Mechanosensitive channels (MSCs) and primary cilium possess a possible relevance for the sensation of intraocular pressure (IOP). However, there is only limited data on their expression and localization in the ciliary body epithelium (CBE). The purpose of this study was to characterize the expression and localization of TRPP2 in a human non-pigmented ciliary epithelial cell (HNPCE) line.
Methods
The expression of the TRPP2 was studied by quantitative (q)RT-PCR and in situ hybridization in rat and human tissue. Protein expression and distribution were studied by western blot analysis, immunohistochemistry, and immunoelectron microscopy. Cellular location of TRPP2 was determined in rat and human CBE by immunofluorescence and immunoblot analysis. Electron microscopy studies were conducted to evaluate where and with substructure TRPP2 is localized in the HNPCE cell line.
Results
The expression of TRPP2 in rat and human non-pigmented ciliary epithelium was detected. TRPP2 was mainly located in nuclei, but also showed a punctate distribution pattern in the cytoplasm of HNPCE of the tissue and the cell line. In HNPCE cell culture, primary cilia did exhibit different length following serum starvation and hydrostatic pressure. TRPP2 was found to be colocalized with these cilia in HNPCE cells.
Conclusion
The expression of TRPP2 and the primary cilium in the CB may indicate a possible role, such as the sensing of hydrostatic pressure, for the regulation of IOP. Functional studies via patch clamp or pharmacological intervention have yet to clarify the relevance for the physiological situation or aqueous humor regulation.
Wenxu Zheng and Focke Ziemssen contributed equally to this work.
Publisher's note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
×
Introduction
Impaired sensation of intraocular pressure (IOP) contributes to the imbalance between aqueous humor secretion of the ciliary body (CB) and the outflow in the trabecular meshwork (TM). Although little is known on the specific baroreceptors, recent studies describe the potential role of primary cilia in this context. Cilia localized in TM cells are altered in the rare congenital Lowe syndrome with congenital glaucoma [1]. Primary cilia have also been described as potential mechanosensory organelles in cholangiocytes [2], vascular endothelia [3, 4], renal collecting duct epithelium [5], and chondrocytes [6]. A shortening of the primary cilia is observed with increasing hydrostatic pressure; the transient receptor potential vanilloid 4 (TRPV4) is a responsible mechanosensitive channel of the cilia [1]. Therefore, a structured search of other candidates keeps the focus on the transient receptor potential (TRP) cation channel family [7].
Anzeige
Polycystin-2 (TRPP2) has been reported to be located on primary cilia. The channel contributes to fluid-flow sensation in kidney cells [8], vascular endothelial cells [9], and cholangiocytes [2]. The protein is a Ca2+ permeable transient receptor potential (TRP) cation channel, whose deficiency may cause autosomal-dominant polycystic kidney disease (ADPKD) [10].
This study was initiated to characterize the ocular expression and localization of TRPP2. The colocalization of TRPP2 with primary cilia was analyzed in human non-pigmented ciliary epithelial (HNPCE) cells, at the site of which the active transport of ions makes an important contribution responsible for the production of aqueous humor in the CB [11]. The carbonate anhydrase is important, controlling local pH with bicarbonate transport through the ciliary epithelium (hydration of CO with formation of HCO and protons). Chloride (Cl) is the major anion transported through the epithelium via Cl channels and, with other actively transported molecules, drives ultrafiltration and diffusion via osmotic gradients. It is still unclear which individual forms of glaucoma might be due to the aforementioned ciliopathies [1]. The aim of these studies was to improve the knowledge of the (ultra)structure in the CB, with focus on TRPP2.
Materials and methods
Animal and tissue preparation
Animals were treated according to the Principles of Laboratory Animal Care (NIH publication No. 85–23, revised 1985), the OPRR Public Health Service Policy on the Human Care and Use of Laboratory Animals (revised 1986), and the German animal protection law. Rat eyes of an approved experiment were used (Approval number of the Animal research Committee: HG6/14). Six wildtype female Sprague–Dawley rats (12 weeks old) were sacrificed using carbon dioxide inhalation, and 12 eyes were enucleated immediately after death. After careful dissecting of the whole eyeballs, 3 eyes were fixed for immunohistochemistry, 6 eyes were processed for protein analysis, and 3 eyes were processed for mRNA analysis. For protein and mRNA analysis, the eyes were transferred under a sterile hood and dissected under a microscope into seven parts: the retina, CB, cornea, sclera, optic nerve (ON) iris, and lens. The tissues were subsequently frozen using liquid nitrogen and stored at − 80 °C until further analysis.
Human ocular specimens
Human eye experiments were conducted according to the tenets of the Declaration of Helsinki, and the study was approved by the local ethics committee (Ethics No.: 332/2021BO2). 3 human eyes that were removed due to choroidal melanoma but with a normal anterior segment were obtained (University of Tübingen, no. 38072, 38,282, 38,375). Only eyes with normal structure of ciliary body were used for analysis.
Anzeige
HNPCE cell culture
Primary HNPCE cells were purchased from ScienCell Research Laboratories (cat no. 6580, CA, USA). The cells were cultured in epithelial cell medium (ScienCell Research Laboratories, cat no. 4101, CA, USA) at 37 °C in an incubator with 5% CO2 and 95% humidity according to the instruction of manufacturer. Originally, the cells were derived from clones obtained from a primary culture of human nonpigmented ciliary epithelium [12].
Horizontal Sects. (12 µm) of the rat tissue (n = 6–8/group) were cut with a cryostat by a cryostat (Leica CM3000; Leica, Germany) at -20 °C for immunofluorescence. The slices were fixed with ice-cold methanol for 10 min at room temperature (RT). After washing with Tris-buffered saline (TBS), slices were incubated with Jacalin-FITC, a marker for NPE cell, for 30 min in a dark chamber at RT. Then blocking at RT for 1 h with 5% bovine serum albumin (BSA) in TBS, slices were incubated with the primary antibody TRPP2 (Table 1) at 4 °C overnight. After washing, slices were incubated with the fluorescence-labeled secondary antibody for 1 h at RT. Slides were observed on Axioskop fluorescent microscope (Zeiss, Germany). To ensure avoidance of selection bias for areas of staining, the first field of view of the tissue of interest was selected as start point of analysis. Analysis was performed in a raster fashion to ensure no selection or double counting. Cells were counted as immunopositive or immunonegative, before the percentage of immunopositivity was calculated and compared with the positive control tissue.
Immunohistochemistry staining
Immunohistochemistry was performed to detect the expression of TRPP2 in human eye tissues. After removing paraffin from human eye, tissue Sects. (4 µm) by using xylol the specimen were rehydrated in a graded alcohol series. Antigen retrieval was performed in citric buffer (pH 6.0). Primary antibody TRPP2 for detection of TRPP2 and mouse anti-acetylated α-tubulin for detection of primary cilia axoneme (Table 1) were incubated at 4 °C overnight. After incubation with secondary antibody, the immunoreaction was detected using a commercially available alkaline phosphatase-anti-alkaline phosphatase kit (Dako REAL™ Detection System, Alkaline phosphatase/red, rabbit/mouse, DakoCytomation GmbH, Hamburg, Germany). Sections were counterstained with Mayer’s hematoxylin (n = 4–6/group). For negative controls, sections underwent the same immunohistochemical staining procedure without the primary antibody [13]. The same camera settings (including exposure time) were used for all images. For all analyses, we used an ImageJ macro. After background subtraction, the same lower and upper thresholds were set. The percentage of the labeled areas was measured for each picture using the macro and exported to Excel.
Western blotting
Tissue and cellular samples were homogenized in cell lysis buffer (cat no. FNN0011, Invitrogen, CA, USA), supplemented with phenylmethylsulfonyl fluoride and a protease inhibitor cocktail (#539,134, Calbiochem, San Diego, USA). After homogenization at 13,000 × g (4 °C) for 10 min, the supernatant was collected for protein analysis. The protein content was determined using a BCA protein assay kit (#23,227, Pierce, Rockford, USA). The same amount of protein was separated on sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) gels for expression analysis. 10% SDS-PAGE gels (Mini-PROTEAN® TGX™ Gel, #456–1033, Bio-Rad., CA, USA) were used to detect TRPP2. After SDS gel separation, proteins were transferred onto nitrocellulose membranes using a wet transfer technique (350 mA for 1 h). Membranes were blocked for 1 h in 5% nonfat dry milk in TBST. The membranes were incubated with the primary antibody TRPP2 (Table 1) at 4 °C overnight. After washing three times with TBST and incubation with the appropriate secondary antibody for 1 h at RT, membranes (n = 3) were detected using an Odyssey Imaging System (Li-Cor Bioscience) [14]. Rat kidney tissue was used as a positive control.
Serum starvation of HNPCE cells
HNPCE cells were exposed to serum starvation before cilia length was evaluated. Primary HNPCE cell cultures were seeded on poly-L-lysine (PLL)-coated cover slips in 24-well plate at a density of 4.0 × 104 cells/well. On the next day, the growth medium of HNPCE cells was changed from 1% serum medium to no serum medium. After serum starvation for 24, 48, and 72 h, HNPCE cells were used for immunocytochemistry (n = 5–6/group).
Immunocytochemistry staining
After serum-starvation, the HNPCE cell cultured cover slips were treated with 4% paraformaldehyde (PFA) for fixation for 15 min at RT followed by permeabilization with 0.2% Triton X-100. Samples were then blocked with 1% BSA/PBS for 90 min at RT. Primary antibody mouse anti-acetylated α-tubulin and rabbit anti-γ-tubulin (Table 1) for detection of primary cilia axoneme and basal body, rabbit anti-TRPP2, and mouse anti-acetylated α-tubulin (Table 1) for colocalization of TRPP2 and primary cilia were applied at 4 °C overnight, followed by secondary antibodies for 1 h at RT. Slides (n = 5–6/group) were observed on fluorescent microscope (Zeiss Axioskop). Imaging was analyzed with an Axio (Version 4.8) for cilia measurements.
Total RNA extraction and reverse transcription PCR
mRNA was extracted from rat eye tissue (n = 3–6/group) or HNPCE cells (n = 6–8/group) and directly synthesized to cDNA using the Milteny MultiMACS cDNA Synthesis Kits according to the manufacturer’s instructions. Synthesized cDNA was stored at -20℃ for further analysis. Primers were designed for TRPP2 by using NCBI’s Primer-BLAST. The sequences for human TRPP2 were forward-TCGACAAGATCTCAAAGGGA and reverse-GTCTCACCAGGACTTGAAAC; for rat were forward-AGGACCTAGACTTGGAACAC and reverse-GTGGATCTCACTATCCCGAC. Conventional PCR was performed with Go Taq® Hot Start Polymerase (M5001, Promega, US) in the UNO Cycler PCR system (VWR, UK). 2 μl of undiluted cDNA was used to amplify the TRPP2 sequences in a 25-μl reaction volume. The thermocycling conditions were 5 min at 94 °C, followed by 45 cycles of 30 s at 94 °C, 30 s at 58 °C, and 30 s at 72 °C. The final elongation step was 7 min at 72 °C. After conventional PCR, the amplicons were resolved on 1.0% agarose gels for electrophoresis. Gels were then detected using the Odyssey Imaging System (Li-Cor Bioscience).
Anzeige
Electron microscopy
The HNPCE cell was fixed overnight at 4 °C in 2% glutaraldehyde in 0.1 M cacodylate buffer (pH 7.4) and post fixed with 1% OsO4% at room temperature in 0.1 M cacodylate buffer for 1 h, stained with uranyl acetate, and embedded in Epon after dehydration in a graded series of ethanol. Ultrathin sections were made and analyzed with a Zeiss 900 electron microscope (Zeiss, Jena, Germany) [15].
Statistical analyses
Regarding immunohistology and western blot, data are presented as the mean ± standard error of the means (SEMs), unless otherwise noted. Statistical comparisons were calculated by unpaired Student’s t test using SPSS Statistics (Version 26.0) software (IBM, Armonk, NY, USA). A p value ≤ 0.05 was considered as statistically significant.
Results
Expression of TRPP2 in rat eyes
Positive TRPP2 staining in rat ciliary body (CB) was shown via immunofluorescence. Jacalin confirmed the localization in NPE cells of the ciliary body. Protein expression analysis revealed TRPP2 abundance in the non-pigmented epithelium (NPE), pigmented epithelium (PE), and stroma of CB (Fig. 1a).
Fig. 1
Localization of TRPP2 in rat eye tissue (n = 6). a TRPP2 was distributed in the rat ciliary body. TRPP2 antibody (red); Jacalin-FITC (green); DAPI (blue). Scale bar: 50 µm (n > 20 sections). NPE, non-pigmented epithelium; S, stroma. b Western blot analysis showed the protein expression level of TRPP2 in different tissues of a rat eye (n = 3). The largest band (220 kDa) is the dimer of TRPP2, the 110 kDa and 85 kDa bands represent two different isoforms of TRPP2. c Quantitative analysis of three different forms of TRPP2 protein in different tissue. The expression of TRPP2 was normalized to β-actin. Three times of replications were done. d Reverse transcription PCR showed the mRNA expression level of TRPP2 in different tissues of rat eye (n = 6). A 344 bp band represents the PCR product of TRPP2. CB, ciliary body; ON, optic nerve; NC, negative control
×
Western blot analysis was performed to study the expression level of TRPP2 in different structures of the rat eye. Three different forms of TRPP2 protein were observed by western blot. The largest band (220 kDa) is the dimer of TRPP2, while the 110 kDa and 85 kDa bands represent two different isoforms of TRPP2. The dimer of TRPP2 was highly expressed in the cornea (14.76 ± 1.65), CB (3.03 ± 1.30), and the lens (2.10 ± 1.15), but not in other parts. The isoform with 110 kDa was expressed weakly in the retina (0.62 ± 0.27), sclera (0.32 ± 0.16), CB (0.19 ± 0.06), and iris (0.18 ± 0.05), but not in other tissues. The 85 kDa isoform was highly expressed in the CB (2.06 ± 0.90), cornea (15.28 ± 1.61), sclera (2.51 ± 0.42), ON (1.46 ± 0.70), and lens (1.23 ± 0.43) but weakly expressed in the retina (0.37 ± 0.04) and iris (0.67 ± 0.13) (Fig. 1b and c).
Anzeige
Additional analysis with reverse transcription PCR confirmed expression of TRPP2 in different tissues of the rat eye. A 344 bp band represented the PCR product of TRPP2 (Fig. 1d), further sanger sequencing validated the PCR product (Supplementary Material, Fig. S1).
Expression of TRPP2 in human ciliary body and HNPCE cells
TRPP2 staining was analyzed in human tissue. Similarly to the rats, we observed the expression of TRPP2 in non-pigmented as well as pigmented cells of the human CB (Fig. 2a). Furthermore, the expression of TRPP2 in HNPCE cell culture was tested by using western blot analysis (Fig. 2b), PCR (Fig. 2c), and immunostaining (Fig. 2d). In agreement with the result of immunohistochemistry staining of the human ciliary body, immunostaining, PCR, and western blot results all proved the expression of TRPP2 in HNPCE. Interestingly, we observed that TRPP2 was mainly located in nuclei and in punctate distribution in the cytoplasm of HNPCE cells (Fig. 2d).
Fig. 2
The expression of TRPP2 in human ciliary body and HNPCE cells. a TRPP2 is expressed in the human ciliary body epithelium (n = 6). TRPP2 antibody (red); nuclei (blue). Scale bar: 50 µm (n = 3). b Western blot analysis showed the expression of TRPP2 in HNPCE cells; β-actin was used as loading control (n = 3). c TRPP2 mRNA expression was detected by reverse transcript PCR. d Immunofluorescence staining displays that the TRPP2 (red) localized in nuclei (via DAPI staining; blue) and partly in cytoplasm of HNPCE cells. Scale bar: 10 µm
×
Serum starvation induced the formation of primary cilia in HNPCE cells
The expression of TRPP2 and structure of primary cilia were examined more closely: acetylated α-tubulin and rabbit anti-γ-tubulin for detection of primary cilia axoneme and basal body were observed in cultured HNPCE cells by immunofluorescence staining (Fig. 3a). First, the length of primary cilia was calculated at different time points after serum starvation directly on the AxioVision Viewer (AxioVs40 V 4.8.2.0; Carl Zeiss MicroImaging, Germany). Extension of the starvation time to 24 h, 48 h, and 72 h, respectively, did not affect the length of primary cilia. After 24 h of serum starvation, HNPCE cells formed 4.4 μm (4.4 ± 1.4 μm) primary cilia in length. After 48 h of starvation, the length of primary cilia remained almost the same (4.8 ± 1.0 μm). After 72 h of starvation, the average length of the primary cilia was 5.1 μm (5.1 ± 0.9 μm). No significant difference was observed between different time points (Fig. 3b). Next, the cells with primary cilia were counted at different time points of serum starvation. Interestingly, our results showed that extension of the time of serum starvation could induce the formation of primary cilia in HNPCE cells. Without serum starvation (at 0 h) only 26.0% (± 5.6%) of cells formed primary cilia. After serum starvation for 24 h, the percentage of cells with primary cilia increased to 65% (± 4.9%). Extended serum starvation time to 48 or 72 h caused almost all HNPCE cells to form primary cilia (93.9 ± 6.1% at 48 h and 96.4 ± 4.7% at 72 h) (Fig. 3c).
Fig. 3
Formation of primary cilia in HNPCE cell culture and human ciliary body epithelium. a Serum starvation of HNPCE cells was performed at 0, 24, 48, and 72 h (n = 6). Representative immunofluorescence photomicrographs showing cilia formation with anti-acetylated α-tubulin (green) antibody and γ-tubulin (red) antibody (DAPI, blue). Cilia length (b) and ciliation rate (c) are given. Error bars represent SD (SD). n > 50 cilia, three independent experiments, ANOVA, *p < 0.05. (Scale bar, 5 μm). An increase of cilia from 26.0 ± 5.6% to 96.4 ± 4.7% was seen after 72 h, accompanied only by a slight elongation of 4.4 µm ± 1.0 μm to 5.1 µm ± 0.9 µm. d Electron micrograph showed a primary cilium in HNPCE. Arrow shows the crossing section of primary cilium. (Scale bar, 500 nm). e Immunohistochemical staining detected a primary cilium in HNPCE of the human eye. Arrow shows primary cilium. (Scale bar, 5 μm)
×
Primary cilia formation in HNPCE cells of human ciliary body
In HNPCE cell culture, the typical sign of primary cilia, a “9 + 0” arrangement was observed and confirmed (Fig. 3d). The electron microscopic images verified that HNPCE cells can form primary cilia. Immunohistochemistry staining of cilia structure was performed in human ciliary body epithelium, and we observed primary cilia in the non-pigmented epithelium of the ciliary body (Fig. 3e). Thus, the existence of primary cilia was approved in the HNPCE cells in vitro and in vivo.
Anzeige
Colocalization of primary cilia and TRPP2
The co-localization of TRPP2 and acetylated α-tubulin, primary cilia marker, was examined by using double immunofluorescence staining. TRPP2 was distributed on the axoneme and the basal body of primary cilia in HNPCE cells with 48 h serum-starvation (Fig. 4). Although no functional studies as a function of TRPP2 have yet taken place, previous observations regarding cilia length as a function of hydrostatic pressure have been confirmed.
Fig. 4
Immunostaining for TRPP2 co-localized to primary cilia in HNPCE cells (n = 5). Double immunostaining was performed on HNPCE cells after serum-starved for 48 h. TRPP2 antibody (red); acetylated α-tubulin (green); DAPI (blue). (Scale bar, 5 μm)
×
Discussion
The expression of the mechano-sensitive membrane protein TRPP2 within the CB epithelium was confirmed, in rat (Fig. 1) as well as in human eyes (Fig. 2). The detection was not limited to non-pigmented cells. We found a co-localization of TRPP2 and primary cilia, very similar to the situation as it was pre-described in the trabecular meshwork for TRPV4 [1].
Earlier reports also indicate the role of TRPP2 in sensing mechanical pressure. For example, the polycystin complex, which is assembled by TRPP2 and its molecular chaperones of polycystin-1, can be activated and induced Ca2+ influx to primary by mechanical pressure on several stress-bearing cells, like kidney cells [8], vascular endothelial cells [9], vascular smooth muscle cells [16], and bronchial smooth muscle cells [17]. A case report showed that a polycystic kidney disease (PKD) patient had experienced rapid loss of vision during the terminal stages of his illness, and the postmortem examination revealed glaucomatous changes in both eyes [18]. Thus, there might be a potential connection between glaucoma and polycystic kidney disease secondary to TRPP2.
So far, in eye tissue, TRPP2 has been identified in human TM tissue and primary TM tissue by using immunohisto- and immunocytochemistry staining and western blot and mass spectrometric analyses [19]. Obermüller et al. showed that TRPP2 was punctuated distribution in cytoplasmic of rat corneal epithelium [20]. In mouse retina, TRPP2 expression was also detected through RT-PCR, northern blot, in situ hybridization, and immunodetection [21]. In the retina of a normal SD rat, the endogenous polycystin-2 (TRPP2) was present in the ganglion cell layer, inner nuclear layer (INL), outer nuclear layer (ONL), and photoreceptor cells [22]. Choi et al. using three methods of PCR identified that TRPP2 was expressed in the mouse optic nerve head [23]. Our study for the first time showed the distribution of TRPP2 in both rat and human CB, as well as in HNPCE cells. The formation of aqueous humor is attributed to the ciliary epithelium of CB [11].
Although their significance for certain forms of glaucoma are uncertain or questionable, primary cilia have been described as mechanosensory organelles in a wide range of other cells [2‐6]. The primary cilium membrane is constituted by a microtubule based axoneme and anchored through a basal body [24]. In this study, we observed the primary cilia in a cell line of HNPCE cells and human ciliary body by using immunostaining of acetylated α-tubulin also known as Arl13b, a small GTPase which localized in the cilia. The basal body of primary cilia was detected by using γ-tubulin staining. After immunofluorescence, co-staining of TRPP2, and primary cilia, we observed the colocalization of TRPP2 and primary cilia (Fig. 4), which may support that during the IOP regulation, TRPP2 may sense the IOP or at least participate in this procedure.
Previous reports showed that TRPP2 on primary cilia may function not only as a mechanosensitive channel [25] but also as a regulator of other mechanosensitive channels, because TRPP2 can be assembled as homo-tetramer [26] and hetero-tetramer with polycystin-1 (PKD1) [27], TRPC1 [26], and TRPV4 [28]. TRPP2 interacts with popycystin-1(PKD1) to form a 3:1 complex channel by C-terminal coiled-coil domain [27]. TRPP2 and TRPC1 form a hetero-tetramer with a 2:2 subunit and an alternating arrangement [26]. Similarly, as TRPP2 and TRPC1, TRPP2 and TRPV4 also form a hetero tetramer with a 2:2 alternating subunit arrangement [28]. Hetero-tetramer also could be assembled by three different kinds of TRP subfamily; Du et al. found TRPV4, TRPC1, and TRPP2 can assemble to form a heteromeric TRPV4-C1-P2 complex heteromeric channel. The fourth subunit in this tetrameric channel could be anyone of the three channels [29]. Recently, a hetero-multimer included both TRPM3 and TRPP2 subunits were also found that might exist in primary cilia of renal epithelia cells by Kleene et al. [30]. TRPP2 can not only form a hetero tetramer with other TRP family members but could also interact with other MSCs. For example, TRPP2 may inhibit PIEZO1-dependent stretch-activated channels in renal tubular epithelial cells [31]. TRPP2 can also block the mechanical activation of TREK1 by a filamin A-mediated cytoskeletal mechanism [32]. Interestingly, TRPP2 could be inhibited by high levels of PI(4,5)P2 in the membrane [33], while lack of mutation of OCRL lead to accumulation of PI(4,5)P2. The OCRL, a phosphoinositide 5-phosphatases, is well known to metabolize PI(4,5)P2 into PI(4)P. Mutation of OCRL can cause Lowe syndrome, which includes congenital cataract and glaucoma [34]. Thus, these data indicate that TRPP2 may play an important role in regulating mechanosensitive processes through OCRL [1]. The detection of TRPP2 in the HNPCE cell line should not be confused with the proof of the relevance in human TM cells. Furthermore, the presence of TRPP2 on primary cilia does not necessarily mean that they play a role in regulating IOP in the eye. This evidence remains to be verified by functional/electrophysiological methods.
In the present study, we investigated whether serum starvation affected the formation of primary cilia. Serum starvation is a widely described method of inducing primary cilia [35]. Using this method, we observed that the average lengths of primary cilia did not change significantly when the starvation time is extended from 24 to 72 h. This result is different from Luo’s study in primary human trabecular meshwork (TM) cells in which the average lengths of cilia are increased followed serum deprivation [1]. It is unclear whether these differences are due to the fact that the HNPCE cells are different from TM or primary human cells. Similarly to the TM cells, increasing serum starvation time leads to increased percentage of cells with primary cilia. In TM cells, primary cilia are critical for response to pressure changes, and the primary cilia in TM cells can be shortened in response to fluid flow or elevated hydrostatic pressure [1]. Whether the length of primary cilia in human tissue will change following high pressure needs to be investigated.
We acknowledge that there are some important limitations of this study. The direct connection of TRPP2 and primary cilia to IOP regulation needs further characterization. No causal mutation of TRPP2 has been characterized yet, affecting the function of the ciliary body. The non-selective cation-channel TRPP2 is expressed in various tissues including epithelial cells, vascular smooth muscle cells, endothelial cells, cardiac myocytes, adrenal glands, and ovaries [9, 16, 17, 36]. By forming homomultimeric or heteromultimeric channels with the same or other subfamilies, the function depends on the subcellular distribution [37]. In vascular smooth muscle cells, TRPP2 is primarily located in the sarcoplasmic reticulum (SR) and differentially regulates the myogenic response in different vascular beds [16]. The application of TRPP2-specific siRNA, leading to the knockdown of TRPP2, resulted in a reduction of swelling-induced cation currents in vascular smooth muscle cells and a decrease in pressure-induced constriction in cerebral arteries (resistance size) [38]. In endothelial cells, the role as a mechanosensing Ca2+ channel conveys a flow-induced vascular dilation [39]. Decreased TRPP2 expression was found to be associated with abnormal vascular function and decreased NO levels. In high salt intake-induced hypertensive rats, TRPP2 protein expression was increased in the vascular smooth muscle cells of the thoracic aorta and mesenteric arteries [40].
The breadth and different role in the response to mechanical signals, from shear stress to blood pressure, is explained by the interaction with different molecules [41]. In reconstituted lipid bilayers, the amplitude and frequency of ionic oscillations of TRPP2 were strongly dependent on the applied voltage, the Ca2+ gradient, and the presence of high Ca2+ [42].
In summary, our data demonstrate the expression of TRPP2 in the ciliary body and the colocalization of TRPP2 with primary cilia, suggesting useful/necessary experiments to test the possible role of TRPP2 in the sensation of IOP. Although the importance in the regulation of hydrostatic pressure within the posterior chamber cannot yet be assessed, the involvement of TRPP2 in the complex control seems conceivable.
Acknowledgements
This work was conducted in the Center for Ophthalmology, Eberhard Karl University Tübingen, Tübingen, Germany, and supported by the China Scholarship Council (W. Zheng, 201206170032). We thank the transgenic facility Tübingen for placing animals for this study and the patients for their agreement of using eye samples for research.
Declarations
Ethical approval
All procedures, in particular the use of human material, were in accordance with the ethical standards of the University of Tuebingen and with the 1964 Helsinki declaration and its later amendments or comparable ethical standards. The experiments were conducted after approval by the local ethics committee (Ethics No.: 332/2021BO2). In the interest of animal welfare, rat eyes were used from animals that had been used as controls in other experiments and therefore had not been exposed to any effect (Approval number of the Animal research Committee: HG6/14).
Conflict of interest
FZ received grants and personal fees from AbbVie, Alimera, Apellis, Bayer Healthcare, Biogen, Boehringer Ingelheim, Clearside, Novartis, Novo Nordisk, MSD Sharp & Dohme, Roche/Genentech, Sanofi, and Stada, but none related to this study. The other authors declare no competing interests.
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/.
Publisher's note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Orbitale und periokuläre metastatische Tumoren galten früher als sehr selten. Aber mit der ständigen Aktualisierung von Medikamenten und Nachweismethoden für die Krebsbehandlung werden neue Chemotherapien und Strahlenbehandlungen eingesetzt. Die …
Metastasen bösartiger Erkrankungen sind die häufigsten Tumoren, die im Auge diagnostiziert werden. Sie treten bei ungefähr 5–10 % der Patienten mit soliden Tumoren im Verlauf der Erkrankung auf. Besonders häufig sind diese beim Mammakarzinom und …
Wird ein Glaukom chirurgisch behandelt, ist die anschließende Wundheilung von entscheidender Bedeutung. In diesem CME-Kurs lernen Sie, welche Pathomechanismen der Vernarbung zugrunde liegen, wie perioperativ therapiert und Operationsversagen frühzeitig erkannt werden kann.
Peri- sowie intraokuläre Metastasen sind insgesamt gesehen selten und meist Zeichen einer fortgeschrittenen primären Tumorerkrankung. Die Therapie ist daher zumeist palliativ und selten kurativ. Zudem ist die Therapiefindung sehr individuell. Die …
Update Augenheilkunde
Bestellen Sie unseren Fach-Newsletterund bleiben Sie gut informiert.
