Piezo2 expression and its alteration by mechanical forces in mouse mesangial cells and renin-producing cells

Mochida, Yuki; Ochiai, Koji; Nagase, Takashi; Nonomura, Keiko; Akimoto, Yoshihiro; Fukuhara, Hiroshi; Sakai, Tatsuo; Matsumura, George; Yamaguchi, Yoshihiro; Nagase, Miki

doi:10.1038/s41598-022-07987-7

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Published: 10 March 2022

Piezo2 expression and its alteration by mechanical forces in mouse mesangial cells and renin-producing cells

Yuki Mochida^1,2,
Koji Ochiai^1,2,
Takashi Nagase³,
Keiko Nonomura⁴,
Yoshihiro Akimoto¹,
Hiroshi Fukuhara⁵,
Tatsuo Sakai^6,7,8,
George Matsumura¹,
Yoshihiro Yamaguchi² &
…
Miki Nagase^1,7

Scientific Reports volume 12, Article number: 4197 (2022) Cite this article

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Abstract

The kidney plays a central role in body fluid homeostasis. Cells in the glomeruli and juxtaglomerular apparatus sense mechanical forces and modulate glomerular filtration and renin release. However, details of mechanosensory systems in these cells are unclear. Piezo2 is a recently identified mechanically activated ion channel found in various tissues, especially sensory neurons. Herein, we examined Piezo2 expression and regulation in mouse kidneys. RNAscope in situ hybridization revealed that Piezo2 expression was highly localized in mesangial cells and juxtaglomerular renin-producing cells. Immunofluorescence assays detected GFP signals in mesangial cells and juxtaglomerular renin-producing cells of Piezo2^GFP reporter mice. Piezo2 transcripts were observed in the Foxd1-positive stromal progenitor cells of the metanephric mesenchyme in the developing mouse kidney, which are precursors of mesangial cells and renin-producing cells. In a mouse model of dehydration, Piezo2 expression was downregulated in mesangial cells and upregulated in juxtaglomerular renin-producing cells, along with the overproduction of renin and enlargement of the area of renin-producing cells. Furthermore, the expression of the renin coding gene Ren1 was reduced by Piezo2 knockdown in cultured juxtaglomerular As4.1 cells under static and stretched conditions. These data suggest pivotal roles for Piezo2 in the regulation of glomerular filtration and body fluid balance.

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Introduction

The morphology and function of tissues and organs, including intricate organs such as the kidney, are tightly coordinated, and mechanical forces are key factors that can mediate this coordination¹. For instance, the functions of mesangial cells in the glomeruli and renin-producing cells in the juxtaglomerular apparatus are finely regulated by hemodynamic mechanical factors, which contributes to the homeostasis of the body².

Glomerular endothelial cells, podocytes, and mesangial cells are three cellular components of renal glomerular tufts. The glomerular endothelial cells and podocytes control urinary filtration, whereas the functions of mesangial cells include (1) structural support, (2) secretion of extracellular matrix (ECM), (3) modulation of glomerular filtration through mesangial cell responses to vasoactive stimuli, (4) phagocytosis of macromolecules and immune complexes, and (5) response to and secretion of cytokines^3,4. Among these, functions (1) and (3) suggest the importance of mechanical strain on the morphology and functions of mesangial cells. For example, mesangial cells and the glomerular basement membrane form a contracting framework, thereby supporting the integrity of the glomerular tuft and its capillary wall tension^5,6. Mesangial cells also secrete ECM in response to mechanical stimuli, including collagens and fibronectin^7,8,9,10. This point is clinically important since glomerulosclerosis is characterized by the uncontrolled proliferation of mesangial cells and an increase in ECM deposition³. However, the mechanism by which mechanical stimuli are initially transmitted to mesangial cells and the molecules that act as mechanosensors remain to be elucidated.

Renin secretion from the juxtaglomerular apparatus is a rate-determining factor of the renin angiotensin system, which controls blood pressure and body fluid balance^11,12. Renin-producing cells in the juxtaglomerular apparatus (also known as juxtaglomerular cells, JG cells, or granule cells) are located in the medial layer of the afferent arterioles. Triggers of renin secretion from renin-producing cells include (1) baroreception by renin-producing cells that sense perfusing pressures of the afferent arterioles, (2) Cl⁻ concentration in the macula densa, and (3) neuroendocrine regulation, including β-adrenergic receptor activity. Although some candidate molecules, such as transient receptor potential vanilloid 4 (Trpv4) ion channel, have been considered¹³, the mechanosensing mechanisms of baroreception have not been fully investigated.

Morphologically, mesangial cells and renin-producing cells have the same embryonic origins^14,15. The metanephros (renal primordia) comprises three progenitor groups. The ureteric buds differentiate into collecting ducts, the renal pelvis, and the ureteric epithelium¹⁶. Six2-positive cap mesenchyme differentiates into the entire nephron from podocytes to the distal tubules¹⁷. Foxd1-positive stromal cells differentiate into both glomerular mesangial cells and mural cells of the renal arterial tree (renin cells, smooth muscle cells, perivascular fibroblasts, and pericytes)^14,15,18. However, it is not clear whether mesangial cells and renin-producing cells share a common mechanosensing system.

Piezo proteins, including Piezo1 and Piezo2, are now regarded as bona fide mechanically activated ion channels that mediate various biological phenomena¹⁹. Piezo1 is predominantly expressed in non-neural tissues, such as blood vessels^20,21, where it regulates blood pressure and vascular development. Piezo2 is mainly expressed in neural sensory systems, such as the dorsal root ganglia²², sensory nerve terminals²², Merkel cells^23,24, and muscle spindles²⁵. Piezo2 mediates cutaneous light touch^22,23,24, itching²⁶, proprioception²⁵, baroreception at the carotid sinus and aortic arch (together with Piezo1)²⁷, and airway stretch²⁸. In the urinary system, Piezo1 is expressed in the glomeruli, tubules, and collecting ducts^29,30. Piezo2 also plays an important mechanosensing role in the bladder³¹. However, the distribution of Piezo2 in the kidney, changes in Piezo2 levels during development, and Piezo2 expression regulation in response to altered mechanical load are still unknown.

In this study, we found that Piezo2 was expressed in glomerular mesangial cells and juxtaglomerular renin-producing cells at both the mRNA and protein levels. Embryonic expression of Piezo2 was observed in Foxd1-positive stromal progenitor cells and their derivatives but not in Six2-positive nephron progenitors. In response to the reduction of mechanical load to the glomeruli by dehydration, Piezo2 expression was downregulated in mesangial cells, whereas its expression was upregulated in juxtaglomerular renin-producing cells, along with an overproduction of renin. Piezo2 knockdown in cultured mouse As4.1 cells, juxtaglomerular cell line, showed significant inhibition of the renin coding Ren1 gene expression under static and stretched status. These data suggest important roles of Piezo2 in the physiological regulation of body fluid homeostasis.

Results

Piezo2 transcripts are localized in mesangial cells and juxtaglomerular renin-producing cells

To examine the expression patterns of Piezo2 transcripts, we first performed in situ hybridization using RNAscope technology. Even a single mRNA molecule can be visualized as a dot using RNAscope³². In the normal C57BL/6J mouse kidney, DAB-stained brown dot signals representing Piezo2 transcripts were specifically observed in the glomeruli (Fig. 1a, arrows). No apparent dot signals were detected in tubular or duct cells. There were no specific dot signals when the negative control probe targeting the invertebrate gene dihydrodipicolinate reductase (dapB) was used (Supplementary Fig. S1a). The brownish staining, not dot signals, observed in some tubules was considered as background staining. Ubiquitous dot signals were observed for the positive control mouse housekeeping gene peptidylprolyl isomerase B (Ppib, Supplementary Fig. S1b). Additionally, dot signals for Piezo2 mRNA were detected in the nodose ganglion in a pattern similar to that reported by Zeng et al.²⁷, serving as another positive control (Supplementary Fig. S1c–e). These data validate the applicability of the RNAscope technology in our study.

To characterize the Piezo2-positive cells more precisely, we next performed double RNAscope in situ hybridization of Piezo2 with cell marker probes using fluorescent dyes. Within the glomerular tufts, Piezo2-positive cells were mostly co-expressed with the platelet-derived growth factor receptor, beta polypeptide (Pdgfrb) gene, a marker for mesangial cells^33,34 (Fig. 1b). On the contrary, co-expression of Piezo2 transcripts with the podocyte marker Nphs1 (also known as nephrin) was not observed (Fig. 1c). Piezo2 transcripts were only rarely colocalized with transcripts for the endothelial marker Tek (Fig. 1d). Notably, Piezo2 transcripts were detected in Ren1-positive cells in the juxtaglomerular apparatus (Fig. 1e), indicating Piezo2 expression in the renin-producing cells within the afferent arteriolar walls.

We further evaluated the distribution of Piezo2 mRNA using real-time quantitative RT-PCR of kidney tissues and fractions. Consistent with the staining pattern, Piezo2 expression was concentrated in the glomerular fraction, compared with the low expression in the whole kidney, cortex, and medulla fractions (Fig. 1f). Taken together, these data indicate that Piezo2 mRNA in the kidney is primarily expressed in mesangial cells and renin-producing cells.

Localization of Piezo2-GFP fusion protein indicates Piezo2 expression in mesangial cells and renin-producing cells

We next examined whether Piezo2 is expressed in mesangial cells and renin-producing cells at the protein level. Since the commercially available anti-human Piezo2 antibodies did not cross-react with mouse Piezo2 (data not shown), we analyzed the previously described Piezo2-GFP-IRES-Cre (Piezo2^GFP) reporter mice^23,28, in which the Piezo2-GFP fusion protein is expressed under the control of the native Piezo2 promoter. GFP immunofluorescence staining using an anti-GFP antibody revealed distinct signals within the glomeruli (Fig. 2a, left) in a similar pattern to that seen using in situ hybridization, indicating that the overall histological distributions of Piezo2 transcripts and the Piezo2-GFP protein were the same. No signal was observed in the kidneys of wild-type C57BL/6J mice (Fig. 2a, right). Double immunofluorescence staining revealed that the Piezo2-GFP protein was colocalized with Pdgfrb (Fig. 2b) and Ren1 (Fig. 2e), supporting Piezo2-GFP expression in mesangial cells and renin-producing cells. The Piezo2-GFP fusion protein was not found to be colocalized with the podocyte marker Nphs2 (also known as podocin, Fig. 2c). There was no or only faint co-staining with the endothelial marker platelet/endothelial cell adhesion molecule 1 (Pecam1, Fig. 2d). Although it was technically difficult to perform immunostaining and RNAscope in situ hybridization on the same section, we confirmed that Piezo2-GFP protein and Piezo2 transcripts were mostly colocalized using adjacent serial sections with 4 µm thickness (Fig. 2f).

We further determined the cellular localization of Piezo2-GFP using immunoelectron microscopy. Positive DAB staining for Piezo2-GFP was observed as osmium black dots under a transmission electron microscope, which was detected in the cytoplasmic membrane of mesangial cells (Supplementary Fig. S2a,b, arrows), and of renin-producing cells (Supplementary Fig. S2c,d, arrows).

Taken together, the analysis of Piezo2^GFP reporter mice showed that Piezo2 is expressed in mesangial cells and renin-producing cells at the protein level.

Piezo2 mRNA is developmentally expressed in Foxd1-positive stromal progenitor cells and their derivatives in mouse embryos

To investigate the embryonic origin of Piezo2/Pdgfrb- or Ren1-positive cells, we next examined the developmental changes in Piezo2 gene expression in mouse metanephros from embryonic day (E)14.5 until E17.5 and in the kidneys of postnatal day (P)0 and P15 mice. RNAscope in situ hybridization followed by DAB detection revealed that Piezo2 mRNA was highly expressed in the subcapsular metanephric mesenchyme, developing glomeruli, and some arteriolar cells (Fig. 3a). Quantitative analysis revealed that Piezo2 gene expression in the subcapsular region did not change during the embryonic period and at P0, and that the expression significantly decreased at P15 (Fig. 3b), possibly due to the disappearance of the metanephric mesenchyme.

Fluorescence multiple RNAscope in situ hybridization of the E16.5 metanephros revealed that most of the Piezo2-expressing cells in the subcapsular metanephric mesenchyme were Foxd1-positive stromal progenitor cells and not Six2-positive nephron progenitor cells (Fig. 3c). Piezo2-expressing cells in the developing glomeruli were positive for the mesangial marker Pdgfrb (Fig. 3d). Ren1 transcripts were observed in the arterioles of the E16.5 kidney, where co-expression of Piezo2 signals was noted (Fig. 3e). Ren1 expression was restricted to the juxtaglomerular cells at P15, at which time Piezo2 mRNA was also expressed.

Piezo2 expression is increased in renin-producing cells under dehydration conditions

We further used a mouse model of dehydration to investigate whether Piezo2 expression is altered in response to reduced mechanical strain in the glomeruli and afferent arterioles. RNAscope in situ hybridization followed by DAB detection revealed that overall Piezo2 dot signals were weakened in the dehydration group (Fig. 4a). Quantitative analysis of signal density indicated that glomerular Piezo2 expression was significantly decreased in the dehydration group (P < 0.05 vs. control group, Fig. 4b). Quantitative RT-PCR also showed that Piezo2 expression was lower in the dehydration group (P < 0.01 vs. control group), whereas Ren1 was overexpressed in the dehydration group (P < 0.01) (Fig. 4c).

Double RNAscope in situ hybridization showed that Piezo2 signals in Pdgfrb-positive mesangial cells were diminished by dehydration (Fig. 4d). Notably, Ren1 expression was strongly augmented in the juxtaglomerular area in the dehydration group, where Piezo2 expression was also enhanced (Fig. 4e). Quantitative analysis revealed that both Piezo2 and Pdgfrb expression decreased in the dehydration group (P < 0.05 and P < 0.01 vs. control group, Fig. 4f, upper panels). The colocalized signal density of Pdgfrb and Piezo2 was also significantly reduced in the dehydration group (P < 0.01, Fig. 4f, lower panel). For Piezo2 and Ren1 double staining, although Piezo2 expression was again decreased by dehydration (P < 0.05, Fig. 4g, upper left panel), Ren1 expression and the colocalized density of Ren1 and Piezo2 were enhanced in the dehydration group (P < 0.05 and P < 0.01, respectively, Fig. 4g, upper right and lower panels).

There may be a concern of whether the colocalization of Piezo2 and Ren1 can be evaluated accurately in a plan view because various cells are densely packed in the juxtaglomerular region. Thus, to clarify their co-expression in more detail, we created 3D images of Ren1-expressing cells using the Z-stack system of the confocal laser scanning microscope. When viewed from different directions by rotating the images, Piezo2 transcripts were definitely co-expressed in Ren1-positive cells in the control group (Fig. 4h, left, Supplementary Video S1 and Supplementary Fig. S3). Additionally, we detected a few Piezo2-positive cells outside the Ren1-positive area. These cells were located in the space between the Ren1- or Acta2- positive arterioles and renal tubules in the vascular pole, suggesting that they are extraglomerular mesangial cells (Supplementary Fig. S4). Notably, the juxtaglomerular Ren1-positive area was markedly enlarged in the dehydration group where Piezo2 and Ren1 transcripts were definitely colocalized (Fig. 4h, right, Supplementary Video S2 and Supplementary Fig. S3). The 3D reconstruction data strengthen our conclusion that Piezo2 is expressed in Ren1-positive cells.

We further used Piezo2^GFP reporter mice to confirm the above-mentioned results of the dehydration model. Glomerular GFP staining was enhanced in the dehydration group compared with that in the control group (Supplementary Fig. S5a, left, middle). No GFP signal was detected in the kidneys of wild-type C57BL/6J mice (Supplementary Fig. S5a, right). Double immunofluorescence revealed that Piezo2-GFP protein and mesangial Pdgfrb signals in the glomeruli were lower in the dehydration group than in the control group (Supplementary Fig. S5b). By contrast, Ren1 staining was augmented, and colocalization of Piezo2-GFP and Ren1 was increased in the dehydration group (Supplementary Fig. S5c), recapitulating the results of RNAscope analyses (Fig. 4).

Piezo2 gene knockdown and mechanical stretch suppress Ren1 gene expression in cultured mouse renin-producing cell line As4.1

Finally, we performed in vitro experiments using the cultured mouse renin-producing cell line As4.1 and investigated the effects of Piezo2 knockdown and mechanical load on Ren1 mRNA expression. We confirmed that As4.1 cells abundantly expressed Ren1 mRNA compared with the whole kidney sample (Fig. 5a). The cells also expressed Piezo2 mRNA, although the level was lower than that in the whole kidney (Fig. 5b).

Piezo2 mRNA knockdown was conducted in As4.1 cells with three types of Piezo2 siRNA and control siRNA, using Lipofectamine™ RNAiMAX transfection reagent. After 72 h of transfection, only one Piezo2 siRNA could sufficiently inhibit Piezo2 mRNA expression (79% reduction; P < 0.01 vs. control siRNA) (Fig. 5c). We used this construct in the following experiments. The siRNA-mediated specific knockdown of the Piezo2 gene partially but significantly reduced Ren1 mRNA expression (Fig. 5d).

It was previously reported that cyclic mechanical distension suppresses renin gene transcription in As4.1 cells³⁵. Therefore, we next examined the effects of Piezo2 knockdown and mechanical stretch. Cells were seeded onto silicon stretch chambers coated with collagen I. After transfection of control siRNA and Piezo2 siRNA for 72 h, the cells were exposed to uniaxial cyclic tensile strain (12% elongation, 0.5 Hz) for 24 h. Static cells were plated onto the same chambers, treated with control or Piezo2 siRNA, and were not subjected to cyclic stretch.

As shown in Fig. 5e, Piezo2 knockdown by siRNA lowered Ren1 gene expression under both static and stretched conditions. Cyclic mechanical strain also decreased Ren1 mRNA expression in both control siRNA and Piezo2 siRNA groups. There were statistical significant knockdown effect (P < 0.01) and stretch effect (P < 0.01), while there was no interaction effect (two-way ANOVA, n = 9 per group). The post hoc test revealed that Piezo2 knockdown significantly reduced Ren1 expression in both static (P < 0.01) and stretched (P < 0.05) conditions (Fig. 5e).

Discussion

In the present study, we demonstrated that Piezo2 is expressed in mesangial cells, juxtaglomerular renin-producing cells, and embryonic precursor cells in the mouse kidney. The in vivo alteration of renal Piezo2 expression was observed under dehydration. Furthermore, Ren1 expression in cultured As4.1 cells was downregulated by Piezo2 knockdown, suggesting an indispensable role for Piezo2 in body fluid balance.

We used RNAscope in situ hybridization technology to visualize Piezo2 transcripts and cell marker genes. This method was successfully utilized in a previous study by Zeng et al.²⁷ to detect Piezo2 expression in the nodose ganglion. Compared with the conventional in situ hybridization techniques, RNAscope has high sensitivity and specificity and enables multiplex analysis with fluorescent dyes³². We could not obtain satisfactory results from Piezo2 immunostaining using commercially available antibodies (data not shown); thus, we further used Piezo2^GFP reporter mice to assess the intrarenal distribution of the Piezo2-GFP fusion protein using anti-GFP immunostaining, as described previously^23,28 (Fig. 2a). The expression patterns of Piezo2 transcripts and the Piezo2-GFP fusion protein were similar. Furthermore, we performed immunofluorescence staining of the Piezo2-GFP protein and in situ hybridization of Piezo2 mRNA in serial sections to confirm their similar expression pattern (Fig. 2f). Since it was difficult to perform double staining of immunofluorescence and in situ hybridization on the same section, their consistency was verified using adjacent sections.

We identified clear Piezo2 gene and protein expression in Pdgfrb-positive mesangial cells in normal mouse kidneys. Mesangial cells have pivotal mechanosensitive roles in integrating the morphology of the glomerular tuft against capillary tension^5,6. Indeed, cultured mesangial cells, under mechanical stimuli such as stretching, upregulate growth factors, including transforming growth factor beta 1 (Tgfb1)⁹, vascular endothelial growth factor A (Vegfa)³⁶ and cellular communication network factor 2 (Ccn2, also known as connective tissue growth factor)³⁷, thereby promoting fibrotic change and ECM deposition^7,8. Mechanosensors in mesangial cells remained unidentified for a long time. Quite recently, Fu et al.³⁸ reported that Piezo1 is involved in ECM gene expression in cultured mesangial cells under mechanical stress and in renal fibrosis in a mouse model. They used an unconventional method of culturing cells on hydrogel with different stiffness to evaluate the effects of mechanical stress. They described that the stiffer gels induced more ECM upregulation, which was ameliorated by inhibition of Piezo1 and related signaling molecules. However, Piezo2 was not mentioned in their paper. Data from our present study suggest the possibility that Piezo2 may also contribute to the mechanosensing reactions of mesangial cells, although further studies are necessary to confirm this.

We observed Piezo2 gene and protein expression in Ren1-positive cells in the juxtaglomerular apparatus. Seghers et al.¹³ examined which of various candidate mechanosensitive ion channels mediate renin secretion from the renin-expressing As4.1 cells. They considered that Piezo2 mRNA expression was low, although present, in the cell line, and a detailed analysis was not performed. They demonstrated that knockdown of Trpv4, but not Trpv2 or Piezo1, inhibited the calcium (Ca) response to mechanical strain in the cell line. They further performed an in vivo analysis showing that Trpv4 is expressed in the juxtaglomerular cells and proximal tubules, and that systemic knockout of Trpv4 resulted in higher plasma renin levels. Our data in normal and reporter gene expressing mice, as well as in the dehydration model and in vitro analysis using the same As4.1 cells as discussed below, suggest that Piezo2 may also modulate renin release as another mechanosensor.

Our findings on Piezo2 expression in mesangial cells and renin-producing cells may further be supported by recent single-cell transcriptome analyses of mouse glomerular/mesangial cells. For example, He et al.³⁹ performed single-cell RNA sequencing of mouse glomerular cells and detected heterogeneity in glomerulus-associated Pdgfrb-expressing cells. There were 4 distinct subpopulations, including bona fide intraglomerular mesangial cells, renin-producing cells, vascular smooth muscle cells, and extraglomerular mesangial cells. It was found that Piezo2 was mainly expressed in intraglomerular mesangial cells, but also in renin-producing cells at lower levels, confirming our results. Karaiskos et al.⁴⁰ reported a single-cell transcriptome atlas of the mouse glomerulus, and Piezo2 expression was found in the mesangial and glomerular endothelial populations by searching their database (https://shiny.mdc-berlin.de/mgsca/). Lu et al.⁴¹ also performed single cell RNA-sequencing analysis using 14 mouse glomerular mesangial cell samples, and Piezo2 as well as Trpv2 and P2rx1 was included in the list of mesangial cell essential genes. Our present study suggested that Piezo2 was additionally expressed at lower levels in glomerular endothelial cells and extraglomerular cells, and these findings may not be inconsistent with the above-mentioned single cell RNA analyses.

Piezo2 was found to be expressed in subcapsular Foxd1-positive cells but not in Six2-positive cells in the developing metanephros. In mice, the kidney develops from the intermediate mesoderm-derived metanephric mesenchyme and ureteric bud through reciprocal inductive interactions. The ureteric bud forms the collecting ducts, the renal pelvis, and the ureter¹⁶. The cap mesenchyme around the ureteric bud tips contains Six2-positive nephron progenitor cells, which differentiate into podocytes, parietal epithelial cells of Bowman’s capsule, proximal tubules, the loop of Henle, distal tubules, and connecting tubules¹⁷. The loose mesenchyme around the cap mesenchyme gives rise to Foxd1-positive stromal cells, which in turn give rise to the glomerular mesangial cells and mural cells of the renal arterial tree (renin cells, smooth muscle cells, perivascular fibroblasts, and pericytes)^14,15,18. The expression of Piezo2 in mesangial cells and juxtaglomerular renin-producing cells, but not in the proximal and distal tubules and collecting ducts, is in agreement with the embryonic origin of Foxd1-positive cells. Piezo2 mRNA was expressed in Pdgfrb-positive glomerular cells and Ren1-positive cells in the embryo. Subcapsular Piezo2 expression was parallel to the presence of metanephric mesenchyme. Nephrogenesis is not completed at birth; the metanephric mesenchyme disappears at around P3⁴². Consequently, Piezo2 mRNA expression in the subcapsular metanephric mesenchyme persisted at P0 but disappeared at P15. The functions of Piezo2 in embryonic Foxd1-positive cells should be analyzed in the future.

In the mouse model of dehydration, Piezo2 expression in the whole kidney was reduced. This result may be attributed to the decrease in transcript levels in mesangial cells. The number of mesangial cells does not seem to decrease; thus, Piezo2 expression itself may be directly downregulated, presumably by intraglomerular hypotension. Conversely, the signal intensity of Piezo2 expression in juxtaglomerular renin-producing cells was markedly upregulated. It is noteworthy that the area of renin-producing cells was enlarged. It is known that renin-producing cells have lineage plasticity; when body fluid homeostasis is threatened and demand for renin release is increased, vascular smooth muscle cells adjacent to the juxtaglomerular area acquire the phenotype of renin-producing cells and secrete renin^12,43. It is tempting to speculate that such transdifferentiation might be triggered by mechanotransduction through Piezo2.

In general, an increase in Ca influx promotes exocytosis in secretory cells. On the other hand, renin release from juxtaglomerular cells is suppressed by Ca influx, a phenomenon known as calcium paradox of renin secretion¹³. The increased renin expression in our dehydration model should accompany decreased Ca, and thus Piezo2 inactivation. However, our results revealed Piezo2 upregulation in the dehydration model. We consider that these seeming contradictory Ca changes might be explained by the dual- or triple-feedback control system for the homeostasis of intracellular pressure. It is known that different types of mechanosensitive channels mediating different roles are localized on the same cells. For example, Du et al.⁴⁴ reported that Trpv4, Piezo1, and Piezo2 are expressed on the same chondrocyte, each of which transduces mechanical stimuli differentially, depending on the stimulus intensities. Nakazawa et al.⁴⁵ reported that Trpv1 and Trpv4 are expressed in lens surface cells. Trpv1 senses decreased pressure or hyperosmotic stress, whereas Trpv4 senses increased pressure or hypoosmotic stress. These reciprocal stimuli are transduced through distinct signaling pathways according to Trpv1/4, thereby forming dual-feedback systems controlling intracellular pressure or osmolarity. In such systems, there may be a possibility that reciprocal Ca changes might lead to unexpected observations. Indeed, Trpv4 is reported to be expressed in juxtaglomerular cells and As4.1 cells¹³, suggesting the possibility that the above-mentioned complicated crosstalk of Ca balance exists in juxtaglomerular cells. Further research will be needed to address this point in the future.

For evaluation of Piezo2 functions, in vivo analysis using Piezo2 knockout mice will be ideal. However, systemic Piezo2 knockout mice are lethal at P1. Generation of conditional renin-cell specific knockout mice using Cre recombinase will be rather time-consuming. Thus, in this study, we decided to perform in vitro analysis using As4.1 cells. It was revealed that Piezo2 knockdown resulted in the downregulation of Ren1 expression in both the static and stretched conditions. These findings suggest that Piezo2 functions upstream of Ren1 signaling and positively regulates its expression. Although this positive regulation is again contradictory to the “calcium paradox”, our in vitro data are in agreement with our in vivo finding of reduced mechanical stress and increased Ren1 expression in the dehydration model. It should also be noted that the stretch-induced reduction of Ren1 expression was not rescued by Piezo2 knockdown. This result suggests the possibility that the effect of mechanical stretch in our experimental condition was not mainly transduced by the Piezo2 channel. As discussed above, different mechanosensors in the same cell occasionally mediate different modes of mechanical stimuli, such that Trpv1 and Trpv4 on lens cells sense decreased and increased pressure, respectively. Thus, it should be better to evaluate mechanotransduction of Piezo2 in the context of multimodal mechanical stimuli, including osmotic stress, increased or decreased hydrostatic pressure, and deformation. Further sophistication of the experimental procedures will be necessary in the analysis of mechanical stress.

Our study has several limitations. Our morphological study suggests that Piezo2 is also expressed at low levels in the glomerular endothelial cells and extraglomerular mesangial cells. However, the data are not so convincing. If a good Piezo2 antibody becomes available in the future, it will be possible to identify cells and intracellular localization sites more clearly. Further functional analyses of Piezo2 ares also required. For example, electrophysiological analysis of the Piezo2 channel will clarify how the Ca change against the calcium paradox works. Investigation of molecular pathways upstream and downstream of Piezo2 will be interesting, considering the possible crosstalk of signaling cascades of other mechanosensors, including Piezo1 and Trpv4. In vivo Piezo2-knockout experiments will be very important to really substantiate the indispensability of Piezo2 in body fluid control.

In conclusion, the present study clearly revealed the expression of Piezo2 in the developing and adult mouse kidneys in normal and dehydrated conditions. We also showed that Piezo2 functions upstream of Ren1 in vitro. Our study suggests crucial roles for Piezo2 in renal morphology and physiology. This work may be an initial step toward clinical understanding and intervention of mechanical stress-related kidney diseases, such as hypertensive and diabetic nephropathy.

Methods

Ethical statement

The research protocols were approved by the Animal Research Committee of Kyorin University (Permit Number: Animal 216) and Recombinant DNA Experiments Safety Committee of Kyorin University (Permit Number: 179-2). All animal experiments were performed in strict accordance with the institutional guidelines and the recommendations in the ARRIVE guidelines⁴⁶.

Mice

Male C57BL/6J mice (6 to 8-week-old) and female pregnant C57BL/6J mice carrying E11.5–E15.5 embryos were purchased from Sankyo Labo Service Corporation (Tokyo, Japan). Piezo2-GFP-IRES-Cre (Piezo2^GFP) reporter mice were previously described^23,28.

For developmental analysis, E14.5–E17.5 mouse embryos were dissected out from pregnant mice under isoflurane anesthesia. Whole embryos (E14.5–E16.5), isolated metanephros (E17.5), and kidneys (P0 and P15) were fixed in 4% paraformaldehyde overnight at 4 °C, and paraffin sections (5 μm) were prepared.

To establish the in vivo model of reduced mechanical load to the glomeruli and juxtaglomerular renin-producing cells, 8-week-old male C57BL/6J mice were divided into a control group fed a standard rodent chow and drinking water ad libitum and a dehydration group fed a standard rodent chow and deprived of drinking water for 5 days (n = 6 for each). According to previously reported methods^47,48, we initially performed 1, 3, 4, and 5 days of dehydration as preliminary experiments. Then, we determined a duration of 5 days for the final experiment. The same control and dehydration interventions were also given to Piezo2^GFP mice (n = 2 for each).

Mice were housed in a room maintained at constant temperature (20 to 26 °C), humidity (40 to 60%), and light cycle (12-h light/dark). The health condition of the mice was checked every day. Mice were anesthetized with isoflurane, and all efforts were made to minimize suffering.

RNAscope in situ hybridization

RNAscope in situ hybridization was performed using an RNAscope 2.5 HD detection kit (brown), RNAscope multiplex fluorescent reagent kit v2, commercially available paired double-Z oligonucleotide probes (Advanced Cell Diagnostics, Newark, CA, USA), and a TSA plus system (Akoya Biosciences, Marlborough, MA, USA)³². The target probes used are: Mm-Piezo2-C1, Mm-Piezo2-C2, Mm-Pdgfrb-C2, Mm-Nphs1-C2, Mm-Tek-C1, Mm-Ren1-C1, Mm-Foxd1-C3, Mm-Six2-C1, negative control bacterial dapB-C1, and positive control Mm-Ppib-C1. Briefly, mice were perfusion fixed with 4% paraformaldehyde via the left ventricular apex. The kidneys were excised and immersed in the same fixative for 24 h. Paraffin sections (5-μm-thick) were baked for 1 h at 60 °C, deparaffinized, subjected to hydrogen peroxide for 10 min, boiled in target retrieval buffer for 15 min, and treated with protease plus or protease III for 30 min at 40 °C. Cryosections (8 μm) were baked for 30 min at 60 °C, postfixed in 4% paraformaldehyde for 15 min at 4 °C before hydrogen peroxide treatment. The sections were then hybridized with the target probe(s) for 2 h at 40 °C, followed by signal amplification reactions and DAB chromogen detection or fluorescence (Cy3, Fluorescein, Cy5) detection, according to the manufacturer’s protocols. Brightfield images were acquired using a light microscope (BX51; Olympus, Tokyo, Japan). Fluorescence signals were observed using a confocal laser scanning microscope (LSM 980; Zeiss, Oberkochen, Germany). Signal intensities were compared under the same acquisition conditions. Three-dimensional reconstruction was performed using the Z-stack analysis of LSM 980 and Imaris software 9.6 (Bitplane, Oxford Instruments, Belfast, UK).

Quantitative analysis of RNAscope in situ hybridization

Brightfield images of DAB reaction were analyzed by ImageJ software according to the method by Jensen⁴⁹. The subcapsular region in the embryonic metanephros was selected as the region of interest (ROI) using a rectangular tool. The whole glomerulus in the adult kidney was also selected as ROI. The DAB-mediated brown signals were measured as the integrated density after identical threshold adjustment and compared among groups.

Fluorescent images were analyzed by the Imaris software according to the manufacturer’s instruction. The glomerulus, including the juxtaglomerular apparatus, was selected as ROI, a red or green channel was selected, and the intensity sum was measured after identical threshold adjustment using Imaris Surface command. Colocalization of different colors was measured as colocalized signal density using Imaris Coloc command.

Gene expression analysis

Kidneys were harvested under isoflurane anesthesia, snap frozen in liquid nitrogen, and stored at − 80 °C. Total RNA was extracted using an RNeasy mini kit (Qiagen, Hilden, Germany), and reverse-transcribed to cDNA with high capacity cDNA reverse transcription kit (Applied Biosystems, Waltham, MA). Gene expression was quantitated by real-time quantitative RT-PCR using StepOnePlus (Applied Biosystems), as previously described⁵⁰. We used TaqMan gene expression assays reagent and commercially available primers and probe sets.

Isolation of glomeruli

Glomerular fraction was isolated using Dynabeads method⁵¹. Briefly, mice were perfused with magnetic Dynabeads M-450 (4.5 μm, Dynal, 8 × 10⁷/mouse). Renal cortices were minced, digested in Hank’s balanced salt solution (Thermo Fisher Scientific, Waltham, MA) containing collagenase A (1 mg/ml, Roche Diagnostics, Basel, Switzerland) and DNase I (100 U/ml) for 1 h at 37 °C with gentle agitation. The digested samples were filtered through 100 μm cell strainer. Magnetic beads were trapped in the glomerular capillary tufts, accordingly, glomeruli were separated from nonglomerular cells and connective tissues using a magnet.

Immunofluorescence staining

For GFP immunostaining, 4% paraformaldehyde-fixed renal cryosections (8 μm) from Piezo2^GFP mice and wild-type mice were pretreated with proteinase type XIV (0.02–0.05%, Sigma, Tokyo, Japan) for 10 min, incubated with 0.5% blocking reagent (Roche Diagnostics), then incubated with a chicken anti-GFP antibody (A10262, 1:100; Thermo Fisher Scientific) overnight at 4 °C, and finally incubated with an Alexa Fluor 488-conjugated anti-chicken IgY (H + L) secondary antibody (A11039, 1:200; Thermo Fisher Scientific)^23,28. For double immunostaining, GFP-stained sections were incubated with a rabbit anti-Pdgfrb (3169S, 1:100; Cell Signaling Technology, Danvers, MA, USA), rabbit anti-Nphs2 (29040, 1:100; Immuno-Biological Laboratories, Gunma, Japan), rat anti-Pecam1 (553370, 1:200; BD Biosciences, Franklin Lakes, New Jersey, USA), or rabbit anti-Ren1 (ab212197, 1:1000; Abcam, Cambridge, UK), followed by an Alexa Fluor Plus 555-conjugated anti-rabbit IgG (H + L) secondary antibody (A32794, 1:200; Thermo Fisher Scientific) or Cy3-conjugated Affini Pure F(ab′)₂ fragment anti-rat IgG (H + L) secondary antibody (712-166-153, 1:200; Jackson ImmunoResearch, West Grove, PA, USA). Fluorescence signals were observed using confocal laser scanning microscope (LSM 980; Zeiss).

Immunoelectron microscopy

4% paraformaldehyde-fixed cryosections (10 µm) were treated with 3% hydrogen peroxide, 0.025% proteinase type XIV for 10 min, avidin–biotin blocking solution, 0.5% blocking reagent, incubated with a chicken anti-GFP antibody overnight at 4 °C, and subsequently with a biotin-conjugated anti-chicken IgY (H + L) secondary antibody (703-066-155, 1:200; Jackson ImmunoResearch). Immunosignals were detected using a Vectastain Elite ABC kit (Vector Laboratories, Burlingame, CA) and a metal-enhanced DAB kit (Thermo Fisher Scientific). Sections were postfixed in 2.5% glutaraldehyde, immersed in 1% OsO₄, dehydrated, and embedded in Epon 812. Ultrathin sections were stained with uranyl acetate and lead citrate, and observed using JEM-1010 transmission electron microscope (JEOL, Tokyo, Japan)⁵².

Cell culture

Mouse renin-producing cell line As4.1 was purchased from ATCC (CRL-2193). The cells were maintained in DMEM with high glucose (25 mM) and pyruvate (11995, Thermo Fisher Scientific) supplemented with 10% heat-inactivated FBS (HyClone), penicillin, and streptomycin in a humidified incubator at 37 °C in 5% CO₂/95% air.

siRNA transfection

A set of pre-designed Stealth RNAi™ siRNA for mouse Piezo2 (catalogue No. 1320003 containing 3 siRNA oligonucleotides, ID: MSS212843, MSS212844, and MSS212845) and control siRNA were purchased from Thermo Fisher Scientific, which guarantees high specificity and less unwanted off-target effects. The day before transfection, the cells were seeded on a 6-well plate or stretch chamber (10 cm²). Transfection was carried out with siRNA using Lipofectamine RNAiMAX (Themo Fisher Scientific), according to the manufacturer’s instruction. Knockdown efficacy was evaluated by quantitative RT-PCR.

Cyclic mechanical stretch

As4.1 cells were seeded onto silicon stretch chambers (STB-CH-10, STREX, Osaka, Japan) coated with collagen I (Koken). At 72 h after transfection, a uniaxial cyclic tensile strain (12% elongation, 0.5 Hz) was applied using a cell stretching system (STB-140, STREX) by which a uniform strain can be loaded to the cells along the stretch axis⁵³. The stretch frequency and ratio were determined, according to a previous stretch experiment performed on this cell line³⁵. Control cells were plated onto the same chambers, and were not subjected to cyclic stretch.

Statistical analysis

Data are expressed as mean ± s.e.m. Statistical analysis was performed by a two-tailed unpaired Student’s t-test for comparison between the two groups, and by one-way or two-way ANOVA followed by Bonferroni's post hoc test for multiple comparisons. Statistical significance was set at P < 0.05.

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Acknowledgements

We thank Prof. Ardem Patapoutian for his kind gift of the Piezo2-GFP mouse line; Ms. Naho Suzuki for her technical support; and Ms. Sachie Matsubara and Ms. Junri Hayakawa (Laboratory for Electron Microscopy, Kyorin University School of Medicine) for their technical EM support. This study was supported in part by Japan Agency for Medical Research and Development (JP18gm5810019 and JP17gm5810027), by Grants-in-Aid for Scientific Research from the Japan Society for the Promotion of Science (17K09736, 20K08616), and by the collaborative research fund program for women researchers from the Tokyo Medical and Dental University, funded by “Initiative for Realizing Diversity in the Research Environment”, from MEXT, Japan.

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Department of Anatomy, Kyorin University School of Medicine, 6-20-2 Shinkawa, Mitaka, Tokyo, 181-8611, Japan
Yuki Mochida, Koji Ochiai, Yoshihiro Akimoto, George Matsumura & Miki Nagase
Department of Trauma and Critical Care Medicine, Kyorin University School of Medicine, Tokyo, Japan
Yuki Mochida, Koji Ochiai & Yoshihiro Yamaguchi
Kunitachi Aoyagien Tachikawa Geriatric Health Services Facility, Tokyo, Japan
Takashi Nagase
Division of Embryology, National Institute for Basic Biology, Okazaki, Japan
Keiko Nonomura
Department of Urology, Kyorin University School of Medicine, Tokyo, Japan
Hiroshi Fukuhara
Juntendo University Faculty of Health Science, Tokyo, Japan
Tatsuo Sakai
Department of Anatomy and Life Structure, Juntendo University Graduate School of Medicine, Tokyo, Japan
Tatsuo Sakai & Miki Nagase
Department of Medical History, Juntendo University Faculty of Medicine, Tokyo, Japan
Tatsuo Sakai

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Yuki Mochida
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Y.M. and M.N. conceived and designed the research. Y.M., K.O., M.N. conducted experiments and analysis of data. K.N. contributed materials. Y.A. conducted electron microscopic analysis. Y.M., T.N. and M.N. wrote the main manuscript text. Y.M. and M.N. prepared Figs. 1, 2, 3, 4, 5, Supplementary Fig. S1, S3, S4, S5, Supplementary Video S1 and S2. Y.A. prepared Supplementary Fig. S2. K.N., H.F., T.S., G.M., and Y.Y. discussed and revised the manuscript critically for important intellectual content. All authors reviewed and approved the manuscript.

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Mochida, Y., Ochiai, K., Nagase, T. et al. Piezo2 expression and its alteration by mechanical forces in mouse mesangial cells and renin-producing cells. Sci Rep 12, 4197 (2022). https://doi.org/10.1038/s41598-022-07987-7

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Received: 03 September 2021
Accepted: 01 March 2022
Published: 10 March 2022
DOI: https://doi.org/10.1038/s41598-022-07987-7

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