|Home | About | Journals | Submit | Contact Us | Français|
Although recent evidence indicates that several chemokines and defensins, well-known as inflammatory mediators, are expressed in the male and female reproductive tracts, the location and functional significance of chemokine networks in sperm physiology and sperm reproductive tract interactions are poorly understood. To address this deficiency in our knowledge, we examined the expression and function in sperm of CCR6, a receptor common to several chemoattractant peptides, and screened several reproductive tract fluids for the presence of specific ligands. CCR6 protein is present in mouse and human sperm and mainly localized in the sperm tail with other minor patterns in sperm from mice (neck and acrosomal region) and men (neck and midpiece regions). As expected from the protein immunoblotting and immunofluorescence results, mouse Ccr6 mRNA is expressed in the testis. Furthermore, the Defb29 mRNA encoding the CCR6 ligand, β-defensin DEFB29, is expressed at high levels in the epididymis. As determined by protein chip analysis, several chemokines (including some that act through CCR6, such as CCL20/MIP-3α (formerly Macrophage Inflammatory Protein 3α) and protein hormones were present in human follicular fluid, endometrial secretions, and seminal plasma. In functional chemotaxis assays, capacitated human sperm exhibited a directional movement towards CCL20, and displayed modifications in motility parameters. Our data indicate that chemokine ligand/receptor interactions in the male and female genital tracts promote sperm motility and chemotaxis under non-inflammatory conditions. Therefore, some of the physiological reactions mediated by CCR6 ligands in male reproduction extend beyond a pro-inflammatory response and might find application in clinical reproduction and/or contraception.
A mammalian spermatozoon must locate the female gamete and deliver its genetic material to generate a new individual. The interaction of motile sperm with the oocyte – both at a distance and through physical interaction – represents a series of integrated processes designed to deliver sperm with optimal fertilizing potential to the site of fertilization. Sperm movement patterns appear to depend on external regulatory factors secreted by the oocyte or its surrounding cells that influence sperm motility (chemokinesis) and chemotaxis, which would optimize gamete interactions (Eisenbach, 1999; Eisenbach and Giojalas, 2006; Kaupp, 2012). The development of the fertilization-competent state occurs through an incompletely understood process called “capacitation,” which refers to the physiological changes that render spermatozoa competent to fertilize an egg (Visconti et al., 1998, 2011). Precontact communication by chemotaxis has been demonstrated between gametes in pig, rabbit, human, and mice (Cohen-Dayag et al., 1995; Lee et al., 1994; Sliwa, 1995; Spehr et al., 2003; Teves et al., 2010). The involvement of different molecules in chemokinesis and in the chemotactic attraction of human sperm to the oocyte is a fascinating and evolving concept.
The substances secreted by the male and female reproductive tracts that influence sperm behavior, physiology, and viability are coming to light, as techniques to screen for various substances in biological fluids are developed and improved. For instance, human seminal plasma contains a variety of inflammatory cytokines, which are thought to confer a survival advantage to spermatozoa within the female genital tract (Denison et al., 1999). Chemokines, a family of chemotactic cytokines produced by a wide variety of cell types, have the ability to attract cells in response to the activation of specific cell surface receptors (Baggiolini, 1998). Several types of mammalian β-defensins have also been found in male reproductive tissues (Conejo-Garcia et al., 2004; Li et al., 2001; Rodríguez-Jiménez et al., 2003). Multiple β-defensins have been independently identified as functional ligands for the chemokine receptor CCR6 (Conejo-Garcia et al., 2004; Röhrl et al., 2010a; Taylor et al., 2009; Yang et al., 1999) and, more recently, for CCR2 (Röhrl et al., 2010b).
Chemokine receptors belong to the superfamily of G protein-coupled receptors (GPCR). These canonical receptors have seven transmembrane sequences of 20-25 hydrophobic residues that form α-helices within the plasma membrane, an extracellular N-terminus, three extracellular loops, three intracellular loops, and a C-terminal cytoplasmic tail. These receptors transmit information to the cell about the presence of chemokine gradients in the extracellular environment. They are named depending on the structure of their ligand (CXC, CC or CX3C). The binding of a chemokine or chemoattractant peptide such as a β-defensin to its cognate receptor is followed by the involvement of heterotrimeric G proteins (Reif and Cantrell, 1998; Ward and Westwick, 1998) and the triggering of pathways involving intracellular second messengers such as cAMP and calcium.
The molecular mechanisms involved in the chemoattraction of specific sperm subsets prior to fertilization remain unknown. Moreover, the location and functional significance of chemokines and chemokine receptors in sperm physiology and male and female genital tracts are poorly understood. It is clear that sperm motility characteristics are modified in response to changes in the microenvironment as the sperm move through the male and female genital tracts. Furthermore, human seminal plasma has potent anti-inflammatory properties, which are thought to confer a survival advantage to spermatozoa within the hostile female genital tract (Kelly, 1995, Robertson et al 2007).
In this study, we identified the presence of receptor CCR6, and its chemoattractant ligands (CCL20 and β-defensins) in human and mouse spermatozoa as well as in the gamete microenvironment during capacitation. We also show that mouse Defb29, previously characterized by one of us (Conejo-Garcia et al., 2004), is highly expressed in the cauda epididymis. Our results provide evidence that, in addition to their role in inflammation, certain β-defensins and chemokines have specific functions through ligand/receptor interactions in sperm motility and chemotaxis acting in the male and female reproductive tracts.
Human semen samples were obtained by masturbation from healthy donors with proven fertility after 2-5 days of abstinence. The samples were collected in sterile containers and evaluated within 1 h after ejaculation following World Health Organization guidelines (World Health Organization, 2010). Briefly, semen analysis included evaluation of volume, concentration, motility, morphology, viscosity, and leukocyte count. Semen parameters were consistently superior to WHO reference values, and leukospermia was not found in any of the analyzed samples. Informed consent to use semen samples was obtained from each participant in this study and collection of semen was approved by the University of Pennsylvania Institutional Review Board. To prepare seminal plasma, liquefied semen samples were first centrifuged at 1,000 × g for 5 min, after which the supernatants were re-centrifuged at 10,000 × g for 15 min to remove cellular elements and debris. After centrifugation, the seminal plasma was collected and stored at −80°C until used. For capacitation, sperm samples were prepared as previously described (Caballero-Campo et al., 2006).
Human follicular fluid (FF) and endometrial fluid samples were obtained from women whose routine infertility examination revealed no abnormal findings, and who were undergoing transvaginal follicular aspiration for IVF due to male infertility as previously described (Simón et al., 1996). Fluids were collected under an Institutional Review Board protocol for samples that would otherwise be discarded. No patient identifiers were used in the sample collection nor was specific patient information received. Women with endometriosis, polycystic ovary syndrome, or infectious diseases were excluded from this study. The FF obtained from follicles of >16 mm diameter were pooled, immediately centrifuged for 5 min at 1,500 × g, and then filtered through a 0.5 μm disc filter to remove cells and debris. The filtrates were aliquoted and stored at −20°C until used.
Adult (>12 weeks old) CD-1 male mice were purchased from Charles River Laboratories, Inc. (Wilmington, MA). Mice were used in accordance with the International Guiding Principles for Biomedical Research Involving Animals as promulgated by the Society for the Study of Reproduction, and research protocols involving animals were approved by the University of Pennsylvania Institutional Animal Care and Use Committee.
Mouse cauda epididymal sperm and ejaculated human sperm were analyzed by indirect immunofluorescence (Kim et al., 2001) and flow cytometry (Griffiths et al., 2008). Noncapacitated and capacitated mouse and human sperm samples were washed for 5 min at 300 × g, resuspended in PBS, and attached to poly-L-lysine-coated slides. Spermatozoa were fixed (4% paraformaldehyde in PBS) for 15 min. After washing in PBS, slides were blocked with PBS containing 600 μg/ml BSA for 30 min at room temperature. The slides were then incubated for 1 h at 37°C in a humidified chamber with primary antibody (mouse anti-human CCR6 catalog number MAB195 or rat anti-mouse CCR6 catalog number MAB590, R&D Systems, Minneapolis, MN) diluted in blocking buffer 1:100. Slides incubated without first antibody in 10% normal goat serum were used as negative controls. After three washes in PBS, the slides were incubated in blocking buffer containing FITC-goat anti-mouse IgG (1:5000) and FITC-goat anti-rat IgG (1:5000) (Santa Cruz Biotech) for 1 h. Following several washes in PBS, sperm were examined by phase contrast/fluorescence microscopy (modified from Kim et al. (2001)). Analysis by flow cytometry of cells labeled with the antibodies was carried out as described by Lasso et al. (1994) with a FACSCalibur flow cytometer with CellQuest 3.2.1fl software (Becton Dickinson).
Mouse and human sperm proteins were separated by SDS-PAGE according to the method of Laemmli (1970) and transferred to Immobilon (PVDF) transfer membranes (Towbin et al., 1979; Turner et al., 1999, 2001). Blots were blocked in 5% non-fat dry milk in Tween-Tris buffered saline (TTBS) and incubated overnight at 4°C with primary antibody (goat anti-human/mouse CCR6, Catalog number C10129, Capralogics, Gilbertville, MA) in blocking buffer 1:500. Blots were then treated with secondary antibody (horseradish peroxidase-conjugated chicken anti-goat IgG, Santa Cruz Biotechnology, Santa Cruz, CA) in TTBS buffer (1:2000) for 1 h at room temperature, and developed using enhanced chemiluminescence (ECL) substrate (Pierce). Bound antibody was visualized by chemiluminescence exposure of X-ray film. In some experiments blots were developed using enhanced chemifluorescence (ECL Plus RPN2132) substrate (Amersham), utilizing a novel acridine-based chemistry and horseradish peroxidase to generate a light signal and also a stable fluorescent product that can be visualized by chemifluorescence densitometry (blue laser) on a Storm 860 phosphoimager (Molecular Dynamics. Sunnyvale, CA).
Samples from mouse testes and the different parts of the epididymis (caput, corpus, cauda) were used to study the expression of Defb29 (GenBank accession number AF515626) compared to other male and female tissues by real-time quantitative RT-PCR (Conejo-Garcia et al., 2004) Levels of mRNA encoding various gene products were determined by real-time RT-PCR as previously described by García et al. (2001). Briefly, after RNA extraction, complementary DNA was generated by reverse transcription with TaqMan® and SYBR® Green One-Step Real-Time RT-PCR Master Mix (Applied Biosystems, Foster City, CA). Complementary DNA primers were designed using Primer3 software (http://frodo.wi.mit.edu/). The primers used were previously designed as Defb29: (forward: 5’–CTG ATC CTG GTT GAC GAG ACC–3’; reverse: 5’–CTG GTA AAG CTC ACA CGC AAT C–3’) and Gapdh: (forward: 5’–CCT GCA CCA CCA ACT GCT TA–3’; reverse: 5’–CAT GAG TCC TTC CAC GAT ACC A–3’) (Conejo-Garcia et al., 2004; Cubillos-Ruiz et al., 2009). For Ccr6, the primers were (forward: 5’–GGA CTG AGA GCC CTG GAA AG–3’; reverse: 5’–CTT GAA TGG CAG ACA CTC ACA GT–3’). Standard curves for Defb29, Ccr6, and Gapdh were constructed. Two microliters of RT product were used for real-time PCR. The amplification reaction (25 μl) contained RT product, forward primer, and reverse primer. Reactions were performed with previously established thermal cycling conditions in the ABI 7700 Sequence Detector (Applied Biosystems). Collection and analysis of data were performed with ABI 7700 sequence detector software.
To evaluate the presence of chemokines in seminal plasma (4 specimens), follicular fluid (3 specimens), and endometrial fluid (3 specimens), samples were analyzed with the RayBio Human Cytokine Antibody Array I and IV membranes (RayBiotech, Norcross GA), which allow the detection of 42 and 38 different cytokines and chemokines, respectively. Membranes were analyzed following the manufacturer’s instructions. Briefly, membranes with pre-spotted capture antibodies were incubated with samples for 2 h at room temperature. Chemokines were detected by incubation with biotinylated detection antibodies for another 2 h at room temperature. Following addition of horseradish peroxidase-conjugated streptavidin and overnight incubation at 4°C, signals were revealed by ECL and (ECL Plus RPN2132 substrate Amersham). ECL Plus can be visualized by chemifluorescence densitometry (blue laser) on a Storm 860 phosphoimager (Molecular Dynamics. Sunnyvale, CA). Positive controls included in the blot were used to normalize the results from different membranes.
To demonstrate a functional role for CCR6 in human sperm, we investigated the dynamic response of capacitated spermatozoa to treatment with several CCR6 ligands. To perform an objective evaluation, computer assisted sperm analysis (CASA; IVOS system version 12, Hamilton-Thorne Biosciences, Beverly, MA) was performed to assess changes in motility patterns after exposure to CCR6 ligands. The kinetic parameters classify sperm movement into different types of progressive motility as “rapid” or “slow” according to the CASA settings, and as “hyperactivated” motility using the criteria defined previously (Burkman, 1991; Caballero-Campo et al., 2006). Capacitated human sperm samples were incubated with the ligands for CCR6 to assess effects on sperm motility kinetics and chemotaxis. After capacitation, 10 million cells per ml were incubated with increasing concentrations (0, 10, 100, 1000 pg/ml) (Isobe et al., 2002) of recombinant human CCL20 (R&D Systems, Minneapolis, MN), recombinant human DEFB4A (also known as DEFB2, formerly hBD-2; Catalog No. HBD25-R from Alpha Diagnostics International, San Antonio, TX) (Hoover et al., 2002; Pérez-Cañadillas et al., 2001) and human DEFB103A (also known as DEFB3, formerly hBD-3; Catalog No. HBD37-R from Alpha Diagnostics International) (García et al., 2001) proteins diluted in HTF medium at 37°C and 5% CO2. As a control, several dilutions of FF were used. At the end of the incubation times, manual motility assessments (World Health Organization, 2010) were performed on sperm from different concentration treatments. The 1,000 pg/ml point was chosen as the working concentration for the following motility assay experiments. The motility patterns of capacitated sperm were examined with a double sperm motility and chemotactic evaluation approach, after treatment with ligands for CCR6. The analysis of sperm motility parameters was performed using CASA. For this evaluation, 5 μl aliquots of treated or control sperm samples were placed in a 20 μm depth standard count analysis chamber (Leja Products, Nieuw-Vennep, The Netherlands) that had been preheated at 37°C, and analyzed using the CASA system with settings according to the manufacturer’s instructions. For every sample, approximately 10 randomly selected fields were evaluated for a minimum total of 300 sperm. Average values were obtained for sperm motion parameters such as: curvilinear velocity (VCL), straight-line velocity (VSL), average path velocity (VAP), amplitude of lateral head displacement (ALH), linearity (LIN=VSL/VCL), and straightness (STR=VSL/VAP). Progressive motile sperm were defined by values of VAP > 20 μm/s and STR > 80%. Rapid or slow motile sperm cells were classified according to the CASA standard cutoff values for VAP and VSL. Slow cells were defined as cells with either of the following attributes: VAP < 20 μm/s or VSL < 30 μm/s. In addition, we also analyzed individual parameters and recorded sperm tracks (Caballero-Campo et al., 2006).
To investigate the chemotactic effect of CCL20, the percentage of chemotactic sperm after the different treatments was analyzed by the directionality-based method described by Fabro et al., (2002), with minor modifications, using the Zigmond chemotaxis chambers (Zigmond, 1977). These devices, kindly provided by Dr. Sally Zigmond of the University of Pennsylvania, consist of two wells separated by a partition wall and closed with a cover slip. As a control for human sperm chemotaxis, we used follicular fluid, which is well-established as a sperm chemoattractant (Cohen-Dayag et al., 1995; Eisenbach and Tur-Kaspa, 1999; Makler et al., 1992; Ralt et al., 1991; Villanueva-Diaz et al., 1990). Briefly, the system allows the formation of a concentration gradient of the chemoattractant test substance between both compartments. The spermatozoa are put in one well, whereas the testing well is filled with FF or a CCR6 ligand. The movement of the cells in the partition wall separating the wells is recorded at 10X magnification. Our video microscopy system consists of an inverted microscope Nikon TE2000 equipped with a Princeton Instruments MicroMax CCD camera with a time-lapse video recorder (Roger Scientific, Trenton NJ) (Buffone et al., 2009). The system allows the formation of a concentration gradient from the one well, filled with the chemoattactrant (CCL20), to the other well, filled with spermatozoa (capacitated sperm). Sperm cells were recorded onto the partition wall (in the middle of the two wells) at using a 10X objective for 10-15 minutes. As controls for human sperm chemotaxis, we used FF which is a well-established sperm chemoattractant (Eisenbach and Tur-Kaspa, 1999), and non-capacitated human sperm cells as negative control, only capacitated cells are chemotactically responsive (Cohen-Dayag et al., 1995). In each recording, the sperm tracks where analyzed semiautomatically (Fabro et al., 2002) for 5-10 minutes after the distribution of the cells was stable. Defining X-axis as the direction of the gradient, the tracks were analyzed as the percentage of the cells traveling longer distance in the direction of the chemoattractant gradient than in the gradient-less direction, perpendicular defined by Y-axis. We evaluated the chemotactic sperm tracks using a grid, in by the means of the percentage of cells having ΔX/ΔY>1 (± SD), apart from the sperm speed and pattern of movement (Fabro et al., 2002). The results shown in Figure 7 correspond to 4 independent experiments from two donors. In addition, under the same CCL20 and FF treatment conditions as for sperm motility evaluation, we analyzed individual motility parameters and recorded sperm tracks (Caballero-Campo et al., 2006). All data were transferred and processed in Excel files prior to statistical analysis.
The Statistical Package for the Social Science (SPSS Inc., Chicago, IL) was used for statistical analysis. The analysis of variance (ANOVA) for multiple comparisons was carried out between groups and p<0.05 was considered statistically significant.
To define the presence of chemokines in reproductive fluids, we performed protein arrays using human seminal plasma, endometrial fluid, and follicular fluid. An unexpectedly high number of chemokines were identified in fluids from both the female and male genital tracts. These included the specific CCR6 ligand CCL20, as well as CXCL8 (interleukin 8), CX3CL1 (fractalkine), and CCL2 (monocyte chemotactic protein 1), traditionally associated with the recruitment of multiple immune cell populations. In addition, CCL5 (RANTES) was found in follicular fluid, but not in seminal plasma nor endometrial fluid (Figure 1). Relevant expressions patterns for IL-8, CCL2/MCP-1, CCL5/Rantes, CXC3CL1/Fraktalkine, and CCL20/MIP-3α are summarized in Table 1.
In complementary studies in mice, we next determined the expression of the corresponding receptors in a variety of tissues, and we found that Ccr6 mRNA is expressed at high levels in the testis but it was undetectable in samples from the uterus (Figure 2A). To define the expression of alternative CCR6 ligands in reproductive tissues, we focused on the unknown expression pattern of the Defb29 mRNA encoding mouse DEFB29, a proven CCR6 ligand and the counterpart of human DEFB116 (Conejo-Garcia et al., 2004). Surprisingly, the highest level of Defb29 expression was found in the cauda epididymis, relative to any other tissue (Figure 2B). Defb29 mRNA was also expressed by other regions of the epididymis at significantly lower levels.
Because Ccr6 mRNA is expressed in the male mouse genital tract, but not at detectable levels in uterine tissue, we next aimed to define the presence and localization of the CCR6 protein in mouse and human sperm. Indirect immunofluorescence revealed that CCR6 was clearly detected in human sperm and was mainly localized in the tail and in the post-acrosomal region (Figure 3A). CCR6 was also found in the midpiece and basal region (neck) in a small percentage of sperm cells. In mouse sperm, CCR6 was also primarily identified in the principal piece and neck region of the tail, although a small percentage of sperm cells showed staining in the acrosomal area (Figure 4A).
Curiously, some human sperm cells did not display detectable CCR6 signal. In examining this issue further, it appeared that the detectability of CCR6 may be related to the state of sperm capacitation. To address this in an objective manner, we utilized flow cytometry analysis of human and mouse sperm before and after capacitation (Figure 3B, Figure 4B). In sperm from both species and states of capacitation, we found two subpopulations of sperm that differed in their staining with antibody to CCR6. Following capacitation, the more intensely labeled sperm became more abundant, suggesting that capacitation causes the exposure or unmasking of epitopes recognized by the CCR6 antibodies. Thus, the percentage of sperm showing CCR6 staining may reflect different levels of sperm maturation. Alternatively, the variability could result from differences in the expression levels of the protein from cell to cell during spermatogenesis, from contributions by epididymosomes during transit through the epididymis, or from the mixing with prostasomes during ejaculation (human only). Immunoblotting analyses confirmed the presence of CCR6 in mouse and human sperm with the expected molecular weights (Figure 5). Therefore, the chemokine receptor CCR6 was present mainly in the tail of sperm cells, where it may play a role in sperm motility as a chemokine sensor.
CASA demonstrated that the number of sperm showing kinetic parameters related to progressive motility (VSL and VAP) was higher after CCL20 treatment compared to the rest of the treatments (FF and β-defensins) (Figure 6). Moreover, maximal chemotactic responsiveness was observed with CCL20. CASA analysis showed that the percentage of cells with a progressive motility pattern also increased after CCL20 treatment. In FF treated cells, the percentage showing a linear swimming pattern decreased, whereas the percentage of hyperactivated sperm increased. On the other hand, motility pattern changes were negligible after treatment with DEFB4 and DEFB103A (also known as DEFB2 and DEFB3), both of which are known ligands of CCR6, although these are considered weaker than CCL20 (Ghannam et al., 2011; Yang et al., 1999) (Figure 7). Therefore, CCR6-displaying sperm cells increase their motility in response to the CCR6-specific chemokine ligand CCL20, demonstrating that CCR6 is functional in sperm and may also respond to CCL20 in fluids from the male and/or female genital tracts.
Before fertilization, sperm must receive and process environmental signals to locate the oocyte (Yanagimachi, 1994). Experiments performed in sea urchin and in other marine species (Guerrero et al., 2010; Kaupp et al., 2003), demonstrated that these chemoattractants originate from the oocyte and its surrounding investments (Sun et al., 2005). In addition, seminal plasma is not just a carrier for spermatozoa. It contains high concentrations of cytokines, chemokines, and other biological compounds that are able to exert potent effects on the immune system of the receptive partner (Robertson et al., 2006; Sharkey et al., 2012). Previous studies have shown that semen induces an acute inflammatory response at the female genital mucosa after coitus in mammals (for review Robertson et al. (2007), including humans (Sharkey et al., 2012). The interactions of the sperm with these chemoattractants primarily influence sperm movement, directing the sperm to the site of fertilization.
Potential chemoatractant molecules (chemokines and β-defensins) also arise from the reproductive tract, as shown in the present study. Chemokines are involved in several human reproductive events (García-Velasco and Arici, 1999; Simón et al., 1998), including regulatory mechanisms that allow the embryo to grow and develop in the uterus (Caballero-Campo et al., 2002; Dominguez et al., 2003), and also sperm chemotaxis (reviewed by Eisenbach and Giojalas (2006)). Although β-defensins have been described in association with sperm, the function of the β-chemokine receptor CCR6 and its specific ligand CCL20 have never been characterized in sperm, normal reproductive tissues, or genital tract fluids.
In the present study, we found that Ccr6 mRNA is expressed in the mouse testis, and the protein was located on the plasma membrane of mouse and human sperm. These results were confirmed by immunoblotting analyses. We believe that the majority of CCR6 in human and mouse sperm originate in the spermatogenic cells based upon our RNA expression studies (Figure 2) and data available at the Mammalian Reproductive Genetics website at the University of Washington [http://mrg.genetics.washington.edu/index.cgi?mrg_id=328109] although it is formally possible that that some CCR6 is contributed to the sperm by epididymosomes (Sullivan et al., 2007). In both species, the receptor was primarily localized to the principal piece of the tail, which represents the first evidence for the presence of CCR6 on the surface of human and mouse spermatozoa. This region is involved in motility and hyperactivation, a specialized motility pattern associated with capacitation (Suarez, 1996). Moreover, using flow cytometry with non-capacitated and capacitated sperm, we determined that the ability of the anti-CCR6 antibody to detect the protein was dependent on the capacitation state of the sperm. In studies with other cytokine receptors, such as CX3CR1, only half of the sperm population was found positive for the receptor (Zhang et al., 2004). Based on this prevalence, it was suggested that chemokine receptor cell surface levels vary according to receptor endocytosis and recycling (Oppermann, 2004). However, we propose that chemokine receptor detection on the sperm surface may actually be dependent upon the capacitation state of the individual sperm cell.
With demonstration of the presence of CCR6 on the surface of human and mouse sperm, we next looked at whether ligands for this receptor were expressed in the male and female reproductive tract fluids. We found the CCR6-specific ligand CCL20 in human seminal plasma, endometrial fluid, and follicular fluid. As previously described, other chemokines such as CX3CL1, CXCL8, CCL5, and CCL2 were also detected in these reproductive fluids (Caballero-Campo et al., 2002; García-Velasco and Arici, 1999; Isobe et al., 2002; Kawano et al., 2001; Zeyneloglu et al., 1998; Zhang et al., 2004). Seeking to identify the presence of alternative CCR6 ligands in mouse reproductive tissues, we focused on mouse DEFB29, which is the β-defensin with the clearest human counterpart in terms of sequence similarity (DEFB116). DEFB29 is a proven CCR6 ligand (Conejo-Garcia et al., 2004) and the expression patterns of either mouse DEFB29 or human DEFB116 (human counterpart) were previously completely unknown. As shown in this study, we now know that the mRNA encoding mouse DEFB29 is very highly expressed in the cauda epididymis.
The β-defensins have been mostly described in the male (Patil et al., 2005), but they are also found in the female genital tract (Quayle et al., 1998; Valore et al., 1998). In the female mouse endometrium, β-defensins are regulated by estradiol (Soboll et al., 2006). In addition, the expression of β-defensins in the human endometrium varies in relation to the stage of the menstrual cycle (King et al., 2003). This is similar to what we have previously seen with chemokines (Caballero-Campo et al., 2002). This suggests a common regulatory role for these molecules in reproductive tract maintenance, host defense, and also fertility (García et al., 2001; Yudin et al., 2005). It is possible that chemokines and β-defensins modulate sperm–oocyte or sperm–reproductive tract interactions as well as sperm motility (Eisenbach and Giojalas, 2006; Tollner et al., 2008a, 2008b, 2012). Moreover, mutations in certain human β-defensins may cause impaired sperm function and subfertility (Tollner et al., 2011). In particular, we hypothesized that these molecules play a role in sperm physiology while protecting the male reproductive tract from invading microbial pathogens. In addition, we demonstrated that CCR6 specific ligands were relevant for sperm motility and sperm-egg interactions, unveiling their potential contribution to the pre-fertilization processes. We employed the previously described directionality-based assay (videomicroscopy in a Zigmond chamber) for sperm chemotaxis (Fabro et al., 2002; Zigmond, 1977) and CASA analysis of sperm motility parameters (Caballero-Campo et al., 2006). Capacitated sperm were treated with human follicular fluid and the recombinant CCR6 specific ligands (CCL20 and β-defensins). Furthermore, human FF was used as a source of substances secreted from the egg and its surrounding cells, including CCL20 as shown in this study. We found that capacitated cells respond chemotactically to a gradient of human FF, which is in agreement with earlier studies (Fabro et al., 2002; Giojalas and Rovasio, 1998; Ralt et al., 1991). These investigations also described the independence of chemotactic responsiveness from other kinetic behaviors (chemotaxis versus chemokinesis), such as hyperactivation, due to the presence of progesterone in FF (Jaiswal et al., 1999; Mbizvo et al., 1990). Significantly, the chemotactic response was more intense to CCL20 compared to FF, exhibiting an increase in the number of progressively motile sperm and illustrating the absence of an effect on hyperactivation. In future studies, the effects of CCL20 on motion of hyperactivated sperm should be more thoroughly studied in light of recent observations suggesting that hyperactivation is part of the chemotactic response (Armon and Eisenbach, 2011).
Human β-defensins use the same receptor (CCR6) as does the chemokine CCL20, suggesting that these proteins share similar structural features and, possibly, an analogous mechanism of receptor recognition and activation. Comparison of the structures of both human and murine β-defensins with human and murine CCL20 indicated a single aspartate (Asp 1 in human DEFB1), followed by the hydrophobic residue Tyr3 or Val6 (DHYNCV motif in human DEFB1), as a potentially important determinant of CCR6-mediated chemotactic activity of defensin. The DHYNCV fragment is equivalent to the DCCL motif in CCL20, and in human DEFB1(Hoover et al., 2002; Pérez-Cañadillas et al., 2001; Rodríguez-Jiménez et al., 2003). These proteins chemoattract and regulate dendritic cells through binding the CCR6 receptor (Yang et al., 1999). Recently, mononuclear phagocytes with properties similar to dendritic cells have been located in a dense network at the base of the epididymal epithelium in the mouse (Da Silva et al., 2011).
CCR6 characterization experiments were performed using an antipeptide antibody. The region used as an antigen corresponds to amino acid residues 18-46 of human CCR6, and the antibody also cross-reacts with the mouse orthologue. CCR6–deficient mice appear to be healthy and breed well (Cook et al., 2000; Varona et al., 2001). However, as far as we know, no specific studies on reproduction and sperm function have been reported. Multiple sequence alignments with other chemokine receptor sequences showed approximately 38% amino acid identity with the α-chemokine receptors hCXCR1 and hCXCR2, which represents only slightly more identity than the closest β-chemokine receptor hCCR4, which is approximately 36% identical (Greaves et al., 1997). The similarity between the human and murine CCR6 sequences is 73.8% over the entire sequence (Varona et al., 1998). However, hDEFB4 and hDEFB103A, together with their mouse orthologues (mDEFB4 and mDEFB14), are chemotactic for a broad spectrum of leukocytes in a CCR6– and, also, CCR2–dependent manner (Röhrl et al., 2010a). Expression of several chemokine receptors in sperm has been previously reported (Muciaccia et al., 2005; Zhang et al., 2004; Zuccarello et al., 2011). Taken together, our results suggest that β-defensins and chemokines present in reproductive fluids may modulate sperm movement through interaction with their cognate receptors in the membrane of the sperm cells.
Functional experiments with capacitated human sperm in the present study indicated that CCR6 and specific ligands might be involved in motility changes related to the capacitation process, especially kinetic alterations and chemotaxis. Thus, the CCR6 location in sperm might potentially identify capacitated sperm subpopulations (Eisenbach, 1999). Considering that receptors for progesterone and mannose identify a subset of sperm (Aitken, 1994; Benoff et al., 1993), it might be possible that functionally viable sperm express receptors, e.g., CCR6 or other G-protein coupled receptors such as olfactory receptors (Spehr et al., 2003).
The interaction of motile human sperm with the oocyte represents a series of integrated processes designed to deliver sperm with optimal fertilizing potential to the site of fertilization. These functions may be extremely significant from a medical standpoint. Determining the prevalence of these factors in fertile and infertile patients might provide relevant clinical information about certain mechanisms of male reproductive function and dysfunction. More importantly, these molecules could play a role in the etiology of idiopathic immunological infertility and may provide tools for its specific diagnosis and possible treatment. In addition, these mechanisms may expose new targets for contraceptive interventions. Ongoing studies will elucidate the molecular signaling pathways associated with these receptors in human and mouse sperm.
The authors would like to thank Dr. Caballero-Peregrin and the Andrology Laboratory group at Clinica Tambre (Madrid, Spain) with human sperm analysis assistance. We also thank Prof. Gerton and Prof. Rinaudo laboratory members for their technical help, especially Xiaoe Liu with immunoblotting. PCC is very grateful to instructors and participants of the 2012 FIR course and Symposium for technical assistance and constructive criticism, and Fundacion Tambre for research funding. PCC would also like to thank Professors Luis Blasco and Jerome Strauss for their encouragement to work in the Center for Research on Reproduction and Women’s Health. We dedicate this study to Professor Emeritus Bayard T. Storey on the occasion of his 80th birthday; Professor Storey was a wonderful resource and advisor during the execution of these studies.
Support: This study was supported in part by CONRAD (GLG), NIH HD-41552 (GLG), Beca de Investigación 26302 from Fundación Salud 2000 and Fundación Tambre, Madrid, Spain (PCC); NIH RO1TW008662 and PICT 2010-2426 from Agencia Nacional de Promoción Científica y Tecnológica, Buenos Aires, Argentina (MGF); NIH 15 CA137499-01 and NSF CBET-1039869 (FB); NCI 2RO1CA124515, NCI RO1CA157664, and DoD grant OC100059 (JRCG); NIH HD-RO1 062803-01A1 (PFR); PCC, MGB, FB, JRCG and PFR worked previously at the CRRWH, Perelman School of Medicine at the University of Pennsylvania, where this study was developed.
Final version of this study was presented at the 2012 Frontiers in Reproduction (FIR) 15th Anniversary Symposium (Marine Laboratory, Woods Hole, MA, USA).
The authors have declared that no competing interests exist.