Long-range cellular communication between the sperm and egg is critical for external fertilization. Sperm-activating peptides (SAPs) are diffusible components of the outer layer of eggs in echinoderms, and function as chemoattractants for spermatozoa. The decapeptide named speract is the best-characterized sea urchin SAP. Biochemical and physiological actions of speract have been studied with purified or chemically synthesized peptides. In this work, we prepared recombinant speract fused to a fluorescent protein (FP; FP-speract) using three color variants: a cyan (eCFP), a yellow (mVenus) and a large Stokes shift yellow (mAmetrine) FP. Although these fluorescence tags are 20 times larger than speract, competitive binding experiments using mAmetrine-speract revealed that this FP-speract has binding affinity to the receptor that is comparable (7.6-fold less) to that of non-labeled speract. Indeed, 10 nmol l−1 eCFP-speract induces physiological sperm responses such as membrane potential changes and increases in intracellular pH and Ca2+ concentrations similar to those triggered by 10 nmol l−1 speract. Furthermore, FP-speract maintains its fluorescence upon binding to its receptor. Using this property, we performed fluorescence resonance energy transfer (FRET) measurements with eCFP-speract and mVenus-speract as probes and obtained a positive FRET signal upon binding to the receptor, which suggests that the speract receptor exists as an oligomer, at least as a dimer, or alternatively that a single speract receptor protein possesses multiple binding sites. This property could partially account for the positive and/or negative cooperative binding of speract to the receptor.
In most marine animals, spermatozoa and eggs are released into the ocean, where the distance between gametes increases upon dilution, which implies a potential problem in achieving successful fertilization for any species. To overcome this problem, marine animals commonly produce a large number of gametes, although there is a trade-off between their number and size. In the case of echinoderms, female gametes employ two additional strategies to improve sperm–egg interactions. One is an increase in physical size by swelling an extracellular matrix, called the egg jelly, through the absorption of seawater (Podolsky, 2002). The other is the release of specific chemoattractants for spermatozoa, sperm-activating peptides (SAPs) (Suzuki, 1995). SAPs initiate their physiological action on spermatozoa through an increase in cyclic guanosine monophosphate (cGMP) levels (Garbers, 1989; Kaupp et al., 2003), which induces membrane potential (Vm) changes (Galindo et al., 2000; Strünker et al., 2006), leading to increases in intracellular pH (pHi) and Ca2+ concentrations ([Ca2+]i) (Nishigaki et al., 2001; Seifert et al., 2015). Changes in [Ca2+]i in particular play a fundamental role in the regulation of the shape of flagellar beating (Böhmer et al., 2005; Wood et al., 2005), namely, in the process of sperm chemotaxis (Alvarez et al., 2012; Guerrero et al., 2010).
Since the first SAP (speract) was purified and structurally determined (Suzuki, 1995), almost 100 SAPs have been identified from many species of echinoderms (Nishigaki et al., 1996; Suzuki, 1995). SAPs are classified into five or six groups depending on their structures and cross-activities (Suzuki, 1995). There are many isoforms in the same class of SAPs given the existence of isoforms within and among species. The diversity of SAPs within species is attributed to the biosynthesis of these peptides. The mRNA encoding speract and asterosap (SAP isolated from the starfish Asterias amurensis) revealed that SAPs are produced as large precursor proteins containing many SAPs isoforms: 9–12 isoforms of speract separated by a single amino acid (Lys) (Kinoh et al., 1994; Ramarao et al., 1990) and approximately 10 isoforms of asterosap separated by a 12–22 amino acid spacer peptide (Matsumoto et al., 1999; Nakachi et al., 2008). Multiple copies of the same peptide in a single precursor protein were also reported for sarafotoxin in a snake venom (Ducancel et al., 1993), suggesting an efficient strategy for producing a high concentration of similar peptides.
The signal transduction of SAPs has been intensively studied in two species of sea urchin, Strongylocentrotus purpuratus (Darszon et al., 2011) and Arbacia punctulata (Kaupp et al., 2008), using their corresponding SAPs, speract and resact, respectively. Although the overall signaling cascades are quite similar between these two species, the molecular identities of the ligand receptors are different. Although the resact receptor is a membrane form of guanylyl cyclase (GC) (Singh et al., 1988), speract binds to a 77 kDa Cys-rich protein (Dangott and Garbers, 1984; Dangott et al., 1989) that somehow activates a membrane GC. One fascinating question is how distinct ligand–receptor combinations evolved without altering the overall signaling cascade in echinoderms. It is worth mentioning that speract and its isoforms are produced in accessory cells (somatic cells) of the oocyte (Kinoh et al., 1994), whereas asterosap, which directly binds to GC, is produced in the oocyte itself (Matsumoto et al., 1999).
Speract is the first identified SAP (Gly-Phe-Asp-Leu-Asn-Gly-Gly-Gly-Val-Gly) and its structure–function relationship is well known thanks to the existence of many natural isoforms (Suzuki, 1995) and some synthetic analogues (Garbers et al., 1982; Nomura and Isaka, 1985; Tatsu et al., 2002) of this peptide. Interestingly, the most important residue is the Gly at position six, as its substitution by any amino acid results in at least a 1000-fold decrease in the affinity to its receptor (Tatsu et al., 2002). For biochemical and physiological studies, speract and its analogues (or isoforms) have been obtained by purification of natural peptides or by chemical synthesis. To explore the usefulness of recombinant speract in this study, we prepared three recombinant versions of this peptide fused to fluorescent proteins (FPs) produced in Escherichia coli as fluorescent analogues. Although these FP-labeled speracts (FP-speracts) are more than 20 times larger than the intact speract, these ligands are active and have binding affinity comparable to that of the natural ligand. The existence of many color variations of FPs facilitated preparation of FP-speract with different optical properties, which allowed us to perform distinct bioassays using fluorescence spectroscopy to evaluate the ligand activity of FP-speract. Moreover, we determined the proximity of speract binding sites on the sperm plasma membrane using the cyan and yellow variant of FP-speract as a FRET pair, which provided us with new insight into the speract receptor.
bovine serum albumin
intracellular Ca2+ concentration
cyclic guanosine monophosphate
diluted artificial seawater
a variant of enhanced cyan fluorescent protein
speract tagged with a fluorescent protein
fluorescence resonance energy transfer
sperm-specific Na+/H+ exchanger
MATERIALS AND METHODS
Sexually mature Strongylocentrotus purpuratus (Stimpson 1857) sea urchins were obtained from Pamanes (Ensenada, Baja California, México) and Lytechinus pictus (Verrill 1867) from Marinus (Long Beach, CA, USA). Dry sperm were collected after intracoelomic injection of 0.5 mol l−1 KCl, and were kept on ice until used. Klenow Fragment, HindIII, XhoI, XbaI, NcoI, T4 ligase, GeneJET Plasmid Miniprep kit, GeneJET Gel Extraction Kit, DNA Ladders and Ni-NTA Superflow agarose were from Thermo Scientific (Waltham, MA, USA). Vent DNA polymerase was from New England Biolabs (Ipswich, MA, USA). Citifluor was from Electron Microscopy Sciences (Hatfield, PA, USA). The fluorescent dyes BCECF-AM, 3,3′-dipropylthiadicarbocyanine iodide [DiSC3(5)] and Fluo-4-AM were obtained from Invitrogen-Molecular Probes (Eugene, OR, USA). cOmplete™ Protease Inhibitor Cocktail Tablets were from Roche (Basel, Schweiz). Luria Broth (LB; containing tryptone, yeast extract and NaCl), kanamycin and the rest of the reagents were from Sigma-Aldrich. Synthetic speract was provided by Dr Tatsu (AIST, Ikeda, Japan) and fluorescein-labeled speract (F-speract) was prepared as described previously (Nishigaki and Darszon, 2000). Artificial seawater (ASW) contained in mmol l−1: 486 NaCl, 27 MgCl2, 29 MgSO4, 10 CaCl2, 10 KCl, 2.5 NaHCO3, 0.1 EDTA, 10 HEPES, pH 8.0 and 1000 mOsm l−1. Low-Ca2+ ASW contained 1 mmol l−1 Ca2+, pH 7.0. Sperm were swollen as described elsewhere (Babcock et al., 1992; Reynaud et al., 1993) in 10-fold diluted ASW (DASW) supplemented with 20 mmol l−1 MgSO4, 120–160 mOsM, pH 6.8. The E. coli strains JM109(DE3) and BL21(DE3) were obtained from the National BioResource Project E. coli strain, National Institute of Genetics, Mishima, Japan. Plasmids encoding eCFP-pRSETB (Kotera et al., 2010), mVenus-pRSETB (Nagai et al., 2002) and pmAmetrine1.2 (Ding et al., 2011) were provided by Dr T. Nagai (Osaka University), Dr A. Miyawaki (RIKEN) and Dr R. Campbell (University of Alberta, Addgene plasmid no. 42171), respectively.
Construction of plasmids for FP-speract
We used a modified pET28c (Novagen) as expression vector for the recombinant proteins. Using the following two primers, 5′ CCC TCT AGA AAT AAT TTT GTT TAA CTT TAA GA and CCC AAG CTT ATA TCT CCT TCT TAA AGT TAA AC 3′, a double-stranded DNA was synthesized using Klenow Fragment. This double-stranded DNA was double digested with XbaI/HindIII and inserted into a pET28c vector using the same restriction enzymes as cloning sites. Consequently, the modified pET28c, called pET28HindIII, lost approximately 120 bp of pET28c, including NcoI as translation initiation site and the majority of other multi-cloning sites of the original vector.
The three plasmids encoding enhanced cyan fluorescent protein (eCFP), mVenus and mAmetrine (mAmetrine1.2) were separately used as a template and the PCRs were carried out to obtain a single DNA fragment that encodes the entire open reading frame of each FP-speract. Oligonucleotide primers for the PCR are as follows: a forward primer (5′ CCA AGC TTA TGC ATC ATC ATC ACC ACC ACG TGA GCA AGG GCG AGG AGC TGT TC 3′) and a reverse primer (5′ CCC CTC GAG TTA GCC CAC ACC GCC ACC GTT CAG ATC AAA GCC GCC ACC GCC GCT ACC ACC ACC CTT GTA CAG CTC GTC CAT GCC GAG 3′). The forward primer encodes a HindIII site and 6xHis tag followed by the N terminus of these FPs. The reverse primer encodes an XhoI site, a stop codon, speract, seven amino acids as a linker (Gly-Gly-Gly-Ser-Gly-Gly-Gly) and the C terminus of these FPs. All PCRs were performed with two units of Vent DNA Polymerase, 0.3 µmol l−1 primers, 100 ng template and 200 µmol l−1 of each dNTP in 50 µl using the following thermal cycle: 3 min at 96°C, 35× (30 s at 96°C; 50 s at 58°C; 1 min at 72°C) and 1 min at 72°C. Each PCR produced a single DNA band of approximately 800 bp. The PCR products were purified, double digested with HindIII/XhoI, and inserted into pET28HindIII vector using the same restriction enzymes as cloning sites. The ligated products were used to transform Ca2+-competent JM109(DE3) cells. Several colonies were inoculated in 3 ml LB medium without isopropyl-β-D-1-thiogalactopyranoside (IPTG) and incubated overnight at 37°C at 200 rpm. After centrifugation of the cell suspension, the pellets of bacteria containing the expected plasmids showed the corresponding colors of each FP (we confirmed the presence of mAmetrine through excitation with 405 nm light as it had a faint yellow color). DNA sequences of the open reading frame of each FP-speract were confirmed by the DNA sequencing facility of our institute.
Preparation of FP-speract
Each FP-speract expression vector was transformed in the E. coli strain BL21(DE3). A single colony was grown in 50 ml LB medium with kanamycin (30 µg ml−1) for 12 h at 37°C. Subsequently, 2 ml were transferred to 200 ml LB medium with kanamycin (30 µg ml−1) and incubated at 37°C. When the OD600 reached 0.8, 300 µmol l−1 IPTG was added and the incubation continued at 30°C over 24 h. The cells were centrifuged (4000 g for 20 min at 4°C) and the pellet was washed three times with NaCl 150 mmol l−1, Tris-HCl 10 mmol l−1, pH 7.4 (solution A), and re-suspended with 8 ml of solution A containing cOmplete™. The cells were lysed by sonication with a GE50T Ultrasonic processor (three treatments of 30 s at 20 watts on ice separated by 1-min intervals) and centrifuged (15,000 g for 15 min at 4°C). The supernatant was passed through a nickel column, Ni-NTA Superflow and washed with solution A containing 50 mmol l−1 imidazole. Then, FP-speract was eluted with solution A containing 250 mmol l−1 imidazole. The purification process was carried out at room temperature. The concentration of each FP-speract was determined by the Bradford protein assay using bovine serum albumin (BSA) as a standard. For physiological measurements (Vm, pHi and [Ca2+]i), we used 10 nmol l−1 of eCFP-speract that was determined by its absorbance (molar extinction coefficient of eCFP: 32,500 M−1 cm−1). The quality of each purified FP-speract was confirmed by electrophoresis on a 15% SDS-PAGE (Fig. S1).
Vm, pHi and [Ca2+]i of S. purpuratus spermatozoa were determined using DiSC3(5), BCECF-AM and Fluo-4-AM, respectively, as previously reported (Beltrán et al., 2014). In the three cases, 10 nmol l−1 speract or 10 nmol l−1 eCFP-speract was added to stimulate the sperm, and the change in fluorescence was recorded over 1 min with an SLM8000 spectrofluorometer modified by Olis Global Works Software. Vm and pHi measurements were performed in DASW as well as in normal ASW. To normalize the [Ca2+]i changes, the cells were permeabilized with 0.05% Triton X-100 and the maximum fluorescence of Fluo-4 was obtained in each recording.
Visualization of mVenus-speract binding to L. pictus sperm receptor
Lytechinus pictus sperm were diluted 10-fold in low-Ca2+ ASW and then 100-fold in ASW containing 0.1% BSA and 10 nmol l−1 mVenus-speract or 10 nmol l−1 mVenus-speract with 500 nmol l−1 speract (as competitor). The samples were centrifuged (1000 g for 7 min at 4°C) and the supernatant was discarded to remove the unbound protein. Sperm (25 μl suspensions) were attached to a three-well slide (Electron Microscopy Sciences) at 4°C for 1 h and fixed with 25 μl 4% paraformaldehyde in ASW for 10 min. Subsequently, the cells were washed three times with phosphate buffered saline (in mmol l−1: 137 NaCl, 2.7 KCl, 10 Na2HPO4 and 1.8 KH2PO4, pH 7.4), and 5 μl of Citifluor were added to minimize fluorescence bleaching. The samples were protected with a coverslip (0.13–0.17 mm thick) and the edges were sealed with nail polish. The fluorescence of the mVenus-speract on the sperm was observed with a 100× objective on a Zeiss LSM510 confocal microscope using an argon laser (488 nm) for excitation. Sperm images were obtained with the LSM 5 Image Browser program.
Competitive binding assays with a chemically synthesized fluorescent speract analogue (F-speract)
Competitive binding assays using F-speract were performed as previously reported (Tatsu et al., 2002), with some modifications. In this work, we measured the fluorescence of 10 nmol l−1 of F-speract in L. pictus sperm suspension, which contained 10 nmol l−1 equivalents of the speract receptor, using a small-volume cuvette (45 μl). As a binding competitor, 1, 3.16, 10, 31.6, 100, 316 and 1000 nmol l−1 of either speract or mAmetrine-speract were added to the sample and their fluorescence intensities (λex 494/λem 524 nm) were determined. Even though the fluorescence intensity of mAmetrine excited at 494 nm is quite small at the equivalent concentration of F-speract, its fluorescence at a much higher concentration is not negligible. Therefore, net F-speract fluorescence intensities were obtained by subtraction of the fluorescence intensities of mAmetrine-speract (in the sperm suspension) from the total fluorescence intensities.
FRET assays using eCFP-speract and mVenus-speract
A sperm suspension (L. pictus) containing 10 nmol l−1 equivalents of speract receptor was mixed with a combination of eCFP-speract and mVenus-speract in the presence or absence of 1 µmol l−1 speract. Two different compositions of ligands were used as follows; 5 nmol l−1 eCFP-speract and 5 nmol l−1 mVenus-speract for a 1/1 (donor/acceptor) ratio, and 2 nmol l−1 eCFP-speract and 8 nmol l−1 mVenus-speract for a 1/4 ratio. Subsequently, the emission spectrum (λex=433 nm) of the sample (with and without competitor) was recorded in the spectrofluorometer.
Fluorescence spectra or intensities were acquired with 4.2 Olis Global Works Software and processed with Microsoft Excel or R project 3.0.1 (Freeware). In figures, all values represent the means±s.e.m. unless otherwise indicated. We performed at least three different experiments with three distinct sea urchins. The Shapiro–Wilk test showed that all data obtained in this study showed a normal distribution (P>0.05). Statistical significance was evaluated using the Student’s t-test. Differences were considered statistically significant at P<0.05.
Design of FP-speract
It has been reported that modification of the amino terminus of speract by small molecules does not affect its ligand activity (Dangott and Garbers, 1984; Nishigaki and Darszon, 2000). Therefore, we decided to fuse speract with an FP at the amino terminus of this peptide ligand. Fig. 1 shows a schematic structure of FP-speract. Considering that a bulky FP could interfere with speract–receptor interactions, a relatively long spacer composed of seven non-structural amino acids (Gly-Gly-Gly-Ser-Gly-Gly-Gly) was inserted between the FP and speract. To facilitate the process of purification, we added 6xHis to the amino terminus of FP using a forward primer of PCR. As described in the Materials and methods, three different FP-speracts were produced in BL21(DE3) and purified by the Ni2+ column. The purified proteins have the expected molecular weights (∼28 kDa) as indicated by a 15% SDS-PAGE (Fig. S1).
Speract and eCFP-speract induce similar Vm, pHi and [Ca2+]i changes in the sperm
To evaluate the activity of FP-speract, we first determined the capacity of eCFP-speract to induce physiological sperm responses: Vm changes and increases in pHi and [Ca2+]i using the fluorescent indicators DiSC3(5), BCECF-AM and Fluo-4-AM, respectively (Beltrán et al., 2014). Fluorescence signals of 10 nmol l−1 eCFP (λex=433 nm, λem=476 nm) did not interfere with the fluorescence measurements of these indicators.
Because the speract-induced initial hyperpolarization is difficult to detect in S. purpuratus sperm in normal ASW, we measured the Vm (as well as the pHi) changes in swollen sperm in DASW, where the hyperpolarization can be easily observed (Babcock et al., 1992). Our results show that 10 nmol l−1 eCFP-speract and 10 nmol l−1 speract induce similar changes in Vm (Fig. 2A). Likewise, 10 nmol l−1 eCFP-speract elicited an increase in pHi (Fig. 2B) and [Ca2+]i (Fig. 2C), as intact speract does. It is worth mentioning that the magnitude of the pHi increase induced by speract is larger in DASW than that observed in normal ASW (Fig. 2B). Considering that the sperm-specific Na+/H+ exchanger (sNHE) is activated by Vm hyperpolarization (Lee and Garbers, 1986) and that this hyperpolarization is larger in DASW (Fig. 2A), the enhanced increase in pHi in DASW supports the involvement of sNHE in the signaling cascade of speract.
Visualization of mVenus-speract binding to the sperm receptor
We previously prepared F-speract as a synthetic fluorescent analogue of speract (Nishigaki and Darszon, 2000). F-speract is a useful speract analogue with which to study ligand–receptor interactions because its fluorescence quenches upon binding to its receptor. However, F-speract does not allow for the visualization of its binding to the receptor under fluorescence microscopy. In contrast, mVenus-speract maintained its fluorescence upon receptor binding and allowed us to visualize the localization of speract receptors with this fluorescent ligand (Fig. 3). In the presence of an excess of speract, the fluorescence signal of mVenus was not observed, indicating that the fluorescence signal from the sperm flagellum is specific.
Competitive binding activity of FP-speract using F-speract as a fluorescent probe
Although 10 nmol l−1 of both FP-speract and speract induced similar sperm responses (Fig. 2), it was necessary to perform quantitative experiments to precisely evaluate the activity of FP-speract. To this end, we performed a competitive binding assay using F-speract as a fluorescent probe, which is supposed to be the most efficient method to evaluate the ligand activity of speract analogues (Tatsu et al., 2002). For this experiment, we used L. pictus spermatozoa because the number of speract binding sites of this species is three times higher than that of S. purpuratus. One of the problems in performing this experiment is the fluorescence overlap between F-speract and FP-speract. As mentioned earlier, the fluorescence emission peak of eCFP is different from that of fluorescein (F-speract). However, a high concentration of eCFP completely masked the fluorescence signal of F-speract because of a significant fluorescence overlap between fluorescein and eCFP. Afterwards, we tried to use a blue FP (mEBFP2)-tagged speract for this experiment, but we were unable to produce a sufficient amount of the soluble mEBFP2-speract in BL21(DE3) for an unknown reason. We thus employed mAmetrine as a useful alternative for this purpose. mAmetrine is a yellow FP (λem=526 nm), with an excitation peak around 400 nm (Ai et al., 2008; Ding et al., 2011) that is classified as a large Stokes shift fluorophore (120 nm between excitation and emission peaks). Even though the fluorescence emission of mAmetrine excited by 490 nm is negligible compared with that obtained by excitation at 400 nm at a comparable concentration of F-speract, this small fluorescence intensity is not negligible at higher concentrations of the fluorophore. Therefore, for this experiment, we subtracted the fluorescence intensity of mAmetrine itself from the total fluorescence intensity to obtain the net F-speract quenching. Fig. 4 shows the competitive binding curves of mAmetrine-speract and speract upon F-speract binding to its receptor in L. pictus spermatozoa. The IC50 values of mAmetrine-speract and speract were 61±9 and 8±0.8 nmol l−1 (n=3), respectively, indicating that this fluorescent analogue of speract has 7.6-fold less affinity for the receptor than speract.
FRET measurements between eCFP-speract and mVenus-speract upon binding to the receptor
As mentioned in the Introduction, the speract receptor is a 77 kDa protein that possesses a single transmembrane segment. Although it has some sequence homology to the Cys-rich scavenger protein found in mammals, its biochemical properties have not been studied in detail (Dangott et al., 1989). To explore whether the speract receptors form an oligomer or exist as a monomer in sea urchin sperm, we performed a binding experiment based on FRET. Fig. 5 shows the fluorescence emission spectra (λex=433 nm) of a mixture of 2 nmol l−1 eCFP-speract and 8 nmol l−1 mVenus-speract (1/4 ratio) with L. pictus spermatozoa (equivalent to 10 nmol l−1 speract receptor) in the presence or absence of an excess amount of speract. We observed a significant difference (15.1±2.0%, n=3) of CFP fluorescence intensities between the two conditions (Fig. 5A). In the normalized fluorescence spectra (Fig. 5B), the fluorescence intensities around 528 nm, which correspond to the fluorescence peak of mVenus (Nagai et al., 2002), are higher in the absence of the competitor than those in the presence. These results indicate that there is FRET between these two speract analogues when they are bound to the receptor, suggesting that the speract receptors exist as a cluster forming an oligomer, at least a dimer, on the sperm plasma membrane. Alternatively, a single speract receptor protein possesses multiple binding sites for this ligand.
Development of FP-speract
In this study, we prepared a recombinant speract analogue tagged with an FP (FP-speract, Fig. 1) and evaluated its functionality. In spite of the relatively large size of FP (25 kDa) compared with speract (decapeptide), FP-speract induced physiological sperm responses (Vm, pHi and [Ca2+]i) in a manner similar to that of speract (Fig. 2). The competitive binding curves of FP-speract and speract (Fig. 4) indicate that FP-speract maintained a comparable affinity to the receptor (only 7.6-fold less potent than intact speract), confirming that FP-speract is indeed a useful ligand for spermatozoa. A non-structural seven-amino-acid spacer between FP and speract probably facilitated this favorable result. To our knowledge, there are a few cases of functional FP-tagged peptide ligands such as parathyroid hormone and bradykinin (Charest-Morin et al., 2013). Although both are functional ligands and induce the expected cell responses, the exact affinity to the corresponding receptor has not been determined.
Application of FP-speract to determine the formation of clusters by the speract receptor
Previously, we prepared fluorescent speract analogues tagged with fluorescein (F-speract), whose fluorescence quenches upon binding to its receptor (Nishigaki and Darszon, 2000). In contrast, FP-speract maintains its fluorescence even after binding to its receptor (Fig. 3). Taking advantage of this property, we applied two color variants of FP-speract, cyan and yellow, to study the proximity of the speract binding sites.
The receptors for resact and asterosap are known to be membrane-bound GC (Matsumoto et al., 2003; Singh et al., 1988). Previously, it was estimated that there are approximately 100,000 asterosap binding sites in the starfish sperm flagellum (Nishigaki et al., 2000). Recently, it was reported that a single cell of A. punctulata spermatozoa possesses 300,000 molecules of GC (Pichlo et al., 2014). Comparing these numbers, the speract receptors are less abundant: 60,000 binding sites in L. pictus and 20,000 binding sites in S. purpuratus (Nishigaki et al., 2001). The speract receptor is a 77 kDa Cys-rich protein distinct from GC that is supposed to be coupled to GC (Dangott and Garbers, 1984; Dangott et al., 1989). It is known that the receptor for the atrial natriuretic peptide, a membrane-bound guanylyl cyclase A, exists as a dimer (Chinkers and Wilson, 1992; Ogawa et al., 2004). However, there is no such information for SAP receptors either in resact-type receptors (GC) or in speract-type receptors.
In this study, we explored the proximity between the speract binding sites on the sperm plasma membrane using multicolor FP-speract. Conventional optical microscopy is unable to resolve the distance between two objects localized at less than 200 nm. In contrast, the current techniques of super-resolution microscopy can increase the resolution up to 20 nm (Fernández-Suárez and Ting, 2008; Huang et al., 2009). However, those techniques require sophisticated experimental conditions and analyses. Therefore, we performed a FRET measurement using cyan and yellow variants of FP-speract. In practice, we can obtain higher spatial resolution applying FRET (<10 nm) than with super-resolution microscopy (Fernández-Suárez and Ting, 2008; Huang et al., 2009). It was reported that the Förster distance (50% of FRET) between eCFP and mVenus is estimated to be around 5 nm (Patterson et al., 2000). Because FRET efficiency decreases by a function of the sixth power of the distance, twice the Förster distance (10 nm in this study) should result in less than 2% FRET efficiency. In this work, we obtained approximately 15% FRET efficiency in our experimental condition (1/4 donor/acceptor ratio). When we performed the same experiment using the 1/1 ratio, the FRET efficiency was lower (10.1±0.8%, n=4), probably because larger fractions of the adjacent binding sites were occupied with the donor fluorophore in this condition. Although the speract receptors are abundant in the plasma membrane of L. pictus sperm flagella (60,000 binding sites per cell), the average distance between the binding sites is estimated to be approximately 40 nm if the binding sites are homogeneously distributed on the plasma membrane of the sperm flagellum (0.3 μm diameter and 45 μm long). Therefore, our results (Fig. 5) suggest that the speract binding sites are not homogeneously distributed, but exist as clusters. This is the first experimental evidence about a cluster formation of SAP receptors. Considering that the speract receptor contains four repeats of Cys-rich domains (Dangott et al., 1989), we cannot rule out the possibility that the single polypeptide receptor has multiple speract binding sites. Further experiments, such as precise determination of molecular stoichiometry between speract receptor and speract binding sites, are required to address this question. It was reported that the speract receptor is localized in a lipid raft (Loza-Huerta et al., 2013; Ohta et al., 2000), which may partially explain its formation of the clusters. Regardless of the type of cluster (intermolecular, intramolecular or both), a cluster of binding sites might provide cooperative bindings, as reported in speract and other SAPs (Nishigaki et al., 2000, 2001; Pichlo et al., 2014).
FP-speract as a tool for experimental training
The sea urchin has been used as a classical and excellent model to observe the process of fertilization in the field of reproductive and developmental biology. Although it is not trivial to document sperm chemotaxis in some species, it is quite easy to observe speract (SAPs in general) activity by recovering suppressed sperm motility in slightly acidified seawater (see Movie 1) (Ohtake, 1976). Considering that preparation of recombinant protein expressed in E. coli is a standard protocol in molecular biology, FP-speract would be quite useful for experimental training. The coloration of a FP-speract facilitates the visualization of the modified speract throughout the preparation along with the determination of its protein concentration.
In this study, we developed recombinant speract analogs tagged with an FP (FP-speract). Although the size of the fluorescent tag is more than 20 times larger than this ligand, FP-speract maintains activity comparable to that of speract, indicating that FP-speract is a useful tool with which to study the action of this peptide on spermatozoa. Using cyan and yellow variants of FP-speract, we were able to determine a cluster formation of the speract binding sites, which might imply some roles for positive and/or negative cooperativity in speract–receptor interactions. We believe that FP-speract is a useful tool not only for scientific research but also for experimental training. Furthermore, FP-tagged recombinant peptide could be generally useful for other types of peptide ligand.
We thank Dr T. Nagai (Osaka University), Dr A. Miyawaki (RIKEN) and Dr R. Campbell (University of Alberta) for providing eCFP-pRSETB, mVenus-pRSETB and pmAmetrine1.2, respectively, and Dr Y. Tatsu (AIST, Ikeda) for providing synthetic speract. We are grateful to the National Institute of Genetics (Mishima, Japan) for providing two E. coli strains, JM109(DE3) and BL21(DE3). We thank T. Olamendi (IBT-UNAM) for HPLC analysis of F-speract, X. Alvarado (IBT-UNAM) for the confocal images, and E. López, S. Becerra, J Yañez and P. Gaytán (IBT-UNAM) for oligonucleotide synthesis and DNA sequencing of plasmids. We thank A. Blancas (IBT-UNAM) for taking care of the sea urchins. We appreciate Dr A. Darszon's critical reading of the manuscript. We thank T. Liévano for reviewing the English grammar of the manuscript. We also thank an anonymous reviewer for their suggestion to improve our FRET experiment.
C.A.-H. performed almost all experiments and prepared all figures, F.R. prepared the plasmid encoding eCFP-speract, Y.S.-G. supervised preparation of plasmids encoding mVenus-speract and mAmetrine-speract and all recombinant proteins, C.B. supervised determination of all sperm physiological responses and visualization of speract binding site, and T.N. designed the entire project and wrote the manuscript. All authors participated in the interpretation of results and reviewed the manuscript.
This work was supported by Dirección General de Asuntos del Personal Académico - Programa de Apoyo a Proyectos de Investigación e Innovación Tecnológica (DGAPA-PAPIIT) - UNAM [IN204112 to C.B. and IN203513 to T.N.] and by Consejo Nacional de Ciencia y Tecnología (CONACyT) [128566 and 177138 to T.N.]. F.R. and Y.S.-G. are PhD students supported by CONACyT.
The authors declare no competing or financial interests.