Open access peer-reviewed chapter

Physiological and Clinical Aspects of the Endocrinology of the Estrous Cycle and Pregnancy in Mares

Written By

Katy Satué and Juan Carlos Gardon

Submitted: September 9th, 2019 Reviewed: November 5th, 2019 Published: June 10th, 2020

DOI: 10.5772/intechopen.90387

Chapter metrics overview

866 Chapter Downloads

View Full Metrics


The use of advanced reproductive endocrinology can generate important economic benefits for equine breeding farms. Pregnancy in the mare involves considerable endocrine changes, which can be explained in part by the development of different structures such as embryonic vesicles, primary and secondary CL, endometrial cups and development of fetoplacental units. Both the pregnant mare and the fetus adapt to this development with unique mechanisms, such as alterations in the maternal endocrine metabolism and hormonal feedback. Since the ability to produce a viable foal is critical for the broodmare, the maintenance of the gestation implies almost a year of physiological effort. Therefore, the joint knowledge of basic reproductive science and current clinical endocrinology allows veterinarians and breeders to be better positioned to achieve their objectives. This chapter reviews normal and abnormal endocrine patterns during the equine estrual cycle, pregnancy. We also consider hormonal evaluation related to placentitis, abortions, recurrent pregnancy loss, and premature deliveries. Also, several aspects associated with endocrinological control of the reproductive cycle, ovulation, parturition, high-risk mare, and hormone supplementation will be developed.


  • estrous
  • clinical endocrinology
  • mare
  • pregnancy

1. Introduction

The gestation in the mare begins with the fertilization of the ovum, then the implantation of the blastocyst in the uterus followed by the development of the placenta and fetus until delivery. Therefore, gestation is a dynamic and coordinated process involving systemic and local changes in the mare that support the supply of nutrients and oxygen to the fetus for growth and development in the uterus [1]. In part, these changes occur through the secretion of hormones in the placenta, which in turn interact with each other and exert extensive effects on maternal tissues during gestation [2]. These endocrine changes in maternal physiology adaptations to gestational status result from modifications in the maternal environment of steroids such as progesterone (P4), estrogens, androgens, and other hormones such as relaxin and prostaglandins (PG). However, an inadequate adaptation of maternal physiology can lead to gestational complications, such as restriction or overgrowth of the fetus and premature delivery [3].

Since an understanding of endocrinology in equine species is useful when considering hormone treatment of cyclic and pregnant mares, this chapter considers a basic review and applications of this information in clinical therapeutic situations. For this reason, this chapter aims to provide an overview of the endocrine changes that occur in the mare in response to gestation and to discuss the key role of hormones in mediating pathological processes.


2. Neuroendocrine control of the estrus cycle in cycling mares

The estrous cycle is defined as the interval of time between two consecutive ovulations. The approximate length varies between 18 and 22 days, considering on average a period of 21 days [4, 5]. The current nomenclature stipulates that the estrous cycle consists of two differentiated stages: estrus or follicular phase and diestrus or luteal phase. These phases are characterized by internal modifications of the sexual organs and glandular system as well as behavioral alterations based on the levels of oestradiol (E2) and P4 [6, 7].

2.1 Follicular phase

Estrus, heat or follicular phase is characterized by the presence of follicles at different stages of development, and the simultaneous increase in the secretion of E2. It has a duration of about 5–7 days, with a variability of 3–9 days related to the season. Thus, estrus is extended in autumn (7–10 days) and is shortened considerably, in late spring and early summer (4–5 days). During this period the mare is sexually receptive to the stallion genital tract and is ready to receive and transport of sperm and finally culminates with ovulation [5, 6, 8].

2.1.1 Follicular dynamics

Ovarian follicular development is a complex dynamic process, characterized by marked proliferation and differentiation of follicular cells, providing an optimal environment for oocyte maturation and preparation for fertilization after ovulation [9]. Among the recruited follicles in each follicular wave, dominance takes place and one follicle of the cohort acquires the ability to continue growing while others undergo atresia. The regulation of each wave and follicular selection involves interactions between specific circulating gonadotropins and intrafollicular factors, ensuring that each follicle is properly stimulated to grow or regress at any stage of development [8]. From an experimental point of view, the occurrence of a wave is defined as follicular growth or simultaneous emergence of a variable number of follicles below 6–13 mm in diameter [10, 11]. In the mare, these follicular waves are classified depending on their ability to develop the dominant follicle (primary waves) or, in contrast, generate only small follicles (smaller waves). Thus, the main waves or greater originate several follicles subordinate and a dominant follicle, while smaller waves, the follicles are not larger than 30 mm in diameter and then regress [12, 13].

During each cycle produces 1 or 2 major follicular waves, differentiated according to time of onset at primary and secondary. The primary major wave occurs near the middle of the diestrus, in which the dominant follicle ovulates at the end or near the end of estrus. The largest wave precedes the previous secondary and emerges during late estrus or early diestrus. There are two anovulatory follicular waves followed by an ovulatory surge during the estrous cycle [14, 15].

Steroidogenesis in the ovaries involves both theca and granulosa cells. The antral follicles acquire receptors for follicle-stimulating (FSH) and luteinizing (LH) hormones in the membranes of the granular cells and theca, respectively. Cholesterol passes through theca cell plasma membrane attached to a lipoprotein, is stored in cytoplasmic vacuoles, and is transported to the outer membrane of the mitochondria. The LH is released in a pulsating form from the anterior pituitary gland and binds to its receptor in the theca cell membrane, mobilizing cholesterol. Inside theca cells, the StAR protein helps transfer cholesterol to the internal mitochondrial membrane, where the cytochrome P450 (CYP) enzyme system divides cholesterol into pregnenalone (P5), and subsequently, P5 becomes to androstenedione (A4). The A4 produced in theca cells is transported through the basal membrane to the granulose cells. There FSH supports the steroidogenic pathway and converts A4 into E2 [16].

Increased concentrations of estrogen stimulate the secretion of LH, which in turn induces greater estrogen synthesis. This progressive increase in estrogen also promotes the onset of LH receptors in granulosa cells, which facilitates the transition from the antral stage to the preovulatory stage, when the oocyte reaches the final stage of maturation. At 6 days after the emergence of major follicular wave deviation occurs. This event relates to the growth rate difference of the preovulatory follicle size (22.5 mm) compared to the subordinate follicles (19 mm) [12, 13, 17]. Deviation is related to inhibin secretion [12] and insulin-like growth factor-1 (IGF-1) [13, 17]. Specifically, inhibin reduces FSH secretion, making it impossible to continue the development of the subordinate follicle. However, the dominant follicle continues to grow at a constant rate of 2.3 mm per day until reaching a size of 40 mm in response to the increased sensitivity to FSH. As has been mentioned, at this stage of development, granulosa cells also develop receptors for LH required for final oocyte maturation and ovulation after the LH surge [18].

As has been demonstrated in different horse breeds such as Quarter Horse, Arabian, Thoroughbred, and Spanish Purebred, the maximum diameter of the ovulatory follicle usually varies between 40 and 45 mm [19], although the range may be higher (30–70 mm) [7, 20]. Moreover, size differences were established concerning the breeding season or the presence of multiple ovulations. Thus, the follicles reach a size 5–8 mm higher in spring than in summer or autumn and are 4–9 mm lower in multiple ovulations compared to the simple [20, 21].

The highest concentrations of estrogen secreted by the granulosa cells of the preovulatory follicle also induce the appearance of typical behavioral manifestations of estrus. Estrogens are also responsible for reproductive changes that ensure the reception, transport of sperm and oocyte fertilization [4, 6]. After the preovulatory LH surge, ovulation occurs spontaneously 24–48 h before the end of the follicular phase. The ovulatory process brings rapid evacuation of the oocyte and follicular fluid after follicular rupture at ovulation fossa. Once completed, E2 concentrations return to basal levels and at the same time completing the oestrus behavior in mares [11, 22, 23, 24].

2.2 Luteal phase

The diestrus or luteal phase begins at the time of ovulation with the formation of CL, which is responsible for the synthesis of P4. Unlike the follicular phase, the insensitivity of the corpus luteum (CL) photoperiod makes the length of this period more constant. Most research estimates an average duration of 14–15 days but can be more durable in mid-summer (16 days) than in spring or autumn (13 days) [5, 6].

2.2.1 Formation of corpus luteum

The disorganization of the follicular wall after ovulation allows blood vessels and fibroblasts invade the follicular cavity. Luteinization involves structural and functional changes in granulosa and theca cells. These are the same cells that initially produced E2 and become into luteal cells that produce P4. P4 remains high from day 5 post-ovulation until the end of the diestrus and exerts specific functions related to the preparation of the endometrium to accept and maintain pregnancy, endometrial gland development and inhibition of myometrial contractility [24].

Have been described two types of CL regarding the presence or absence of central blood clot. In a high percentage of cases (50–70%) in place of ovulation, a core clot develops surrounded by luteal tissue. This type of condition is defined as a corpus hemorrhagic. The cavity begins to fill with blood, fibrin, and transudate for the first 24 h, reaching the maximum size at 3 days. Around day 5 post-ovulation CLs that develop a central cavity usually, have a significantly higher size (32.8 mm) to those without it (26.0 mm). The ratio of the maximum diameter of the CL is 65–80% compared to pre-ovulatory follicle size and has an outer wall thickness of 4–7 mm corresponding to the portion of luteinized tissue. As happens with the size, texture also changes depending on the type of CL. The CL that develops the central cavity is denser than those that lack it, in which the structure is more spongy [25]. Usually, the ratio of non-luteal luteal tissue of the corpus hemorrhagic is minimal during the early diestrus and maximum in halfway of diestrus. These events are associated with the gradual decrease of fluid as a result of the production and organization of connective tissue associated with the clotting mechanism [26, 27]. Notably, the formation of one type or another of CL is a random event. The morphology luteal repeatability is not always observed in subsequent ovulation [26, 27, 28].

Furthermore, continuous P4 levels during diestrus reduce the frequency and intensity of gonadotrophin-releasing factor (GnRH) pulses by a feedback mechanism. However, because the pulses of FSH are higher than those of LH, a new follicular wave is developed during this period. In the absence of pregnancy, the end luteal phase culminates with the lysis of CL induced by the PGF of endometrial origin and decreased concentrations of P4 [5, 6]. Luteal regression involves several structural and functional events characterized by decreased vascularization, an increase of connective tissue, hyalinization, atrophy and fibrosis [29].

2.3 Neuroendocrine control of the estrus cycle

Physiological events that occur during the estrous cycle are regulated by the coordinated interaction of various hormones and releasing factors like GnRH, FSH, LH, E2, P4, and PGF, among others [22]. In this section we will describe a synthesis of the most notable changes and the physiological participation that all these factors have during the estral cycle in the mare.

2.3.1 Gonadotrophin releasing factor

The increased photoperiod during spring and summer causes decreased secretion of melatonin. This signal has a positive effect on the pulses of hypothalamic GnRH, which in turn controls the release of gonadotropins [27]. GnRH pulses produced every 45 min originate predominantly LH secretion whereas those occur every 6 h stimulate the secretion of FSH. The high-frequency pulses of GnRH (2 pulses per hour) during estrus favors an increase in LH and FSH decline, while reducing the frequency to 2 pulses per day, leads an increase of FSH and LH inhibition [30]. These endocrine events, allowing the emergence of follicular waves, E2synthesis, and ovulation during estrus and appearance of the CL with P4 release during diestrus [24].

2.3.2 Follicle stimulating hormone

Follicle-stimulating hormone describes two types of secretion patterns during the estrous cycle in the mare: uni or bimodal. The bimodal pattern occurs frequently during the spring transition period and the ovulatory season. The first peak of FHS appears between the 8th and 14th day of the cycle, the moment in which the largest follicle reached a diameter of 13 mm [18]. This initial increase precedes the beginning of the deviation and is associated with increased synthesis of inhibin by the largest follicle [8, 13, 15, 18, 31] and persists until the preovulatory follicle reaches 22 mm of diameter. The second peak of FSH begins on day 15 of the cycle and it is necessary to complete the development of the preovulatory follicle [19, 31]. Unlike the bimodal pattern, the first peak of FSH would be absent in the unimodal pattern [18]. In the latter pattern, FSH levels remain low during estrus, rise in times around ovulation, maintaining increased during diestrus [31].

FSH is also involved in the development of the LH receptors in the preovulatory follicle [32, 33]. At the start of follicular growth, low levels of estradiol exert negative feedback on the hypothalamic-hypophysis axis (HHA) controlling the tonic or basal release of gonadotropin. This mechanism controls the follicular growth and E2 synthesis continuously preventing ovarian overstimulation. After the period of follicular growth, once the dominant follicle has been selected, the E2 and inhibin levels are significantly increased. This elevation of E2 is responsible for the characteristic changes of the genital tract and signs of heat during estrus. Furthermore, this response exerts positive feedback on the HHA, favoring the emergence of preovulatory LH surge, necessary to produce the ovulation. Additionally, the stimulatory effects of E2 on LH combined to the inhibitory action of inhibin on FSH create the ideal microenvironment for the final maturation of the oocyte, inhibiting the development of immature follicles [4].

2.3.3 Luteinizing hormone

LH levels gradually increase from day 5 to the day of ovulation, when it reaches the maximum concentration [7, 34]. The pre-ovulatory LH surge occurs as a result of the positive feedback mechanism exerted in the adenohypophysis by E2 concentrations secreted by the granulosa cells of the preovulatory follicle. However, the peak of E2 is reached 2 days before the LH surge. During diestrus, LH is released in a pulsatile manner, with a frequency of 1.4 pulses per 24 h and for a period of 20–40 min at the central level, or 2–4 h per pulse at the peripheral level [34]. Therefore, P4 secretion is maintained by basal levels of LH. The decline of LH at the end of diestrus is a result of the combined effect of decreased estrogen positive feedback, and the resurgence of negative feedback induced by P4 on the HHA. This gonadotropin not only participates in the development and maturation of the primary follicles but also in the development and maintenance of CL during the luteal phase [8, 13, 22].

2.3.4 Estradiol-17β

The ability of estrogen synthesis is dependent on the effect of FSH on granulosa cells. In the absence of P4, estrogens begin to be actively secreted by the preovulatory follicle 5–7 days before ovulation. This event coincides with the time of departure and reaches the peak 2 days before ovulation [5, 22], and will be responsible for the preovulatory release of LH. After ovulation, E2 levels begin to decrease, reaching basal levels at day 5 post-ovulation [13, 19].

Although estrogen levels are directly related to the degree of ovarian activity, sexual receptivity and reproductive tract changes [4, 6, 13, 31, 35] there is no evidence of a direct relationship between the intensity of endometrial edema and E2 concentration. This situation is much clearer on P4. Swelling occurs when P4 levels are <1 ng/ml, so this hormone could be responsible in principle on the intensity of edema, among other behavioral and morphological changes of the cervix and uterus [35]. However, at the time of ovulation inverse correlations are established between E2 and FSH levels associated with the negative feedback effect of inhibin, as previously referred [31].

2.3.5 Progesterone

The steroidogenic activity of P4 depends on the action of LH on theca cells. As noted above, levels of P4 are <1 ng/ml during estrus [19, 36]. After ovulation, it increases progressively and significantly to the 5th or 6th day, with values similar to those of pregnant mares during the first 14 days of gestation. At this time the CL is fully functional and P4 levels remain high until day 9 [35, 37], consistent with the maximum diameter reached by the CL [7, 20, 35, 37]. However, peripheral concentrations of P4 are highly variable between mares. This variability is associated with secretory capacity CL and hormonal catabolic rate. Perhaps this fact may explain the differences in P4 levels between different breeds during the first 5 days of the luteal period, despite the similarity in length of estrous cycles. Among other factors related to variations in levels of P4 highlights the number of ovulations. In fact, double ovulations induce higher concentrations of P4 compared to simple ones [35].

P4 inhibits the secretion and pulsatile release of GnRH and LH but does not modify the pattern of FSH [7, 13, 15]. This event, unlike what happens in other species, enabling a new wave of follicular growth and in some cases the presence of ovulation during diestrus related to high levels of this hormone [18, 22, 38]. After lysis of the CL at the end of diestrus, P4 is drastically reduced to levels <1 ng/ml, a fact which promotes the mare returns to estrus [19, 36].

2.3.6 Prostaglandin F

In the absence of pregnancy, the average life span of the CL is controlled by the release of endometrial PGF source, establishing a bimodal pattern of discharge around day 13–16 of diestrus. While the first 4-h peak precedes the decline of P4, the second occurs during and after luteolysis. Luteolysis involves decreased blood supply, leukocyte infiltration, cell disruption and loss of lutein steroidogenic capacity by apoptotic or non-apoptotic mechanisms intended to disintegrate the CL and therefore secretion P4 [39, 40].


3. Recent advances in hormonal control of estrous cycle

In mares, the natural breeding season extends from spring to early autumn. Until now, various methods have been used to advance the onset of the breeding season or to synchronize the estrus during the reproductive season. Ovulation induction protocols have also been developed for use in artificial insemination or embryo transfer programs [41, 42].

3.1 Gonadotropin releasing hormone

Seasonal reproductive inactivity in mares is due to reduced synthesis and storage in the hypothalamus of GnRH and decreased amounts of FSH and LH in the anterior pituitary gland [27]. Taking this physiological basis into account, it would be expected that the administration of gonadotropins to anestrous mares will restart reproductive capacity.

The administration of a single dose of GnRH to mares causes an increase in the circulating concentrations of FSH and LH [43]. However, constant infusions result in a continuous release of both hormones [44]. An experience conducted in the late 1980s reported that 50% of mares treated during the seasonal anestrous had fertile estrous after infusion of GnRH for 28 days (100 ng/kg; SC). However, this same experiment showed that mares with transitional anestrous were more likely to respond to GnRH than mares with deep anestrous [45].

In another study, daily but not continuous administration of GnRH to induce ovulation in anestrous mares only induced the development of preovulatory follicles [46]. Also, another report [47] showed that the administration of 0.5 mg GnRH three times daily for 7 or 7.5 days induced normal follicular maturation and normal luteinization in anestrous mares. From these studies, it has been demonstrated that the administration of GnRH in diverse protocols is not profitable and requires a lot of manpower. It also results in variable response to treatment among mares, especially deep anestrous mares.

3.2 GnRH agonists

GnRH is known to be responsible for the secretion of FSH and LH, but studies performed to evaluate the efficacy of GnRH-agonists are conflicting. GnRH agonists were used as injections or slow-releasing implants to induce estrus and ovulation in anestrous and transitional mares. The GnRH agonists available for mares include deslorelin, buserelin, and historelin [48].

According to Allen et al. [49] two injections of GnRH agonists each day or continuous administration of GnRH agonists were able to induce follicular development and ovulation in acyclic mares. In the same way, Bergfelt and Ginther [26], demonstrate the same result where mares where about 60% of treated mares with GnRH-agonist ovulated within a 21-day long treatment.

In a study conducted in transition mares for 28 days, Harrison et al. [50] administered buserelin twice daily (40 μg, IM, q 12 h) for 28 days, or as SC implants releasing 100 μg/day. 45% of the mares ovulated between the 10th and 25th day after the start of treatment, in response to the two daily injections. However, 60% of the mares ovulated between 4 and 30 days after implant treatment. The same results were observed when the GnRH agonist was combined with E2 [51].

Deslorelin has also been used to induce cycle and ovulation in mares. Slow liberation subcutaneous deslorelin implants are effective in increasing LH and accelerating ovulation in mares [52, 53].

It is important to indicate that the response is in correlation with the follicular size at the beginning of the treatment and the depth of anestrus. This means that due to the insensitivity of GnRH, mares that are already in the transition period are more likely to respond to the treatment compared to those who are in deep anestrus [54]. Another negative aspect of GnRH treatment in anestrous mares is the risk of early pregnancy losses due to inadequate luteal function [26].

3.3 Progesterone and progestins

The administration of P4 suppresses the release of LH from the anterior pituitary gland. Once P4 supplementation ceases, the so-called “rebound effect” induces follicular maturation and ovulation. Its use in equine reproduction is a common practice and the available protocols include progestogens administered orally or parenterally. However, its use in mares with seasonal anestrous is questionable.

Different studies indicate that mares in deep anestrous or early transition do not anticipate the first ovulation of the year with P4 treatments [30, 55]. However, it has been shown that, if treatment is carried out at the end of the transition period and the mares have at least one follicle of more than 20 mm in diameter in the ovaries, they show regular post-treatment cycles [56].

Intravaginal devices containing P4 (CIDR, PRID, and intravaginal sponges) have been used in mares. Indeed, Hanlon and Firth [57] examined the effect of intravaginal devices placed during 10 days in transitional Thoroughbred mares. The results of the experiment showed that the use of P4 has a positive effect in bringing forward the first estral cycle of the breeding season. Compared to control mares, in the first 21 days of the season, 95.2% treated mares were served and conceived sooner after the start of the breeding season.

Regumate is the most commonly used orally administered progestogen. Its active ingredient is allyl trenbolone, also called Altrenogest. Allen et al. [55] evaluated the effect of oral P4 treatment in mares with seasonal anestrous. Within 8 days, 88% of the treated mares showed estrous behavior and within 18 days of treatment interruption, 84% had ovulated. Based on these figures, the treatment gave a positive result in the acceleration of cyclicity in mares, but its response depends on the depth of the anestrus.

3.4 Recombinant equine FSH (reFSH) and LH (reLH)

The use of recombinant equine FSH (reFSH) has been reported to induce follicular growth in cyclic mares [58, 59]. A study reviewed in 2013 however determined the efficacy of it in deep anestrous mares to be very successful with ovulation rate of 76.7% in response to FSH treatment followed by human chorionic gonadotropin (hCG) administration [60].

Mares in deep anestrous treated with reFSH alone or reFSH and reLH in combination under natural photoperiod showed a significant increase in follicular development within 6 days on average and all of them ovulated within 10 days. In comparison, the control group needed a significantly longer time for follicular growth and only 30% of the control mares had ovulated at the end of the 14 days used for the experiment [61].

3.5 Dopamine antagonists and prolactin

Studies in sheep found that dopamine antagonists are effective in increasing LH secretion during estrus by inhibiting the release of dopamine in the brain [62]. In mares, the increased release of dopamine during winter anestrous has been confirmed in studies measuring a higher concentration of dopamine in the cerebrospinal fluid during deep anestrous. It has also been shown that inhibition of dopamine D2 receptors may accelerate the onset of the ovulatory season in mares. Sulpiride, domperidone, and perphenazine have been studied [63].

Mari et al. [64] compared the efficacy of sulpiride and domperidone, two long-acting dopamine antagonists, to induce ovarian activity in mares with deep anestrous. The results showed that sulpiride administration was effective in accelerating the transition period and first ovulation in mares with deep anestrous.

On the other hand, as daylight increases, the concentration of prolactin (PRL) also increases. Dopamine is an inhibitor of PRL release, and it has been suggested that the administration of this hormone may help stimulate cycling in mares in anestrus [65]. Various studies have confirmed that the administration of recombinant prolactin from different animal species (equine, porcine and ovine) has a stimulating effect on mares in anestrus. Thompson et al. [66] examined the effect of subcutaneous administration of recombinant porcine prolactin (rpPRL) pony mares for 45 days. About 17 days after the start of treatment, a high percentage of treated mares showed signs of heat and ovulation accelerated by more than 1 month. However, another study examined the effect of a single dose of recombinant ovine prolactin (ovPRL). As a result, significant stimulation of follicular development was observed, but only one mare ovulated [67].

3.6 Induction of ovulation in mares

A reliable ovulation-inducing drug is one that can trigger ovulation within a certain “fixed” period of time. This pharmacological action can provide enormous advantages in anticipating the right time for artificial insemination. Several pharmacological agents such as GnRH and GnRH agonist, hCG, recombinant equine LH, and equine pituitary extracts, prostaglandins and kisspeptin have been used to determine their efficacy in ovulation induction [68].

3.6.1 GnRH

The frequency of GnRH pulses is the main regulator of LH secretion by the adenohypophysis [69]. Because of this stimulation, they can be used as an ovulatory agent and therefore can be used to induce ovulation in mares. On the other hand, due to its natural origin, it does not cause an immune response after being administered in several sessions. There is also little risk of contamination as GnRH is a synthetic product. In the 1990s, several experiments were conducted to evaluate the efficacy of GnRH in ovulation induction in cyclic mares [70, 71]. In one of them, the effect of a single administration of 2 mg of synthetic GnRH was tested but did not affect ovulation induction. However, daily injections of the same compound from day 2 of heat to ovulation resulted in a shortening of the duration of heat and the time for ovulation [72]. Likewise, Duchamp et al. [73] conducted a study to try to identify a more suitable ovulatory agent. To do that, they compared the effect of an intramuscular injection of 2.500 i.u. hCG and 2 mg GnRH (not synthetic). The use of hCG, injected when the follicle reached 35 mm in diameter, induced ovulation in 24 or 48 h. However, GnRH was not effective in shortening ovulation time compared to the control group.

On the other hand, the pulsatile infusion of endogenous GnRH was effective in advancing ovulation time in cyclic mares [70]. Treatments with low doses of endogenous GnRH (2.5 μg) continuous infusion for 14 days demonstrated increased LH and ovulation in all treated mares compared to controls [74].

3.6.2 GnRH-agonist Deslorelin (ovuplant and other products)

Deslorelin is a potent GnRH agonist and is marketed as a controlled-release subcutaneous implant under the trade name Ovuplant™. In the past, several authors have investigated the efficacy of Deslorelin in inducing ovulation in mares [29, 75, 76].

It has been shown that between 84 and 93% of mares ovulate after 2 or 3 days of treatment, respectively [77]. However, adverse effects have been reported for this drug. Mares treated with Ovuplant™ showed a prolonged interovulatory interval and estrual cycles of 3–7 days longer than controls [78]. In this sense, it was suggested that the GnRH agonist may cause a decrease in the regulation of the pituitary gonadotropic cells [79]. Besides, additional studies reported suppression of follicular growth and decreased FSH levels in mares treated with Ovuplant™ [80]. A study conducted by McCue et al. [81] showed that the extraction of Ovuplant™ after 48 h prevented a prolonged interovulatory interval. These authors also observed an alteration in ovulation rates. However, Ovupant™ is currently not commercially available.

A short-term release product of deslorelin was developed in a biocompatible liquid vehicle called BioRelease™ [82]. This product releases deslorelin for approximately 6–36 h. An increase in the number of ovulations within 48 h has been demonstrated (75% vs. 7% for controls). There was also no effect of fertility and the number of coverages per conception decreased in treated mares (1.6 vs. 2.9).

Subsequently, a greater number of injectable deslorelin products have been developed. Many of them are suspensions in saline or sterile water and do not contain any slow-release mechanism. McCue et al. [83] compared several deslorelin formulations and reported that all of the formulations tested in their study resulted in a shortening of the follicular phase, acceleration of ovulation and a similar response to human chorionic gonadotropin (hCG). It is important to note that these studies were conducted in the middle of the breeding season. Buserelin

Different works have also tested Buserelin for its effect of inducing ovulation in mares [84]. Treatment with 40 μg de buserelin (4 doses/12 h) caused ovulation without altering fertility in mares [84, 85]. Also, the effect of treatments with 20 μg or 13.3 μg of buserelin (4 doses/12 h; or 3 doses/6 h respectively) was comparable with treatment with 2.500 IU of hCG (iv).

However, some problems with Buserelin to induce ovulation were also reported [86]. Mares treated with 40 μg iv. of Buserelin (2 times daily), 2.500 IU of hCG (single dose iv) and 2 ml of water distilled as placebo (iv) were compared. The highest ovulation rate was found in hCG treatments where 88% of the mares ovulated between 36 and 48 h. However, Buserelin treatment caused only 22.7% ovulation within 48 h.

Buserelin has also been given during early diestrus to pregnant mares as a means of improving pregnancy rates [87, 88]. These studies used doses of 20–40 mg of Buserelin between days 8 and 12. The results showed that pregnancy rates after ovulation increased by approximately 10%. The exact mechanism of how GnRH increases pregnancy rates is unclear since P4 does not appear to be increased. Human chorionic gonadotropin

hCG is a glycoprotein hormone and has a biological function like LH. It is composed of two subunits (α-subunit and β-subunit). The biological activity of hCG is determined by β-subunit, which is composed of 145 amino acids [89]. Several experiments have been conducted to test the efficacy of hCG in ovulation induction [73, 90, 91]. The results of these studies showed that administration of 1.500–3.300 IU of hCG to mares with a follicle in the ovary 35 mm in diameter, or after estrus day 2, induced ovulation within 48 h. The administration of hCG to mares with a follicle in the ovary 35 mm in diameter, or after estrus day 2, induced ovulation within 48 h. The administration of hCG to mares with a follicle in the ovary 35 mm in diameter, or after estrus day 2, induced ovulation within 48 h. However, the adverse effect of consecutive administration of hCG has been reported. The results demonstrate a null effect from the second administration of hCG.

On the other hand, significant levels of antibodies to hCG were also observed after repeated injections [91, 92]. However, there is much conflicting evidence as to whether antibody formation affects the efficacy of hCG [93]. Equine recombinant LH

The recombinant equine LH (reLH) was successfully developed and tested for both in vitro and in vivo efficacy [94, 95]. To test the efficacy of reLH in ovulation induction, a study was performed in mares with 35 mm follicles that were treated with 0.3, 0.6, 0.75, 0.9 mg reLH, 2.500 IU hCG and the number of ovulations within 48 h of injection was monitored. With a total of 84 mares of various breeds 28.6, 50, 90, and 80% ovulated within 48 h in response to 0.3, 0.6, 0.75, and 0.9 mg reLH, respectively. Changes in hormonal profiles (LH, FSH, P4, E2) in response to 5, 0.65, or 10 mg reLH were similar to those of mares of the control group, except for the early increase in LH after reLH injection. The result of this study indicates that reLH is a drug that induces ovulation in mares with a follicle size of 35 mm in 48 h. It is important to point out that as a synthetic product it offers good potential by having, for example, a low production cost. Equine pituitary extracts

The raw extract of equine gonadotropin (CEG) from the pituitary, contains FSH and LH. These extracts have been tested to determine if they can be used as agents to control the estrual cycles of mares. Also, due to their LH content, the effect of CEG for ovulation induction has been tested. Duchamp et al. [73] showed that 80% of ponies and 57% of mares ovulated 2 days after the administration of 50 mg and 25 mg of CEG, respectively. However, there is one major obstacle to these results; the FSH and LH relationship in cEG is not always consistent. Another important factor to keep in mind is that CEG may be contaminated with other pituitary hormones. Also, the potential transmission of certain associated diseases between animals or between animals and humans [96, 97, 98]. Prostaglandins

Savage and Liptrap [99], reported on the use of PGF was able to induce ovulation in mares. By administering 250 μg PGF synthetic (Fenprostalene) 60 h after the onset of estrus, the interval between treatment and ovulation and the duration of estrus were significantly reduced.

Despite these good results, no other PGF could be found that could give similar results [100]. It is therefore believed that the prolonged action of Fenprostalene was responsible for these results. Another PGF (Luprostiol), has also been shown to induce a release of LH from the anterior pituitary gland [101]. Kisspeptin

Kisspeptin is a neuropeptide that induces the secretion of gonadotropins through the stimulation of GnRH secretion and has also been described as having a role in triggering the onset of puberty [102, 103]. A study in pony mares demonstrated the anticipated ovulation when treated with 10 mg of kisspeptin. Another report identified that the administration of 500 μg and 1.0 mg of kisspeptin induces indistinguishable LH and FSH responses to 25 μg GnRH. However, a single injection of 1.0 mg of kisspeptin (iv) was insufficient to induce ovulation in the mare in heat [104].


4. Hormonal regulation of pregnancy in normal mares

4.1 Progesterone

“Maternal recognition of gestation-MGR” it is essential to establish a complete and uninterrupted interaction between the uterus and the conceptus to prevent the regression of primary CL as a result of the blocking of luteolysis. The mobility of the conceptus within the uterine lumen between days 11 and 15 (or “first luteal response of pregnancy”); [27] seem to compensate for the reduced contact surface due to the relatively small size of the equine trophoblast, demonstrating that restriction of movement only partially leads to early embryo loss [105]. The PGs synthesized and secreted by the concept itself stimulate myometrial contractions that promote their migration through the uterus, avoiding premature regression of CL. Additionally, the longitudinal direction of the uterine folds, as well as the spherical shape of the embryo due to the persistence of the glycoprotein capsule, contribute to facilitating this movement [106, 107]. During the mobility phase and its subsequent fixation uterine high amounts of estrogen, mainly oestrone sulfate (E1S) by the equine conceptus are synthesized, related to the development of the embryonic and endometrial vasculature and local effects on myometrial activity, uterine mobility and endometrial gland secretion [108, 109].

Embryo implantation begins around day 36 post-ovulation and involves the development of the chorionic band from the trophoblast, whose cells invade the maternal endometrium giving rise to endometrial cups [110]. Ginther [28] reported that the embryonic cup cells produce a hormone called equine chorionic gonadotropin (eCG), formerly known as pregnant mare’s serum gonadotropin. This hormone is first detectable systemically between days 35 and 40 of pregnancy. The cups are mature and robustly secreting eCG at approximately days 50–60, but they will subsequently undergo sloughing by days 100–150 in most mares This resurgence phase of P4 secretion by the primary CL is termed the “secondary luteal phase or output 2,” whereas the production by supplementary CL is termed the “third luteal phase” or “output 3”. These accessory CLs formed, respectively, causing an increase in P4 secretion around the 75th day of gestation [27, 28, 111]. Thus, during this period, two secretion peaks of P4 are described, which gradually decreasing to undetectable levels at the 200 days of gestation [112, 113].

Ovarian P4 is necessary for the early maintenance of gestation in the mare until 150 days of pregnancy. After the regression of CLs, the placenta is then the organ in charge of maintaining gestation [114]. Several studies describe maximum levels of P4 during the second and third months of gestation, followed by a significant decrease to minimum values (<1 ng/ml) from mid-gestation to term [115]. Additionally, the presence of eCG causes a change in luteal steroidogenesis. In this case, CL changes from synthesizing only P4 to secreting also estrogens and androgens, increasing plasma levels rapidly and tripling the basal values [116]. However, it is not until approximately day 35 that systemic estrogen rises. The source of this estrogen is the ovary, more specifically, the CL and possibly follicles. The stimulation of the ovaries by eCG is responsible for the timing of this increase in estrogen. It appears that estrogen is not actually necessary for pregnancy maintenance, because ovariectomized mares administered only exogenous progestins will maintain pregnancy without the administration of estrogens [28]. The origin of both steroids is found in the primary CL, since their increase takes place before the formation of the secondary CLs and is absent in mares without functional CL. Although the mechanism by which gonadotropin exerts this activity is unknown, an increase in the expression of the enzyme 17α-hydroxylase in charge of the conversion of P5 into dehydroepiandrosterone (DHEA) and P4 into A4 has been described. Both events coincide with the secretion of eCG, they seem to be limited to the first period since they are not detected towards the middle of gestation [116]. The increase in P4 responds primarily to the growth of primary CL and the development of secondary and accessory CLs [4, 117].

During the period of endometrial cups activity, secretion peaks are described for testosterone (T) and A4 [118, 119], whose activity may be decisive in uterine processes related to cell transformation associated with decidualization [120]. In addition, estrogen production depends on the increased synthesis and availability of androgens that are subsequently metabolized by the enzyme aromatase, present in luteal tissue even before eCG secretion. Thus, total estrogen levels are like right-handed during the first 35 days of gestation and increase around day 40 due to follicular development before the formation of CL [121]. Additionally, primary gestational CL produces E1S in response to eCG stimulation [113, 115, 118].

The regression of the endometrial cups to 100–120 days of gestation causes the cessation of eCG secretion and luteal development, observing a progressive decrease in plasma levels of P4 to reach basal values around 200 days of gestation [115]. Currently, all the luteal structures present in the ovary have completely involuted [27]. From this moment onwards, various metabolites derived from P4 (progestins) increase in the systemic circulation, that exceed 500 ng/ml during the last weeks of gestation, which subsequently fall in the 24–48 h prior to birth [122].

4.2 Progestagens

Progestins can be subclassified as pregnenes and 5α-pregnenes. The pregnenes includes P5, P4 and 5-pregnene-3β,20β-diol (P5ββ), while 5α-pregnenes includes 5α-pregnane-3,20-dione (5αDHP), 3β-hydroxy-5α-pregnan-3-one (3β5P), 20α-hydroxy-5α-pregnan-3-one (20α5P), 5α-pregnane-3β,20β-diol (ββ-diol) and 5α-pregnane-3β,20α-diol (βα-diol). Of them, the most important ones in maternal plasma during this period are the 5αDHP and its derivatives, 20α5P, and βα-diol. The origin of all of them is found in P5, synthesized mainly in the fetal adrenal gland, with a production rate exceeding 10 μmol/min. In the placenta, P5 is converted to P4 and this is transformed into 5αDHP in the endometrium [123]. The pattern of secretion of 5αDHP at beginning of gestation runs parallel to that of P4, while around 90 days the onset of P4 decline gives way to fetoplacental synthesis of the different progestogens whose concentrations continue to increase during the second half of gestation. Thus, 20α5P, which is initially at 5 ng/ml, reaches 69 ng/ml at 200 days of gestation and 300 ng/ml at term. In addition, the concentrations of βα-diol increase to 484 ng/ml [112], while 3β5P, P5ββ and ββ-diol reach values of 100, 10 and 100 ng/ml, respectively, towards the end of gestation [124].

The 5αDHP is found primarily at the uterine level during midgestation, but as labor approaches, its distribution changes and is predominantly in fetal circulation. This metabolite is an immediate precursor of allopregnanolone, a potent gamma-aminobutyric acid (GABA) receptor agonist with activity on myometrial relaxation in other species [125, 126, 127]. Serum allopregnanolone increases similarly to its precursor, reaching maximum values at the middle of gestation and a term [112]. However, both P4 and 5αDHP prevent weakly myometrial contractions induced by oxytocin in vitro, suggesting the intervention of the other hormones in the maintenance of uterine quiescence [128]. On the other hand, an umbilical increase of P4 after 300 days of gestation related to a greater expression in the trophoblast of the enzyme necessary for the conversion of P5 into P4 has been described [129].

Simultaneously with the production of progestagens, the feto-placental unit (FPU) synthesizes phenolic estrogens, E1S and E2 17β and 17α, through the aromatization of dihydroandrosterone (DHA), DHEA and its precursors (3β-hydroxyl C-19). The estrogens β unsaturated, equilin and echinelin, specific to the equine species, derive from farnesyl pyrophosphate, through a noncholesterol-dependent pathway. In general, the pattern of estrogen secretion during gestation is characterized by the first peak of secretion around day 40 in relation to follicular development before the formation of secondary and accessory CLs and a subsequent increase from day 80, reaching maximum levels around 210 days of gestation [130, 131, 132]. Thus, the initial plasma concentrations of E1S, corresponding to ovarian synthesis and are affected by ovariectomy. On the contrary, the subsequent peak of liberation comes only from fetoplacental synthesis, descending drastically after fetal death [108, 113, 115, 133].

This increase in estrogens temporarily coincides with the hypertrophy of fetal gonads, which together with local expression of the enzyme 17α-hydroxylase, lead to elevated umbilical levels of P5, T and DHEA [134]. At the same time, maternal plasma concentrations of T and DHEA increase after 100 days of gestation, reaching maximum values at 6 months [116, 135] to promote greater perfusion in the fetal compartment and the uterine tonicity [27, 136]. Legacki et al. [112] describe DHEA values that increase since the first 2 months of gestation to at 6–8 months, decreasing afterward.

The mitochondrial cytochrome P450 side-chain cleavage enzyme (P450scc), necessary for the conversion of cholesterol into P5 is present in the glomerulosa and reticularis zone of the fetal adrenals from 150 days of gestation. However, its expression increases noticeably at the end of gestation, is also found in the fasciculata zone, in the placenta, and the utero-placental tissues. At the same time, fetal plasma levels of P5 and its uteroplacental diffusion are doubled and tripled between 200 and 300 days of gestation and that subsequently descend in the days prior to birth [132, 137]. One of the main metabolites of P4, the 5α-DHP, returns to umbilical circulation after synthesis in the endometrium, excreting only 30% of its production to the maternal circulation. Thus, it has been suggested that it could play a relevant role within fetoplacental tissues [137].

4.3 Estrogens

Estrogen production can likewise be determined in serum obtained from the mare and used as an indicator of feto-placental health [136]. Although total estrogen levels decrease in term gestation, E2 increases dramatically hours before parturition with accentuated myoelectric activity at the uterine level, suggesting the involvement of E2 in myometrial activation [132, 138]. In fact, estrogens promote PGs synthesis and increase endometrial sensitivity to oxytocin, stimulating myometrial contractile activity during delivery [137].

4.4 Cortisol

A few days before parturition, fetal adrenals change from mainly synthesizing P5 to producing cortisol in response to the stimulation of adrenocorticotropic hormone (ACTH). The increase of fetal cortisol is related to preparing the fetus for extra-uterine life by stimulating different processes necessary for the maturation of organs such as the liver, thyroid gland, lungs, digestive system, bone marrow and cardiovascular system [137]. In addition, cortisol activates the enzymes responsible for the synthesis of PGs which, without the presence of progestogens, increase continuously stimulating the onset of myometrial contractions. In addition, E2 favors the uterine response to PGs and may also promote their synthesis [139].

4.5 Prostaglandins

PGF play an important role during delivery by promoting myometrial contractibility, along with oxytocin, and cervical ripening and relaxation (PGE2). Utero-placental tissues are capable of synthesizing PGs and can be found in maternal plasma, fetal plasma and allantoic fluid [140]. However, its bioactivity is controlled by the enzyme 15-hydroxyprostaglandin dehydrogenase (PGDH), which converts the PGs into inactive metabolites, present in the maternal endometrium since approximately 150 days of pregnancy. Since the labile nature of PGs makes it difficult to measure one of these metabolites, 13,14-dihydro-15-keto-prostaglandin F-2α (PGFM) remained at low levels until day 200, then increased to peak pregnancy levels by day 300 and remained at this value until parturition. PGFM uses one of its metabolites as an indicator of its circulating levels, with a term increasingly being described, although it is during the second labor stage when its value increases up to 50 times [141].

4.6 Relaxin

Relaxin is produced by the trophoblastic cells of the placenta and its activity is related to myometrial [137] as well as of the cervix and pelvic ligaments relaxation [142]. Maternal plasma levels increase at the end of gestation and during the second labor stage. After the expulsion of the placenta, it returns to basal values below the detection limit at 36 h, remaining elevated in cases of placental retention [143].


5. High-risk mares and hormone supplementation

5.1 Progesterone

P4 concentrations above 4.0 ng/ml are considered adequate to support early pregnancy. However, when levels are <2.0 ng/ml, P4 supplementation is considered [137]. Several types of P4 products have been used to maintain pregnancies in mares. After oral administration altrenogest is readily absorbed, reaching peak levels after 3–6 h [144]. Altrenogest acts by binding to the P4 receptors but has little effect on endogenous plasma total progestagen concentrations. Specifically, altrenogest is not metabolized to 5α-pregnanes in the horse [128]. For this reason, the only scientific evidence that altrenogest prevents loss pregnancy in mares is during the first trimester, when it prevented abortion induced by repeated administration of PGF (cloprostenol) [145]. P4 may exert its effects by interfering with PG production stimulated by proinflammatory cytokines. Daels et al. [146] demonstrated that the rise in endogenous PGF concentrations was inhibited by altrenogest treatment. Indeed, when early pregnant mares (21–35 days post-ovulation) were exposed to Salmonella typhimurium endotoxin all mares supplemented with altrenogest until day 70 remained pregnant, whereas 6 out of 7 mares aborted when altrenogest therapy was discontinued on day 50 [147].

Mares with suspected luteal insufficiency can be supplemented with altrenogest (0.044 mg/kg per os once or twice daily) or P4 (150 mg/day IM) starting on day 3 after ovulation and continuing until 100–120 days of pregnancy. Long-acting injectable formulations of P4 and altrenogest are available in some countries [148]. Administration of the GnRH analog, buserelin (40 μg), 10 or 11 days after ovulation has been reported to improve luteal function and reduce early pregnancy loss [149]. Panzani et al. [150] showed that the use of altrenogest improved recipient pregnancy rates compared to untreated controls. A recent clinical study showed a positive effect of altrenogest supplementation on embryonic growth rates between 35 and 45 days after ovulation in Warmblood mares older than 8 years [151]. P4 may need to be supplemented generally in early pregnant mares showing estrus signs, with a history of repeated pregnancy loss in case of endotoxemia and of stressful events. In mares under P4 supplementation continuation of pregnancy has to be monitored regularly, since many will lose their pregnancy despite supplementation of P4 and this will prevent those mares return to estrus [152].

The latter sentence has been checked. It has been reported that the administration of a single dose of 20–40 μg of buserelin between day 9 and day 10 after ovulation increases the number of multiple ovulations and gestation up to 5–10% [153]. Buserelin does not increase circulating P4 levels or preventing the luteolysis, acting independently of CL in the mare [154]. These effects preventing pregnancy loss that operating between day 9 to day 10 and day 13 to day 14 of pregnancy.

In a recent study Köhne et al. [155] reported that hCG administration for induction of ovulation in mares increased progestin concentration in plasma of early pregnancy as well as the embryo size at the time of the start of placentation. Periovulatory treatment of mares with hCG may thus be a valuable tool to enhance conceptus growth during early pregnancy by stimulation of endogenous P4 secretion. However, Biermann et al. [156] report that hCG-treatment of mares on day 5 or day 11 post-ovulation influenced peripheral P4 concentrations due to secondary luteal tissue but did not alter ovarian and uterine blood flow or increase pregnancy rates.

5.2 Progestagens

Several pathological conditions as placentitis, placental separation or fetus as, alteration in umbilical blood flow attributable to a cord pathologic condition stimulates inflammatory and immune responses leading disrupt the endocrine capacity of the FPU and alterations in endocrine profile in plasma maternal attributed to disturbances to the normal synthetic pathway for these pregnanes [126, 157].

Fetal death or imminent fetal expulsión due to uterine torsion, colic, maternal stress, or acute cases of experimentally induced placentitis when the mares abort rapidly (within 7 days of infection) are related with the rapidly declining of P5 and P4 (less than the 95%), consistent with failure of the fetus and feto-placental tissues to produce and metabolize progestagens [158, 159].

In mares with chronic placentitis, placental edema, and placentas with poorly developed or sparse microvilli [159, 160] unusually high concentrations of all the progestagens. This pattern indicates that the fetus and the uteroplacental tissues are metabolically active despite the presence of bacteria or their products. In addition, Shikichi et al. [157] demonstrated that mares with a high concentration of progestins and low concentration of estrogens after day 241 of pregnancy were likely to deliver aborted/dead foals with placentitis. These authors demonstrated elevated and low concentrations of progestins and estrogens in the maternal sera of all cases with placentitis in pregnant mares, respectively.

The mare’s exposure to ergopeptine alkaloids from the endophyte fungus found on tall fescue grass (fescue toxicosis), ergot alkaloids inhibit fetal corticotropin-releasing hormone (CRH), inhibiting the normal function of the adrenal gland to produce the cortisol surge and associated changes in pregnane metabolism [137]. In mares with fescue toxicosis, prepartum total plasma progestagen concentrations remain low, their foals have low cortisol concentrations, indicating suppression of fetal adrenocortical activity and P5 production [161].

Recent studies demonstrated that altrenogest, when given in combination with antimicrobials, pentoxifylline and nonsteroidal anti-inflammatory (NSAIDs) drugs to mares with placentitis, decreased the incidence of abortion [162]. In these cases, altrenogest counteracts uterine contractility induced by inflammation of the fetal membranes. In the same way, in bacterial placentitis, a combination of trimethoprim sulfamethoxazole, pentoxifylline and a double dose of altrenogest (0.088 mg/kg bwt per os s.i.d.) were successful in maintaining pregnancies to term [163], while that untreated control mares aborted. When mares were treated with trimpethoprim sulfamethoxazole and pentoxifylline without altrenogest, only one live foal was born [163, 164]. Despite this, it is not clear what role, if any, altrenogest plays within this multi-treatment approach. However, the mares can still abort while receiving altrenogest treatment in the last trimester of pregnancy.

5.3 Estrogens

In late gestation total estrogen (including E1S, E2, and its metabolites, equilin, and equilenin) may be used for fetal and placental health monitoring. However, it is doubtful that total estrogen concentration can predict fetal death as the fetal gonads are unlikely to respond to fetal stress [157, 165].

Since the production of estrogens requires both contributions by the fetus and placental, reduced concentrations in maternal circulation may indicate or predict a stressed or hypoxic fetus that is not producing the estrogen precursors [165]. Indeed, E2 [166] and E1S [167] concentrations decreased sharply in mares with placental dysfunction and after the induction of abortion. If the fetus is severely compromised or die in the uterus, maternal plasma E1S are baseline because of the absence of the C19 precursors secreted by the fetal gonads. However, pregnancies compromised by equine herpesvirus-1 infection or severe colic can present normal or transiently decreased E1S concentrations [168]. Compared with the adrenal glands, the gonads are unlikely to respond to fetal stress; consequently, so it is doubtful that total estrogen concentrations can predict fetal death. Frequent blood sampling of mares induced to abort with PG between 90 and 150 days of pregnancy indicated that E1S levels did not decline until within 5 h of abortion [145].

In cases of placentitis at gestational ages between 150 and 280 days, Douglas [169] and Shikichi et al. [157] showed hormonal alterations common as elevated progestogens and low estrogens in mares that aborted. Although the decline in E2 associated with placental dysfunction is thought to reflect placental disease per se, Esteller-Vico et al. [170] recommended the estrogen supplementation as a means to reduce the risk of abortion associated with placentitis in mares. Recently, Curcio et al. [171] showed that in addition to basic treatment with trimethoprim-sulfamethoxazole and flunixin meglumine, mares with experimentally induced ascending placentitis benefited from E2 cypionate supplementation. Conversely, altrenogest did not appear to make a difference in outcomes.

After fetal death and stress or fetal weakness, androgens and estrogens levels drop rapidly. For better determination of the health state of the fetus, due to the metabolism of both steroids, it is recommended to monitor androgens and estrogens simultaneously [126].

5.4 Relaxin

Relaxin is a useful biomarker to assess placental health and can be monitored in high-risk mares. Ryan et al. [172] reported a positive relationship between circulating levels of relaxin and poor outcomes in high-risk pregnancies. Relaxin is detectable in the blood after the 80th day of pregnancy without any changes until the second stage of labor. In mares with impaired placental function, in cases of placentitis, placental abruption, hydroallantois, and hydramnios relaxin concentrations decrease below 4 ng/mL [143, 172]. Low circulating levels of relaxin have been reported both in pony mares affected by fescue toxicosis associated with placental disease and agalactia and in Thoroughbred mares, with other forms of placental disease or insufficiency [172].

In the case of placental hydrops, the risk of spontaneous rupture of the fetal membranes increases significantly [173]. Relaxin has been explored as a potential marker of treatment success in placentitis due to its level decrease in cases of spontaneously occurring and experimentally induced pregnancy loss [174].

5.5 Prostaglandins

Placentitis is characterized by the production of proinflammatory cytokines (such as IL-6 and IL-8) and PGs [175, 176]. PG release increases uterine contractility and consequently the risk of premature delivery [138]. Proinflammatory cytokines and the PGs of the FPU increases both in response to inflammation/infection, inducing premature activation of the fetal hypothalamic-pituitary-adrenal (HPA) axis [177], accelerating fetal maturation before parturition [138, 178]. The fetal adrenal produces both progestins and, once sufficiently mature, cortisol. Fetal cortisol, in turn, enhances placental and uterine PGs production, further enhancing uterine contractility and resulting in fetal delivery. Since the maturation of the equine fetus occurs later in gestation [137] this implies that placentitis or maternal disease could be devastating to the newborn foal. However, early fetal maturation likely counterbalances premature delivery and may help improve the chances for foal survival [138, 178]. The supplementation with progestin and PG synthetase inhibitor can maintain equine pregnancy in the presence of PGF2 insults [146, 147]. In addition, Esteller-Vico et al. [170] showed that estrogen suppression resulted in a decrease in circulating PGFM, which suggests that estrogens partially regulate PG production during pregnancy since PGFM concentrations were lower but still increased during the last trimester of equine gestation in letrozole-treated mares.


6. Conclusions

Knowledge of the physiological basis of the estrous cycle allows us to understand the interaction of reproductive hormones and the factors or events that interact in the cyclicity of mares. These basic studies have made possible the correct manipulation of the estrous cycle, the advancement of the reproductive season or the synchronization of ovulation. A great contribution in this sense has been possible through the description of the follicular dynamics and the study of the different structures present in the ovaries of the mares throughout the year.

Likewise, the adequate interaction between the ovary, the placenta, and the fetus guarantees the secretion of the correct hormonal patterns necessary for a successful pregnancy. Measurements of progestogens, estrogens, and relaxin, among other hormones, are useful for monitoring the health status of the placenta and fetal viability. This is mainly because placental pathologies or fetal death are mainly due to alterations of these hormones. On the other hand, the hormonal diagnosis allows temporizing and early detection of pathological conditions to propose an adequate treatment for the maintenance of gestation and with it, the production of a viable foal. Substantial progress has been made in recent years in the identification of risk pregnancies and their treatment.

All this knowledge helps greatly to improve the work of professionals and achievements for the improvement of reproductive outcomes. It is important to bear in mind that the constant production of basic knowledge and applied in equine reproduction will allow in the future to improve and generate new guidelines in reproductive technologies.


  1. 1. Fowden AL, Moore T. Maternal-fetal resource allocation: Co-operation and conflict. Placenta. 2012;33(2):e11-e15. DOI: 10.1016/j.placenta.2012.05.002
  2. 2. Napso T, Yong HEY, Lopez-Tello J, Sferruzzi-Perri AN. The role of placental hormones in mediating maternal adaptations to support pregnancy and lactation. Frontiers in Physiology. 2018;9:1091. DOI: 10.3389/fphys.2018.01091
  3. 3. Fowden AL, Giussani DA, Forhead AJ. Intrauterine programming of physiological systems: Causes and consequences. Physiology (Bethesda, Md.). 2006;21:29-37. DOI: 10.1152/physiol.00050.2005
  4. 4. Bergfelt DR. Estrous synchronization. In: Samper JC, editor. Equine Breeding Management and Artificial Insemination. Philadelphia: Saunders Company; 2000. pp. 165-177
  5. 5. Ginther OJ, Beg MA, Neves AP, Mattos RC, Petrucci BP, Gastal MO, et al. Miniature ponies: 2. Endocrinology of the estrous cycle. Reproduction, Fertility and Development. 2008;20(3):386-390. DOI: 10.1071/rd07165
  6. 6. Crowell-Davis SL. Sexual behaviour of mares. Hormones and Behavior. 2007;52(1):12-17. DOI: 10.1016/j.yhbeh.2007.03.020
  7. 7. Aurich C. Reproductive cycles of horses. Animal Reproduction Science. 2011;124(3-4):220-228. DOI: 10.1016/j.anireprosci.2011.02.005
  8. 8. Ginther OJ, Beg MA, Gastal MO, Gastal EL, Baerwald AR, Pierson RA. Systemic concentrations of hormones during development of follicular waves in mares and women: A comparative study. Reproduction. 2005;130:379-388. DOI: 10.1530/rep.1.00757
  9. 9. Armstrong DG, Webb R. Ovarian follicular dominance: The role of intraovarian growth factors and novel proteins. Reviews of Reproduction. 1997;2(3):139-146. PMID: 9414477
  10. 10. Ginther OJ, Bergfelt DR. Effect of GnRH treatment during the anovulatory season on multiple ovulation rate and on follicular development during the ensuing pregnancy in mares. Reproduction. 1990;88(1):119-126. DOI: 10.1530/jrf.0.0880119
  11. 11. Ginther OJ, Beg MA, Bergfelt DR, Donadeu FX, Kot K. Follicle selection in monovular species. Biology of Reproduction. 2001;65(3):638-647. DOI: 10.1095/biolreprod65.3.638
  12. 12. Donadeu FX, Ginther OJ. Changes in concentrations of follicular fluid factors during follicle selection in mares. Biology of Reproduction. 2002;66(4):1111-1118. DOI: 10.1095/biolreprod66.4.1111
  13. 13. Ginther OJ, Gastal MO, Gastal EL, Bergfelt DR, Baerwald AR, Pierson RA. Comparative study of the dynamics of follicular waves in mares and women. Biology of Reproduction. 2004;71:1195-1201. DOI: 10.1095/biolreprod.104.031054
  14. 14. Ginther OJ. Folliculogenesis during the transitional period and early ovulatory season in mares. Journal of Reproduction and Fertility. 1990;90(1):311-320. DOI: 10.1530/jrf.0.0900311
  15. 15. Irvine CHG, Alexander SL, Mckinnon AO. Reproductive hormone profiles in mares during the autumn transition as determined by collection of jugular blood at 6 h intervals throughout ovulatory and anovulatory cycles. Journal of Reproduction and Fertility. 2000;118:101-109. PMID: 10793631
  16. 16. Watson ED, Bae SE, Steele M, Tomassen R, Michele S, Pedersen H, et al. Expression of messenger ribonucleic acid encoding for steroidogenic acute regulatory protein and enzymes, and luteinizing hormone receptor during the spring transitional season in equine follicles. Domestic Animal Endocrinology. 2004;26(3):215-239. DOI: 10.1016/j.domaniend.2003.10.006
  17. 17. Ginther OJ. Selection of the dominant follicle in cattle and horses. Animal Reproduction Science. 2000;2(60-61):61-79. PMID: 10844185
  18. 18. Gastal EL. Recent advances and new concepts on follicle and endocrine dynamics during the equine periovulatory period. Animal Reproduction. 2009;6(1):144-158. DOI: 10.1111/j.1439-0531.2007.01003.x
  19. 19. Satué K, Montesinos P, Gardon JC. Influence of oestrogen and progesterone on circulating neutrophils and monocyte during ovulatory and luteal phase in healthy Spanish Purebred mares. In: Proceeding of XIX Congress of Societa Italiana Veterinari per Equini (SIVE); 1-3 February 2013; Arezzo, Italy. pp. 383-384
  20. 20. Bergfelt DR, Adams GP. Ovulation and corpus luteum development. In: Samper JC, Pycock JF, McKinnon AO, editors. Current Therapy in Equine Reproduction. W.B. Saunders-Elsevier; 2007. pp. 1-13
  21. 21. Davies Morel MC, Newcombe JR, Hayward K. Factors affecting pre-ovulatory follicle diameter in the mare: The effect of mare age, season and presence of other ovulatory follicles (multiple ovulation). Theriogenology. 2010;74(7):1241-1247. DOI: 10.1016/j.theriogenology.2010.05.027
  22. 22. Gastal EL. Ovulation. Part 1. Follicle development and endocrinology during the periovulatory period. In: AO MK, Squires EL, Vaala WE, Dickson DV, editors. Equine Reproduction. Ames, IA: Wiley-Blackwell; 2011. pp. 2020-2031. ISBN: 978-0-813-81971-6
  23. 23. Gastal EL. Ovulation. Part 2: Ultrasonographic morphology of the preovulatory follicle. In: McKinnon AO, Squires EI, Vaala WE, Varner DD, editors. Equine Reproduction. 2nd ed. Vol. 2. Oxford: Blackwell Publishing Ltd; 2011. pp. 2032-2054. ISBN: 978-0-813-81971-6
  24. 24. Younqquist RS, Threlfall WR. Current Therapy in Large Animal Theriogenology. 2nd ed. St Louis: Saunders Elsevier; 2007. pp. 47-67
  25. 25. Dickson SE, Fraser HM. Inhibition of early luteal angiogenesis by gonadotropin-releasing hormone antagonist treatment in the primate. The Journal of Clinical Endocrinology and Metabolism. 2000;85(6):2339-2344. DOI: 10.1210/jcem.85.6.6621
  26. 26. Bergfelt D, Ginther O. Embryo loss following GnRH-induced ovulation in anovulatory mares. Theriogenology. 1992;38(1):33-43. DOI: 10.1016/0093-691x(92)90216-e
  27. 27. Daels PF, DeMoraes JJ, Stabenfeldt GH, Hughes JP, Lasley BL. The corpus luteum: Source of oestrogen during early pregnancy in the mare. Journal of Reproduction and Fertility. Supplement. 1991;44:501-508. PMID: 1665517
  28. 28. Ginther OJ, editor. Reproductive Biology of the Mare: Basic and Applied Aspects. 2nd ed. Cross Plains, WI: Equiservices Publishing; 1992. pp. 224-226. ISBN: 0964007215
  29. 29. Samper JC. Induction of estrus and ovulation: Why some mares respond and others do not. Animal Reproduction Science. 2008;70:445-447. DOI: 10.1016/j.theriogenology.2008.04.040
  30. 30. Alexander SL, Irvine CHG. Control of onset of breeding season in the mare and its artificial regulation by progesterone treatment. Journal of Reproduction and Fertility. Supplement. 1991;44:307-318. PMID: 1795275.
  31. 31. Medan MS, Nambo Y, Nagamine N, Shinbo H, Watanabe G, Groome N, et al. Plasma concentrations of Ir-inhibin, inhibin A, inhibin pro-αC, FSH, and estradiol-17β during estrous cycle in mares and their relationship with follicular growth. Endocrine. 2004;25(1):7-14. DOI: 10.1385/ENDO:25:1:07
  32. 32. Irvine CHG, Alexander SL. Secretory patterns and rates ofgonadotrophin-releasing hormone, follicle-stimulating hormone, and luteinizing hormone revealed by intensive sampling of pituitary venous blood in the luteal phase mare. Endocrinology. 1993;132:212-218. DOI: 10.1210/endo.132.1.8419124
  33. 33. Reichert LE Jr. The functional relationship between FSH and its receptor as studied by synthetic peptide strategies. Molecular and Cellular Endocrinology. 1994;100(1-2):21-27. DOI: 10.1016/0303-7207(94)90273-9
  34. 34. Pantke P, Hyland J, Galloway DB, Mclean AA, Hoppen HO. Changes in luteinizing hormone bioactivity associated with gonadotrophin pulses in the cycling mare. Journal of Reproduction and Fertility. Supplement. 1991;44:13-18. PMID: 1795256
  35. 35. Honnens A, Weisser S, Welter H, Einspanier R, Bollwein H. Relationships between uterine blood flow, peripheral sex steroids, expression of endometrial estrogen receptors and nitric oxide synthases during the estrous cycle in mares. The Journal of Reproduction and Development. 2011;57(1):43-48. DOI: 10.1262/jrd.10-023t
  36. 36. Amer HA, Gamal S, Randa I. Profile of steroid hormones during oestrus and early pregnancy in Arabian mares. Slovenian Veterinary Research. 2008;45(1):25-32. UDC 636.1.082.455:612.621.9:637.047:577.175.6
  37. 37. Nagy P, Huszenicza G, Reiczigel J, Juhász J, Kulcsár M, Abaváry K, et al. Factors affecting plasma progesterone concentration and the retrospective determination of time of ovulation in cyclic mares. Theriogenology. 2004;61(2-3):203-214. DOI: 10.1016/s0093-691x(03)00211-5
  38. 38. Donadeu FX, Pedersen HG. Follicle development in mares. Reproduction in Domestic Animals. 2008;43(2):224-231. DOI: 10.1111/j.1439-0531.2008.01166.x
  39. 39. Shand N, Irvine CH, Turner JE, Alexander SL. A detailed study of hormonal profiles in mares at luteolysis. Journal of Reproduction and Fertility. Supplement. 2000;56:271-279. PMID: 20681138
  40. 40. Ginther OJ, Beg MA. Hormone concentration changes temporally associated with the hour of transition from preluteolysis to luteolysis in mares. Animal Reproduction. 2011;129(1-2):67-72. DOI: 10.1016/j.anireprosci.2011.09.013
  41. 41. Greco GM, Fioratti EG, Segabinazzi LG, Dell’Aqua JA Jr, Crespilho AM, Castro-Chaves MMB, et al. Novel long-acting progesterone protocols used to successfully synchronize donor and recipient mares with satisfactory pregnancy and pregnancy loss rates. Journal of Equine Veterinary Science. 2016;39:58-61. DOI: 10.1016/j.jevs.2015.07.012
  42. 42. Pinto MR, Miragaya MH, Burns P, Douglas R, Neild DM. Strategies for increasing reproductive efficiency in a commercial embryo transfer program with high performance donor mares under training. Journal of Equine Veterinary Science. 2017;54:1-5. DOI: 10.1016/j.jevs.2016.09.004
  43. 43. Alexander SL, Irvine CHG. Effect of graded doses of gonadotrophin-releasing hormone on serum LH concentrations in mares in various reproductive states: Comparison with endogenously generated LH pulses. The Journal of Endocrinology. 1986;110:19-26. DOI: 10.1677/joe.0.1100019
  44. 44. Garcia MC, Ginther OJ. Plasma luteinizing hormone concentration in mares treated with gonadotropin-releasing hormone and estradiol. American Journal of Veterinary Research. 1975;36:1581-1584. PMID: 1103666
  45. 45. Hyland JH, Wright PJ, Clarke IJ, Carson RS, Langsford DA, Jeffcott LB. Infusion of gonadotropin-releasing hormone (GnRH) induces ovulation and fertile estrus in mares during seasonal anestrous. Journal of Reproduction and Fertility. Supplement. 1987;35:211-220. PMID: 3316638
  46. 46. Turner JE, Irvine CHG. The effect of various gonadotropin-releasing hormone regimens on gonadotrophins, follicular growth and ovulation in deeply anestrous mares. Journal of Reproduction and Fertility. Supplement. 1991;44:213-225. PMID: 1839039
  47. 47. Minoia P, Mastronardi M. Use of GnRH to induce oestrus in seasonally anoestrus mares. Equine Veterinary Journal. 1987;19:241-242. DOI: 10.1111/j.2042-3306.1987.tb01394.x
  48. 48. Lindholm A, Ferris R, Scofield D, Mccue P. Comparison of deslorelin and histrelin for induction of ovulation in mares. Journal of Equine Veterinary Science. 2011;31(5-6):312-313. DOI: 10.1016/j.jevs.2011.03.144
  49. 49. Allen WR, Sanderson MW, Greenwood RES, Ellis DR, Crowhurst JS, Simpson DJ, et al. Induction of ovulation in anestrous mares with a slow-release implant of GnRH analogue (ICI 118630). Journal of Reproduction and Fertility. Supplement. 1987;35:469-478. PMID: 2960804
  50. 50. Harrison LA, Squires EL, Nett TM, McKinnon AO. Use of gonodotrophin-releasing hormone for hastening ovulation in transitional mares. Journal of Animal Science. 1990;68:690-699. DOI: 10.2527/1990.683690x
  51. 51. Mumford EL, Squires EL, Jasko DJ, Nett TM. Use of gonadotropin-releasing hormone, estrogen, or combination to increase releasable pituitary luteinizing hormone in early transitional mares. Journal of Animal Science. 1994;72:174-177. DOI: 10.2527/1994.721174x
  52. 52. Mumford EL, Squires EL, Jochle W, Harrison LA, Nett TM, Trigg TE. Use of deslorelin short-term implants to induce ovulation in cycling mares during three consecutive estrous cycles. Animal Reproduction Science. 1995;39:129-140. DOI: 10.1016/0378-4320(95)01383-B
  53. 53. Squires EL, Moran DM, Farlin ME, Jasko DJ, Keefe TJ, Meyers SA, et al. Effect of dose of GnRH analog on ovulation in mares. Theriogenology. 1994;41:757-769. DOI: 10.1016/0093-691x(94)90185-l
  54. 54. Dascanio J. In: McCue P, editor. Equine Reproductive Procedure. John Wiley & Sons, Inc; 2014. DOI: 10.1002/9781118904398
  55. 55. Allen WR, Urwin V, Simpson DJ, Greenwood RES, Crowhurst RC, Ellis DR, et al. Preliminary studies on the use of an oral progestogen to induce oestrus and ovulation in seasonally anoestrous Thoroughbred mares. Equine Veterinary Journal. 1980;12(3):141-145. DOI: 10.1111/j.2042-3306.1980.tb03405.x
  56. 56. Webel SK, Squires EL. Control of oestrous cycle in mares with altrenogest. Journal of Reproduction and Fertility. Supplement. 1982;32:193-198.PMID: 6962854
  57. 57. Hanlon DW, Firth EC. The reproductive performance of Thoroughbred mares treated with intravaginal progesterone at the start of the breeding season. Theriogenology. 2012;77(5):952-958. DOI: 10.1016/j.theriogenology.2011.10.001
  58. 58. Raz T, Carley S, Card C. Comparison of the effects of eFSH and deslorelin treatment regimes on ovarian stimulation and embryo production of donor mares in early vernal transition. Animal Reproduction Science. 2009;71:1358-1366. DOI: 10.1016/j.theriogenology.2008.09.048
  59. 59. Meyers-Brown GA, McCue PM, Niswender KD, Squires EL, DeLuca CA, Bidstrup LA, et al. Superovulation in mares using recombinant equine follicle stimulating hormone: Ovulation rates, embryo retrieval, and hormone profiles. Journal of Equine Veterinary Science. 2010;30(10):560-568. DOI: 10.1016/j.jevs.2010.09.007
  60. 60. Meyers-Brown GA, McCue PM, Troedsson MH, Klein C, Zent W, Ferris RA, et al. Induction of ovulation in seasonally anestrous mares under ambient lights using recombinant equine FSH (reFSH). Theriogenology. 2013;80(5):456-462. DOI: 10.1016/j.theriogenology.2013.04.029
  61. 61. Meyers-Brown GA, Loud MC, Hyland JC, Roser JF. Deep anestrous mares under natural photoperiod treated with recombinant equine FSH (reFSH) and LH (reLH) have fertile ovulations and become pregnant. Theriogenology. 2017;98:108-115. DOI: 10.1016/j.theriogenology.2017.05.001
  62. 62. Havern RL, Whisnant CS, Goodman RL. Hypothalamic sites of catecholamine inhibition of luteinizing hormone in the anestrous Ewe1. Biology of Reproduction. 1991;44(3):476-482. DOI: 10.1095/biolreprod44.3.476
  63. 63. Panzani D, Zicchino I, Taras A, Marmorini P, Crisci A, Rota A, et al. Clinical use of dopamine antagonist sulpiride to advance first ovulation in transitional mares. Theriogenology. 2011;75(1):138-143. DOI: 10.1016/j.theriogenology.2010.07.019
  64. 64. Mari G, Morganti M, Merlo B, Castagnetti C, Parmeggiani F, Govoni N, et al. Administration of sulpiride or domperidone for advancing the first ovulation in deep anestrous mares. Theriogenology. 2009;71(6):959-965. DOI: 10.1016/j.theriogenology.2008.11.001
  65. 65. McCue PM. Clinical cases in equine reproduction. In: Proceedings of the 52nd Annual Convention of the American Association of Equine Practitioners (AAEP); 2-6 December 2006; San Antonio, Texas. Vol. 52. pp. 591-596
  66. 66. Thompson DL, Hoffman R, Depew CL. Prolactin administration to seasonally anestrous mares: Reproductive, metabolic, and hair-shedding responses. Journal of Animal Science. 1997;75(4):1092-1099. DOI: 10.2527/1997.7541092x
  67. 67. Nequin LG, King SS, Johnson AL, Gow GM, Ferreira-Dias GM. Prolactin may play a role in stimulating the equine ovary during the spring reproductive transition. Journal of Equine Veterinary Science. 1993;13:631-635. DOI: 10.1016/S0737-0806(07)80391-1
  68. 68. Yoon M. The estrous cycle and induction of ovulation in mares. Journal of Analytical Science and Technology. 2012;54(3):165-174. DOI: 10.5187/JAST.2012.54.3.165
  69. 69. Alexander SL, Irvine CH. Secretion rates and short-term patterns of gonadotrophin-releasing hormone, FSH and LH throughout the periovulatory period in the mare. The Journal of Endocrinology. 1987;114:351-362. DOI: 10.1677/joe.0.1140351
  70. 70. Johnson AL. Induction of ovulation in anestrous mares with pulsatile administration of gonadotropin-releasing hormone. American Journal of Veterinary Research. 1986;47:983-986. PMID: 3521408
  71. 71. Becker SE, Johnson AL. Effects of gonadotropinreleasing hormone infused in a pulsatile or continuous fashion on serum gonadotropin concentrations and ovulation in the mare. Journal of Animal Science. 1992;70:1208-1215. DOI: 10.2527/1992.7041208x
  72. 72. Irvine DS, Downey BR, Parker WG, Sullivan JJ. Duration of oestrus and time of ovulation in mares treated with synthetic Gn-RH (AY-24,031). Journal of Reproduction and Fertility. 1975:279-283. PMID: 1107542
  73. 73. Duchamp G, Bour B, Combarnous Y, Palmer E. Alternative solutions to hCG induction of ovulation in the mare. Journal of Reproduction and Fertility. Supplement. 1987;35:221-228. PMID: 3479577
  74. 74. Williams GL, Amstalden M, Blodgett GP, Ward JE, Unnerstall DA, Quirk KS. Continuous administration of low dose GnRH in mares. I. Control of persistent anovulation during the ovulatory season. Theriogenology. 2007;68:67-75. DOI: 10.1016/j.theriogenology.2007.03.024
  75. 75. Samper JC, Jensen S, Sergenat J. Timing of induction of ovulation in mares treated with ovuplant or chorulon. Journal of Equine Veterinary Science. 2002;22:320-323. DOI: 10.1016/S0737-0806(02)70080-4
  76. 76. Meinert C, Silva JFS, Kroetz L, Klug E, Trigg TE, Hoppen HO, et al. Advancing the time of ovulation in the mare with a short-term implant releasing the GnRH analogue deslorelin. Equine Veterinary Journal. 1993;25:65-68. DOI: 10.1111/j.2042-3306.1993.tb02904.x
  77. 77. Farquhar V, McCue P, Vanderwall DK, Squires EL. Efficacy of the GnRH agonist deslorelin acetate for inducing ovulation in mares relative to age of mare and season. Journal of Equine Veterinary Science. 2000;20:8-11. DOI: 10.1016/S0737-0806(00)80183-5
  78. 78. Vanderwall DK, Juergens TD, Woods GL. Reproductive performance of commercial broodmares after induction of ovulation with hCG or Ovuplant™ (deslorelin). Journal of Equine Veterinary Science. 2001;21:539-542. DOI: 10.1016/S0737-0806(01)70158-X
  79. 79. Johnson CA, Thompson DL, Kulinski K, Guitreau AM. Prolonged interovulatory interval and hormonal changes in mares following the use of Ovuplant™ to hasten ovulation. Journal of Equine Veterinary Science. 2000;20:331-336. DOI: 10.1016/S0737-0806(00)70421-7
  80. 80. Farquhar VJ, McCue PM, Nett TM, Squires EL. Effect of deslorelin acetate on gonadotropin secretion and ovarian follicle development in cycling mares. Journal of the American Veterinary Medical Association. 2001;218:749-752. DOI: 10.2460/javma.2001.218.749
  81. 81. McCue PM, Farquhar VJ, Carnevale EM, Squires EL. Removal of deslorelin (Ovuplant™) implant 48 h after administration results in normal interovulatory intervals in mares. Theriogenology. 2002;58(5):865-870. DOI: 10.1016/S0093-691X(02)00923-8
  82. 82. Stich KL, Wendt KM, Blandchard TL, Brinsko SP. Effects of a new injectable short-term release deslorelin in foal-heat mares. Theriogenology. 2004;62:831-836. DOI: 10.1016/j.theriogenology.2003.12.004
  83. 83. McCue PM, Magee C, Gee EK. Comparison of compounded deslorelin and hCG for induction of ovulation in mares. Journal of Equine Veterinary Science. 2007;27:58-61. DOI: 10.1016/j.jevs.2006.12.003
  84. 84. Barrier-Battut I, Le Poutre N, Trocherie E, Hecht S, Grandchamp des Raux A, Nicaise JL, et al. Use of buserelin to induce ovulation in the cyclic mare. Theriogenology. 2001;55:1679-1695. DOI: 10.1016/s0093-691x(01)00512-x
  85. 85. Miki W, Oniyama H, Takeda N, Kimura Y, Haneda S, Matsui M, et al. Effects of a single use of the GnRH analog buserelin on the induction of ovulation and endocrine profiles in heavy draft mares. Journal of Equine Science. 2016;27(4):149-156. DOI: 10.1294/jes.27.149
  86. 86. Camillo F, Pacini M, Panzani D, Vannozzi I, Rota A, Aria G. Clinical use of twice daily injections of buserelin acetate to induce ovulation in the mare. Veterinary Research Communications. 2004;28(1):169-172. DOI: 10.1023/b:verc.0000045398.62134.e4
  87. 87. Newcombe JR, Martinez TA, Peters AR. The effect of the gonadotropin-releasing hormone analog, buserelin, on pregnancy rates in horse and pony mares. Theriogenology. 2001;55:1619-1631. DOI: 10.1016/s0093-691x(01)00507-6
  88. 88. Kanitz W, Schneider F, Hoppen HO, Unger C, Nurmberg G, Becker K. Pregnancy rates, LH and progesterone concentrations in mares treated with GnRH agonist. Animal Reproduction Science. 2007;97:55-62. DOI: 10.1016/j.anireprosci.2005.12.011
  89. 89. Cole LA, Kardana A. Discordant results in human chorionic gonadotropin assays. Clinical Chemistry. 1992;38:263-270. PMID: 1371722
  90. 90. Kilicarslan MR, Horoz H, Senunver A, Konuk SC, Tek C, Carioglu B. Effect of GnRH and hCG on ovulation and pregnancy in mares. The Veterinary Record. 1996;139:119-120. DOI: 10.1136/vr.139.5.119
  91. 91. Wilson C, Downie C, Hughes J. Effects of repeated hCG injections on reproductive efficiency in mares. Journal of Equine Veterinary Science. 1990;10:301-308. DOI: 10.1016/S0737-0806(06)80015-8
  92. 92. Newcombe JR, Wilson MC. The effect of repeated treatment with human chorionic gonadotrophin to induce ovulation in mares. In: Proceedings of the 46th Congress British Equine Veterinary Association (BEVA): 12-15th September 2007; Edinburgh. p. 291
  93. 93. Newcombe JR. Human chorionic gonadotrophin. In: McKinnon AO, Squires EL, Vaala WE, Varner DD, editors. Equine Reproduction. United Kingdom: Blackwell Publishing Ltd.; 2011. pp. 1804-1810. ISBN: 978-0-813-81971-6
  94. 94. Jablonka-Shariff A, Roser JF, Bousfield GR, Wolfe MW, Sibley LE, Colgin M, et al. Expression and bioactivity of a single chain recombinant equine luteinizing hormone (reLH). Theriogenology. 2007;67:311-320. DOI: 10.1016/j.theriogenology.2006.06.013
  95. 95. Yoon MJ, Boime I, Colgin M, Niswender KD, King SS, Alvarenga M, et al. The efficacy of a single chain recombinant equine luteinizing hormone (reLH) in mares: Induction of ovulation, hormone profiles, and inter-ovulatory intervals. Domestic Animal Endocrinology. 2007;33:470-479. DOI: 10.1016/j.domaniend.2007.06.001
  96. 96. Goldfarb LG, Cervenakova L, Gajdusek DC. Genetic studies in relation to kuru: An overview. Current Molecular Medicine. 2004;4(4):375-384. DOI: 10.2174/1566524043360627
  97. 97. Chakraborty C, Nandi S, Jana S. Prion disease: A deadly disease for protein misfolding. Current Pharmaceutical Biotechnology. 2005;6(2):167-177. DOI: 10.2174/1389201053642321
  98. 98. Zou WQ , Gambetti P. Prion: The chameleon protein. Cellular and Molecular Life Sciences. 2007;64(24):3266-3270. DOI: 10.1007/s00018-007-7380-8
  99. 99. Savage NC, Liptrap RM. Induction of ovulation in cyclic mares by administration of a synthetic prostaglandin, fenprostalene, during oestrus. Journal of Reproduction and Fertility. Supplement. 1987;35:239-243. PMID: 3479578
  100. 100. Harrison LA, Squires EL, McKinnon AO. Comparison of hCG, Burserelin and Luprostiol for induction of ovulation in cycling mares. Journal of Equine Veterinary Science. 1991;11:163-166. DOI: 10.1016/S0737-0806(07)80039-6
  101. 101. Jöchle W, Irvine CH, Alexander SL, Newby TJ. Release of LH, FSH and GnRH into pituitary venous blood in mares treated with a PGF analogue, luprostiol, during the transition period. Journal of Reproduction and Fertility. Supplement. 1987;35:261-267. PMID: 3119828
  102. 102. Caraty A, Franceschini I. Basic aspects of the control of GnRH and LH secretions by kisspeptin: Potential applications for better control of fertility in females. Reproduction in Domestic Animals. 2008;43(2):172-178. DOI: 10.1111/j.1439-0531.2008.01158.x
  103. 103. Clarke H, Dhillo WS, Jayasena CN. Comprehensive review on Kisspeptin and its role in reproductive disorders. Endocrinology and Metabolism. 2015;30(2):124-141. DOI: 10.3803/EnM.2015.30.2.124
  104. 104. Magee C, Foradori CD, Bruemmer JE, Arreguin-Arevalo JA, McCue PM, Handa RJ, et al. Biological and anatomical evidence for kisspeptin regulation of the hypothalamic-pituitary-gonadal axis of estrous horse mares. Biomedizinische Technik. 2009;150(6):2813-2821. DOI: 10.1210/en.2008-1698
  105. 105. Ginther OJ. Mobility of the early equine conceptus. Theriogenology. 1983;19(4):603-611. DOI: 10.1016/0093-691x(83)90180-2
  106. 106. Ginther OJ. Equine pregnancy: Physical interactions between the uterus and conceptus. In: Proceedings of the 44th Annual Convention of the American Association of Equine Practitioners (AAEP); 6-9 December 1998. Baltimore, Maryland. pp. 73-104
  107. 107. Stout TA, Allen WR. Role of prostaglandins in intrauterine migration of the equine conceptus. Reproduction. 2001;121(5):771-775. DOI: 10.1530/rep.0.1210771
  108. 108. Raeside JI, Christie HL, Renaud RL, Waelchli RO, Betteridge KJ. Estrogen metabolism in the equine conceptus and endometrium during early pregnancy in relation to estrogen concentrations in yolk-sac fluid. Biology of Reproduction. 2004;71(4):1120-1127. DOI: 10.1095/biolreprod.104.028712
  109. 109. Raeside JI, Christie HL, Waelchli RO, Betteridge KJ. Biosynthesis of oestrogen by the early equine embryo proper. Reproduction, Fertility, and Development. 2012;24(8):1071-1078. DOI: 10.1071/RD11275
  110. 110. Wilsher S, Allen WR. Factors influencing equine chorionic gonadotrophin production in the mare. Equine Veterinary Journal. 2011;43(4):430-438. DOI: 10.1111/j.2042-3306.2010.00309.x
  111. 111. Ginther OJ, Santos VG. Natural rescue and resurgence of the equine corpus luteum. Journal of Equine Veterinary Science. 2015;35:1-6. DOI: 10.1016/j.jevs.2014.10.004
  112. 112. Legacki EL, Scholtz EL, Ball BA, Stanley SD, Berger T, Conley AJ. The dynamic steroid landscape of equine pregnancy mapped by mass spectrometry. Reproduction. 2016;151(4):421-430. DOI: 10.1530/REP-15-0547
  113. 113. Satué K, Marcilla M, Medica P, Ferlazzo A, Fazio E. Sequential concentrations of placental growth factor and haptoglobin, and their relation to oestrone sulphate and progesterone in pregnant Spanish purebred mare. Theriogenology. 2018;115:77-83. DOI: 10.1016/j.theriogenology.2018.04.033
  114. 114. Davies Morel MC. Equine Reproductive Physiology, Breeding and Stud Management. 3rd ed. Wallindorf, UK: CABI; 2008. ISBN: 9781845934507
  115. 115. Satué K, Domingo R, Redondo JI. Relationship between progesterone, oestrone sulphate and cortisol and the components of renin angiotensin aldosterone system in Spanish purebred broodmares during pregnancy. Theriogenology. 2011;76(8):1404-1415. DOI: 10.1016/j.theriogenology.2011.06.009
  116. 116. Satué K, Marcilla M, Medica P, Ferlazzo A, Fazio E. Testosterone, androstenedione and dehydroepiandrosterone concentrations in pregnant Spanish purebred mare. Theriogenology. 2019;1(123):62-67. DOI: 10.1016/j.theriogenology.2018.09.025
  117. 117. Albrecht BA, MacLeod JN, Daels PF. Differential transcription of steroidogenic enzymes in the equine primary corpus luteum during diestrus and early pregnancy. Biology of Reproduction. 1997;56(4):821-829. DOI: 10.1095/biolreprod56.4.821
  118. 118. Daels PF, Chang GC, Hansen B, Mohammed HO. Testosterone secretion during early pregnancy in mares. Theriogenology. 1996;45(6):1211-1219. DOI: 10.1016/0093-691x(96)00076-3
  119. 119. Daels PF, Albrecht BA, Mohammed HO. Equine chorionic gonadotropin regulates luteal steroidogenesis in pregnant mares. Biology of Reproduction. 1998;59(5):1062-1068. DOI: 10.1095/biolreprod59.5.1062
  120. 120. Kajihara T, Tanaka K, Oguro T, Tochigi H, Prechapanich J, Uchino S, et al. Androgens modulate the morphological characteristics of human endometrial stromal cells decidualized in vitro. Reproductive Sciences. 2014;21(3):372-380. DOI: 10.1177/1933719113497280
  121. 121. Ferraz LES, Vicente WRR, Ramos PRR. Progesterone and estradiol 17-β concentration, and ultrasonic images of the embryonic vesicle during the early pregnancy in Thoroughbred mares. Arquivo Brasileiro de Medicina Veterinária e Zootecnia. 2001;53(4):1-7. DOI: 10.1590/S0102-09352001000400015
  122. 122. Holtan DW, Houghton E, Silver M, Fowden AL, Ousey J, Rossdale PD. Plasma progestagens in the mare, fetus and newborn foal. Journal of Reproduction and Fertility. Supplement. 1991;44:517-528. PMID: 1795295
  123. 123. Han X, Rossdale PD, Ousey J, Holdstock N, Allen WR, Silver M, et al. Localisation of 15-hydroxy prostaglandin dehydrogenase (PGDH) and steroidogenic enzymes in the equine placenta. Equine Veterinary Journal. 1995;27(5):334-339. DOI: 10.1111/j.2042-3306.1995.tb04067.x
  124. 124. Ousey JC, Houghton E, Grainger L, Rossdale PD, Fowden AL. Progestagen profiles during the last trimester of gestation in Thoroughbred mares with normal or compromised pregnancies. Theriogenology. 2005;63(7):1844-1856. DOI: 10.1016/j.theriogenology.2004.08.010
  125. 125. Scholtz EL, Krishnan S, Ball BA, Corbin CJ, Moeller BC, Stanley SD, et al. Pregnancy without progesterone in horses defines a second endogenous biopotent progesterone receptor agonist, 5α-dihydroprogesterone. Proceedings of the National Academy of Sciences of the United States of America. 2014;111(9):3365-3370. DOI: 10.1073/pnas.1318163111
  126. 126. Conley AJ. Review of the reproductive endocrinology of the pregnant and parturient mare. Theriogenology. 2016;86(1):355-365. DOI: 10.1016/j.theriogenology.2016.04.049
  127. 127. Wynn MAA, Esteller-Vico A, Legacki EL, Conley AJ, Loux SC, Stanley SD, et al. A comparison of progesterone assays for determination of peripheral pregnane concentrations in the late pregnant mare. Theriogenology. 2018;106:127-133. DOI: 10.1016/j.theriogenology.2017.10.002
  128. 128. Ousey JC, Rossdale PD, Palmer L, Houghton E, Grainger L, Fowden AL. Effects of progesterone administration to mares during late gestation. Theriogenology. 2002;58:793-795. DOI: 10.1016/S0093-691X(02)00743-4
  129. 129. Ousey JC, Forhead AJ, Rossdale PD, Grainger L, Houghton E, Fowden AL. Ontogeny of uteroplacental progestagen production in pregnant mares during the second half of gestation. Biology of Reproduction. 2003;69(2):540-548. DOI: 10.1095/biolreprod.102.013292
  130. 130. Henderson K, Stewart J. A dipstick immunoassay to rapidly measure serum oestrone sulfate concentrations in horses. Reproduction, Fertility, and Development. 2000;12(3-4):183-189. DOI: 10.1071/rd00062
  131. 131. Henderson KM, Eayrs K. Pregnancy status determination in mares using a rapid lateral flow test for measuring serum oestrone sulphate. New Zealand Veterinary Journal. 2004;52(4):193-196. DOI: 10.1080/00480169.2004.36428
  132. 132. Fowden AL, Forhead AJ, Ousey JC. The endocrinology of equine parturition. Experimental and Clinical Endocrinology & Diabetes. 2008;116:393-403. DOI: 10.1055/s-2008-1042409
  133. 133. Pashen RL, Allen WR. The role of the fetal gonads and placenta in steroid production, maintenance of pregnancy and parturition in the mare. Journal of Reproduction and Fertility. Supplement. 1979;27:499-509. PMID: 289829
  134. 134. Hasegawa T, Sato F, Nambo Y, Ishida N. Expression of steroidogenic enzyme genes in the equine feto-placental unit. Journal of Equine Science. 2001;12(1):25-32. DOI: 10.1294/jes.12.25
  135. 135. Canisso IF, Ball BA, Esteller-Vico A, Squires EL, Troedsson MH. Dehydroepiandrosterone sulfate and testosterone concentrations in mares carrying normal pregnancies. In: Proceedings of the Society for Theriogenology Annual Conference; 6-9 August 2014; Portland, OR, USA. p. 383
  136. 136. Ousey JC. Endocrinology of pregnancy. In: McKinnon AO, Squires EL, Vaala WE, Varner DD, editors. Equine Reproduction. Hoboken NJ: Wiley-Blackwell; 2011. pp. 2222-2231. ISBN: 978-0-813-81971-6
  137. 137. Ousey JC. Hormone profiles and treatments in the late pregnant mare. The Veterinary Clinics of North America. Equine Practice. 2006;22(3):727-747. DOI: 10.1016/j.cveq.2006.08.004
  138. 138. McGlothlin JA, Lester GD, Hansen PJ, Thomas M, Pablo L, Hawkins DL, et al. Alteration in uterine contractility in mares with experimentally induced placentitis. Reproduction. 2004;127(1):57-66. DOI: 10.1530/rep.1.00021
  139. 139. Kelleman AA, Act D. Equine pregnancy and clinical applied physiology. In: Proceedings of the 59th Annual Convention of the American Association of Equine Practitioners (AAEP); 7-11 December, 2013. Nashville, Tennessee, USA. pp. 350-358
  140. 140. Silver M, Barnes RJ, Comline RS, Fowden AL, Clover L, Mitchell MD. Prostaglandins in maternal and fetal plasma and in allantoic fluid during the second half of gestation in the mare. Journal of Reproduction and Fertility. Supplement. 1979;27:531-539. PMID: 289833
  141. 141. Vivrette SL, Kindahl H, Munro CJ, Roser JF, Stabenfeldt GH. Oxytocin release and its relationship to dihydro-15-keto PGF2alpha and arginine vasopressin release during parturition and to suckling in postpartum mares. Journal of Reproduction and Fertility. 2000;119(2):347-357. DOI: 10.1530/jrf.0.1190347
  142. 142. Bryant-Greenwood GD. Relaxin as a new hormone. Endocrine Reviews. 1992;3(1):62-90. DOI: 10.1210/edrv-3-1-62
  143. 143. Stewart DR, Addiego LA, Pascoe DR, Haluska GJ, Pashen R. Breed differences in circulating equine relaxin. Biology of Reproduction. 1992;46(4):648-652. DOI: 10.1095/biolreprod46.4.648
  144. 144. Machnik M, Hegger I, Kietzmann M, Thevis M, Guddat S, Schänzer W. Pharmacokinetics of altrenogest in horses. Journal of Veterinary Pharmacology and Therapeutics. 2007;30:86-90. DOI: 10.1111/j.1365-2885.2007.00820.x
  145. 145. Daels PF, Hussni M, Montavon SME, Stabenfeldt GH, Hughes JP, Odensvik K, et al. Endogenous prostaglandin secretion during cloprostenol-induced abortion in mares. Animal Reproduction. 1995;40:305-321. DOI: 10.1016/0378-4320(95)01429-2
  146. 146. Daels PF, Besognet B, Hansen B, Mohammed H, Odensvik K, Kindahl H. Effect of progesterone on prostaglandin F2 alpha secretion and outcome of pregnancy during cloprostenol-induced abortion in mares. American Journal of Veterinary Research. 1996;57:1331-1337. PMID: 8874729
  147. 147. Daels PF, Stabenfeldt GH, Hughes JP, Odensvik K, Kindahl H. Evaluation of progesterone deficiency as a cause of fetal death in mares with experimentally induced endotoxemia. American Journal of Veterinary Research. 1991;52:282-288. PMID: 2012339
  148. 148. Vanderwall DK. Early embryonic loss in the mare. Journal of Equine Veterinary Science. 2008;28:691-702. DOI: 10.1016/j.jevs.2008.10.001
  149. 149. Pycock J, Newcombe J. The effect of the gonadotrophin-releasing hormone analog, buserelin, administered in diestrus on pregnancy rates and pregnancy failure in mares. Theriogenology. 1996;46:1097-1101. DOI: 10.1016/s0093-691x(96)00274-9
  150. 150. Panzani D, Crisci A, Rota A, Camillo F. Effect of day of transfer and treatment administration on the recipient on pregnancy rates after equine embryo transfer. Veterinary Research Communications. 2009;33:113-116. DOI: 10.1007/s11259-009-9303-7
  151. 151. Willmann C, Schuler G, Hoffmann B, Parvizi N. Effects of age and altrenogest treatment on conceptus development and secretion of LH, progesterone and eCG in early-pregnant mares. Theriogenology. 2011;75:421-428. DOI: 10.1016/j.theriogenology.2010.05.009
  152. 152. Sieme JL, Sielhorst J, Martinsson G, Bollwein H, Thomas S, Burger D. Improving the formation and function of the corpus luteum in the mare. Revista Brasileira de Reprodução Animal. 2015;39:117-120. DOI: 10.5167/uzh-116508
  153. 153. Newcombe JR, Peters AR. The buserelin enigma: How does treatment with this GnRH analogue decrease embryo mortality? Journal of Veterinary Science and Technology. 2014;5:151. DOI: 10.4172/2157-7579.1000151
  154. 154. Stout TA, Tremoleda JL, Knaap J, Daels P, Kindahl H, Colenbrander B. Mid-diestrus GnRH-analogue administration does not suppress the luteolytic mechanism in mares. Theriogenology. 2002;58:567-570. DOI: 10.1016/S0093-691X(02)00860-9
  155. 155. Köhne M, Ille N, Erber R, Aurich C. Treatment with human chorionic gonadotrophin before ovulation increases progestin concentration in early equine pregnancies. Animal Reproduction Science. 2014;149:187-193. DOI: 10.1016/j.anireprosci.2014.07.002
  156. 156. Biermann J, Klewitz J, Otzen H, Martinsson G, Burger D, Meinecke-Tillmann S, et al. The effect of hCG, administered in diestrus, on luteal, ovarian and uterine blood flow, peripheral progesterone levels and pregnancy rates in mares. Journal of Equine Veterinary Science. 2014;34:166. DOI: 10.1016/j.jevs.2013.10.119
  157. 157. Shikichi M, Iwata K, Ito K, Miyakoshi D, Murase H, Sato F, et al. Abnormal pregnancies associated with deviation in progestin and estrogen profiles in late pregnant mares: A diagnostic aid. Theriogenology. 2017;98:75-81. DOI: 10.1016/j.theriogenology.2017.04.024
  158. 158. LeBlanc MM, Macpherson M, Sheerin P. Ascending placentitis: What we know about pathophysiology, diagnosis and treatment. In: Proceedings of the Annual Convention of the American Association of Equine Practitioners (AAEP); 4-8 December 2004; Denver, Colorado, USA. pp. 127-143
  159. 159. Morris S, Kelleman AA, Stawicki RJ, Hansen PJ, Sheerin PC, Sheerin BR, et al. Transrectal ultrasonography and plasma progestin profiles identifies feto-placental compromise in mares with experimentally induced placentitis. Theriogenology. 2007;67:681-691. DOI: 10.1016/j.theriogenology.2006.05.021
  160. 160. Wynn MAA, Ball BA, May J, Esteller-Vico A, Canisso I, Squires E, et al. Changes in maternal pregnane concentrations in mares with experimentally-induced, ascending placentitis. Theriogenology. 2018;122:130-136. DOI: 10.1016/j.theriogenology.2018.09.001
  161. 161. Brendemeuhl JP, Williams MA, Boosinger TR, Ruffin DC. Plasma progestagen, trioiodothyronine and cortisol concentrations in postdate gestation foals exposed in utero to the tall fescue endophyte Acremonium coenophialum. Biology of Reproduction. 1995;1:53-59. DOI: 10.1093/biolreprod/52.monograph_series1.53
  162. 162. Troedsson MHT, Miller LMJ. Equine placentitis. Pferdeheilkunde. 2016;32(1):49-53. DOI: 10.21836/PEM20160109
  163. 163. Bailey CS, Macpherson ML, Pozor MA, Troedsson MH, Benson SM, Giguere S, et al. Treatment efficacy of trimethoprim sulfamethoxazole, pentoxifylline and altrenogest in experimentally induced equine placentitis. Theriogenology. 2010;74:402-412. DOI: 10.1016/j.theriogenology.2010.02.023
  164. 164. Graczyk J, Macpherson ML, Pozor MA, Troedsson MHT, Eichelberger AC, LeBlanc MM, et al. Treatment efficacy of trimethoprim sulfamethoxazole and pentoxifylline in equine placentitis. Animal Reproduction Science. 2006;94:434-435. DOI: 10.1016/j.theriogenology.2010.02.023
  165. 165. LeBlanc MM. Ascending placentitis in the mare: An update. Reproduction in Domestic Animals. 2010;45:28-34. DOI: 10.1111/j.1439-0531.2010.01633.x
  166. 166. Canisso IF, Ball BA, Esteller-Vico A, Williams NM, Squires EL, Troedsson MH. Changes in maternal androgens and oestrogens in mares with experimentally induced ascending placentitis. Equine Veterinary Journal. 2017;49(2):244-249. DOI: 10.1111/evj.12556
  167. 167. Kasman LH, Hughes JP, Stabenfeldt GH, Starr MD, Lasley BL. Estrone sulfate concentrations as an indicator of fetal demise in horses. American Journal of Veterinary Research. 1988;49(2):184-187. PMID: 2831761
  168. 168. Santschi EM, LeBlanc MM, Weston PG. Progestagen, oestrone sulphate and cortisol concentrations in pregnant mares during medical and surgical disease. Journal of Reproduction and Fertility. Supplement. 1991;44:627-634. PMID: 1665522
  169. 169. Douglas RH. Endocrine diagnostics in the broodmare: What you need to know about progestins and estrogens. In: Annual Meeting for the Society for Theriogenology and American College of Theriogenologists; 4-7 August, 2004; Lexington, KY. pp. 106-115
  170. 170. Esteller-Vico A, Ball BA, Troedsson MHT, Squires EL. Endocrine changes, fetal growth, and uterine artery hemodynamics after chronic estrogen suppression during the last trimester of equine pregnancy. Biology of Reproduction. 2017;96:414-423. DOI: 10.1095/biolreprod.116.140533
  171. 171. Curcio BR, Canisso IF, Pazinato FM, Borba LA, Feijo LS, Muller V, et al. Estradiol cypionate aided treatment for experimentally induced ascending placentitis in mares. Theriogenology. 2017;102:98-107. DOI: 10.1016/j.theriogenology.2017.03.010
  172. 172. Ryan PL, Christiansen DL, Hopper RM, Bagnell CA, Vaala WE, LeBlanc MM. Evaluation of systemic relaxin blood profiles in horses as a means of assessing placental function in high-risk pregnancies and responsiveness to therapeutic strategies. Annals of the New York Academy of Sciences. 2009;1160:169-178. DOI: 10.1111/j.1749-6632.2008.03802.x
  173. 173. Christensen BW, Troedsson MHT, Murchie TA, Pozor MA, Macpherson ML, Estrada AH, et al. Management of hydrops amnion in a mare resulting in birth of a live foal. Journal of the American Veterinary Medical Association. 2006;228:1228-1233. DOI: 10.2460/javma.228.8.1228
  174. 174. Klein C. The role of relaxin in mare reproductive physiology: A comparative review with other species. Theriogenology. 2016;86:451-456. DOI: 10.1016/j.theriogenology.2016.04.061
  175. 175. LeBlanc MM, Giguere S, Lester GD, Bauer K, Paccamonti L. Relationship between infection, inflammation and premature parturition in mares with experimentally induced placentitis. Equine Veterinary Journal. Supplement. 2012;41:8-14. DOI: 10.1111/j.2042-3306.2011.00502.x
  176. 176. Lyle SK. Immunology of infective preterm delivery in the mare. Equine Veterinary Journal. 2014;46:661-668. DOI: 10.1111/evj.12243
  177. 177. Lyle SK, Hague M, Lopez MJ, Beehan DP, Staempfil S, Len JA, et al. In vitro production of cortisol by equine fetal adrenal cells in response to ACTH and IL-1b. Animal Reproduction Science. 2010;121:322. DOI: 10.1016/j.anireprosci.2010.04.127
  178. 178. Canisso IF, Ball BA, Erol E, Squires EL, Troedsson MHT. Comprehensive review on equine placentitis. In: Proceedings of the 61st Annual Convention of the American Association of Equine Practitioners (AAEP); 5-9 December 2015; Las Vegas, Nevada, USA. pp. 490-509

Written By

Katy Satué and Juan Carlos Gardon

Submitted: September 9th, 2019 Reviewed: November 5th, 2019 Published: June 10th, 2020