoskeleton). BSA (1 μM) was used as a control. After incubation of PKCα and F-actin for 30 min at room temperature, the F-actin separation was performed by centrifuging the tubes at 150,000 g for 1.5 h at 24°C. The supernatant was carefully removed and 10 μl of 5 × Laemmli reducing sample buffer was added. The pellet was resuspended in 60 μl of Laemmli reducing sample buffer. Both supernatant and pellet were run on 10% SDS-PAGE and transferred to nitrocellulose membranes for Western blot analysis using PKCα antibodies.
Immunoprecipitation and immunoblot analysis.
After treatment of Caco-2 cells with 5-HT (0.1 μM for 60 min), cells were washed with phosphate-buffered saline, and lysates were prepared in 20 mM Tris·HCl, pH 7.5, 150 mM NaCl, 1% Triton X-100, 1 mM EDTA, 1 mM EGTA, and 1 × complete protease inhibitor mixture. The cells were homogenized by passing 10 times through a 26-gauge needle. The lysate was centrifuged at 5,000 rpm for 5 min at 4°C. The protein content of the resulting supernatant was adjusted to contain 0.5–2 mg in 200 μl of lysis buffer and incubated with the polyclonal antibody against specific isoforms PKC (2 μg) overnight at 4°C. After incubation, immune complexes were precipitated using protein G plus agarose beads. The immunoprecipitates were collected by centrifugation and washed four times with the lysis buffer. Proteins were separated by electrophoresis on 8 or 12% SDS-polyacrylamide gels and transblotted to nitrocellulose membranes. To detect association with actin, the protein-bound nitrocellulose membranes were incubated with monoclonal anti-actin antibody (1:15,000 dilution for 1 h). The blots were stripped and reprobed with specific PKC isoform antibody (1:800 dilution) to normalize for immunoprecipitated input (PKC isoforms). The membranes were washed with the wash buffer containing 1 × PBS and 0.1% Tween 20 for 15 min with agitation, during which time the wash buffer was changed every 5 min. Finally, the membranes were probed with horseradish peroxidase-conjugated goat anti-rabbit or goat anti-mouse IgG antibody (1:2,000 dilution), and bands were visualized with enhanced chemiluminescence detection reagents.
Statistical analysis was performed by paired Student's two-tailed t-test. P < 0.05 was considered statistically significant.
5-HT alters brush-border architecture.
In our initial studies to examine the potential effects of 5-HT on human intestinal epithelial cell architecture, we performed ultrastructural analysis utilizing Caco-2 as an in vitro cell model. Cell monolayers grown on Transwell inserts were treated with 5-HT (0.1 μM, 1 h) and subjected to transmission electron microscopy (TEM). 5-HT treatment of Caco-2 cells caused modification in the cellular architecture that was especially apparent at the apical membrane. The brush-border membrane assumed a convex dome shape (Fig. 1A) that was associated with shortening of microvilli (Fig. 1B). The quantitative measurements of microvillus length and brush-border membrane curvature were performed by morphometric analysis. There was a significant increase (P < 0.05) in membrane curvature in response to 5-HT treatment compared with control (Fig. 1C). Furthermore, the microvillus length was decreased ∼30% in response to 5-HT treatment compared with control intestinal epithelium (Fig. 1C). These results suggested that brush-border ultrastructure is altered in human intestinal epithelial cells in response to 5-HT treatment.
5-HT modifies actin cytoskeleton.
Previous studies suggest that epithelial ion transport function in intestinal epithelia may be differentially influenced by dynamic alterations in F-actin (22, 35). Also, our TEM data showed alterations in cell shape changes, which could be actin cytoskeleton driven. Therefore, to examine whether 5-HT influences actin cytoskeleton organization, F-actin content was assessed by quantitative analysis of phalloidin binding (33). Latrunculin A was used as a positive control and showed a decrease in F-actin content. Within 1 h of 5-HT treatment, phalloidin binding significantly increased with 0.1 and 10 μM 5-HT concentrations, respectively (Fig. 2). This was not due to an increase in actin synthesis, since SDS-PAGE immunoblot analyses showed no significant change in total actin content in response to 5-HT treatment (not shown). These studies indicated that 5-HT causes reorganization of the actin cytoskeleton.
5-HT induces prominent basal stress fibers.
To examine how 5-HT influences F-actin assembly, morphological assessment of F-actin utilizing fluorescent microscopy was performed in control and 5-HT-treated cells. Treatment of Caco-2 monolayers with 5-HT resulted in induction of prominent basal stress fibers, which correlates with increase in actin polymerization (Fig. 3A). Examination of the apical surface indicated subtle curvature changes, which were more obvious in the TEM (Fig. 1). The basal stress fibers are clearly distinguished in the 3D projections created from the series of images of F-actin taken from apical to basolateral surface as shown in Fig. 3B.
5-HT sidedness and receptor subtypes mediating stress fiber assembly.
Since enterochromaffin cells release 5-HT both from the apical and basolateral side (12, 15, 30); we investigated whether sidedness plays a role in 5-HT-mediated effects on stress fiber assembly. Results as depicted in Fig. 4A demonstrated that induction in stress fiber assembly was observed when 5-HT was applied from either the apical side or the basolateral side of the Caco-2 cells. These studies correlate with our previous functional studies showing that 5-HT inhibits NHE activity when applied from either the apical or basolateral side (16).
Our previous studies demonstrated that 5-HT modulates Na+ and Cl− transport in human intestinal epithelial cells via involvement of 5-HT4 and 5-HT3/4 receptor subtypes, respectively (16, 31). Therefore, we examined which receptor subtype(s) is involved in stress fiber formation. For these studies, Caco-2 cells were treated apically with 5-HT3 and 5-HT4 receptor-specific agonists for 1 h, followed by staining with actin phalloidin. Both 5-HT3 and 4 receptor agonists mimicked the effects of 5-HT in inducing stress fibers (Fig. 4B).
Role of signal transduction pathways.
5-HT is well known to induce various signaling pathways (16, 31). Therefore, it was important to investigate the role of signal transduction pathways in 5-HT induced stress fiber reorganization. For these studies, Caco-2 cells were pretreated with specific inhibitors of signaling pathways and then treated in the absence or presence of 5-HT followed by labeling with actin phalloidin. As represented in Fig. 5, inhibition of intracellular Ca2+ by BAPTA-AM (10 μM), PKC by BIM (0.5 μM) (not shown) or conventional PKC isoforms by Go6976 partially prevented the increases in stress fiber reorganization. Also, treatment of inhibitor alone to Caco-2 cells had no effect on actin reorganization (not shown). These results indicated that 5-HT-mediated increase in Ca2+ and conventional PKC isoforms are involved in 5-HT-mediated modulation of actin cytoskeleton.
Activation of PKCα and δ.
Our previous studies revealed that 5-HT activates both PKCα and PKCδ in human intestinal epithelial cells (16, 31). To ascertain the role of PKCα and δ in stress fiber reorganization, we examined the activation of both PKCα and δ isoforms in response to 5-HT treatment of Caco-2 cells by confocal microscopy. As shown in Fig. 6A, in control cells, most of PKCα staining (green) was localized to the cytoplasm. However, treatment with 5-HT either from the apical or basolateral side caused the translocation of PKCα from cytoplasm to the membrane compartments. Colocalization of PKCα (green) with actin (red) was observed in 5-HT-treated cells (Fig. 6A). Similarly, 5-HT caused activation of PKCδ as evidenced by translocation of the cytoplasmic/nuclear staining in untreated cells to the membranes in response to 5-HT. Interestingly, unlike PKCα, which was translocated to both apical and basolateral membranes, PKCδ (green) was translocated specifically to the apical membranes (Fig. 6B). We then asked whether PKCδ signaling pathway is involved in 5-HT-mediated stress fiber induction at the basal surface. However, inhibition by rottlerin (PKCδ inhibitor at 10 μM) was ineffective in preventing stress fiber formation (Fig. 6B). These results suggest that differential activation of PKCα and PKCδ to the distinct membranes might explain the involvement of PKCα but not PKCδ in the induction of basal stress fiber assembly by 5-HT in Caco-2 cells.
In vitro interaction of PKCα with F-actin.
PKC isoforms are also known to be associated with a range of cytoskeletal components. Previous studies have shown that PKCδ binds to F-actin through its C2 domain (26). However, the direct interaction of PKCα with actin has not been reported. As a direct evidence of PKCα interaction with F-actin, an in vitro actin spin-down assay was performed utilizing recombinant PKCα. In this assay, F-actin binding proteins cosediment with actin filaments and form a pellet at the bottom of the centrifugation tube, whereas F-actin severing proteins, G-actin binding proteins, or non-actin-binding proteins remain in the supernatant. Bovine serum albumin (BSA) was used as a negative control (non-actin-binding protein) and was only found in the supernatant fraction (Fig. 7A). Our results as shown in Fig. 7B suggested that rPKCα was detected mostly in the pelleted fractions, indicating its association with actin under basal conditions.
5-HT increases association of PKCα with actin.
To gain further insight into mechanisms of 5-HT induced stress fiber assembly formation, coimmunoprecipitation studies were performed. Lysates from control and 5-HT-treated cells (0.5, 1.0, and 2 mg protein) were immunoprecipitated with different PKC isoform antibodies and immunoblotted with antibodies against actin. Figure 8A shows that 5-HT treatment increased the association of PKCα with actin. Densitometric analysis of actin association by normalizing to the PKCα values showed that 5-HT treatment increased the association of PKCα with actin by ∼1.8 fold (Fig. 8B). The interaction of PKCδ, PKCζ, or PKCβ1, however, was not altered (Fig. 8C). These studies suggest that 5-HT-mediated increased PKCα interactions with actin may be involved in modulation of the basal stress fiber assembly in Caco-2 cells.
5-HT has been shown to exhibit numerous effects on mammalian physiology in both health and disease. In the gut, 5-HT plays an important role in the regulation of the gut motility; absorption of sugars, amino acids, and electrolytes; and fluid transport via specific 5-HT receptor subtypes (2, 3, 16, 21, 28, 31, 32). We previously suggested that 5-HT-mediated inhibition of NHE3 and Cl−/OH− exchange activities might contribute to the pathophysiology of diarrheal diseases associated with 5-HT (16, 31). Since actin cytoskeleton influences the optimal function of many transporters including NHE3 (22), we investigated whether 5-HT is capable of modulating actin cytoskeleton and brush-border membrane architecture. Our present studies provide novel data that 5-HT treatment of human intestinal Caco-2 cells caused alterations in brush-border membrane architecture and actin cytoskeleton. We also show that 5-HT induced Ca2+ and PKCα signaling pathway mediates the actin cytoskeleton reorganization via the participation of both 5-HT3 and 5-HT 4 receptor subtypes. Also, the effects of 5-HT on induction of stress fibers were observed when applied from either the apical or basolateral side.
Ultrastructural analysis by TEM to understand the plasma membrane architecture revealed that 5-HT-treated cells displayed a small but significant decrease in microvillus length. Microvilli are actin-rich membrane protrusions present in all sensory and transporting epithelial cell types. The apical microvillus surface of the intestinal epithelial cell is supported by an extensive cytoskeletal apparatus composed of actin filaments and associated binding proteins. Interestingly, our studies showed that total F-actin content in 5-HT-treated cells was increased correlating with increase in cortical actin and induction of basal stress fiber reorganization. In this regard, previous studies have shown NHE3 activity to be inhibited by actin-disrupting agents such as latrunculin A and cytochalasin B as well F-actin stabilizing agents such as jasplakinolide (22). It was implied from these studies that NHE3 activity is not a simple function of the cellular F-actin content but an intact F-actin network is required for optimal NHE3 function. Therefore, the induction of basal stress fiber assembly by 5-HT might underlie the 5-HT-mediated effects on intestinal ion transport processes such as inhibition of NHE3 or Cl−/OH− exchangers. Furthermore, our results showed for the first time that 5-HT treatment of intestinal epithelial cells promoted convex dome shape of the brush-border membrane. Interestingly, recent studies have shown that changes in plasma membrane curvature (convex shaped) resulting from hypoosmolar exposure caused stimulation of NHE3 isoform activity (1). In contrast, our data with TEM suggest that 5-HT induced convex dome shape may be associated with inhibition of NHE3 (16). Therefore, cell volume changes are not likely involved in the observed membrane curvature alterations and inhibition of NHE3 by 5-HT. It is more likely that convex deformation of the apical membrane per se does not regulate the NHE3 activity but is a critical marker of cytoskeletal reorganization that impacts association of NHE3 with other plasma membrane proteins or accessory factors resulting in either stimulation as shown previously (1) or inhibition of NHE3 activity as implied in present studies. Thus our studies suggest that redistribution of F-actin from microvilli and the cortical ring to basal stress fibers may imply a more global change in cellular function. Moreover, PKCα activation is closely linked to both actin reorganization and NHE3 inhibition. We and others have clearly shown that PKCα activation can downregulate NHE3 activity by multiple mechanisms (8, 16, 24, 25).
Whether cytoskeleton plays a role in 5-HT induced modification of membrane architecture is not known. Interestingly, morphological assessment of F-actin utilizing fluorescent microscopy revealed that basal stress fibers were induced in response to 5-HT treatment. Previous studies from our laboratory have shown that 5-HT induces tyrosine phosphorylation that activates downstream targets such as PLCγ1 and PKCδ (16, 31). PLCγ1 activation was further shown to increase intracellular Ca2+ and activate the PKCα isoform in Caco-2 cells (16). Our present studies revealed that both Ca2+ and PKCα were partially involved in 5-HT-mediated effects on actin cytoskeleton reorganization. Functional involvement of PKC in this process appears to be isoform selective as PKCδ was not involved in stress fiber formation by 5-HT.
PKC isoforms are known to be associated with a wide range of cytoskeletal elements (7, 20). For example, PKCδ directly binds F-actin through its C2 domain, and these interactions were shown to be important in regulating actin redistribution in neutrophils (26). PKCα has been implicated in actin remodeling during cell motility, phagocytosis, and neurite overgrowth as well as acting as a ligand and substrate for actin-associated proteins such as filamin (19, 38). However, a direct interaction of PKCα with actin has not been defined. In present studies, analysis of interaction between recombinant PKCα and actin was done via an in vitro actin spin-down assay. Our data showed that majority of recombinant PKCα was found to bind to F-actin. Interestingly, immunoprecipitation assays suggested that 5-HT specifically increased the association of PKCα (but not other PKC isoforms) with actin. Therefore, although both PKCα and PKCδ are activated in response to 5-HT treatment; however, only PKCα was partially involved in inducing stress fiber formation. These findings highlight the complexity of signaling pathways and actin interactions that underlie the molecular events leading to stress fiber formation. In this regard, previous studies suggest that the subcellular localization of inactive PKC isoforms and their dynamic translocation to other subcellular compartments upon activation might determine the specificity of regulation of various biological processes as well as define a unique physiological role for each PKC isoform (6, 11, 17, 27). Our studies, for the first time, demonstrated differences in localization of PKCα and δ isoforms to the antipodal membranes of Caco-2 cells in response to 5-HT treatment. Notably, PKCδ was only translocated to the apical membranes, whereas PKCα was observed on both apical and basolateral membranes upon activation by 5-HT. Previous studies of Song et al. (35) demonstrated that PKCα and PKCε translocate to the basal but not apical membranes upon activation. This difference in PKCα translocation may represent differences in the epithelial cell type studied. Song et al. utilized T84 cells to demonstrate that activation of PKCα antagonized the ability of PKCε to disassemble F-actin and stimulate basolateral membrane endocytosis.
The membrane-associated F-actin cytoskeleton has widely been proposed as the regulatory site of membrane trafficking events (29). Our previous studies suggested that 5-HT might be involved in modulating endocytic/exocytic processes since alterations in Vmax values of NHE activity were observed in response to 5-HT treatment (16). Similarly, membrane deformation is known to be essential for various cellular processes such as cell division, locomotion, organelle biogenesis, and creation of the high-curvature vesicles and tubules that mediate cargo transport along the endocytic and exocytic pathways (18). The observed decrease in microvillus length along with deformation in membrane curvature in response to 5-HT might suggest initiation of membrane trafficking events such as endocytosis (9, 13) that might underlie effects of 5-HT on ion transporters in human intestinal epithelial cells. In this regard, our previously published studies showed that 5-HT (0.1 μm for 1 h) inhibited the activities of apical ion exchangers including NHE2, NHE3, and Cl−/OH− exchange but did not affect the activities of the apical sodium-dependent bile acid transporter or d-glucose uptake. Our studies also showed that the basolaterally expressed NHE1 isoform was not affected by 5-HT. Furthermore, 5-HT was shown to inhibit NHE and Cl−/OH− exchange activities via distinct signaling pathways (16, 31), indicating that the effects of 5-HT are through specific pathways. Our present findings showed that 5-HT influences actin cytoskeleton via Ca2+ and PKCα mediated signaling pathways, which are also involved in inhibition of NHE3 but not of Cl−/OH− exchange activity by 5-HT. These studies indicate potential mechanisms by which activation of 5-HT-mediated specific signaling mechanisms may trigger distinct physiological responses, some of which may be partly related to downstream events such as modification of cellular cytoskeleton.
In summary, our results demonstrated that 5-HT treatment of Caco-2 cells induces alterations in brush-border membrane architecture and basal stress fiber reorganization. Actin cytoskeletal reorganization occurred via 5-HT3/4 receptor subtypes and was partially dependent on Ca2+ and PKCα-dependent pathways. Further studies are warranted to directly link the basal stress fiber assembly formation with the apical membrane curvature changes that might underlie the pathophysiology of irritable colon or diarrheal conditions associated with elevated levels of 5-HT.
These studies were supported by the Department of Veterans Affairs and the National Institute of Diabetes and Digestive and Kidney Diseases Grants P01 DK-067887 (P. K. Dudeja, K. Ramaswamy, J. R. Turner), DK-54016 (P. K. Dudeja), DK-33349 (K. Ramaswamy) DK-09930 (W. A. Alrefai) and DK-074459 (R. K. Gill).
↵* R. K. Gill and P. K. Dudeja are co-senior authors.
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