Medaka villin 1-like protein (VILL) is associated with the formation of microvilli induced by decreasing salinities in the absorptive ionocytes
Frontiers in Zoologyvolume 11, Article number: 2 (2014)
Villin 1 is an actin-regulatory protein involved in the formation of microvilli of mammalian enterocytes. The microvilli, finger-like protrusions, are more abundant on the apical surfaces of gill ionocytes in various freshwater (FW) teleosts than in seawater (SW) fishes. However, the plasticity in the mechanisms of microvillus formation in the gill ionocytes are poorly understood, and the actin-regulatory proteins involved in the formation of microvilli have not been identified in fishes. The present study used the euryhaline medaka (Oryzias dancena) as a model to explore the role of a homolog of villin 1 in the actin-organization of cellular morphologies induced by decreasing salinities.
By ultrastructural observation, there are numerous actin filaments organized on the apical cortex of ion-absorptive ionocytes in the FW-acclimated medaka. From gills of the euryhaline medaka, we have identified the VILL sequence. The phylogenetic tree and functional domains suggest that VILL is the homolog of villin 1 in fishes. Immunofluorescence using a specific antibody revealed that VILL was specifically localized to the apical region of gill ionocytes along with microvilli in the FW medaka, but not in SW fish. The expression levels of Odvill mRNA and VILL protein were higher in the gills of the FW individuals than in the SW group and were induced when fish were transferred from SW to FW. A morpholino oligonucleotide for VILL knockdown eliminated the apical protrusions of ionocytes and pavement cells in the trunk epithelia of embryos.
From a novel aspect of cytoskeletal functions, our findings highlighted the important role of VILL protein in the ionoregulation of aquatic vertebrates in response to different osmotic challenges. This study is the first to show that the expression of VILL is associated with the formation of microvilli in the absorptive ionocytes of a euryhaline fish. Loss-of-function experiments showed that the distribution of VILL may represent the molecular link between the cytoskeletal organization and cellular morphology of the absorptive ionocytes during hypoosmotic adaptation in aquatic vertebrates.
Teleostean fishes are aquatic osmoregulators that can maintain plasma homeostasis in environments with many fluctuating components. The gill, which is exposed to the external environment, is one of the major osmoregulatory organs in fishes. In recent years, several review articles have illustrated the regulatory systems of crucial ion transporters in gill ionocytes, also called mitochondrion-rich cells or chloride cells [1–8]. Ionocytes are polar, with apical and basolateral membranes that face the external media and internal plasma, respectively . Gill ionocytes express Na+, K+-ATPase (NKA) on the basolateral membrane, providing the driving force that enables other ion transporters or channels on the plasma membrane to absorb ions in fresh water (FW) and to secrete ions into seawater (SW) [1–8]. According to ultrastructural observations by scanning electron microscopy (SEM) and transmission electron microscopy (TEM), two typical types of gill ionocytes can be identified by their apical morphologies and the acclimated salinities. In various teleosts, the SW-type cells exhibit deeply invaginated surfaces with smaller orifices, while the FW-type ionocytes generally show large openings and membrane surfaces with finger-like cytoplasmic protrusions, similar to microvilli. The microvilli of gill ionocytes serve to enlarge the apical surface area to enhance ion absorption in the FW teleosts [5, 8–13].
The gill ionocytes modulate the expression of ion transporters and remodel their cellular morphologies to regulate ion concentrations between their blood and the environment. The apical morphologies of ionocytes in fish gills transform and change in size or shape for different ionoregulatory functions in euryhaline teleosts when exposed to environments with various salinities or concentrations of ions [5, 10, 12, 13]. This plasticity involves the appearance and disappearance of microvilli upon exposure to decreasing or increasing environmental salinities, respectively [12, 13]. In the epithelial cells of mammals, microvilli are composed of actin filaments that originate from the terminal web of the “cell cortex” (i.e., the cytoplasmic area close to the apical region) [14, 15]. The reorganization of actin filaments is associated with the plasma membrane dynamics, which remodel the cell morphology to perform specific functions of epithelial cells [14–16]. According to previous TEM observations, more cytoskeletal filaments were found in the cell cortex rather than the cytoplasm of gill ionocytes in fishes [10, 17–19]. On the other hand, Wong et al.  reported that the ionocytes express actin protein in the Japanese eel. These findings imply that the actin cytoskeleton is involved in the formation of microvilli in the apical membrane of gill ionocytes. To date, however, there is no known actin-regulatory molecule that governs the remodeling of the apical microvilli in fish ionocytes in response to changes in environmental salinities.
Villin 1, an actin-regulatory protein, was first isolated from chicken intestinal brush border . Based on the structural and functional domains of villin 1, its gelsolin and headpiece domains exhibit actin-capping, -severing, -nucleating, and -bundling for the reorganization of actin filaments [22–24]. The villin 1 of mammals can polymerize G-actin and depolymerize F-actin to influence cell morphology, migration, invasion, and survival . Human villin 1 is expressed prominently in renal, gastrointestinal, and urogenital epithelial cells, where it is localized to the microvillar core and the terminal web of apical structures [24–26]. Villin 1 plays roles in the initiation, organization, and formation of microvilli, which absorb and reabsorb nutrients in enterocytes and proximal tubule cells . Different levels of villin 1 expression influence the microvillus structures of two cell lines [28, 29]. Thus, villin 1 is an important factor in the cell morphologies of mammals. In the fish cells, however, no homolog of villin 1 has been identified.
The brackish medaka (Oryzias dancena) is a small euryhaline fish with good salinity tolerance [30, 31]. Our previous studies have demonstrated the mechanisms of ionoregulation in gill ionocytes of this medaka [13, 32–35]. The present study verified the microvillus ultrastructures on the apical surfaces of ionocytes in gills of the FW-acclimated medaka by SEM and TEM. When searching for a homolog of villin 1 that is associated with the organization of cytoskeletal filaments in FW-type ionocytes, we identified the gene sequence of villin 1-like protein (VILL) from the euryhaline medaka, detected the gene and protein expression of VILL in gill ionocytes with different microvillus ultrastructures, and demonstrated the function of VILL in determining the apical morphologies of embryonic ionocytes. These findings suggest an important role for VILL in a novel aspect of cytoskeletal function in the ionocytes of aquatic vertebrates in response to different osmotic challenges.
Finger-like protrusions of ionocytes in the FW medaka
In the FW medaka, SEM and TEM observations showed numerous finger-like protrusions extending from the cell membrane in the apical opening of the ionocytes (Figure 1). The diameters and lengths of the protrusions were approximately 100 and 500 nm, respectively. Close to the apical membrane, there was a region rich in cytoskeletal filaments with high electron density. No membrane-formed tubule (i.e., the tubular system) was found in this region like the other part of the cytoplasm. The finger-like protrusions exhibited longitudinally arranged filaments (Figure 1B). The microvilli on apical surfaces were mainly found in ionocytes of FW-acclimated medaka but not in the hole-type ionocytes of SW-acclimated individuals (Additional file 1: Figure S1). However, 50%-SW-acclimated medaka exhibited some hole-type ionocytes with microvilli but other hole-type ionocytes without microvilli (Additional file 1: Figure S2).
Cloning and characterization of villin-like (VILL) protein from the fish gill
A 3114 bp full-length Odvill cDNA (KF011977) encoding an 864 amino acid protein was isolated from gills of the brackish medaka (Additional file 1: Figure S3). The cDNA contained 118 bp of 5′ UTR and 404 bp of 3′ UTR. There were six gelsolin domains and a headpiece domain in the deduced VILL protein of the brackish medaka (Figure 2A). The present study surveyed databases of the 11 fish species from the ensemble genome browser (Table 1). According to the phylogenetic tree (Figure 2B), the homologous proteins of the vertebrates could be divided into two subclasses: villin 1 and VILL. The gene of vill was found in all examined vertebrates. However, the villin 1 was found in three fishes (among the 11 surveyed species) and the frog, chicken, and human. In these vertebrates, the specific sequences of villin 1 were identified, and their differences with VILL were illustrated in the Additional file 1: Figure S3. The derived amino acid sequence of VILL from the brackish medaka showed 89% identity to that of the Japanese medaka and about 63-73% identity to those of the other fishes, 47-58% identity to the VILL clade of other higher vertebrates, and 46-55% identity to members of the villin 1 clade. RT-PCR analysis of 11 organs revealed that Odvill (735 bp) were expressed mainly in the gill, kidney, intestine, ovary, and testis (Figure 2C). In addition, lower levels of Odvill were found in the muscle, liver, and fin.
Apical distribution of VILL protein in FW-type ionocytes
A polyclonal antibody against the headpiece domain of medaka VILL was produced (Additional file 1: Figure S3). Figure 3 shows the distribution of VILL protein in the afferent epithelia of gill filaments of the FW- and SW-acclimated medaka using the whole-mount double immunofluorescence staining. The merged images (Figure 3C,D) revealed that VILL protein was localized in the NKA immunoreactive (NKA-IR) cells in gills of the FW fish rather than in the SW group. The magnified merged 3D image (Figure 3E) revealed that the VILL signals were localized to the apical region of NKA-IR cells in the gill filaments of FW-acclimated medaka. In addition, double immunofluorescence staining with T4 antibody and VILL antibody showed that T4 signals of the apical Na+-K+-2Cl- cotransporter were colocalized with VILL signals at the apical region of some ionocytes in the gill filaments of FW-acclimated medaka (Additional file 1: Figure S4).
Chronic and acute expression of VILL in gills
Quantification of branchial Odvill mRNA in medaka acclimated to SW, 50% SW, or FW revealed the highest abundance in the FW fish, approximately 6-fold and 24-fold of the expression in 50% SW and SW fish, respectively (Figure 4A). The medaka VILL antibody was used to detect its localization and abundance. Compared to the negative control (immunoblots using the rabbit pre-immune serum; Additional file 1: Figure S5), there were two immunoreactive bands, at 100 kDa and 90 kDa, in the total lysates of gill samples. The major band at 100 kDa was detected in all groups, while the minor band at 90 kDa was found in the FW and 50% SW groups (Figure 4B). Combining the amounts of these two immunoreactive bands, FW fish expressed the highest level of VILL in gills (approximately 3-fold of the level in the 50% SW group and 10-fold of the level in the SW group) (Figure 4B). The amounts of VILL of the 50% SW group were significantly higher (approximately 3-fold) than in the SW fish. Time-course experiments showed increased expression of VILL gene and protein in gills when SW medaka were transferred to FW (Figure 4C,D). The abundance of branchial Odvill mRNA increased significantly (approximately 5-fold) at 1/2 day post-transfer. At 2 days after transfer, the Odvill mRNA of the FW-exposed fish increased to approximately 17-fold higher than the SW group (Figure 4C). In the immunoblots of the SW-acclimated medaka and the fish transferred to FW for 1/2, 1, 2, 4, or 7 days, gill VILL also displayed a major immunoreactive band at 100 kDa in all groups, while a minor band at 90 kDa was found in the 2-, 4-, and 7-day-transfer groups (Figure 4D). Compared to the SW group, the abundance of VILL in FW-exposed medaka increased significantly (approximately 3-fold) at 2 days post-transfer. The amounts of VILL in the 4- and 7-day-transfer groups were approximately 5-fold higher than in the SW group (Figure 4D).
VILL-MO inhibited expression of VILL in embryonic ionocytes
The whole-mount double immunofluorescence staining with VILL and NKA antibodies showed the VILL-IR/NKA-IR cells on the posterior trunks of embryo incubated in the FW at 6 dpf (Additional file 1: Figure S6). The magnified merged confocal microscopic 3D images revealed that the VILL signals were localized at both basolateral (compared to NKA) and apical regions of NKA-IR cells. In addition, the circular patterns of VILL signals were also found in the pavement cells adjacent to NKA-IR cells. The medaka embryos were microinjected with VILL-MO to evaluate the morphological changes of trunk ionocytes. Quantification of the number of NKA-IR cells with VILL signals in the fixed region of the posterior trunk (Figure 5A-F) revealed that there was no significant difference in the number of NKA-IR cells between the VILL-MO- and SC-injected groups (VILL-MO vs. SC: 28.3 ± 1.4 vs. 27.1 ± 1.7). Meanwhile, the number of NKA-IR cells with VILL signals in the VILL-MO-injected group was significantly lower (approximately 24-fold) than in the SC-injected group (Figure 5G). In addition, strong VILL-IR signals were found in the guts of VILL-MO and SC-injected embryos (Figure 5). Using the VILL antibody, immunoblots of embryos injected with VILL-MO and SC at 6 dpf revealed a single immunoreactive band at 100 kDa (Figure 5H). The abundance of VILL in the VILL-MO-injected group was approximately 3-fold lower than in the SC-injected group (Figure 5H). The apical surfaces of ionocytes were investigated by SEM on the posterior trunks of embryos injected with VILL-MO and SC at 6 dpf (Figure 6A,B). The apical surfaces of embryonic ionocytes were found to exhibit smaller apical and fewer protrusions in the VILL-MO group than the SC group. In addition, there were numerous protrusions in the apical surfaces of pavement cells of SC-injected embryos compared to those of the VILL-MO group (Figure 6C,D).
Lee et al.  reported that cytoskeletal filaments were rich in the cell cortex of tilapia ionocyte with microvilli. In the FW medaka, SEM and TEM showed numerous finger-like protrusions extending from the cell membrane in the apical openings of the ionocytes. The finger-like protrusions exhibited parallel bundles of cytoskeletal filaments. The parallel bundles of filaments were originated from the terminal web with web-like cytoskeletal filaments in the cell cortex of the medaka ionocyte. According to the known characteristics of microvilli in the epithelial cells of mammals [14–16], the filament-rich protrusions of medaka ionocytes were microvilli. Among the ionocytes of the brackish medaka acclimated to different salinities, abundant microvilli were found on the apical surfaces of the lower-salinity groups. Microvilli are densely packed on the apical surfaces of the ionocytes responsible for ion absorption in FW fishes [5, 8–13]. Similar to the other euryhaline teleosts exposed to hypoosmotic challenges, the gill ionocytes of the brackish medaka enlarged their apical surface area with microvilli when transferred from SW to FW . Therefore, the plasticity in the formation of ionocyte microvilli was hypoosmotic-dependent in the medaka gills.
Like villin 1, the predicted VILL of the medaka also exhibited six gelsolin segments and one headpiece domain. These domains indicated that medaka VILL could bind with G- and F-actin to play the roles of actin-capping, -severing, -nucleating and -bundling . We surveyed databases of the 11 fish species in the Ensembl Genome Browser (Table 1) and compared the fish genomes . According to the phylogenetic tree, VILL of the brackish medaka was more similar to the other VILL orthologs of the teleosts. In addition, the agnathan, an early vertebrate, only exhibited VILL. The phylogenetic tree presented in this study suggests that VILL is an ancestor of vertebrate villin 1.
By RT-PCR analysis of 11 organs, we found that Odvill was expressed mainly in the gill, kidney, intestine, ovary, and testis. In humans, villin 1 is expressed in the intestine, colon, kidney, and testis . Among these tissues, the human ileum exhibited the highest abundance of villin 1. Wang et al.  reported the expression of the villin 1 gene in the intestine of the zebrafish. In the brackish medaka Odvill would be expected to conduct some critical functions of the enterocytes of the intestine because of lacking villin 1. Furthermore, this study is the first to identify the expression of the Odvill mRNA in the gill, the respiratory and ionoregulatory organ of the teleost.
Ultrastructural observations revealed that the apical openings of gill ionocytes in the FW-acclimated medaka had microvilli. In different epithelial cells of mammals, the apical surfaces with various types of microvilli are the major locations of villin 1 protein [23, 24, 39–41]. Villin 1 organizes the actin filaments for the formation of microvilli in the apical region of mammalian enterocytes [25, 26]. In the chicken, villin 1 is also expressed in the microvilli of enterocytes [21, 42]. On the other hand, villin 1 protein is located in the apical microvilli of enterocytes and taste cells of the amphibian [43, 44]. In the brackish medaka, gill ionocytes expressed NKA on the basolateral membrane [13, 32–35]. The images of whole-mount double immunofluorescence staining revealed that VILL protein was localized in the apical region of the NKA immunoreactive (NKA-IR) cells in gills of the FW fish but not in the SW group. Additionally, because a monoclonal antibody, T4, has been successfully used to label the apical Na+, Cl- cotransporter in gill ionocytes of FW-acclimated fish [33, 45], the present study used double immunofluorescence staining with the T4 antibody to illustrate that VILL was localized at the apical region of absorptive ionocytes. Some VILL-immunoreactive (IR) cells, however, exhibited no apical T4-IR signals in the FW medaka. Hiroi et al.  reported that type III (apical T4-IR negative) and type II (apical T4-IR positive) ionocytes are involved in the absorption of Na+ and Cl-, respectively, in gills of tilapia when exposed to hypoosmotic environments. The results revealed that the apical VILL expressed in the absorptive ionocytes of medaka gills. Our TEM observations demonstrated that gill ionocytes exhibited more cytoskeletal filaments in the region of the cell cortex of FW ionocytes. Therefore, we speculated that the VILL protein would accumulate in the cytoskeleton-rich region so that it could participate in the formation of microvilli in the FW ionocytes. Across diverse taxa and broad evolutionary distances, epithelial cells express conserved molecules for the formation of microvilli. The antibody of VILL would be a relevant marker to identify the apical region of the absorptive ionocytes in gills of teleosts.
Based on our observation of superior salinity tolerance of the euryhaline medaka [13, 33], the correlation between VILL expression and the formation of microvilli in gill ionocytes was investigated in chronic and acute salinity-exposure experiments. Quantification of branchial Odvill mRNA revealed the hypoosmotic-dependent expression in gills of medaka acclimated to SW, 50% SW, or FW. The VILL antibody detected the major and minor immunoreactive bands at 100 kDa and 90 kDa, respectively, in the protein lysates of medaka gills. Immunoblots showing two bands have been reported in frog embryos labeled with an anti-frog villin 1 antibody . Based on the predicted weight of 96–98 kDa from its deduced amino acid sequence, the larger band was most likely intact VILL protein of the brackish medaka. In the mouse kidney, the villin 1 protein (92 kDa) is degraded to fragments with lower molecular weights of 83 kDa and 53 kDa by meprins . We proposed that the minor bands of VILL immunoblots might be degraded forms of medaka VILL in the gill ionocytes with microvilli. Combining the amounts of these two immunoreactive bands, the expression of VILL protein showed a similar pattern to that of Odvill mRNA and corresponded to the signals of immunofluorescence staining. The formation of ionocyte microvilli was correlated with the expression levels of VILL protein in gills of the medaka when acclimated to environments with decreasing salinities. On the other hand, time-course experiments indicated the increased gene and protein expression of VILL in gills of the SW medaka after being transferred to FW. In line with the typical model of protein synthesis, the mRNA level of VILL increased more quickly than the protein level after transfer. The highest level of VILL protein was detected in the medaka transferred from SW to FW for 4 days. In fish at the same time-point, microvilli were observed on the apical surface of gill ionocytes . The occurrence of microvilli in ionocytes coincided with increasing levels of VILL protein in gills of the brackish medaka upon hypoosmotic challenge. When villin 1 was overexpressed in the fibroblasts, numerous microvilli were formed on their plasma membrane [27, 28]. Therefore, the results of the chronic and acute salinity-exposure experiments in this study confirm that decreasing environmental salinity can induce the expression of VILL at both mRNA and protein levels in gill ionocytes of the euryhaline medaka. Because the constant expression of villin 1 mRNA is useful to measure the variation in the mammalian enterocyte content of biopsies , the elevated expression of Odvill mRNA implies that a specific promoter in the upstream region of Odvill in the brackish medaka is induced in response to decreasing environmental salinity. The expression of VILL protein was hypoosmotic-dependent and correlated with the formation of microvilli on the apical surfaces of gill ionocytes. To our knowledge, this study is the first to illustrate the expression of fish VILL protein associated with the changes in cellular morphology for ionoregulation in gills.
The antisense morpholino oligonucleotide (MO) is a popular and reliable approach for gene knockdown to demonstrate the in vivo functions of target genes using the embryos of the zebrafish and Japanese medaka [48, 49]. We developed a microinjection system of MO knockdown in the transparent embryo of the brackish medaka to examine the cellular function of VILL protein in the present study. Ionocytes were found in the epithelia of the yolk sac of the Japanese medaka embryos as early as 2 dpf. At 4 dpf, the ionocytes of the trunk epithelia appeared in the embryos . Similar to the gill ionocytes, the apical openings of the ionocytes remodel the epithelial cell morphology of the embryonic trunk and yolk sac of the tilapia , sea bass , and zebrafish  in the early developmental stages as the ambient ion concentrations change. Recent studies have performed MO knockdown of ion transporters in embryonic ionocytes to elucidate the ionoregulatory functions of proteins in fish gills [53–55]. The duration of MO efficiency in the inhibition of protein translation is 7–10 days in the embryos of the zebrafish and Japanese medaka [48, 49]. In the developmental stages of the brackish medaka, numerous apical openings of ionocytes were observed in the trunk of FW-incubated embryos at 6 dpf. The embryonic ionocytes exhibited basolateral and apical patterns of VILL-IR signals (compared to NKA) in the trunks that were different from those in the ionocytes of adult gills, which had only apical signals. The results indicated that the embryonic ionocytes could express VILL for the formation of apical microvilli. According to the results of immunoblotting and immunostaining, the efficiency and specificity of VILL-MO blocked the translation initiation of Odvill mRNA and thus reduced the expression of VILL protein in the ionocytes of the microinjected embryos. Differentiation of ionocytes, however, might not have been affected by the VILL-MO treatment in the posterior trunk of the embryos at 6 dpf. On the other hand, SEM observation was used to verify the disrupting effects on the cellular morphologies of the ionocytes after VILL-MO knockdown in the embryos at 6 dpf. The apical surfaces of ionocytes without VILL expression showed smaller openings with fewer protrusions in the morphants compared to the SC-injected group. In addition, circular patterns of VILL signals and numerous apical microridges were found in the pavement cells (PVCs) adjacent to apical openings of the embryonic ionocytes, but these were not found in the PVCs of the gills of adult medaka. The apical surfaces of PVCs lacked microridges in the morphants. In a mammalian intestinal cell line, the suppression of villin 1 impairs the formation of microvilli . Therefore, the results of MO knockdown indicate that the fish VILL protein plays an important role in remodeling cellular morphology, including the formation of microvilli and microridges on the apical surfaces of epithelial cells in vivo.
In the brackish medaka when environmental salinity is decreasing, the hypoosmotic-dependent microvilli are enhanced on the apical surfaces of gill ionocytes. The phylogenetic tree and functional domains suggest that VILL is the homolog of villin 1 in fishes. This study is the first to show that the expression of VILL, an actin-regulatory protein, is associated with the formation of microvilli in the absorptive ionocytes of a euryhaline fish. Loss-of-function experiments show that the distribution of VILL may represent the molecular link between the cytoskeleton organization and cellular morphology. Consequently, the availability of VILL protein will be helpful in improving our understanding of the molecular evolution of microvilli in relation to the functional morphologies of the absorptive ionocytes during hypoosmotic adaptation in aquatic vertebrates.
Experimental animals and environments
The brackish medaka (Oryzias dancena; 2.5 ± 0.3 cm) was reared in 50% SW. The water was continuously circulated through fabric-floss filters and partially refreshed every two weeks and temperature was held at 28 ± 1°C. Fish received a constant photoperiod cycle of 14:10 hrs light: dark cycle and were fed a daily diet of commercial pellets. The facilities and protocols for experimental animals were approved by the Institutional Animal Care and Use Committee of the National Chung Hsing University (IACUC approval no. 96–48 to THL). Following the experiment, fish were not fed and were anaesthetized with MS-222 (100–200 mg/l) before sampling. For chronic (long-term) experiments, the fish were acclimated to FW, 50% SW (15%), or SW (35%) for at least one month. On the other hand, SW-acclimated medaka was transferred directly to FW for acute (short-term) experiments. The FW-exposed groups were sampled at 1/2, 1, 2, 4, or 7 days.
Electron microscopic observations
The gills or embryos were fixed at 4°C in a fixative consisting of 5% (v/v) glutaraldehyde and 4% (w/v) paraformaldehyde in 0.1 M phosphate buffer (PB, pH 7.2) for 12 hrs. Fixed samples were post-fixed with 1% (w/v) osmium tetroxide in 0.1 M PB for 1.5 hrs. After post-fixation, the samples were rinsed in PB and dehydrated in ascending concentrations of ethanol. For observation in the scanning electron microscope (SEM, JSM-6700 F, JEOL, Tokyo, Japan), samples were prepared by our previous method . For observation in the transmission electron microscope (JEM-1400, JEOL), the dehydrated gills were transferred to propylene oxide and embedded in Spurr’s resin. Ultrathin sections (75 nm) of gill filaments were cut with MTX Ultramicrotome (RMC, Tucson, AZ, USA and mounted on grids. The sections were stained with uranyl acetate and lead citrate before observation.
Double immunofluorescence staining
Gills of medaka were fixed in the neutral formalin (pH 7.2) in 4°C for 3 hrs. After washing in phosphate buffer saline (PBS), the samples of whole-mount immunofluorescence staining were permeated with methanol for 30 min at -20°C. The samples were then stored in the methanol at -20°C before performing the following experiments. Whole-mount samples were rehydrated by rinsing with PBS three times. Subsequently, the samples were incubated in 5% bovine serum albumin (Sigma, St. Louis, MO, USA) at room temperature for 30 min. Samples were then incubated with the rabbit polyclonal VILL antibody (1: 5000 dilution) at room temperature for 2 hrs. Samples were then washed with PBS, incubated with the secondary antibody (Dylight-488 goat anti-rabbit IgG) at room temperature for 1 hr and washed again with PBS. After the first staining, samples were incubated with the mouse monoclonal antibody (α5, 1:200 or T4, 1:100) for 2 hrs at room temperature. Samples were then washed and incubated with the secondary antibody (Dylight-549 goat anti-mouse IgG) at room temperature for 1 hr followed by several PBS washes. Samples were then mounted in 50% glycerol with PBS and examined using a fluorescent microscope (BX50, Olympus, Tokyo, Japan) with the Olympus DP72 CCD camera or a laser scanning confocal microscope (FV1000, Olympus).
The template of cDNA for gene cloning and SMART RACE cDNA amplification kit (Clontech, Palo Alto, CA, USA) were described in our previous study . Amino acid sequences for villin and VILL from different organisms (Table 1) were aligned by CLUSTALW and a phylogenetic tree was constructed using MEGA 4.1. For tissue distribution of gene expression, PCR amplification (28 cycles) was done by the Hot start EX-Taq polymerase (Takara, Shiga, Japan). β-actin was used as an internal control for all tissues. The sequences of the primers used in the gene identification were listed in the Table 2.
The Odvill mRNA of gills was detected by the SYBR Green PCR Master Mix (Bio-Rad Laboratories, Hercules, CA, USA) and quantified with the Mini Opticon real-time PCR system (Bio-Rad). The Odvill mRNA values were normalized using the expression of the β-actin mRNA from the same DNA samples. One identical cDNA sample from the 50% SW-acclimated fish was used as the internal control among different groups. For each unknown sample, the comparative Ct method with the formula 2^-[(CtOdvill,n-Ctβ-actin,n)-(CtOdvill,c-Ctβ-actin,c)] was used to obtain the corresponding Odvill and β-actin values, where Ct corresponded to the threshold cycle number.
Protein extraction and western immunodetection
According to the method of Kang et al. , homogenates of medaka gills or embryos were prepared. Aliquots containing 20 μg of homogenates were heated at 65°C for 25 min and fractionated by electrophoresis on SDS-containing 7.5% polyacrylamide gels. Transferred PVDF blots were incubated with VILL polyclonal antibody (1:200,000 dilution) or β-actin monoclonal antibody (1:10,000 dilution; 8226, Abcam, Cambridge, UK) for 2 hrs, followed by a 1-hr reaction with horseradish peroxidase-conjugated goat anti-mouse or anti-rabbit IgG (Pierce, Rockford, IL, USA). Blots were developed using the SuperSignal West Pico Detection Kit (#34082, Pierce) and analyzed with Image Lab software version 3.0 (Bio-Rad) after densitometric scanning of membranes using a ChemiDoc XRS+ (Bio-Rad). Results were converted to numerical values to compare relative intensities of immunoreactive bands.
Microinjection of morpholino oligonucleotides
Morpholino oligonucleotides (MOs) of antisense Odvill were designed and manufactured by Gene Tools (Philomath, OR, USA). The VILL-MO sequence was 5′-TGTTCGGAAAGTCATCCTTCATCAT-3′. This morpholino overlapped the start codon (underlined) and acted as a translational blocker. Gene Tools’ standard control (SC) morpholino (5′-CCTCTTACCTCAGTTACAATTTATA-3′) was used as a morpholino injection control. Morpholinos were dissolved to 0.5 mM injection stocks in RNase-free water. The microinjection system consisted of an Olympus SZ60 stereomicroscope, an air-pressure-driven microinjector (IM-300; Narishige, Tokyo, Japan), and a three-axis micromanipulator (M-152, Narishige). The fertilized eggs of FW-acclimated medaka at the one- or two-cell stage were collected for operation with the microinjection system in a protocol modified from Kinoshita et al. . The injection volumes of VILL-MO and SC ranged from 2 to 5 nl. Injection pressure was varied to compensate for variable needle opening size to ensure an appropriate injection volume. The injected eggs were incubated in FW at 28±1°C. The morphologies of developing embryos were investigated and recorded for 6 days after fertilization (dpf). The 6 dpf embryos were collected in a microcentrifuge and stored in -80°C for Western blotting. For immunofluorescence staining and SEM, the embryos were fixed after performing the dechorionation procedure.
Bioinformatics and statistical analysis
The open reading frame of Odvill was predicted with the ORF Finder (http://www.ncbi.nlm.nih.gov/gorf/gorf.html). Six gelosolin and one head piece domains of the medaka VILL were analyzed in the website of Conserved Domains and Protein Classification (http://www.ncbi.nlm.nih.gov/Structure/cdd/cdd.shtml). Values were expressed as the means ± S.E.M. (the standard error of the mean). Results were compared using Student’s t-test or one-way ANOVA followed by Tukey’s pairwise method. The significance level was set as p < 0.05.
- NKA-IR cells:
Scanning electron microscopy
Transmission electron microscopy
Villin 1-like protein.
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The monoclonal antibodies, T4 and α5, were purchased from the Developmental Studies Hybridoma Bank (DSHB) maintained by the Department of Pharmacology and Molecular Sciences, John Hopkins University School of Medicine, Baltimore, MD 2120521205, and the Department of Biological Sciences, University of Iowa, Iowa City, IA 52242, under Contract N01-HD-6-2915, NICHD, USA. The work was supported in part by a grant from the ATU plan of the Ministry of Education, Taiwan, to THL (CC-97118).
The authors have no commercial, proprietary or financial interest in any companies or products described in this article.
CKK and THL conceived the study. CKK and THL discussed and designed the experiments. CKK performed the experiments and wrote the manuscript. Both authors read and approved the final manuscript.