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Intraluminal pressure elevation can cause degenerative disorders, such as ileus and hydronephrosis, and the threshold is fairly low and constant, 20–30 cm H2O. We previously devised a novel two-chamber culture system subjecting cells cultured on a semipermeable membrane to increased culture medium height (water pressure up to 60 cm H2O). Here, we sought to determine how a continuous pressure load of ~30 cm H2O affects proliferating epithelial cells with special interest in the link with cell morphology. We cultured several different cell lines using the low static pressure-loadable two-chamber system, and examined cell growth, cell cycle, and cell morphology. Madin–Darby canine kidney (MDCK) columnar epithelial cells were growth-suppressed in a manner dependent on static water pressure ranging from 2 to 50 cm H2O, without cell cycle arrest at any specific phase. Two other types of columnar epithelial cells exhibited similar phenotypes. By contrast, spherical epithelial and mesenchymal cells were not growth-suppressed, even at 50 cm H2O. Phalloidin staining revealed that 50 cm H2O pressure load vertically flattened and laterally widened columnar epithelial cells and made actin fiber distribution sparse, without affecting total phalloidin intensity per cell. When the mucosal protectant irsogladine maleate (100 nM) was added to 50-cm-high culture medium, MDCK cells were reduced in volume and their doubling time shortened. Cell proliferation and morphology are known to be regulated by the Hippo signaling pathway. A pressure load of 50 cm H2O enhanced serine-127 phosphorylation and cytoplasmic retention of YAP, the major constituent of this pathway, suggesting that Hippo pathway was involved in the pressure-induced cell growth suppression. RNA sequencing of MDCK cells showed that a 50 cm H2O pressure load upregulated keratin 14, an intermediate filament, 12-fold. This upregulation was confirmed at the protein level by immunofluorescence, suggesting a role in cytoskeletal reinforcement. These results provide evidence that cell morphology and the cytoskeleton are closely linked to cell growth. Pathological intraluminal pressure elevation may cause mucosal degeneration by acting directly on this linkage and the Hippo pathway.
Intraluminal pressure exists at various sites in the body, such as the digestive, biliary, and urinary tracts, and intraocular, intracranial, and intraventricular spaces. The normal mean values range approximately from 5 to 20 cm H2O (Enevoldsen et al., 1976; Schmidt et al., 1978; Coelho et al., 1985; Bratt and Nilsson, 1987; Liu et al., 2003; Kawoos et al., 2015). Increases in intraluminal pressure are thought to cause several diseases and disorders, such as ileus, jaundice, hydronephrosis, hydrocephalus, and glaucoma (Lindahl et al., 1995; Leske et al., 2003; Kumar et al., 2010). These pathological conditions involve degenerative lesions of the mucosa and nervous system, and are known to emerge when intraluminal pressure is persistently elevated over 20–30 cm H2O (Bratt and Nilsson, 1987; Leske et al., 2003; Kawoos et al., 2015). Thus, the threshold for pressure-induced degeneration is fairly low and constant, regardless of the tissues or organs where the pressure is loaded. This suggests that there is a common mechanism by which such low pressure causes cell and/or tissue degeneration, but the precise molecular basis has not yet been intensively examined.
Recently, we devised a new two-chamber culture system, in which small amounts of water pressure can be loaded on cells without disturbing the standard culture conditions, such as normal pH and partial pressures of oxygen and carbon dioxide (Yoneshige et al., 2017). Using this system, we demonstrated that mouse superior cervical ganglion neurons degenerated when water pressure was over 30 cm H2O (Yoneshige et al., 2017). Cell adhesion molecule 1, an immunoglobulin superfamily member, appeared to be involved in this neuronal degeneration through increased ectodomain shedding to produce a C-terminal fragment that accumulates in neurites (Yoneshige et al., 2017).
On the other hand, mucosal degeneration associated with intraluminal pressure elevation is thought to involve the retardation of mucosal epithelial renewal, suggesting that pressure directly suppresses epithelial cell proliferation. This speculation is reasonable but its mechanisms have not been carefully examined. The Hippo signaling pathway may be involved because it is crucial for controlling epithelial cell growth by regulating contact inhibition (Gumbiner and Kim, 2014; Yu et al., 2015). This pathway consists of a molecular cascade involving MST2, LATS1, LATS2, YAP, and TAZ (Yu et al., 2015). When the pathway is inactive, YAP is present in the nucleus and transactivates target genes, promoting cell proliferation (Yu et al., 2015). When the pathway is activated, YAP is phosphorylated and retained in the cytoplasm, resulting in suppression of target gene transactivation and cell proliferation (Yu et al., 2015).
Irsogladine maleate (IM) has long been widely used as a mucosal protectant that promotes the healing of gastric ulcers, based on its ability to reinforce epithelial cell adhesion by increasing adhesion-related molecule expression, gap junctional cell–cell communication, and cAMP production (Akagi et al., 2013). Thus, IM may counteract the action of water pressure on epithelial cells.
The aim of the present study is to examine how a continuous pressure load of ~30 cm H2O affects proliferating epithelial cells, as we intend to reproduce the in vivo process when erosive surfaces of the mucosa are being re-epithelialized by epithelial cell growth under the condition of intraluminal pressure elevation. We had a special interest in cell shape change induced by pressure load, because mucosal epithelia consist generally of columnar-shaped cells. We cultured various types of epithelial and mesenchymal cells using a water pressure-loadable two-chamber system, and examined changes in cell growth profiles and cell morphology. Next, we analyzed protein expression of the Hippo pathway molecules and addressed the Hippo signaling activity, and we comprehensively compared gene expression between pressure-loaded and non-loaded epithelial cells by RNA sequencing. In addition, we examined whether IM rescued the pressure-induced phenomena of epithelial cells. Pressure-induced phenotypes revealed a close link among morphology, cytoskeleton, and proliferation in columnar epithelial cells.
Madin–Darby canine kidney (MDCK), NIH3T3, and TIG-1 cells were purchased and cultured as described in our previous reports (Ito et al., 2000, 2008; Hosokawa et al., 2011). Human lung adenocarcinoma NCI-H441 cells (lot no. 58294188) were purchased from the American Type Culture Collection (Manassas, VA, USA) and grown as previously described. Human colon adenocarcinoma Caco-2, and human gastric adenocarcinoma (signet-ring cell carcinoma) KATO-III and NUGC-4 cells were purchased from the Riken BioResource Center, Tsukuba, Japan. All experiments using these cells were performed within 4 months after resuscitation. MDCK, Caco-2, and NCI-H441 cell monolayer cultures on semipermeable membranes were used as representative in vitro models of columnar epithelia (Volpe, 2011; Ren et al., 2016). KATO-III and NUGC-4 cells were used as representatives that are of epithelial origin but have a spherical morphology; this morphology well resembles that of signet-ring cell carcinoma cells in vivo (Sekiguchi et al., 1978; Nakashio et al., 1997).
Primary antibodies used in this study targeted MST2 (#3952; Cell Signaling, Beverly, MA, USA), LATS1 (C66B5; Cell Signaling), LATS2 (#A300-479A, Bethyl Laboratories, Montgomery, TX, USA), YAP (#4912; Cell Signaling), Phospho-YAP (Ser127; #4911, Cell signaling), TAZ (#HPA007415; Sigma-Aldrich, St. Louis, MO, USA), keratin 14 (LL002; Dako, Glostrup, Denmark), lamin B (M-20; Santa Cruz, Dallas, TX, USA), MCM7 (DCS-141; Medical & Biological Laboratories, Nagoya, Japan), β-actin (Medical & Biological Laboratories), and GAPDH (Medical & Biological Laboratories). Peroxidase-conjugated secondary antibodies used for western blot analysis were purchased from Amersham (Buckinghamshire, England). Phalloidin (rhodamine conjugated) and DAPI were purchased from Molecular Probes (Carlsbad, CA, USA) and Dojindo (Kumamoto, Japan), respectively. IM was kindly provided by Nippon Shinyaku Co., Ltd. (Kyoto, Japan), and was dissolved in DMSO at a concentration of 1 mM (stock solution). Blebbistatin and jasplakinolide were purchased from Wako Pure Chemical Industries (Osaka, Japan) and BioVision, Inc. (San Francisco, CA, USA), and was dissolved in DMSO at concentrations of 150 and 1.5 mM (stock solution), respectively.
The water pressure-loadable two-chamber culture device was previously described in detail (Yoneshige et al., 2017). Briefly, the upper chamber composite consisted of a long plastic cylinder with a water-tight connection with a culture insert lined with a semipermeable membrane, and the unit was placed vertically in a 10-cm dish lower chamber. Between the two chambers, a porous (150 μm, 200 cm2) silicon sheet was inserted to support the semipermeable membrane against the medium (water pressure) applied to the upper chamber cylinder. Using this device, cells were subjected to water pressure levels (cm H2O) dictated by the height of the medium from the surface to the semipermeable membrane. Partial pressures of oxygen and carbon dioxide and pH were confirmed to be comparable in the upper and lower chambers (Yoneshige et al., 2017).
4 × 104 MDCK or Caco-2 cells, 8 × 104 NCI-H441 cells, and 1 × 105 NIH3T3, TIG-1, KATO-III, or NUGC-4 cells were seeded onto the bottom of a culture insert lined with a semipermeable membrane (transparent PET membrane, pore size 1.0 μm; Corning Life Sciences, Durham, NC, USA) placed in a 6-well plate, and cells were grown in 2-cm-high Eagle's minimum essential medium (EMEM, for MDCK, Caco-2, and TIG-1), RPMI1640 (for NCI-H441, KATO-III, and NUGC-4), or Dulbecco's modified Eagle's medium (DMEM, for NIH3T3) (Wako Pure Chemical Industries) containing 10% fetal bovine serum (FBS). The following day, when the cells grew to ~40–50% confluency, the insert was set in the pressure-loadable two-chamber system, and the upper and lower chambers were filled with the appropriate medium containing 10% FBS. In some experiments, the IM, blebbistatin or jasplakinolide stock solution or DMSO was added to the upper chamber at 10,000 × (100 nM for IM), 7,500 × (20 μM for blebbistatin) or 75,000 × (20 nM for jasplakinolide) dilution, respectively.
Cell doubling time was calculated as described previously (Nakamoto et al., 2001) with some modifications (see Fluorescent staining and confocal microscopy). Cell cycle analysis was performed using propidium iodide and flow cytometry, as described previously (Ito et al., 2000). Cell viability was examined by trypan blue (0.4 v/w% solution; Wako Pure Chemical Industries) staining. Experiments were done in triplicate, and repeated independently at least three times with essentially similar results.
Total RNA was extracted from MDCK cells cultured in 2- and 50-cm-high media using a miRNeasy Mini Kit (Qiagen, Valencia, CA, USA) according to the manufacturer's protocol. Library preparation was performed using a TruSeq stranded mRNA sample prep kit (Illumina, San Diego, CA, USA) according to the manufacturer's instructions. Sequencing was performed on an Illumina HiSeq 2500 platform in 75-base single-end mode. Illumina Casava 1.8.2 software was used for base-calling. Sequenced reads were mapped to the dog reference genome (CanFam3.1) using TopHat v. 2.0.13 in combination with Bowtie 2 v. 2.2.3 and SAMtools v. 0.1.19. The fragments per kilobase of exon per million mapped fragments (FPKMs) was calculated using Cuffnorm v. 2.2.1. Among the genes calculated with a normalized FPKM value >1.0 in both MDCK cell cultures, 730 genes were more than 2-fold up- or downregulated from the 2-cm H2O to 50-cm H2O pressure load. A total of 730 significantly changed genes was queried against functional annotations in the NextBio, Gene Ontology, Broad MSigDB Regulatory Motif, and Broad MSigDB Canonical Pathways databases (http://software.broadinstitute.org/gsea/index.jsp), and more than 100 biological groupings (biogroups) were identified to have a P < 0.01 (see Table S2).
Protein extraction from cultured cells and western blot analysis were performed as described previously (Koma et al., 2008). Immunoreactive band intensities were quantified using ImageJ software (National Institutes of Health, Bethesda, MD, USA), as described previously (Mimae et al., 2012).
Phalloidin staining and nuclear labeling with DAPI were performed as previously described (Ito et al., 2012; Mimae et al., 2012). Immunofluorescence coupled with phalloidin labeling was performed as previously described (Ito et al., 2012). Briefly, cells were fixed in paraformaldehyde, blocked with 2% bovine serum albumin, and incubated with an antibody against keratin 14 or MCM7, then visualized with Alexa Flour 488-conjugated secondary antibody (anti-mouse IgG; Jackson ImmunoResearch, West Grove, PA, USA). After washing three times with phosphate buffered saline, phalloidin staining was performed for 10 h at 4°C. Nuclei were labeled with DAPI. Fluorescence images were captured using a C2+ confocal scanning system equipped with 488-nm argon and 543-nm helium–neon lasers (Nikon, Tokyo, Japan). The vertical sectional (Z-plane) images were generated by Z-stack confocal microscopy using a 0.4-μm motor step. Captured images were analyzed on the Nikon C2+ computer system using Analysis Controls tools. Length and area were measured with Annotations and Measurements, cell numbers were counted as the number of DAPI-stained nuclei identified using Object Count, and phalloidin intensity (arbitrary unit) was calculated using ROI Statistics. The mean total phalloidin intensity per cell was calculated as follows: in a high-power field view using a 60 × objective lens, the total intensities were measured in three XY planes that were in the middle of the Z-axis, and 0.8 μm up and 0.8 μm down, and the mean value was calculated and expressed as phalloidin intensity per XY plane. The total intensity of phalloidin per cell was calculated as follows: the mean phalloidin intensity of 10 randomly selected ZX planes was multiplied by the area of the XY plane, then divided by the cell number. Ten randomly selected high-power field views were examined per experimental group, and the mean and standard deviation were calculated. In some experiments, Z-projected 3-dimentional images were constructed, and used for analyses of phalloidin intensity (see Figure 2B).
To calculate cell doubling time, cells were observed through a 20 × objective lens on days 1, 2, and 3 of culture, and total cell numbers per field view were counted as the number of DAPI-stained nuclei identified using Object Count. Ten randomly selected field views were examined per sample, and their mean value was calculated in triplicate cell cultures (30 field views in total) for each day of culture. The mean cell numbers of 3 timepoints were input into Doubling Time Calculator (http://www.doubling-time.com/compute_more.php). The mean and standard deviation of doubling time were calculated by repeating the cell count experiment independently five times.
For assessment of cell proliferation, the number of MCM7-positive nuclei was counted in the randomly selected high-power field views, and its ratio to the total cell number (MCM7 positivity; %) was calculated. The mean ratio and standard deviation were calculated in triplicate experiments.
Differences among experimental groups were analyzed statistically; ANOVA was applied for time-course plots of cell numbers using the software “EZR” (Easy R) (Kanda, 2013), and paired Student's t-test for cell doubling time, cell morphological variables, phalloidin and western blot intensities, and immunofluorescence positivity. A P ≤ 0.05 was considered to indicate statistical significance.
MDCK cells, which are of epithelial origin with a columnar morphology, were cultured on a semipermeable membrane below culture medium that was 2, 15, 30, or 50 cm in height, and the cell numbers were counted after 1, 2, and 3 days. The cell growth curve showed a slow ascent and the doubling time lengthened in a culture medium height-dependent manner (Figure (Figure1A).1A). Two other columnar epithelial cell lines, NCI-H441 and Caco-2, and two mesenchymal cell lines, TIG-1 and NIH3T3, were cultured in 2- or 50-cm-high culture medium. NCI-H441 and Caco-2 cells produced results similar to those of MDCK cells (Figures S1A,D), whereas TIG1 and NIH3T3 cells did not exhibit significant differences between the two culture conditions (Figures S2A,C). KATO-III and NUGC-4 cells, which are of epithelial origin but have a spherical morphology, were not growth-suppressed by a static pressure of 50 cm H2O (Figures S3A,C). Cell cycle profiles of MDCK, NCI-H441, and Caco-2 cells were analyzed by flow cytometry. There were no apparent growth-arrested phases or no appearance of sub-G1 populations detectable in cells in 50-cm-high-medium cultures (Figure (Figure1B;1B; Figures S1B,E). Consistent results were obtained by immunofluorescence of MDCK cells against MCM7, a marker for DNA replication; the MCM7-positive cell proportions were comparable between 2- and 50-cm-high-medium cultures (Figure (Figure1C).1C). There were practically no MDCK cells positive for trypan blue staining in 50-cm-high-medium cultures. These results suggested that growth suppression in pressure-loaded cells was not due to increased cell death or apoptosis.
Cultured cells were stained with phalloidin. MDCK cells were found to change drastically in shape with the application of a static pressure of 50 cm H2O. The cell area tripled in the XY plane and the cell height roughly halved in the Z-axis, resulting in 1.5-fold enlargement of the cell volume (cell area × cell height) (Figure (Figure2A).2A). Phalloidin staining was markedly weakened in the cytoplasm and on the cell membrane when XY planes around the middle of the Z-axis were observed, but the total intensity per cell was unchanged when the cell volume increase was taken into consideration (Figures 2A,B), suggesting that actin fibers became sparsely distributed as the cell volume increased. Similar results were obtained with NCI-H441 and Caco-2 cells (Figures S1C,F). By contrast, in 50-cm-high-medium cultures of KATO-III and NUGC-4 cells, some cells showed a little flattened morphology, but there was no apparent decrease in phalloidin staining intensities (Figures S3B,D). Neither TIG-1 nor NIH3T3 cells exhibited substantial differences in cell shape or phalloidin staining intensity between 2- and 50-cm-high-medium cultures (Figures S2B,D).
MDCK cells were cultured in 2- or 50-cm-high culture medium for 3 days, and their protein extracts were fractionated into cytosolic and nuclear fractions. Successful fractionation was confirmed by western blot analyses with antibodies against glyceraldehyde 3-phosphate dehydrogenase (GAPDH) and lamin B (Figure (Figure3;3; the original image Figure S4). The duplicate blots were examined for expression of the Hippo pathway molecules, MST2, LATS1, LATS2, YAP, and TAZ. No appreciable differences were detected in the expression levels of the four molecules, i.e., MST2, LATS1, LATS2, or TAZ, between the two culture conditions in either fraction (Figure (Figure3).3). Similar results were obtained with NCI-H441 and Caco-2 cells (Figure (Figure3).3). In contrast, significant differences were detected in the YAP expression. Total YAP levels were decreased in the nuclear fractions of the three cell lines cultured in 50-cm-high medium, and in line with this, serine-127 phosphorylated YAP was increased in their cytoplasmic fractions (Figure (Figure33).
RNAs were extracted from MDCK cells cultured in 2- and 50-cm-high culture medium, and gene expression differences were compared by RNA sequencing. The raw data have been deposited in the NCBI Gene Expression Omnibus database (GSE100794). Top 10 up- or down-regulated genes are listed in Table S1. The gene most upregulated in 50-cm-high-medium cultures was keratin 14, encoding a type I intermediate filament, with an 11.869-fold change (Figure (Figure4A).4A). This upregulation was confirmed at the protein level by western blot analyses (Figure (Figure4B).4B). MDCK cells were double-stained with phalloidin and an anti-keratin 14 antibody. Keratin 14 expression was at trace levels in 2-cm-high-medium cultures, whereas it was clearly detected in the cytoplasm of MDCK cells cultured in 50-cm-high medium, in contrast to a marked decrease in phalloidin staining (Figure (Figure4C).4C). Using 730 genes that were more than 2-fold up- or down-regulated from the 2-cm H2O to 50-cm H2O pressure load, we performed gene ontology analysis to annotate their biological functions. Gene categories significantly altered (P < 0.01) are listed in Table S2. Most significantly up- and down-regulated were the genes associated to transcriptional regulation related to activator protein 1 (AP-1), and those associated to biosynthesis and metabolism related to lipids and derivatives, respectively (Table S2).
MDCK cells were cultured on a semipermeable membrane for 3 days in 2- or 50-cm-high culture medium containing either IM or vehicle (dimethyl sulfoxide, DMSO) alone (final concentrations of IM and DMSO, 100 nM and 10,000× dilution, respectively). Cell doubling times in 2-cm-high-medium cultures were comparable in the IM and vehicle groups, whereas in 50-cm-high-medium cultures, the IM group had a significantly shorter doubling time than the vehicle group (Figure (Figure5A).5A). Cell cycle analyses did not indicate any apparent differences between the two groups (Figure (Figure5B).5B). MDCK cells were stained with phalloidin. Cell morphology and phalloidin staining intensity were comparable between the IM and vehicle groups in 2-cm-high-medium cultures (Figure (Figure6).6). When cultured in 50-cm-high medium, the IM group had a smaller XY plane cell area, a larger cell height, and a smaller cell volume than the vehicle group (Figure (Figure6).6). IM-treated cells stained more strongly with phalloidin than the vehicle-treated cells, when observed in XY planes around the middle of the Z-axis. The total intensity per cell, however, was comparable in the IM and vehicle groups (Figure (Figure6),6), suggesting that IM did not affect the kinetics of actin polymerization/depolymerization.
We performed similar cell cultures in the presence of either blebbistatin (20 μM), a myosin II inhibitor that relieves F-actin tension, or jasplakinolide (20 nM), an inhibitor of actin filament depolymerization. Both drugs extended the MDCK cell doubling time even in 2-cm-high-medium cultures, consistent with past reports (Senderowicz et al., 1995; Hirata et al., 2017), but blebbistatin, not jasplakinolide, significantly shortened the time in 50-cm-high-medium cultures when compared with DMSO alone (Figure (Figure5C;5C; Figure S5).
In the present study, we found that relatively small increases in water pressure significantly suppressed the growth of columnar epithelial cells in association with cell height shortening and lateral widening. This cell shape change was associated with decreased intensity of phalloidin staining in the XY plane. By contrast, spherical epithelial-origin cells and mesenchymal cells were not growth-suppressed by the pressure load of 50 cm H2O, and did not exhibit noticeable changes in cell morphology or phalloidin staining. These results suggest that cell morphological changes and cytoskeletal remodeling are involved in growth suppression induced by modest static pressure, and are consistent with the notion that actin fibers act as a mechano-sensing apparatus (Hayakawa et al., 2011). A pressure of 50 cm H2O is nearly equal to 0.05 atm = 5 kPa = 5 fN nm−2. Nanometer-sized molecules in live cells fluctuate with forces on the piconewton order because the thermal energy of each molecule at room temperature is on the order of multiplying nanometers by piconewtons (kBT = 4.1 × 10−21 J = 4.1 pN·nm) (Merkel et al., 1999). This means that under a pressure of 5 fN nm−2, the force loaded on each molecule is fN order, and is too small to perturb the molecular fluctuation. How can cells convert this weak force into biological signals? According to our present study, the primary event caused by the pressure appeared to be cell-shape change, a kind of physical response. This event may trigger particular biological responses, including growth suppression and gene transactivation.
A pressure of 50 cm H2O made columnar epithelial cells 1.5-fold larger in cell volume, with lateral widening and cell height shortening. This cell volume increase is likely associated with an increase in cell membrane tension. Actin fibers appeared to become sparsely distributed as a result of cell volume increase because their total amount per cell was unchanged. At this time, individual actin fibers may be stretched out, as they have an extensibility as high as 200% (Labouesse et al., 2016). These events may be involved in pressure-induced cell growth retardation. Increased tension of the cell membrane may interfere with the progression of the cell cycle into the S phase because in cells proceeding to cell division, cell volume gradually increases but cell membrane tension remains low (Chang et al., 2014). Sparse distribution and/or stretching of actin fibers may do the same because preexisting actin filaments are used preferentially for the formation of the contractile ring in dividing cells (Cao and Wang, 1990). These notions are supported by the results obtained from adding IM to cultures: when 50 cm H2O pressure-loaded MDCK cells were treated with IM, their doubling time and cell volume decreased significantly, and phalloidin staining strengthened in the XY planes. Blebbistatin also negated the growth-suppressive effect of 50 cm H2O pressure load on growing MDCK cells, consistent with the recent studies reporting actin cytoskeletal tension-dependent arrest of epithelial proliferation (Furukawa et al., 2017; Hirata et al., 2017). On the other hand, some past articles clearly demonstrate that stretch-induced membrane/cytoskeletal tension has a promotive effect on epithelial cell proliferation (Aragona et al., 2013; Benham-Pyle et al., 2015). This effect is detected when dense, quiescent monolayers of epithelial cells are stretched, suggesting that it stimulates cell cycle reentry. This experimental condition is essentially different from that of the present study, in which cells were loaded with pressure when they should grow actively from sparse cultures to confluent monolayers. Thus, mechanistic force may produce opposite effects on epithelial cells between growth-suppressive or quiescent and proliferative phases.
Notably, YAP appeared to be involved in pressure-induced growth suppression of epithelial cells. YAP is known to bind angiomotin, a component of the intracellular complex of tight junctions, in the back of epithelial lateral membrane (Zhao et al., 2011). The most apparent event induced by static pressure was the lowering of epithelial cell height, i.e., the shortening of the lateral membrane in the Z-axis direction. This structural change in the lateral membrane may activate anigiomotin and/or increase angiomotin–YAP binding, resulting in enhancement of YAP phosphorylation.
RNA sequencing indicated that keratin 14 was upregulated by modest static pressure in MDCK cells. This upregulation is reasonable because intermediate filaments including keratin 14 act to reinforce cell stiffness and to resist physical strain imposed on the cell (Ma et al., 1999; Nolting et al., 2014). Expression levels of keratin 14 are shown to change dynamically among cell cycle phases, and this change is apparently required for the cell division process to progress (Confalonieri et al., 2017). Constant upregulation of this keratin in MDCK cells can be regarded as one of the causes of cell growth suppression induced by pressure loading. In addition, RNA sequencing suggested that pressure-loaded cells had a general suppression of metabolism and thereby decline in molecular functions. These conditions appear similar to those under starvation. Future studies should clarify the differences between low pressure load, which extends cell doubling time without cell cycle arrest, and starvation, which induces cell cycle arrest at the G1 phase (Cooper, 2003).
Intraluminal pressure elevation often causes the formation of tissue degenerative lesions. Hydronephrosis/obstructive nephropathy leads to renal tubular injury through urinary intraluminal pressure increase (Bratt and Nilsson, 1987; Kipari et al., 2006). Obstruction of pancreatic and biliary ducts results in ductal dilatation through intraductal pressure elevation (Turowski et al., 2011). Mechanical ventilation often leads to alveolar damage through excess airway pressure (Cabrera-Benítez et al., 2012). Delayed tissue regeneration and re-epithelialization are assumed to underlie the development of these lesions (Kipari et al., 2006; Turowski et al., 2011; Cabrera-Benítez et al., 2012). Intraluminal pressure elevation can be a direct cause of delayed tissue regeneration/re-epithelialization through the suppression of epithelial cell proliferation. The present study identified IM as a potent drug that can protect against degenerative lesion formation.
In conclusion, the growth of columnar epithelial cells appeared to be suppressed by a static pressure burden as low as a few tens of cm H2O. The precise mechanisms by which cells can sense such modest pressure remain unknown; however, this study highlights an important role for mutual links among the cytoskeleton, cell morphology and Hippo pathway in the proliferative responses of epithelial cells to modest pressure. These links may underlie a general mechanism of the development and progression of columnar epithelial degeneration and the delay in re-epithelialization of erosive mucosa under pathological conditions of intraluminal pressure elevation.
The raw data of RNA sequencing are deposited in the NCBI Gene Expression Omnibus database (accession number, GSE100794). The URL is as follows https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE100794.
MH: carried out the cell culture, cell staining, western blotting, and laser microscopic examinations, and performed the statistical analyses; TI, YT, RK, and AR: participated in the western blot analysis and microscopic examinations; NY: supervised the western blot analysis and data interpretation; DO: carried out RNA sequencing and deposited the data into the public database; AI: conceived and designed the study, and drafted the manuscript. All authors read and approved the final manuscript.
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Funding. This study was supported by Japan Society for the Promotion of Science KAKENHI grants (15K19079, 17K08680 to MH, and 15K15113 to AI); the Ministry of Education, Culture, Sports, Science and Technology-Supported Program for the Strategic Research Foundation at Private Universities 2015-17 (to AI); a twenty-first Century Joint Research Enhancement Grant of Kindai University (to AI); and the Grant for Joint Research Projects of the Research Institute for Microbial Diseases, the University of Osaka (to AI).
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fphys.2017.00997/full#supplementary-material