KCa3.1 Inhibition Abrogates Suppression of Cell Migration and F-Actin Assembly Caused by Selective PIEZO1 Activation in Transformed Mouse Fibroblasts

Abstract

PIEZO1 are Ca²⁺-permeable mechanogated channels that play a crucial role in numerous fundamental cellular responses. Ca²⁺ influx via PIEZO1 could control the activity of various Ca²⁺-dependent molecules within the cells, thus activating Ca²⁺-dependent signaling processes and reactions. Previously, we demonstrated Ca²⁺-mediated coupling between PIEZO1 and KCa channels in the plasma membranes of transformed mouse fibroblasts, where a Ca²⁺ influx through PIEZO1 stimulates the activity of functionally co-localized KCa channels. Importantly, the selective PIEZO1 activator Yoda1 inhibited transformed fibroblast migration, induced F-actin assembly, and stress fiber formation. However, the impact of PIEZO1-KCa channel coupling on the observed effects remains unknown. Here, we performed the molecular identification of KCa channels in transformed mouse fibroblasts. Importantly, TRAM-34, a specific KCa3.1 channel blocker, abrogated the effect of Yoda1 on F-actin organization and fibroblast motility. We conclude that KCa3.1 channels in the plasma membrane are primary downstream effectors and critical contributors to the decrease in transformed fibroblast migration and F-actin assembly caused by selective PIEZO1 activation.

1. Introduction

Mechanosensitive ion channels (MSCs) are present in a wide variety of cells and tissues, where they play a key role in mechanotransduction, a fundamental physiological process that converts extracellular mechanical stimuli into intracellular signals. MSCs are the only mechanosensory molecules within the cells that are capable of providing the fastest (less than 1 ms) responses to external mechanical forces. Among MSCs, PIEZO1 channels, as Ca²⁺-permeable mechanogated channels, are a central focus of attention. The key role of PIEZO1 channels in physiological processes both in health and disease has been confirmed in a large number of studies that have been summarized in numerous reviews [1,2,3,4]. PIEZO1 allows cells to sense various mechanical forces, including membrane stretch, compression, shear stress, matrix stiffness, ultrasound, osmotic pressure, and others. When exposed to any mechanical force, a PIEZO1 channel is activated and allows the flux of physiologically relevant monovalent and bivalent ions, including Ca²⁺, a ubiquitous secondary messenger. To date, it has been shown that the activity of various molecules depends on the influx of Ca²⁺ via PIEZO1, and this results in a significant impact on intracellular and membrane Ca²⁺-dependent processes [5,6,7,8]. In particular, PIEZO1 could control the activity of Ca²⁺-activated ion channels, forming mechanogated channel complexes in the plasma membrane [9]. The presence of such complexes is thought to be a universal property of cells of different origins. However, the question of how these complexes could control and determine PIEZO1-dependent reactions remains unanswered.

Previously, using low-noise single-channel patch-clamp recordings, we identified functional complexes of PIEZO1 and Ca²⁺-activated potassium (KCa) channels in the plasma membrane of transformed mouse 3T3B-SV40 fibroblasts [10]. We also reported that Yoda1 (2-(5-(((2,6-Dichlorophenyl)methyl)thio)-1,3,4-thiadiazol-2-yl)pyrazine), the selective chemical PIEZO1 activator, induced F-actin assembly and suppressed fibroblast migration [11]. Thus, it was of specific interest to elucidate whether PIEZO1-coupled KCa activity contributes to Yoda1-mediated alterations of cell migration and F-actin organization. In the present study, we used 3T3B-SV40 cells as an experimental model to identify the molecular correlates of KCa channels that are coupled with PIEZO1 using a selective inhibitor analysis. Importantly, we determined the crucial impact of KCa activity on migration suppression and F-actin assembly caused by selective activation of PIEZO1 in 3T3B-SV40 cells.

2. Results and Discussion

In our previous study, we demonstrated the presence of functional complexes of PIEZO1 and KCa channels in the plasma membrane of transformed mouse 3T3B-SV40 fibroblasts [10,11]. Particularly, plasma membrane stretch-induced Ca²⁺ influx via PIEZO1 resulted in the stimulation of functionally co-localized KCa channel activity. Here, we aimed at identification of a particular KCa channel that is activated by a PIEZO1-mediated Ca²⁺ entry. Based on single-channel conductance (about 9 pS, [10]) measured under quasi-physiological ionic conditions (Na⁺-based extracellular solution, e.g., Ringer’s), the molecular correlates of KCa channels in 3T3B-SV40 cells could potentially be from the small conductance (SK1-3, or KCa2.1, 2.2 and 2.3) KCa channel family or, alternatively, KCa channels of intermediate conductance (IK, [12]), also known as KCa3.1 or Gardos channels.

Importantly, SK and IK channels can be easily distinguished from each other due to their sensitivity to specific pharmacological blockers, such as apamin and TRAM-34 (1-((2-chlorophenyl)-di(phenyl)methyl)pyrazole) [13], respectively. Taking this KCa channel pharmacological property as a useful tool for channel identification, we aimed to determine the specific PIEZO1 partner in the plasma membrane of transformed mouse fibroblasts. Particularly, in the case of 3T3B-SV40 cells, the absence blockage of KCa channels by apamin would undoubtedly indicate their molecular identity as KCa3.1 channels. The range of apamin blocking concentration varies from picomoles to tenths of nanomoles, depending on the specific SK channel subtype and/or SK channel subunit combination [13]. To reliably block all possible SK channel correlates, we performed the electrophysiological experiments in a cell-attached configuration (registration of ion currents from the membrane fragment of the intact cell) to probe whether PIEZO1-KCa coupling remains in the presence of an extremely high concentration (200 nM) of apamin in the patch pipette. As in the previous study [10], we used the application of “negative” pressure (suction, ΔP < 0) to evoke mechanogated PIEZO1 currents and monitored to see whether PIEZO1 activation stimulates coupled KCa channel activity in the presence of an SK blocker. One of the significant experimental drawbacks is that (in the case of PIEZO1-KCa coupling in the plasma membrane fragment) we are limited in the use of a selective agonist, Yoda1, to stimulate PIEZO1 in cell-attached experiments. Particularly, the inclusion of Yoda1 in the patch pipette would result in uncontrolled PIEZO1 activity, that, if PIEZO1-KCa coupling is present in the membrane fragment, would lead to channel interference, thus complicating the determination of whether PIEZO1 are indeed coupled with KCa channels. At the same time, the controllable application and the removal of “negative” pressure allow us to correctly determine if channel coupling is indeed present in the particular experiment (see below).

Importantly, in n = 7 independent experiments (about 30%, from n = 23) with 200 nM apamin in the patch pipette, we observed the channel coupling phenomenon (Figure 1a), which indicates that the KCa channels are not blocked by apamin and thus could not belong to the SK channel family. The mean single-channel conductance of coupled KCa channels in the presence of apamin is 8.7 ± 1.0 pS (n = 7), which coincides with the KCa conductance that was reported previously in these cells under controlled conditions [10]. Note that KCa channels remain active for >20 s after the removal of mechanical stimuli (followed by deactivation of PIEZO1), which indicates that effective local [Ca²⁺]_i increase via PIEZO1 is sufficient to induce KCa currents that persist within the seconds after PIEZO1 closure. In other patches (n = 16), the stretch-activated PIEZO1 channels were either observed alone (without KCa channel activity) or no channel activity was recorded in response to stretch. This is also similar to the statistical data reported earlier in cell-attached patches on 3T3B-SV40 cells [10]. Taken together, our results indicated that KCa3.1 channels are the only suitable candidates for molecular correlates of KCa channels coupled to PIEZO1 in the plasma membrane of transformed mouse 3T3B-SV40 fibroblasts. Further, in line with this, we revealed the presence of KCa3.1 mRNA (gene KCNN4) in the cell lysates (Figure 1b). Consistently, immunofluorescent staining with specific antibodies confirmed the expression of KCa3.1 channels in the 3T3B-SV40 cells (Figure 1c). Interestingly, the analysis of the immunofluorescent images allows one to detect significant differences in the IK staining pattern between the cells; several cells show almost no or very low staining intensity. The quantification of the percentages of KCa3.1-positive and KCa3.1-negative stained cells allowed us to determine that the mean percent of KCa3.1-negative cells is 12 ± 2% of the population. Potentially, the phenomenon could be explained by a number of factors, including the heterogeneity of the transformed 3T3B-SV40 cell population, by the differences in cell cycle stage, a known regulator of potassium channel expression, (including KCa3.1 channels [14,15]), or by KCa3.1 channel trafficking processes [16]. It should be noted that the presence (or absence) of KCa3.1 channels in the plasma membrane could be an efficient regulator of PIEZO1-KCa3.1 channel functional interplay in cellular processes and reactions [9].

To confirm the presence of functional KCa3.1 channels in the plasma membrane of 3T3B-SV40 cells we performed whole-cell patch-clamp experiments with the selective KCa3.1 channel blocker TRAM-34. We used a cytosol-like (pipette) solution containing high concentration of intracellular free Ca²⁺ (1 μM or pCa6) for reliable activation of KCa3.1 currents. At the start of the experiment, we recorded whole-cell currents in a standard extracellular solution (mM): 145 NaCl, 1 MgCl₂, 2 CaCl₂, 10 HEPES/TrisOH. Then, TRAM-34 dissolved in the same extracellular solution was added to the cells. The application of TRAM-34 resulted in the decrease of whole-cell currents in 3T3B-SV40 cells (in n = 4 independent experiments), which indicates the presence of KCa3.1 channels in the plasma membrane (Figure S1).

To summarize the first part of the study, we identified KCa3.1 channels as molecular correlates of KCa channels whose activity is controlled by local Ca²⁺ entry via PIEZO1 using selective inhibitory analysis supported by the experimental evidence obtained using molecular biology techniques. It was shown that different members of the KCa family can act as the Ca²⁺-activated molecular partner of PIEZO1 in various cells. For example, coupled activation of PIEZO1 and KCa channels of big conductance (BK) has been recorded in renal intercalated cells in the cortical collecting duct, vascular smooth muscle cells, and atrial fibroblasts of patients with sinus rhythm [17,18,19]. We have previously shown that there is a coupling between PIEZO1 and BK channels in human endometrial mesenchymal stem cells, while the activity of other KCa channels does not depend on PIEZO1 activation, despite their greater sensitivity to intracellular Ca²⁺ compared to BK [20].

The experimental model that we used in the study, that is simian virus (SV)-transformed BALB/3T3 clone A31 mouse fibroblasts (see Section 3), implies that PIEZO1-KCa3.1 coupling could potentially be a result of viral transformation that causes changes in gene expression profiles [21], including ion channels. However, we report in our previously published paper on the observation of PIEZO1-KCa coupling in pseudo-normal BALB/3T3 fibroblasts that its abundance was significantly lower compared to that found in transformed 3T3B-SV40 cells [22]. Also, as a PIEZO1-KCa3.1 coupling was demonstrated in other cell types, this channel interplay in the plasma membrane is unlikely due to the specific transformation of the fibroblasts with the virus. The coupling of PIEZO1-KCa3.1 channels in red blood cells (RBC) has been the most studied, as their functioning is crucial for erythrocyte physiology [23]. Similar PIEZO-KCa3.1 coupling was also detected in A431 human epidermoid carcinoma cells [5]. However, it should be emphasized that functional complexes with different representatives of the KCa family can also be simultaneously found in cells. Both PIEZO1-BK and PIEZO1-KCa3.1 channels are present in U87-MG glioblastoma cells [24]. However, despite the identification of PIEZO1 molecular partners from the KCa family, the role of such functional complexes in cellular reactions of different cell types remains unclear and requires further study.

In our next series of experiments, we aimed to determine whether coupled KCa3.1 activity has an impact on previously reported effects induced by selective PIEZO1 activation. In particular, we performed an analysis of 3T3B-SV40 cell migration in the presence of a specific KCa3.1 blocker, TRAM-34, together with Yoda1, a selective PIEZO1 activator. The use of Yoda1 to stimulate PIEZO1 is the only relevant ability for the analysis of the impact of PIEZO1 activation on cell migration. It was previously used in our study to reveal the inhibition of the motility of 3T3B-SV40 cells [11]. It was recently shown that Yoda1 induces conformational changes in PIEZO1 channels that are similar to those induced by membrane stretch [25]. Importantly, when TRAM-34 and Yoda1 were applied together, we observed the absence of the inhibitory effect on 3T3B-SV40 migration caused by Yoda1 alone (Figure 2). At the same time, the application of the SK channel blocker apamin (200 nM) together with Yoda1 did not prevent Yoda1-induced inhibition of cell migration and Yoda1-induced F-actin assembly (Figure S3). We must note that we are not claiming that 3T3B-SV40 transformed fibroblasts do not express SK channels at all. However, if they do express functional SK channels, their activity is not functionally coupled with PIEZO1, as the application of apamin had no effect on Yoda1-induced suppression of cell migration and F-actin organization (Figure S3). These results, together with single-channel patch-clamp analysis (no effect on channel coupling in the presence of apamin in the patch pipette, Figure 1a), further confirm the molecular identity of KCa3.1 channels as well as their functional coupling with PIEZO1 in the plasma membrane of 3T3B-SV40 cells.

Previously, we reported that the selective PIEZO1 activator Yoda1 induced F-actin assembly and stress fiber formation in transformed fibroblasts, and this effect (at least partly) seems to underlie migration suppression [11]. The same effect on F-actin was observed in Madin-Darby canine kidney (MDCK) cells, where activation of PIEZO1 by Yoda1 stimulated the formation of thick F-actin fibers [26]. Also, in macrophages, a positive feedback loop was demonstrated between PIEZO1 and the cytoskeleton; treatment with Yoda1 induced F-actin assembly, promoting the inflammatory activation of macrophages [27].

Further, we aimed to elucidate whether the application of TRAM-34 together with Yoda1 had any effect on F-actin organization, and we demonstrated that TRAM-34 prevented F-actin assembly induced by Yoda1 (Figure 3). Thus, the restoration of the migratory characteristics of 3T3B-SV40 via the addition of TRAM-34 to a Yoda1-containing medium was due to the prevention of F-actin assembly and stress fiber formation. Interestingly, TRAM-34 alone had no significant effect on cell migration, indicating little or no participation of KCa3.1 channels in transformed fibroblast motility under normal conditions (without a selective PIEZO1 activator, Figure S4). The application of selective KCa3.1 blockers was previously shown to affect fibroblast responses that were stimulated by various stimuli, including pro-fibrotic chemokines and growth factors [28]. At the same time, there are contradictory data obtained on pancreatic cancer cells, where the use of the TRAM-34 stimulated cell migration [29]. It should be noted that the effect of KCa3.1 blockers could be dependent on a particular state of the cells. As a relevant example, in human fibrocytes KCa3.1 inhibition only had an effect on migration when the cells were freshly isolated or had been detached from the surface (“rounded”). At the same time, no effect was observed when the cells were adherent (elongated shape, [30]. Thus, the role of KCa3.1 channels in cell reactions and the effect of channel inhibition could be rather different, depending on the particular cell type and its state, the type of stimuli, and/or the cell-specific signaling pathways in which the KCa3.1 channels are integrated.

Our data clearly indicated that KCa3.1 channel activity underlies the suppression of transformed fibroblast migration and F-actin assembly caused by PIEZO1 activation by Yoda1 (Figure 4).

Importantly, despite the differences in the KCa3.1 staining pattern within cell populations that indicate the variability in the level of KCa3.1 channel activity in the plasma membrane of 3T3B-SV40 cells, the abrogation of the effects of PIEZO1 activation by TRAM-34 is clearly observed. This could be justified by a relatively low percentage (12 ± 2%, see Figure 1c) of distinct KCa3.1-negative cells (that are potentially insensitive to TRAM-34). However, this low percentage is not enough to significantly impact cell migration restoration caused by the addition of TRAM-34 to Yoda1-containing culture media. Also, we cannot exclude the dynamical changes of KCa3.1 expression during cell migration. The tight interconnection between PIEZO1 activity caused by Yoda1 and KCa3.1 activation is highlighted by the observation that TRAM-34 alone had no effect on 3T3B-SV40 cell migration. This implies that the proper function of the PIEZO1-KCa channel complex could be crucial to cell physiology. The importance of “correct” functioning of the PIEZO1-KCa3.1 complex was emphasized in the study of epidermal growth factor (EGF) mediated—macropinocytosis in A431 cells [5]. Particularly, it was shown that Yoda1-induced PIEZO1 activity leads to persistent KCa3.1 activation, which prevents actin rearrangement and induces the disruption of ruffle formation and the completion of macropinosome cup formation. Thus, chemical stimulation of PIEZO1 leads to inhibition of EGF-stimulated macropinocytosis, which contributes to a decrease in cancer cell viability. Another striking example of the finely regulated function of the PIEZO1-KCa3.1 channel complex is the adaptation of erythrocytes to constantly changing volumes. Dysregulation of this channel complex leads to disruptions in the osmoregulatory mechanisms of erythrocytes, which are the cause of several hemolytic diseases [31].

The specific molecular mechanisms that underlie the effects of PIEZO1-KCa3.1 channel activity and its impact on cell signaling remain to be elucidated. Particularly, KCa3.1 channel activation could result in the change of membrane potential and the increase of the driving force for Ca²⁺ thus acting as a “positive feedback loop” allowing more Ca²⁺ to enter the cell via PIEZO1 [32]. At the same time, the activation/inhibition or modulation of other downstream effectors or ion channels in 3T3B-SV40 cells by the changes in the plasma membrane potential could not be excluded. Another possibility is that the activation of KCa3.1 channels by Ca²⁺ influx via PIEZO1 could interfere with the processes of cell volume regulation that in turn affect cell motility and migration [33]. In conclusion, it should be noted that our data highlight the importance of precise functioning of the PIEZO1-KCa3.1 channel complex and demonstrate that KCa3.1 channel activity in the PIEZO1-KCa3.1 complex underlies the effects of cell motility inhibition and cytoskeleton reorganization induced by selective PIEZO1 activation in 3T3B-SV40 cells.

3. Materials and Methods

3.1. Cell Culture and Reagents

Transformed mouse 3T3B-SV40 fibroblast cell line (simian virus-transformed BALB/3T3 clone A31 [34], obtained from the shared research facility “Vertebrate Cell Culture Collection”, St. Petersburg, Russia, https://incras-ckp.ru/catalog/3t3b-sv40/, accessed on 25 September 2025) were cultured in DMEM medium (Biolot, St. Petersburg, Russia) containing 10% fetal bovine serum (Biowest, Nuaille, France) and 40 μg/mL antibiotic gentamicin in 5% CO₂ at 37 °C. Cells were seeded in culture dishes on 4 × 4 mm or 12 × 12 mm glass coverslips for patch-clamp and fluorescence analysis, respectively. Working solutions of selective PIEZO1 agonist Yoda1 (10 μM, Tocris, Bristol, UK) and selective blocker of KCa3.1 channels TRAM-34 (5 μM, Tocris, Bristol, UK) were prepared from 10 mM Yoda1 and 5 mM TRAM-34 stocks dissolved in DMSO. Selective SK blocker apamin (Santa Cruz Biotechnology, Santa Cruz, CA, USA) was dissolved in distilled water (to 100 μM stock) and was added at 200 nM final concentration to the patch pipette prior to patch-clamp experiments.

3.2. Patch-Clamp Experiments

The electrophysiology setup was based on the patch-clamp amplifier Axopatch 200B and analog-to-digital converter Axon Digidata 1550A (Molecular Devices LLC, San Jose, CA, USA), controlled by a personal computer with Axon PClamp 10.7 Software Suite (Molecular Devices LLC, San Jose, CA, USA) for data registration, processing, and analysis. Pipettes were pulled from borosilicate glass capillaries with filament (BF-150-86-10, Sutter Instruments, Novato, CA, USA); the resistance was ~5–10 MΩ when filled with a working solution. Single-channel recordings were detected using the cell-attached mode of the path-clamp technique. The cells were placed in an experimental chamber filled with a bath solution containing (in mM): 145 KCl, 1 MgCl₂, 2 CaCl₂, 10 Hepes/TrisOH to nullify resting membrane potential. The recording patch pipette was filled with an external standard working solution (in mM): 145 NaCl, 1 MgCl₂, 2 CaCl₂, 10 Hepes/TrisOH and 200 nM apamin. The pH of all solutions was 7.2–7.3. To stimulate the activity of mechanogated PIEZO1 channels, the classical method, that is the application of “negative” pressure (suction, ΔP < 0) through a patch pipette, was applied. All experiments were performed at room temperature (RT, 22–23 °C). The single-channel conductance of KCa channels in each experiment was calculated from the slope of the I-V relationship after linear approximation, and the mean conductance value (±S.E.M.) was averaged from n = 7 independent cell-attached experiments.

3.3. RT-PCR

The PCR primers were designed using the GeneRunner v5.0.59 software. The primer sequences used for hKCNN4: 5′-GGC CAA GCT TTA CAT GAA C-3′ (forward) and 3′-ATC ATG AAG TTG TGC ACG TG-5′ (reverse). The predicted amplicon size was 325 bp. PCR was performed in a volume of 15 µL using 10 ng of cDNA, 0.3 µM of each primer, 100 µM of each dNTP, 2.5 mM MgCl₂, 1X CoralLoad PCR buffer and 1 unit Hot-Taq polymerase (Qiagen, Germantown, MD, USA). The PCR cycling conditions were 9 min 30 s at 94 °C; 35 cycles of 30 s at 94 °C, 30 s at 55 and 57 °C, and 30 s at 72 °C; 5 min at 72 °C; and 10 °C in the end for storage. 10 µL of the PCR reaction was subjected to electrophoresis on a 6% polyacrylamide gel, then was stained with DNA-binding dye Gel Red (1:10,000, Biotium, Fremont, CA, USA). The visualization of reaction was performed by UV fluorescence in the E-Gel Imager System (Thermo Fisher Scientific, Waltham, MA, USA).

3.4. Wound Healing Migration Assay

For the wound healing assay, the cells were trypsinized, resuspended in fresh medium, and placed to each well of 3-well culture silicon inserts (Ibidi, Gräfelfing, Germany) pre-installed to culture dishes at a concentration of 30,000 cells per well. Then, the cells were incubated for 6–7 h to allow spreading and monolayer formation. After the gentle removal of the culture inserts, the experimental cell-free wounds (starting points at 0 h) were photographed on the stage of an inverted microscope with a 10× objective and CCD camera. Then, the following reagents: DMSO (control, 0.2%), 10 µM Yoda1, 5 µM TRAM-34, and 10 µM Yoda1 + 5 µM TRAM-34 were added to the cells. As a control, DMSO (0.2% DMSO) was added to the culture medium. After 18 h of incubation, the same wounds were photographed and analyzed. Particularly, the wounds captured before the addition of the reagents and after 18 h of treatment were outlined in the ImageJ software 1.54n (NIH, Bethesda, MD, USA) using the “freehand selection” tool, and then the area of the wounds was determined using the “Measure—Area” command. A minimum of n = 33 wounds were analyzed for each experimental condition. The results are presented as the mean (±S.D) remaining (after 18 h) percentage of the initial wound size.

3.5. Immunofluorescence

For immunofluorescent staining, specific primary antibodies against KCa3.1 channels (anti-KCa3.1, Cat. No GB114347, ServiceBio, Wuhan, China) were used. Cells were fixed in 4% paraformaldehyde for 10 min at RT, then the cells were permeabilized with 0.25% Tween-20 (10 min, RT). Nonspecific binding of the antibodies was blocked by incubating the samples in phosphate-buffered saline (PBS) containing 10% goat serum (1 h, RT). Then, the cells were incubated with the primary antibodies at 1:100 dilution overnight at +4 °C. Staining with fluorescently labeled secondary antibodies (1:200, Goat anti-rabbit conjugated to Cy3, Santa Cruz Biotechnology, Santa Cruz, CA, USA) for 40 min at RT in the dark was performed for fluorescent detection of KCa3.1 channels. Cell nuclei were counterstained with 4′,6-diamidino-2-phenylindole (DAPI, Sigma-Aldrich, St. Louis, MO, USA, 0.05 μg/mL, 30 min at RT). Then the cells were mounted on glass slides using Vectashield mounting medium (Vector Laboratories, Newark, CA, USA). Between all staining steps cells were washed 2–3 times with PBS. The specificity of the staining was confirmed by eliminating the primary antibodies, followed by incubation of the cells only with secondary fluorescent antibodies (a fluorescent signal was not observed under these conditions, see Figure S4). Visualizations of the fluorescently labeled preparations were performed on Olympus FV3000 (Olympus, Shinjuku, Tokyo, Japan) confocal microscope with a 40× oil immersion objective using excitation at 405 (DAPI) and 561 (Cy3) nm. Images were analyzed and processed in ImageJ software 1.54n.

3.6. F-Actin Labeling

Cells were incubated in the presence of 10 µM Yoda or combination of 10 µM Yoda1 + 5 µM TRAM-34 or 10 µM Yoda1 + 200 nM apamin for 18 h before F-actin labeling. F-actin staining with rhodamine-phalloidin (TRITC-phalloidin, Sigma-Aldrich, USA) was performed as previously described [10]. Particularly, F-actin was stained using a standard procedure. The cells were fixed in 4% paraformaldehyde (10 min, RT) followed by permeabilization with 0.1% Triton X-100 for 8 min. After each step, the cells were washed 2–3 times with PBS 1×. Then, the cells were incubated with 2 µM TRITC-phalloidin at 37° C for 15 min, mounted on glass slides using a Vectashield mounting medium, and visualized with Olympus FV3000 using a 40× oil objective and excitation wavelength of 561 nm. Acquisition parameters were kept constant during the experiments for correct comparison of cell fluorescence. Fluorescent images were processed with ImageJ 1.54n. Cell cytoskeletons were outlined using the “Freehand selection tool”, and then fluorescence intensity was quantified and averaged for at least 25 cells in each experiment. The results are presented as the mean fluorescent intensities ± S.D.

3.7. Statistical Analysis

The statistical analysis was performed in the GraphPad Prism 8.0 program (GraphPad Software, Inc., San Diego, CA, USA). Before the statistical procedures, the data was tested for normality (Shapiro–Wilk’s test) and the absence of the outliers (ROUT). The comparisons of experimental wound areas (to control) were performed using the Mann–Whitney test. F-actin fluorescence intensities were compared with the corresponding control values using Student’s t-test; p < 0.05 was considered as significant.