PMCCPMCCPMCC

Search tips
Search criteria 

Advanced

 
Logo of scirepAboutEditorial BoardFor AuthorsScientific Reports
 
Sci Rep. 2017; 7: 44339.
Published online 2017 March 13. doi:  10.1038/srep44339
PMCID: PMC5347088

Quality of seminal fluids varies with type of stimulus at ejaculation

Abstract

The theory of ejaculate economics was mainly built around different sperm competition scenarios but also predicts that investments into ejaculates depend on female fecundity. Previous tests of this prediction focused on invertebrates and lower vertebrate, and on species with high female reproductive potential. It remains unclear whether the prediction also holds for polygynous mammals with low female reproductive potential (due to low litter size and long inter-birth intervals). We used horses (Equus caballus) to experimentally test whether semen characteristics are adjusted to the oestrous cycle of the mare a stallion is exposed to during few moments before ejaculation. We analysed 122 weekly semen samples collected from 16 stallions during exposure to either an oestrous or a dioestrous mare. Semen volume and the rate of motile sperm were higher when stallions were exposed to an oestrous than to a diestrous mare, while total sperm counts and sperm velocity remained unchanged. Sperm collected after exposure to an oestrous mare also showed reduced oxidative degeneration of cell membranes over a period of 48 hours. We conclude that stallions invest more into their seminal fluids when the chance of fertilization is elevated, and that this adjustment of ejaculate quality can happen very quickly.

The theory of ejaculate economics1 makes strong prediction about the evolution of reproductive traits and about phenotypic plasticity in male reproductive parameters. Many of these predictions have successfully been tested in comparative studies and in experimental work within species. For example, testes differ morphologically and ejaculates generally contain more sperm in species or populations with more sperm competition2,3,4, and males can quickly adjust their investment into an ejaculate to the expected level of sperm competition5,6,7,8. A general conclusion from this theoretical and empirical work is that sperm competition favours large and high-quality ejaculates, and, because the possibility of sperm competition is probably ubiquitous, costs and benefits of ejaculates therefore need to be optimized. These costs and benefits are predicted to not only depend on the number of rival males but also on female quality. Males are expected to differentially invest into ejaculate quality if females vary in fecundity1,9.

Regardless of whether an ejaculate is adjusted to the number of rivals or the fecundity of a female, an important question in ejaculate economics is always whether each sperm has the same chance of fertilizing an egg1, i.e. whether the raffle is “fair” or “loaded”. Reasons for a loaded raffle can be extrinsic, including differences in the timing of insemination (e.g. relative to the timing of oestrus), or intrinsic, due to differences in sperm quality or the quality of seminal fluids. Key factors in ejaculate economics are therefore not only sperm number per ejaculate but also sperm velocity and sperm longevity. Arguably, variation in sperm velocity may be more relevant in external fertilizers where fertilization happens within seconds and sperm longevity is typically in the range of few seconds or minutes10, while variation in sperm longevity may be more relevant in internal fertilizers where sperm may need to remain functional for longer times to successfully fertilize an ovum (e.g. several hours or days in many mammals, including humans and horses). In the latter case, the ability of seminal fluids to support sperm longevity (e.g. to protect them from oxidative damage) may play a decisive rule11.

Seminal fluids often make up a larger part of an ejaculate. They may contain specific proteins, hormones, antimicrobials, immunity suppressors, fats, sugars, salts, and different types of cells, including immunity cells12,13. The composition of seminal fluids is generally expected to vary with male genetics, condition, life history, and social situation13, with different functions for different components14,15. Little is known about the relative cost of the various components. However, seminal fluids have important effects on female reproductive physiology16 and on male and female fitness17, and the availability of seminal fluids has been found to limit remating18. Males are therefore predicted to rapidly modify the composition of ejaculates in response to female characteristics. Such a rapid adjustment may be under hormonal control, e.g. by testosterone that can rise quickly in response to the presence of a female19 and that has been found to influence characteristics of seminal fluids20,21.

We chose the polygamous horse (Equus caballus) to test experimentally whether blood testosterone concentration, behavioural indicators of sexual arousal, and ejaculate characteristics vary with oestrous cycle of a stimulus mare that a stallion is exposed to shortly before and during ejaculation. We used a within-subject experimental design to control for possible variance among stallions. Semen quality was determined immediately after ejaculation and over a period of 48 hours thereafter.

Material and Methods

Sixteen clinically healthy and sexually experienced stallions (mean age = 12.1 years, range 5–19) and mares A and B (11 and 13 years old, respectively, with regular oestrous cycles) were used for the experiments (all of Franches-Montagnes breed and unrelated to each other). They were kept in individual boxes bedded with straw, with other horses of only the same sex in the same stable each, i.e. the sexes were separated in different stables and there was no contact between the sexes other than during experimental exposure. All horses were regularly exercised and had daily access to a paddock. The study was approved by the Etat de Vaud, Service Vétérinaire (permit no 2667.1). All methods were performed in accordance with the relevant guidelines and regulations (Vaud canton and Swiss Confederation).

The experiments lasted over a period of 7 weeks and took place every Tuesday in a building that was separated from the housing stables. One of the two mares was led to this building and tethered close to a dummy. Stallions were then individually led to this building where they were first exposed to this mare’s faeces for 15 seconds (presented on a plastic plate on the ground). The stallion was then held in front of the mare’s head at a distance of about 2 meters and for about 30 seconds, then led to a dummy that the stallion could mount and that was used to collect the semen in an artificial vagina (type “Avenches”). A second faeces sample of the stimulus mare was hung in a perforated bag above the dummy. The stallion was then returned to its box, the hind part of the dummy was wrapped with a new plastic film (routine sanitary procedure), and the procedure was repeated with the next stallion. After 8 stallions, the mare was replaced by the other one, and the experiments continued with the remaining 8 stallions and with new faeces samples from this other mare. In order to ensure a crossover study design, the order of presentation changed over the first 6 weeks so that by the end of the 7th week, each stallion had been exposed to each mare once in oestrus and 2 or 3 times in dioestrus. The stallions were always handled by the same person who was not informed about the study design and its objectives.

The cycles of the two mares were regularly assessed by rectal ultrasonography of ovaries and uterus. The mares were in dioestrus on two or three consecutive Tuesdays and in oestrus the following Tuesday. Oestrus was defined as existence of a follicle >35 mm, uterus oedema at stage >222 combined with typical oestrous behaviours that include “sawhorse” posturing with lowered pelvis, vocalizations, frequent urination, and rhythmic eversion of the clitoris23,24. Oestrous mares were given 1500 IE hCG (Chorulon®, Intervet, Boxmeer, Netherlands) intravenously on the Monday evening before the experimental exposures on the following Tuesday in order to induce ovulation.

The behaviour of both the mare and the stallion was filmed (two cameras from different angles) to record time until erection, first mount on the dummy, and ejaculation confirmed by rhythmic tail flagging25,26. Mare vocalisation was recorded by an observer who did not know the oestrous cycle of the mare. Blood samples were obtained by jugular venipuncture from stallions 15 minutes before semen collection and immediately afterwards. Plasma testosterone concentrations were determined via electrochemiluminescence immunoassay (Elecsys 2010, Roche Diagnostics, Basel, Switzerland) as described previously27 (inter- and intra-assay coefficients of variation were 2.2 and 1.4%, respectively). Volume of the fresh ejaculate was measured after removal of the gel fraction. Sperm concentration was assessed with the Nucleocounter® SP-100TM system (ChemoMetec A/S, Allerød, Denmark). Semen was then diluted with INRA 96TM (IMV technologies, L’Aîgle, France) to a concentration of 30 × 106 spermatozoa/ml. Diluted semen was placed in a pre-warmed 20 μm standard count analysis chamber (Standard Count Analysis Chambers SC 20-01-C, Leja, Nieuw-Vennep, The Netherlands) and assessed for motility parameters in 10 fields using a computer-assisted sperm analyser (HTM-IVOS, version 12.1, Hamilton Thorne Biosciences, Beverly, USA) and standardized settings for stallion semen28. In each sample, the total motility (%), the average path velocity (VAP μm/s, average velocity of the smoothed cell path), the curvilinear path velocity (VCL μm/s, average velocity measured over the actual point-to-point track followed by the cell), and the straight-line velocity (VSL μm/s, average velocity measured in a straight line from the beginning to the end of track) of sperm cells were determined. A sample of fresh diluted semen was then packaged in an EquitainerTM (Hamilton Thorne Biosciences, Beverly, USA) and sent to the Clinic of Reproductive Medicine, University of Zurich/Switzerland, for analysis of sperm motility, viability and membrane lipid peroxidation after 24 and 48 hours of cold (4 °C) storage. Evaluation of the plasma membrane and acrosome integrity as well as of the lipid peroxidation of spermatozoa was performed using a Cell Lab Quanta SC MPL flow cytometer operated by the Cell Lab Quanta SC Software for instrument Control Data Acquisition (Beckman Coulter Inc., Nyon, Switzerland). The system was equipped with a solid state LASER exciting at 488 nm and emission filters detecting green, orange and red fluorescence at 525, 590, 670 nm, respectively. Flow rate was set to 500 cells/s and for each sample 10000 events were analysed after incubation of stained sperm for 15 min at 38 °C. Membrane integrity and acrosomal status of spermatozoa were evaluated after double staining with propidium iodide (PI) and peanut agglutinin conjugated with fluorescein isothiocyanate (FITC-PNA)29,30. Five μl of the semen previously diluted with 238.5 μl Tyrode’s solution to a final concentration of 0.6 × 106 spermatozoa/ml were stained by adding 1.5 μl of 2,99-mM PI (Sigma-Aldrich, Buchs, Switzerland) and 5 μl FITC-PNA (100 μg/ml) (Sigma-Aldrich Buchs, Switzerland). The percentage of membrane and acrosome intact spermatozoa was defined as viability. For determination of lipid peroxidation in spermatozoa a combined staining with the BODIPY581/591-C11 probe31,32 and PI was used. 2.5 μl of 1000-μM BODIPY581/591-C11 (Thermo Fisher Scientific, Riehen, Switzerland) and 1.5 μl of 2,99-mM PI (Sigma-Aldrich, Buchs, Switzerland) were added to 5 μl of semen and mixed with 241 μl Tyrode’s medium to a final concentration of 0.6 × 106 spermatozoa/ml. Mean BODIPY581/591-C11 fluorescence intensity of live (PI negative) sperm cells was considered for further analysis.

Statistical analyses were done in JMP® 11.2. Effects of stallion and mare identity (ID) on potential measures of sexual arousal and on characteristics of fresh semen were analysed in least square multiple regressions, with oestrous stage nested in mare ID. Repeated measures on consecutive testosterone measurements and on semen characteristics taken 24 h and 48 h after ejaculation were analysed in MANOVAs. Some semen and some blood samples could not be measured due to technical problems. It turned out, however, that no experimental cell of the factorial within-subject design was lost because all missed samples had been taken during exposure to dioestrous mares for which we always had several replicates per combination of stallion and mare. Therefore, using average values per stallion, time point of measurement, mare, and oestrous stage (n = 16 × 2 × 2 × 2 = 128) ensured a balanced data set for all analyses. We used directed testing (pdir) when there was a strong a priori expectancy about the direction of an effect and to avoid inflation of the alpha value33. If directed and two-tailed testing led to the same conclusions, two-tailed p-values (p) are reported. Kendall rank correlation coefficients τ were used to analyse correlations.

Results

The stallions differed in mean time to erection, time to first mount the dummy, and time to ejaculation (Table 1). All these time periods were shorter when stallions were exposed to an oestrous than to a dioestrous mare (Table 1), while mare ID did not significantly influence indicators of male sexual arousal (Table 1). Both mares vocalized more intensely in reaction to a stallion and turned their head longer towards the stallion when in oestrus than when in dioestrus (mean numbers of vocalizations ±95% CI: 0.9 ± 0.5 versus 2.5 ± 1.5, paired t-tests: t = 3.5, d.f. = 15, p = 0.003; mean duration of head towards the stallion: 59.0 ± 21.2 versus 68.6 ± 10.2, paired t-tests: t = 3.3, p = 0.004), in addition to the behaviours that they only showed during oestrus such as clitoral eversion, urination and sawhorse posture.

Table 1
Effects of stallions’ and mares’ ID and oestrous stage on indicators of stallions’ sexual arousal and characteristics of fresh semen.

The stallions differed in average sperm number, concentration, volume, velocity, and motility as determined immediately after semen collection (Table 1), in blood plasma testosterone levels around ejaculation, and sperm viability, velocity, motility, and lipid peroxidation 24 h and 48 h after ejaculation (Tables 2, ,3).3). Mare ID did not seem to have an influence on semen characteristics (Tables 1, ,2,2, ,3).3). When the stimulus mare was in oestrus, sperm motilities were increased (Table 1), and, while sperm velocity and total sperm counts remained unchanged, sperm concentration per ejaculate had declined, i.e. overall semen volume had increased (Table 1).

Table 2
Effects of stallions’ and mares’ ID and oestrous stage on stallions’ plasma testosterone levels before and immediately after semen collection, and on sperm viability and lipid peroxidation 24 h and 48 h after ejaculation. ...
Table 3
Effects of stallions’ and mares’ ID and oestrous stage sperm velocity and motility 24 h and 48 h after ejaculation.

Blood plasma testosterone increased from before to immediately after ejaculation (Table 2) and was not statistically linked to the oestrous stage of the stimulus mare (Table 2). However, whether the stimulus mare was in oestrus or in dioestrus had a marked effect on lipid peroxidation of sperm after 24 and 48 h cold storage (Table 2; Fig. 1). Lipid peroxidation increased and sperm viability decreased over time (Table 2; Fig. 1). Sperm velocity and motility measures taken on sperm after 24 and 48 h of cold storage were not statistically correlated to the respective lipid peroxidation measures (|τ| always ≤0.11, p always >0.29) and did not seem to be affected by the oestrus stage of the stimulus mare but were mainly linked to stallion ID and time (Table 3, see also time × stallion ID interaction effects). While the rate of motile sperm declined from 24 h to 48 h after ejaculation, the average velocity of the motile sperm increased during this observational period (Table 3). None of the observed differences in semen characteristics could be explained by stallion age or size (i.e. withers height; |τ| always <0.32, p always >0.08).

Figure 1
Lipid peroxidation rate (Bodipy fluorescence intensity; medians, quartiles, and deciles) of sperm membranes after 24 h (open bars) and 48 h (closed bars) when the stimulus mare was either in oestrus or dioestrus at ejaculation.

Discussion

The stallions differed significantly in all measurements we took, from indicators of sexual arousal and testosterone blood plasma concentration to all characteristics of fresh and aging ejaculates. It therefore turned out to be important to use a within-subject experimental design that controls for this variance. The origins of such strong male effects are unclear. It has been suggested that reproductive parameters may reveal variance in health and vigour, but this hypothesis is little supported in humans34 (apart from several infertility aetiologies35 or the damaging effects of cigarette smoking and other life-style factors36) or in species with secondary sexual traits that may serve as quality indicators37. The housing conditions that our stallions experience at the stud are expected to minimize variance in health and vigour, and we found no correlations between reproductive parameters and stallion age or size. However, we cannot exclude potential effects of the order of presentation to the mares (the stallions were largely used in the same order each, and smells of previous stallions that had been tested in the experimental set up could not be avoided).

In contrast to the significant stallion effects, the ID of the two mares seemed to play no role here (however, more than two mares would be necessary to study potential mare effect). What mattered instead was whether a mare was in oestrus or not. Stallions showed behaviour that indicated higher sexual arousal when exposed to an oestrous mare and/or her faeces than when exposed to the same mares in dioestrus. The mares’ oestrous cycle also affected semen characteristics. When exposed to an oestrous mare, the stallions ejaculated more seminal fluids. Total sperm number and sperm velocity per ejaculate did not seem to increase, but sperm motility in fresh ejaculates was elevated, and sperm suffered less from oxidative stress over the following 48 hours. We conclude that the seminal fluids supported sperm motility and longevity better when the stallions were stimulated by a mare in oestrus than in dioestrus. It remains to be tested whether these effects are only due to the increased amounts of seminal fluids or also due to changes in their compositions.

It remains unclear whether testosterone played a role in inducing the effects of the mares’ oestrous cycle on semen characteristics. While blood plasma testosterone levels showed a marked increase from before to immediately after the ejaculation, we found no significant effect of the mares’ oestrous cycle on testosterone levels, neither in our between-subject not in the within-subject analyses. This suggests either that testosterone plasma levels do not react strongly to the mares’ oestrous cycle during only a short-term exposure and that the semen quality was regulated differently (for example neutrally mediated or dependent by the interaction of various hormones), or that the temporal dynamics of testosterone release requires a higher time resolution in measurements, e.g. one measurement per minute38, in order to reveal testosterone effects.

In fowls (Gallus gallus), roosters allocate larger ejaculates to more attractive hens, and seminal fluids allocated to more attractive hens support increased sperm velocity8. Previous studies on horses that were based on long-term exposure demonstrated that semen characteristics are plastic and that they depend on the social environments the stallions experience. Stallions showed increased sperm number per ejaculate after exposure to other stallions than after exposure to one mare only39, and ejaculates contained more sperm cells after exposure to mares that were predicted to be more attractive than after exposure to mares that were predicted to be less attractive40 (attractiveness being predicted by the sharing of alleles of the major histocompatibility complex40,41). Both conditions tested in Burger et al.39,40 had no or little effects on sperm velocity. These previous experiments were based on long-term exposure (4–8 weeks), covering at least the second half of the 57 days of spermatogenesis42. Our present experimental set-up only allowed for rapid adjustments of ejaculate characteristics. In contrast to the long-term exposure, short-term exposure seems to only affect semen volume and the ability of seminal fluids to support sperm motility and longevity, but it does not seem to affect total sperm counts. This suggests that either long-term exposure to certain social situations enhance sperm production and hence sperm number per ejaculate, or that the present treatment (oestrous versus dioestrous stimulus mare) provokes a different response than the treatments in Burger et al.39,40.

In feral conditions, stallions either live in harems together with several mares (and their offspring) or in bachelor bands together with other stallions. Harem stallions interact continuously with their harem mares and show signs of sexual interest (including mounting attempts) for both oestrous and dioestrous mares, even if dioestrous mares will typically try to avoid copulation24. Induced ovulation as in cats, rabbits, ferrets or camelids43 is not described for horses. However, exposure to stallion was recently found to affect the mares’ cyclicity44. Such potential fitness-enhancing effects may explain why stallions would try to mount dioestrous mares and ejaculate semen, even if of comparatively low quality.

Female pheromones have been found in other mammals to stimulate immediate reactions45. We therefore exposed the stallions to faeces samples of the mares that may reveal their oestrous stage. However, the mares were also present during semen collection, and they expressed the typical oestrous signals. It is therefore unclear what role the faeces samples played in inducing the strong treatment effects we observed here.

In horses, a typical oestrous cycle takes approximately 3 weeks during the reproductive season44. The typical oestrous signals can normally be observed during approximately 5–7 days during each cycle, i.e. up to several days before ovulation. Longevity of ejaculated sperm may therefore be of critical importance, and stallions who mount an oestrous mare may be expected to invest into sperm longevity, i.e. into the respective components of the seminal fluids. Mammalian seminal fluid include antioxidants like superoxide dismutase, catalase, glutathione peroxidase, and several non-enzymatic agents that protect spermatozoa from oxidative damage13. We found that aging sperm still suffered from increased lipid peroxidation over time, potentially contributing to the observed reduction in sperm viability over time. The oxidative stress was mitigated after exposure to an oestrous mare, i.e. seminal fluids provided increased support for sperm that were ejaculated during exposure to an oestrous stimulus mare. However, the mitigating effects of this treatment condition did not significantly affect viability, motility, or velocity of aging sperm. There was only a non-significant tendency that sperm that suffered less from lipid peroxidation also showed increased viability. Even if oxidative stress is a major cause of damage to sperm46, the link between lipid peroxidation and sperm viability is still not sufficiently understood47.

In stud farms, cooled sperm that are subject to oxidative stress are routinely used, and the per-cycle conception is typically more variable and on average clearly lower than in many other life stock48 (D.B. & H.S. personal observations). We found that semen quality can be significantly increased with the use of stimulus mares in oestrus. The enhanced semen quality may then provide two benefits: (i) it may increase success rates of instrumental fertilization, and (ii) it may reduce the mutational load that is inflicted by oxidative stress on sperm49. Therefore, the use of oestrous stimulus mares during semen collection can have beneficial long-term consequences on the genetics of horse breeds. These insights could also be relevant for other mammals and in other contexts, for example in the management of captive populations or in supportive breeding programs50. Conservation programs for some endangered mammals would benefit from improved protocols of assisted reproductive techniques, for example, to minimize the loss of genetic diversity51 or to reduce mutational load52.

We conclude that sperm differ in their probability of fertilizing an ovum not only because of the female’s state (oestrus or dioestrus) but also because of the male’s reaction to the female’s state (increased quantities of seminal fluids and increased protection of sperm from oxidative stress). Our observations support predictions derived from ejaculate economics if the variation in female state that we studied here sufficiently represents variation in female fecundity as modelled by this theory1,9. This condition may only be fulfilled if the chance of fertilizing an ovum is not zero for sperm deposited in dioestrous females. Indeed, semen deposition and ovulation do not need to be synchronized for successful reproduction in many mammals53. Sperm storage is often possible in the isthmus and the oviduct. Sperm then bind to epithelial cells to form a reservoir that seems much under female control, as gene transcription and translation in these oviductal cells can support sperm storage and fertility54. One of the questions that remain to be answered is why, in response to the female’s cycle, males invest differentially into seminal fluids but not into sperm number per ejaculate.

Additional Information

How to cite this article: Jeannerat, E. et al. Quality of seminal fluids varies with type of stimulus at ejaculation. Sci. Rep. 7, 44339; doi: 10.1038/srep44339 (2017).

Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Acknowledgments

We thank G. Cosentino and F. Flahaut of the Laboratory. Dr. Risch, CH-Liebefeld, for the testosterone analyses, Mathias Siuda for semen evaluations, and R. Bruckmaier, V. Gerber, S. Thomas, the vet team of the Swiss Institute of Equine Medicine for discussion and assistance in the field, and two anonymous reviewers for constructive comments. This work was supported by ISMEquine Research.

Footnotes

The authors declare no competing financial interests.

Author Contributions D.B., H.S. and C.W. designed the study, D.B. supervised the experiments, E.J. performed the experiments and analysed the fresh ejaculates, F.J. guided the analyses on aging sperm, and C.W. did the statistical analyses. E.J., D.B., and C.W. wrote the manuscript that was critically revised by all authors.

References

  • Parker G. A. & Pizzari T. Sperm competition and ejaculate economics. Biol. Rev. 85, 897–934, doi: (2010).10.1111/j.1469-185X.2010.00140.x [PubMed] [Cross Ref]
  • Aron S., Lybaert P., Baudoux C., Vandervelden M. & Fournier D. Sperm production characteristics vary with level of sperm competition in Cataglyphis desert ants. Funct. Ecol. 30, 614–624, doi: (2016).10.1111/1365-2435.12533 [Cross Ref]
  • Firman R. C. & Simmons L. W. Experimental evolution of sperm quality via postcompulatory sexual selection in house mice. Evolution 64, 1245–1256, doi: (2010).10.1111/j.1558-5646.2009.00894.x [PubMed] [Cross Ref]
  • Firman R. C. et al. . Evolutionary change in testes tissue composition among experimental populations of house mice. Evolution 69, 848–855, doi: (2015).10.1111/evo.12603 [PubMed] [Cross Ref]
  • Ramm S. A. et al. . Sperm competition risk drives plasticity in seminal fluid composition. BMC Biol. 13, doi: (2015).10.1186/s12915-015-0197-2 [PMC free article] [PubMed] [Cross Ref]
  • Firman R. C., Klemme I. & Simmons L. W. Strategic adjustments in sperm production within and between two island populations of house mice. Evolution 67, 3061–3070, doi: (2013).10.1111/evo.12164 [PubMed] [Cross Ref]
  • Crean A. J. & Marshall D. J. Gamete plasticity in a broadcast spawning marine invertebrate. Proc. Natl. Acad. Sci. USA 105, 13508–13513, doi: (2008).10.1073/pnas.0806590105 [PubMed] [Cross Ref]
  • Cornwallis C. K. & O’Connor E. A. Sperm: seminal fluid interactions and the adjustment of sperm quality in relation to female attractiveness. Proc. R. Soc. B Biol. Sci. 276, 3467–3475, doi: (2009).10.1098/rspb.2009.0807 [PMC free article] [PubMed] [Cross Ref]
  • Kelly C. D. & Jennions M. D. Sexual selection and sperm quantity: meta-analyses of strategic ejaculation. Biol. Rev. 86, 863–884, doi: (2011).10.1111/j.1469-185X.2011.00175.x [PubMed] [Cross Ref]
  • Browne R. K. et al. . Sperm motility of externally fertilizing fish and amphibians. Theriogenology 83, 1–13, doi: (2015).10.1016/j.theriogenology.2014.09.018 [PubMed] [Cross Ref]
  • Kareskoski M. & Katila T. Components of stallion seminal plasma and the effects of seminal plasma on sperm longevity. Anim. Reprod. Sci. 107, 249–256, doi: (2008).10.1016/j.anireprosci.2008.04.013 [PubMed] [Cross Ref]
  • Kareskoski A. M. et al. . Protein composition of seminal plasma in fractionated stallion ejaculates. Reprod. Dom. Anim. 46, e79–e84, doi: (2011).10.1111/j.1439-0531.2010.01641.x [PubMed] [Cross Ref]
  • Perry J. C., Sirot L. & Wigby S. The seminal symphony: how to compose an ejaculate. Trends Ecol. Evol. 28, 414–422, doi: (2013).10.1016/j.tree.2013.03.005 [PMC free article] [PubMed] [Cross Ref]
  • Poiani A. Complexity of seminal fluid: a review. Behav. Ecol. Sociobiol. 60, 289–310, doi: (2006).10.1007/s00265-006-0178-0 [Cross Ref]
  • Dhole S. & Servedio M. R. Sperm competition and the evolution of seminal fluid composition. Evolution 68, 3008–3019, doi: (2014).10.1111/evo.12477 [PubMed] [Cross Ref]
  • Robertson S. A. & Sharkey D. J. Seminal fluid and fertility in women. Fertil. Steril. 106, 511–519, doi: (2016).10.1016/j.fertnstert.2016.07.1101 [PubMed] [Cross Ref]
  • Chapman T. Seminal fluid‐mediated fitness traits in Drosophila. Heredity 87, 511–521, doi: (2001).10.1046/j.1365-2540.2001.00961.x [PubMed] [Cross Ref]
  • Reinhardt K., Naylor R. & Siva-Jothy M. T. Male mating rate is constrained by seminal fluid availability in bedbugs, Cimex lectularius. PLoS One 6, doi: (2011).10.1371/journal.pone.0022082 [PMC free article] [PubMed] [Cross Ref]
  • Gleason E. D., Fuxjager M. J., Oyegbile T. O. & Marler C. A. Testosterone release and social context: When it occurs and why. Front. Neuroendocrinol. 30, 460–469, doi: (2009).10.1016/j.yfrne.2009.04.009 [PubMed] [Cross Ref]
  • Nass S. J., Miller D. J., Winer M. A. & Ax R. L. Male accessory sex glands produce heparin‐binding proteins that bind to cauda epididymal spermatozoa and are testosterone dependent. Mol. Reprod. Dev. 25, 237–246, doi: (1990).10.1002/mrd.1080250305 [PubMed] [Cross Ref]
  • Zalata A., Hafez T., Verdonck L., Vermeulen L. & Comhaire F. Androgens in seminal plasma: markers of the surface epithelium of the male reproductive tract. Int. J. Androl. 18, 271–277 (1995). [PubMed]
  • Ginther O. J. Reproductive biology of the mare: basic and applied aspects 2nd ed. (Equiservices Publishing, 1992).
  • Aurich C. Reproductive cycles of horses. Anim. Reprod. Sci. 124, 220–228, doi: (2011).10.1016/j.anireprosci.2011.02.005 [PubMed] [Cross Ref]
  • McDonnell S. M. Reproductive behavior of stallions and mares: comparison of free-running and domestic in-hand breeding. Anim. Reprod. Sci. 60/61, 211–219 (2000). [PubMed]
  • McDonnell S. Reproductive behavior of the stallion. Vet. Clin. North Am. Equine Pract. 2, 535–555 (1986). [PubMed]
  • Schumacher J. & Riddell M. Collection of stallion semen without a mount. Theriogenology 26, 245–250, doi: (1986).10.1016/0093-691x(86)90029-4 [PubMed] [Cross Ref]
  • Janett F., Stump R., Burger D. & Thun R. Suppression of testicular function and sexual behavior by vaccination against GnRH (EquityTM) in the adult stallion. Anim. Reprod. Sci. 115, 88–102, doi: (2009).10.1016/j.anireprosci.2008.11.011 [PubMed] [Cross Ref]
  • Janett F., Sacher K., Hassig M. & Thun R. Quality of raw and of cold-stored semen in Icelandic stallions. J. Equine Vet. Sci. 32, 590–595, doi: (2012).10.1016/j.jevs.2012.02.004 [Cross Ref]
  • Nagy S., Jansen J., Topper E. K. & Gadella B. M. A triple-stain flow cytometric method to assess plasma- and acrosome-membrane integrity of cryopreserved bovine sperm immediately after thawing in presence of egg-yolk particles. Biol. Reprod. 68, 1828–1835, doi: (2003).10.1095/biolreprod.102.011445 [PubMed] [Cross Ref]
  • Rathi R., Colenbrander B., Bevers M. M. & Gadella B. M. Evaluation of in vitro capacitation of stallion spermatozoa. Biol. Reprod. 65, 462–470, doi: (2001).10.1095/biolreprod65.2.462 [PubMed] [Cross Ref]
  • Neild D. M., Brouwers J. F., Colenbrander B., Aguero A. & Gadella B. M. Lipid peroxide formation in relation to membrane stability of fresh and frozen thawed stallion spermatozoa. Mol. Reprod. Dev. 72, 230–238, doi: (2005).10.1002/mrd.20322 [PubMed] [Cross Ref]
  • Ortega Ferrusola C. et al. . Lipid peroxidation, assessed with BODIPY-C11, increases after cryopreservation of stallion spermatozoa, is stallion-dependent and is related to apoptotic-like changes. Reproduction 138, 55–63, doi: (2009).10.1530/REP-08-0484 [PubMed] [Cross Ref]
  • Rice W. R. & Gaines S. D. Heads I win, tails you lose’: testing directional alternative hypotheses in ecological and evolutionary research. Trends Ecol. Evol. 9, 235–236, doi: (1994).10.1016/0169-5347(94)90258-5 [PubMed] [Cross Ref]
  • Jeffery A. J., Pham M. N., Shackelford T. K. & Fink B. Does human ejaculate quality relate to phenotypic traits? Am. J. Hum. Biol. 28, 318–329, doi: (2016).10.1002/ajhb.22805 [PubMed] [Cross Ref]
  • Tarin J. J., Garcia-Perez M. A., Hamatani T. & Cano A. Infertility etiologies are genetically and clinically linked with other diseases in single meta-diseases. Reprod. Biol. Endocrinol. 13, 1–11, doi: (2015).10.1186/s12958-015-0029-9 [PMC free article] [PubMed] [Cross Ref]
  • Firns S. et al. . The effect of cigarette smoking, alcohol consumption and fruit and vegetable consumption on IVF outcomes: a review and presentation of original data. Reprod. Biol. Endocrinol. 13, doi: (2015).10.1186/s12958-015-0133-x [PMC free article] [PubMed] [Cross Ref]
  • Mautz B. S., Møller A. P. & Jennions M. D. Do male secondary sexual characters signal ejaculate quality? A meta-analysis. Biol. Rev. 88, 669–682, doi: (2013).10.1111/brv.12022 [PubMed] [Cross Ref]
  • Käser R. et al. . High inter- and intra-individual variation of oxytocin secretion in estrous mares exposed to stallions, but no significant link to mate preferences. Theriogenology 86, 2222–2229, doi: (2016).10.1016/j.theriogenology.2016.07.017 [PubMed] [Cross Ref]
  • Burger D., Dolivo G. & Wedekind C. Ejaculate characteristics depend on social environment in the horse (Equus caballus). PLoS One 10, e0143185, doi: (2015).10.1371/journal.pone.0143185 [PMC free article] [PubMed] [Cross Ref]
  • Burger D., Dolivo G., Marti E., Sieme H. & Wedekind C. Female major histocompatibility complex type affects male testosterone levels and sperm number in the horse (Equus caballus). Proc. R. Soc. B Biol. Sci. 282, doi: (2015).10.1098/rspb.2015.0407 [PMC free article] [PubMed] [Cross Ref]
  • Burger D. et al. . MHC-correlated preferences in diestrous female horses (Equus caballus). Theriogenology 89, 318–323 e311, doi: (2017).10.1016/j.theriogenology.2016.09.015 [PubMed] [Cross Ref]
  • Amann R. P. In Equine Reproduction 2nd Edition (eds McKinnon A. O., Squires E. L., Vaala W. E. & Varner D. D.) 881–908 (Wiley-Blackwell, 2011).
  • Bakker J. & Baum M. J. Neuroendocrine regulation of GnRH release in induced ovulators. Front. Neuroendocrinol. 21, 220–262, doi: (2000).10.1006/frne.2000.0198 [PubMed] [Cross Ref]
  • Wespi B., Sieme H., Wedekind C. & Burger D. Exposure to stallion accelerates the onset of mares’ cyclicity. Theriogenology 82, 189–194, doi: (2014).10.1016/j.theriogenology.2014.03.019 [PubMed] [Cross Ref]
  • Richardson H. N. et al. . Female pheromones stimulate release of luteinizing hormone and testosterone without altering GnRH mRNA in adult male Syrian hamsters (Mesocricetus auratus). Gen. Comp. Endocrinol. 138, 211–217, doi: (2004).10.1016/j.ygcen.2004.06.008 [PubMed] [Cross Ref]
  • Aitken R. J., Smith T. B., Jobling M. S., Baker M. A. & De Iuliis G. N. Oxidative stress and male reproductive health. Asian J. Androl. 16, 31–38, doi: (2014).10.4103/1008-682X.122203 [PMC free article] [PubMed] [Cross Ref]
  • Gibb Z., Lambourne S. R. & Aitken R. J. The paradoxical relationship between stallion fertility and oxidative stress. Biol. Reprod. 91, doi: (2014).10.1095/biolreprod.114.118539 [PubMed] [Cross Ref]
  • Morris L. H. & Allen W. R. Reproductive efficiency of intensively managed thoroughbred mares in Newmarket. Equine Vet. J. 34, 51–60, doi: (2002).10.2746/042516402776181222 [PubMed] [Cross Ref]
  • Menezo Y. et al. . Oxidative stress and fertility: incorrect assumptions and ineffective solutions? Zygote 22, 80–90, doi: (2014).10.1017/s0967199412000263 [PubMed] [Cross Ref]
  • Wedekind C. Sexual selection and life-history decisions: implications for supportive breeding and the management of captive populations. Cons. Biol. 16, 1204–1211 (2002).
  • Andrabi S. M. H. & Maxwell W. M. C. A review on reproductive biotechnologies for conservation of endangered mammalian species. Anim. Reprod. Sci. 99, 223–243, doi: (2007).10.1016/j.anireprosci.2006.07.002 [PubMed] [Cross Ref]
  • Cotton S. & Wedekind C. Male mutation bias and possible long-term effects of human activities. Cons. Biol. 24, 1190–1197, doi: (2010).10.1111/j.1523-1739.2010.01524.x [PubMed] [Cross Ref]
  • Orr T. J. & Zuk M. Reproductive delays in mammals: an unexplored avenue for post-copulatory sexual selection. Biol. Rev. 89, 889–912 (2014). [PubMed]
  • Miller D. J. Regulation of sperm function by oviduct fluid and the epithelium: insight into the role of glycans. Reprod. Dom. Anim. 50, 31–39, doi: (2015).10.1111/rda.12570 [PubMed] [Cross Ref]

Articles from Scientific Reports are provided here courtesy of Nature Publishing Group