Abstract
Equine protozoal myeloencephalitis (EPM) remains an important neurologic disease of horses. There are no pathognomonic clinical signs for the disease. Affected horses can have focal or multifocal central nervous system (CNS) disease. EPM can be difficult to diagnose antemortem. It is caused by either of 2 parasites, Sarcocystis neurona and Neospora hughesi, with much less known about N. hughesi. Although risk factors such as transport stress and breed and age correlations have been identified, biologic factors such as genetic predispositions of individual animals, and parasite‐specific factors such as strain differences in virulence, remain largely undetermined. This consensus statement update presents current published knowledge of the parasite biology, host immune response, disease pathogenesis, epidemiology, and risk factors. Importantly, the statement provides recommendations for EPM diagnosis, treatment, and prevention.
Keywords: Encephalitis, Equine myeloencephalopathy, Equine neurologic, Equine protozoal disease, Myelitis, Neospora hughesi, Sarcocystis neurona
Abbreviations
- BBB
blood–brain barrier
- CNS
central nervous system
- CSF
cerebrospinal fluid
- CVSM
cervical vertebral stenotic myelopathy
- ELISA
enzyme‐linked immunosorbent assay
- EMND
equine motor neuron disease
- EPM
equine protozoal myeloencephalitis
- FDA
Food and Drug Administration
- IFAT
indirect fluorescent antibody test
- PYR
pyrimethamine
- SAG
surface antigen
- SDZ
sulfadiazine
- Se
sensitivity (of a diagnostic test)
- SIG
special interest group
- Sp
specificity (of a diagnostic test)
- WB
Western blot
Parasite Biology and Disease Pathogenesis
EPM was initially called “segmental myelitis” by Rooney in Kentucky in 1970.1 The syndrome was renamed “focal encephalitis‐myelitis” because of brain involvement. Prickett, Rooney, and others described 44 cases of the disease in 19682 and 52 cases of the disease in 19701 at the annual meeting of the American Association of Equine Practitioners (AAEP). Protozoa were first observed in association with characteristic lesions in 1974,3, 4 and the disease was given its current name, equine protozoal myeloencephalitis by Mayhew et al., who reported on 45 cases at the AAEP meeting in 1976.5 It is now well established that EPM can be caused by either Sarcocystis neurona 6 or Neospora hughesi, 7, 8, 9, 10, 11 although the majority of cases are because of infection with S. neurona.
Sarcocystis neurona has a 2‐host life cycle that alternates between the definitive host, and any of multiple mammal intermediate hosts. The opossum Didelphis virginiana is the definitive host for S. neurona in North America.12 As well, South American opossums can act as definitive hosts for S. neurona in the southern hemisphere.13 Sexual reproduction by the parasite in the intestinal epithelium of the infected opossum results in the production of sporozoite‐containing sporocysts that are passed in the feces. The sporozoites are infectious for the intermediate hosts, which include skunks,14 raccoons,15 armadillos,16 and cats.17 S. neurona forms latent sarcocysts in the muscle tissue of the intermediate host; sarcocyst‐laden muscle is the source of infection for the opossum. Opossums are commonly infected with S. neurona 18 and can generate significant contamination of the environment in locations which they frequent.
Horses are infected with S. neurona by ingesting food or water that has been contaminated with feces from an infected opossum. Although S. neurona sarcocysts were described in 1 case of a 4‐month‐old foal with clinical signs of EPM,19 it is unlikely that horses are normal intermediate hosts that contribute to the parasite's life cycle as S. neurona sarcocysts are not found typically in tissues of these animals and equine carcasses are seldom accessible to opossums. Importantly, S. neurona is not transmitted horizontally between horses, nor can it be transmitted to horses from nonequine intermediate hosts. Antibodies against S. neurona in foals before suckling have been reported,20, 21 but vertical transmission of this parasite in horses is probably uncommon. Thus, opossums are the major source of S. neurona infection for horses. The exact mechanisms by which S. neurona enters the CNS are not known, but are thought to involve either infection of endothelial cells or leukocytes.22, 23, 24, 25
The complete life cycle of N. hughesi is unknown, so all mode(s) of transmission of this parasite to horses remain poorly understood. Canids are a definitive host for the related species Neospora caninum, 26 but it has not been established that dogs or wild canids are a definitive host for N. hughesi. Vertical transmission of N. caninum is very efficient in cattle, and several recent studies indicate that N. hughesi can be transmitted transplacentally in horses.27, 28
All horses are believed to be susceptible to EPM, but it is clear that not all horses that are infected with S. neurona or N. hughesi will develop disease. Studies in both mice and horses experimentally infected with S. neurona have demonstrated a critical role for the immune response in preventing disease.29, 30, 31, 32 Additionally, some EPM‐affected horses have demonstrated altered immune responses, some of which are antigen‐specific.25, 33, 34, 35 As is clear from the finding that not all horses have demonstrated decreased immune responses with the methodology employed, the mechanisms involving the development of disease remain poorly understood.
It is unclear what influences the progression to severe neurologic disease. Factors such as variations in protozoal inoculum and stress‐induced immune suppression have been implicated in the occurrence of EPM.36, 37, 38 However, efforts to increase stress (ie, by additional transport of infected horses) and treatment with immunosuppressive steroids did not cause a concomitant increase in disease severity.39, 40 Genetic variation has been observed among the strains of S. neurona that have been analyzed,41, 42, 43 and there is some evidence that specific parasite genotypes may be particularly virulent in marine mammals.44 However, such an association was not apparent in isolates from horses suffering from EPM.
Epidemiology and Risk Factors
A survey using postmortem data from 10 diagnostic centers throughout the United States and Canada found that a majority of EPM cases (61.8%) occurred in horses that were 4 years old or less, whereas only 19.8% of the EPM cases reviewed were in horses 8 years or older.45 Thoroughbreds, Standardbreds, and Quarter Horses were most commonly observed, but no sex or seasonal bias could be established. A smaller retrospective study of 82 horses with histologic lesions compatible with EPM suggested that EPM risk was highest among male Standardbreds.46 The mean age of affected horses was 3.6 ± 2.8 years, similar to that found by Fayer et al.45
The seroprevalence of S. neurona in horses from the United States has varied widely, ranging from as low as 15% to a high of 89%, depending on geographic location.47, 48, 49, 50, 51 Seroprevalences of 35.6% and 35.5% have been observed in horses in Brazil and Argentina, respectively,52, 53 thus indicating that this parasite commonly infects horses in South America.
In general, the seroprevalence of N. hughesi is low in horses. Serum antibodies against N. hughesi have been reported in more than 10% of horses in some geographic regions,7, 54, 55, 56, 57, 58 whereas other studies found antibodies against N. hughesi in much lower proportions of horses (ie, <3%).52, 53, 59, 60, 61, 62 Some of the variation may be because of geographic differences, but studies that used Western blot to confirm serologic results have suggested that seroprevalence to N. hughesi is commonly overestimated.57, 59, 62
A survey reported in 2001 by the National Animal Health Monitoring System (NAHMS) estimated that the annual incidence of EPM in horses 6 months of age or older was 14 ± 6 cases per 10,000 horses.63 While it is now known that N. hughesi can cause neurologic disease in horses,7, 8, 9, 10, 11 the proportion of EPM cases attributable to this parasite species remains uncertain.
EPM usually occurs sporadically and seldom involves more than 1 horse on a farm,5, 64 although clusters of cases can occur.65, 66 A retrospective study found that young horses (1–5 years) and older horses (>13 years) had a higher risk of developing EPM,67 as observed previously. EPM occurred the least in the winter, with the risk 3 times higher in spring and summer and 6 times higher in the fall. On a given premise, the presence of opossums (2.5‐fold), previous diagnosis of EPM (2.5‐fold), and the presence of wooded areas (2‐fold) were also associated with increased risk of EPM. The likelihood of EPM was reduced by one third when wildlife was prevented access to feed and by one‐half when a creek or river was present as a water source.
Immune suppression because of stress or advanced age might predispose a horse to development of EPM.36 Stressful events such as heavy exercise, transport, injury, surgery, or parturition have all been found to increase the risk of EPM.67 Racehorses and show horses had a higher risk of developing EPM compared to breeding and pleasure horses. Not surprisingly, horses with EPM that were treated with an anticoccidial drug were 10 times more likely to improve than untreated horses.36
Clinical Signs
Clinical signs of EPM vary from acute to chronic with insidious onset of focal or multifocal signs of neurologic disease involving the brain, brainstem, or spinal cord.64 Initial signs might include dysphagia, evidence of abnormal upper airway function, unusual or atypical lameness, or even seizures.68 Severely affected horses might have difficulty standing, walking, or swallowing and the disease can progress very rapidly. Occasionally, the clinical signs stabilize, only to relapse days or weeks later.
The variability of clinical signs is because of infection of both white and gray matter at multiple sites in the CNS. Signs of gray matter involvement include focal muscle atrophy and severe muscle weakness, whereas damage to white matter frequently results in ataxia and weakness in limbs caudal to the site of infection. Early signs of EPM such as stumbling and frequent interference between limbs can be confused with lameness. Horses affected with EPM commonly exhibit a gradual progression in severity and range of clinical signs. In some cases, however, a gradual onset can give way to a sudden exacerbation in the severity of clinical illness, resulting in recumbency.
The vital signs in affected horses are usually normal and animals appear bright and alert. Some horses with EPM appear thin and mildly obtunded. Neurologic examination often reveals asymmetric ataxia, weakness, and spasticity involving all 4 limbs. Areas of hyporeflexia, hypalgesia, or complete sensory loss are occasionally present. The most common signs of brain/brainstem disease include obtundation, head tilt, facial nerve paralysis, and difficulty in swallowing, although signs are not necessarily limited to these areas.69
Recommendations for EPM Diagnosis
Definitive diagnosis of EPM requires postmortem confirmation of protozoal infection of the CNS (see below). For highest accuracy in antemortem diagnosis, the following steps are recommended. (1) The presence of clinical signs consistent with EPM should be confirmed by conducting a thorough neurologic examination. (2) Other potential causes should be ruled out using available tools (eg, cervical radiography). (3) Immunodiagnostic testing of serum and CSF should be conducted to confirm intrathecal antibody production against S. neurona or N. hughesi. The ratio of antibody in serum to CSF will reveal intrathecal antibodies in most cases of EPM. The Goldman‐Witmer coefficient (C‐value) or the antigen‐specific antibody index (AI) should be applied for cases that have ELISA titer results that are equivocal (ie, the serum:CSF ratio equals the cut‐off) or when a condition that compromises the blood–brain barrier is suspected. The SnSAG2, 4/3 ELISA serum:CSF titer ratio and NhSAG1 ELISA serum:CSF titer ratio are the only tests currently offered commercially that provide information regarding intrathecal antibody production based on serum and CSF titers. The commercially available S. neurona and N. hughesi IFATs do determine antibody titers in both the serum and CSF, but the laboratory does not calculate ratios at this time.
Basis for Recommendations
In horses with clinical signs consistent with CNS disease, EPM should be considered as a differential. Affected horses should initially have a thorough neurologic examination to identify abnormalities, and localize the lesion(s), which will allow one to further refine the differentials. This, combined with the use of appropriate diagnostic tests, will assist in diagnosing EPM and ruling out other causes. Some of the most consistent/classic clinical signs include asymmetric gait and focal muscle atrophy. When these signs are present, EPM should be considered as a top differential diagnosis. EPM‐affected horses are not painful, and rarely febrile, unless comorbidities exist.
Differential Diagnoses
Almost all neurologic diseases in horses can have clinical signs that are also present in EPM‐affected horses. A thorough neurologic examination and diagnostic tests are needed to distinguish between EPM and other differentials. Some diseases have other more consistent/classic signs that allow one to rule them in or out. With cervical vertebral stenotic myelopathy (CVSM), signs usually are symmetric and, typically, the pelvic limbs are more severely affected than the thoracic limbs. Focal muscle atrophy is not common. Trauma should also be considered as a differential cause of spinal cord damage at any level, potentially causing abnormal neurologic signs in 1 to all limbs.
In horses where there is a history of respiratory disease or an outbreak of abortion, EHV‐1‐associated neurologic disease should be considered as a more likely differential. EHV‐1‐affected horses may be febrile shortly before or at the onset of neurologic signs. In the EHV‐1‐affected horses, neurologic signs typically manifest as symmetric, with primary pelvic limb weakness and ataxia, bladder distention, usually without incontinence, and, more rarely, perineal hypalgesia, tail paralysis, fecal retention and in some cases incontinence as well. Some affected horses show rapidly progressing signs of ataxia and can sometimes have cranial nerve deficits, often involving cranial nerves VII to XII. In other cases, cerebral signs occur.
Another disease which should be considered as a differential diagnosis is equine motor neuron disease (EMND). Affected horses with early stages of disease typically have severe limb weakness with muscle fasciculations and tremors. Horses with chronic EMND can have widespread, profound, muscle atrophy.
Other differentials of spinal cord disease that can result in similar clinical signs include extradural and spinal cord tumors, epidural abscess, migrating metazoan parasites, rabies, West Nile viral encephalomyelitis, equine degenerative myeloencephalopathy/neuroaxonal dystrophy, lead poisoning, creeping indigo toxicity, Lyme neuro‐borreliosis, vascular malformations, and discospondylopathies. If affected horses have signs of cranial nerve or brain involvement, EPM should be considered as a differential. Other rule outs include viral encephalomyelitides, neoplasia, head trauma, brain abscess, migrating parasites, temporohyoid osteoarthropathy, polyneuritis equi, cholesterol granuloma, metabolic derangement, and hepatoencephalopathy.
Postmortem Diagnosis
Confirmation of EPM on postmortem examination is based on demonstration of protozoa in CNS lesions, although the diagnosis frequently is made presumptively even when parasites are not detected if the characteristic inflammatory changes are found. In 2 reported series, organisms were seen in H&E sections of CNS tissue in 10 to 36% of suspected cases.46, 70 Sensitivity was increased from 20 to 51% by immunohistochemical staining with antibody against S. neurona.70 Although it has not been demonstrated experimentally, the use of PCR to detect parasites in CNS tissues might aid postmortem diagnosis of EPM. There is decreased likelihood of finding parasites histologically in tissues from affected EPM horses that have been treated with antiprotozoal drugs.46
Immunodiagnostic Testing
Overview
There are several immunodiagnostic tests currently in use for EPM diagnosis. Importantly, these tests are an adjunct to diagnosis and not the mainstay. Performing serology as part of a general health screen or prepurchase examination is discouraged because of the very low positive predictive value when a nonneurologic horse is tested. In horses showing gait deficits, EPM serology should not be used to distinguish whether the deficits are caused by CNS or musculoskeletal disease. Presence or absence of neurologic disease is determined by the clinical examination, and serology can then help refine the differential diagnoses list for a neurologic horse.
All commonly used tests are based on detection of antiprotozoal antibodies in serum, CSF, or both. As EPM occurs only in a small proportion of horses infected with S. neurona, 63 testing for serum antibodies against S. neurona has minimal diagnostic value unless the serologic results are negative (low positive predictive value but high negative predictive value).71, 72 However, detection of serum antibodies against N. hughesi in a neurologic horse has a higher positive predictive value because of a much lower seroprevalence. A negative serum test usually indicates that the horse has not been infected and alternative diagnoses should be pursued or that the EPM‐suspect horse resides in a geographic area of low exposure to the infecting parasite. However, a recently infected horse might display clinical signs before seroconversion, and repeated serologic testing in 10–14 days is indicated for horses with recent development of compatible clinical signs. Detection of antibodies in the CSF is more informative, but alone is not a definitive indicator of EPM as there is passive transfer of antibody across a healthy blood–brain barrier (BBB).73 Additionally, blood contamination of CSF samples can cause false‐positive results.74, 75, 76 Logically, horses with higher serum titers are more likely to have detectable antibody levels in CSF in both of these circumstances.
Use of quantitative assays to detect intrathecal antibody production, indicating active parasite infection in the CNS, provides an accurate approach for EPM diagnosis. The Goldman‐Witmer coefficient (C‐value) and the antigen‐specific antibody index (AI) are tests of proportionality that assess whether the amount of pathogen‐specific antibody in the CSF is greater than should be present from normal passive transfer across the BBB. These methods have been used in human medicine to diagnose CNS infections caused by a variety of pathogens,77, 78, 79 including the apicomplexan T. gondii.80, 81 The value of these tests for EPM diagnosis was demonstrated initially with a sample set of 29 clinical cases.75 This study also showed that minor blood contamination of the CSF sample (ie, up to 10,000 red cells per μL) will not confound the assay results. Subsequently, 2 additional studies examining a more extensive collection of horses with neurologic disease showed that a simple serum:CSF antibody titer ratio was sufficient in many cases for an accurate diagnosis of EPM caused by S. neurona.71, 72 Although use of a serum:CSF titer ratio should be equally effective for diagnosis of EPM caused by N. hughesi, an optimal serum:CSF titer ratio cut‐off needs to be established.
Available tests for EPM caused by S. neurona
Numerous serologic tests have become available during the past 2 decades to aid in the diagnosis of EPM caused by S. neurona, including Western blot (WB), indirect fluorescent antibody test (IFAT), and surface antigen (SAG) enzyme‐linked immunosorbent assays (ELISAs). Descriptions of testing options and reported test performance are shown in Table 1.71, 72, 82, 83, 84, 85, 86, 87, 88, 89, 90, 91, 92, 93 All tests can be performed on serum or CSF, and none is considered a gold standard. The WB, the first immunodiagnostic test described for EPM, is a qualitative test for antibodies against merozoite lysate. Its use has largely been supplanted by more quantitative tests, and positive WB results have limited diagnostic utility. However, negative WB results retain a high negative predictive value. The IFAT is a quantitative (end‐point titer) test for antibodies against culture‐derived whole merozoites. Although serum titers obtained with the IFAT have been used to predict the likelihood of EPM, with higher titers suggesting greater probability of disease, studies that have used diverse collections of neurologic disease cases have shown that a serum titer alone is a poor predictor of EPM.71, 72 As a quantitative test, the IFAT can be used to calculate a serum:CSF titer ratio. However, this information is not routinely provided by the laboratory.
Table 1.
Test | Laboratory | Interpretation | Reported performance | ||
---|---|---|---|---|---|
Sample | Sensitivity (%) | Specificity (%) | |||
WB87 | EDS | Band pattern read and interpreted visually (subjective) | Serum | 8993, 8082, 8983 | 7193, 3882, 8783 |
UC Davis IDEXX |
Results usually reported as negative, weak positive, low positive, or positive | CSF | 8993, 8782 | 8993, 4482 | |
mWB90 | Michigan State | Similar to standard WB (above) | Serum | 10090, 8983 | 9890, a, 6983 (a n.b., negative cases not from North America) |
IFAT83 | UC Davis | Serum positive at ≥1:80 has ≥55% probabilitya of EPM | Serum | 8983, 8384, 9489, 5971 | 10083, 9784, 8589, 7171 |
Serum negative at ≤1:40 has ≤33% probabilitya of EPM | CSF | 10084, 9289, 6571 | 9984, 9089, 9871 | ||
CSF positive at ≥1:5 has 92% probabilitya of EPM | Serum:CSF titer ratio | 6571 | 9871 | ||
SAG1 ELISA86 | Antech | Serum positive at ≥1:16 but recommended cutoff ≥1:32 | Serum | 6888, 1389 | 7188, 9789 |
SAG2, 4/3 ELISA91 | EDS | Serum positive for exposure at ≥1:250 | Serum | 30–86 (depending on cutoff)72, 7171 | 37–88 (depending on cutoff)72, 5071 |
CSF correlates well with EPM if ≥1:40 | CSF | 77–96 (depending on cutoff)72, 8871 | 58–96 (depending on cutoff)72, 8671 | ||
Serum:CSF titer ratio very predictive of EPM if ≤100 | Serum:CSF titer ratio | 86 (cutoff ≤50) or 93 (cutoff ≤100)72, 8871 | 96 (cutoff ≤50) or 83 (cutoff ≤100)72, 10071 | ||
SAG1, 5, 6 ELISA92 | Pathogenes | Serum positive at ≥1:8, indicating infection | Serum | N/A | N/A |
WB, Western blot; mWB, modified Western blot; IFAT, indirect fluorescent antibody test; SAG, surface antigen; ELISA, enzyme‐linked immunosorbent assay; EDS, Equine Diagnostic Solutions (Lexington, KY); UC Davis, University of California at Davis; EPM, equine protozoal myeloencephalitis; CSF, cerebrospinal fluid.
Based on pretest probability of 10%; see reference 85.
Most recent research has focused on the SAG ELISAs, quantitative (end‐point titer) tests based on S. neurona surface antigens. These molecules have proven to be good serologic targets in the assays because of their high level of expression in the parasite and their immunogenicity in infected horses.94, 95, 96 The SnSAG2 ELISA and the SnSAG4/3 ELISA accurately detect antibodies against S. neurona in equine serum and CSF samples88, 91 and were used to demonstrate the value of detecting intrathecal antibody production for EPM diagnosis.71, 72 An ELISA based on the SnSAG1 surface protein has been described.86 However, this antigen is not expressed by all strains of S. neurona,43 thereby reducing its utility for serologic detection88 and EPM diagnosis.89 An ELISA combining SnSAG1 with 2 additional SnSAGs (SnSAG5 and SnSAG6) is currently offered. However, no published reports describe validation of this assay, so it is unclear whether the test reliably detects antibodies to S. neurona.
Several studies have directly compared different tests for EPM (caused by S. neurona infection);71, 83, 89 these publications and 3 unpublished studies presented at ACVIM EPM Society SIGs97, 98, 99 are detailed in Table 2.71,83,89,97, 98, 99 Although none of the studies examined all of the currently available tests, and the types of samples utilized were variable, some general conclusions are evident. Testing serum alone yielded less accurate results than testing CSF alone or a serum:CSF titer ratio, generally because of low specificity. One notable exception was the SAG1 ELISA, which showed poor sensitivity. Poor to fair test agreement was observed; samples that were split and submitted to multiple labs often had discrepant results. Three of the 6 comparison studies evaluated the SAG2, 4/3 ELISA serum:CSF titer ratio; in all 3 studies this test demonstrated the highest overall accuracy as compared to the WB, IFAT, and SAG1 ELISA. However, the SAG1, 5, 6 ELISA has not yet been evaluated in any comparison study, so its performance is currently unknown.
Table 2.
References | Tests (and samples) compared | Sample origin | Results | Author conclusions |
---|---|---|---|---|
Duarte et al. (2003)83 |
|
|
|
IFAT accuracy was better than WB tests. |
Saville (2007)99 |
|
|
|
WB and IFAT were most accurate, though IFAT was cross‐reactive with S. fayeri. mWB tended to have false‐positive results, whereas SAG1 ELISA tended to have false‐negative results. |
Johnson et al. (2010)89 |
|
|
|
Low Se limited the usefulness of the SAG1 ELISA. |
Reed et al. (2010)97 |
|
|
|
SAG2, 4/3 ELISA serum:CSF ratio was the most accurate. |
Renier et al. (2012)98 |
|
|
|
IFAT advantages include testing for N. hughesi and use as serum stand‐alone test. (n.b., SAG2, 4/3 ELISA serum:CSF ratio had higher overall accuracy.) |
Johnson et al. (2013)71 |
|
|
|
Serum testing alone was least accurate; more accurate methods should be used. SAG2, 4/3 ELISA serum:CSF ratio was most accurate. |
ACVIM, American College of Veterinary Internal Medicine; EPM, equine protozoal myeloencephalitis; SIG, special interest group; WB, Western blot; mWB, modified Western blot; IFAT, indirect fluorescent antibody test; SAG, surface antigen; ELISA, enzyme‐linked immunosorbent assay; Se, test sensitivity; Sp, test specificity; CSF, cerebrospinal fluid.
Available tests for EPM caused by N. hughesi
Two serologic assays are currently offered for measuring antibodies against N. hughesi in equine samples (Table 3). An ELISA based on the major parasite surface antigen NhSAG162 is available from Equine Diagnostic Solutions, LLC, whereas an IFAT using whole N. hughesi tachyzoites is offered by the School of Veterinary Medicine, University of California‐Davis, Veterinary Immunology Laboratory. Based on analysis of 1006 random equine samples, the NhSAG1 ELISA provides an estimated 94% sensitivity and 95% specificity for detecting antibodies against N. hughesi when compared to Western blot results. The N. hughesi IFAT sensitivity and specificity for detecting antibodies against N. hughesi was reported to be 100% and 71.4%, respectively, at a cut‐off of 1:320.100 These values were based on samples from 3 naturally infected, 7 experimentally infected, and 7 naïve horses. Of note, neither the N. hughesi IFAT nor the NhSAG1 ELISA have been fully validated for EPM diagnosis because of an inadequate number of samples from EPM cases caused by this parasite.
Table 3.
Test | Laboratory | Interpretation | Reported performance |
---|---|---|---|
IFAT100 | UC Davis |
|
|
ELISA62 | EDS |
|
|
IFAT, indirect fluorescent antibody test; ELISA, enzyme‐linked immunosorbent assay; UC Davis, University of California at Davis; EDS, Equine Diagnostic Solutions (Lexington, KY); CSF, cerebrospinal fluid; EPM, equine protozoal myeloencephalitis; Se, sensitivity; Sp, specificity; WB, Western blot.
Recommendations for EPM Treatment and Prevention
For treatment of EPM, it is recommended that 1 of the FDA‐approved anticoccidial drugs should be used to control infection. The current FDA‐approved drugs are: a) Ponazuril (Marquis®; Merial, Inc., Duluth, Georgia, 30096, USA); b) Diclazuril (Protazil®; Merck Animal Health, Madison, NJ, 07940, USA); and c) Sulfadiazine/Pyrimethamine (eg, ReBalance®; PRN Pharmacal, Pensacola, Florida, 32514, USA). Additional medical and supportive treatment should be provided based on the severity of neurologic deficits and complications arising from them.
Basis for Recommendations
Folate‐Inhibiting Drugs
A combination of sulfadiazine and pyrimethamine (SDZ/PYR) was 1 of the initial treatment for EPM. Sulfonamides and pyrimethamine act synergistically by interfering with folic acid metabolism and biosynthesis of purine and pyrimidine nucleotides necessary for the parasite's survival.
A dosage regimen of PYR, 1 mg/kg PO q24 h, and SDZ, 20 mg/kg PO q24 h for up to 6 months was the earliest treatment for EPM. As dietary folate can interfere with the uptake of diaminopyrimidine drugs like PYR,101 hay should not be fed for 2 hours before or after treatment. PYR given PO to horses at 1 mg/kg/d achieves a concentration of approximately 0.02 to 0.10 μg/mL in the CSF 4–6 h after administration.102 These experimental horses were allowed free access to prairie hay, potentially reducing the bioavailability of the drug.101 One of the PK characteristics is that steady‐state CSF concentrations of PYR can be obtained after 4–6 hours after a single PO administered dose at 1 mg/kg/d. Further, short half‐lives of these compounds suggest that there will be large fluctuations between peak and trough concentrations in the CSF after single daily administration. Additionally, as PYR is concentrated in CNS tissue relative to plasma,103 the concentration at the desired site of action might be >0.1 μg/mL. Mean peak CSF concentrations of sulfonamide after single or multiple dosing (22–44 mg/kg) have been reported to be approximately 2–8 μg/mL.104 These drugs are available as an FDA‐approved product (ReBalance®; PRN Pharmacal). Treatment efficacy determined by clinical improvement (2 or more improvement grades in the overall neurologic dysfunction) or reversion to a CSF negative status for S. neurona by immunoblot after 90 days of treatment showed success in 60–70% of treated horses.105
The toxic effects of these drugs relate to the inhibition of folate synthesis and include bone marrow suppression, anorexia, urticaria, and self‐limiting diarrhea.102, 106 Typically, there is progressive mild anemia (PCV in the low 20s) over a 6‐month treatment period; neutropenia and thrombocytopenia can be seen in some cases as well. Pyrimethamine is teratogenic, causing abortions in rats and congenital defects in pups.107 In addition, mares treated with pyrimethamine in late pregnancy had a fatal syndrome observed in the foals.108 Of the 4 mares, 3 had been supplemented with folic acid. In other species, folic acid supplementation will not prevent PYR‐induced toxicosis109 or can even exacerbate it.107 Therefore, the use of folic acid in EPM‐affected horses treated with PYR cannot be justified.
Benzeneacetonitrile Drugs
Diclazuril and ponazuril, 2 members of the benzeneacetonitrile group of compounds, have been approved by the FDA for treatment of EPM (US FDA, Protazil® antiprotozoal oral pellets. 1.56% diclazuril. Freedom of Information Summary; US FDA, Marquis™ antiprotozoal oral paste. 15% w/w ponazuril. Freedom of Information Summary). With demonstrated broad‐spectrum anticoccidial activity in many avian and mammalian species, these drugs are related to the herbicide atrazine and are thought to target the parasite's apicoplast organelle.110 The activity of benzeneacetonitrile compounds against S. neurona and N. caninum was initially shown in vitro.111, 112, 113 In horses, pharmacokinetic studies have established that therapeutic steady‐state concentrations of both diclazuril and ponazuril are achieved by day 7 using labeled doses.114, 115, 116 Moreover, use of a loading dose of ponazuril at 15 mg/kg resulted in steady‐state concentrations in blood and CSF by day 2.117 Furthermore, the concurrent administration of vegetable oil (1/2 cup) has shown to increase the bioavailability of the FDA‐approved ponazuril product up to 15% (M. Furr, unpublished observations). A loading dose for the FDA‐approved diclazuril product is not required and use of vegetable oil does not increase its bioavailability (Hunyadi, unpublished observations). The FDA‐approved benzeneacetonitrile compounds exhibited efficacy ranging from 62 to 67% based on a neurologic examination improvement of 1 grade or becoming negative to antibodies against S. neurona in serum and CSF.118 Because ponazuril and diclazuril are highly selective against apicomplexan parasites, little to no toxicity is to be expected at therapeutic doses.119
Duration of treatment will mainly depend on response to antiprotozoal administration. While the FDA‐approved products are labeled for a treatment course of 28 days, the majority of horses with EPM are treated for a longer period of time, generally 6–8 weeks or longer if clinical improvement is still apparent under treatment. Discontinuation of antiprotozoal treatment should be based on neurologic improvement. At this time, antibody retesting in blood, CSF, or both is not recommended to determine discontinuation of antiprotozoal drug administration.
Supportive Medical Treatment
Nonsteroidal anti‐inflammatory drugs such as flunixin meglumine are frequently given to moderately or severely affected horses during the first 3–7 days of antiprotozoal treatment and in an attempt to prevent worsening of neurologic deficits during the early antiprotozoal treatment. In the case of horses which are in danger of falling down or exhibit signs of brain involvement, the additional use of a short course of corticosteroids (0.1 mg/kg of dexamethasone once or twice daily) and dimethyl sulfoxide (1 g/kg as a 10% solution IV or by nasogastric tube once or twice daily) may control the inflammatory response and associated clinical signs. Because the damaged CNS is susceptible to oxidant injury, vitamin E (eg, 20 IU/kg daily per os) is often used as an adjunct antioxidant treatment; it remains to be determined experimentally whether this practice is beneficial.
Biologic Response Modifiers
Based on the assumption that horses that develop EPM may be immune compromised, immunomodulators have anecdotally been included by some in treatment of the disease. The drugs used include levamisole (1 mg/kg PO q12h for the first 2 weeks of antiprotozoal treatment and for the first week of each month thereafter), killed Propionibacterium acnes (Eqstim™; Neogen, Lansing, MI), mycobacterial wall extract (Equimune® IV; Bioniche Animal Health Vetoquinol, Belville, ON, Canada), inactivated parapox ovis virus (Zylexis, Zoetis, Florham Park, NJ), and transfer factor (4Life® Transfer Factor, 4LifeResearch, Sandy, UT). Because no studies have been conducted to evaluate their efficacy in EPM horses, no recommendations can be made.
Prevention of EPM
Preventative approaches to EPM can be achieved by decreasing stress along with reducing exposure to scat from opossums. Practical approaches such not feeding off the ground, providing separate sources of fresh water for horses and preventing wildlife access to horse pastures, paddocks, and stalls may also help reduce the incidence of protozoal infections in horses.
Intermittent use of coccidiostatic and coccidiocidal drugs is another approach used to prevent EPM. Two prophylactic studies have looked at the use of ponazuril after an experimental challenge.120, 121 Treatment at either 2.5 or 5.0 mg/kg PO q24h of ponazuril was administered beginning 7 days before experimental challenge and continued for 28 days.120 In that study, administration of ponazuril reduced clinical signs and delayed seroconversion. Intermittent ponazuril paste administration at 20 mg/kg PO every 7 days was associated with a significantly decreased intrathecal anti‐S. neurona antibody response in horses experimentally inoculated with S. neurona sporocysts.121 Collectively, these 2 studies showed that daily or intermittent treatment with ponazuril minimized but did not eliminate infection in horses experimentally infected with S. neurona. Recently, pharmacokinetics of daily low‐dose diclazuril (0.5 mg/kg PO q24h) given to adult healthy horses were investigated.116 Diclazuril pellets, given at a low‐dose, attained plasma and CSF concentrations known to inhibit S. neurona and N. caninum in cell culture. The daily administration of a low‐dose diclazuril pellet topdressing to healthy foals from a farm with a high exposure rate to S. neurona significantly reduced the monthly seroprevalence to S. neurona when compared to untreated foals.122 The authors of that study suggested that the reported difference in temporal seroprevalence between treated and untreated foals was likely because of the successful reduction of S. neurona infection in foals receiving a daily low‐dose diclazuril. This preventive strategy has the potential to be used in high‐risk horses in an attempt to reduce the incidence of EPM, although, future longitudinal studies will be required before establishing a standard protocol.
Future directions
While considerable progress has been made as the original EPM consensus statement in 2002, many questions remain unanswered. The highest priority areas identified by the EPM organizing committee include: (a) identifying whether S. neurona can establish a persistent but inapparent infection in the horse, (b) elucidating the nature of the immune response in protection and disease, (c) determining how S. neurona causes disease and whether organisms need to be present to cause pathologic changes and clinical signs, (d) elucidating whether S. neurona parasite genotype influences infection and severity of signs, (e) identifying whether co‐infection with other pathogens can be a contributing factor in EPM cases, (f) expanding the fundamental knowledge of N. hughesi as a cause of EPM, including identifying the definitive host, determining all modes of transmission and investigating the host‐pathogen relationship, including the protective immune response. The Committee urges support for the aforementioned projects as the knowledge gained from these studies will lead to earlier and more accurate diagnosis, preventive approaches and more efficacious treatments.
Summary
Based on the currently published information, it is recommended that horses with neurologic signs consistent with EPM, because of S. neurona or N. hughesi, have a thorough neurologic examination performed. With this information, neurologic deficits can be identified and the lesion(s) localized. Differentials can be developed and appropriate diagnostic testing can be performed to rule in EPM and rule out other diseases. Current recommendations are for serum and CSF testing for S. neurona, N. hughesi, or both to identify whether intrathecal antibody production is present. Treatment recommendations for EPM include an FDA‐approved treatment, as well as supportive care. Duration of treatment is based on resolution of clinical signs. Horses that develop recurrent signs should be reassessed. As more knowledge is elucidated on the virulence of S. neurona and N. hughesi and the immune phenotype is elicited, more accurate diagnose, more efficacious treatments, and better preventative approaches will be identified.
Acknowledgments
Conflict of Interest Declaration: Dr. Morrow works for Equine Diagnostic Solutions, LLC, Lexington, KY, that offers commercial diagnostic testing for S. neurona and N. hughesi. Dr. Pusterla works for the William R. Pritchard Veterinary Medical Teaching Hospital, School of Veterinary Medicine, University of California at Davis that offers commercial testing for S. neurona and N. hughesi.
Off‐label Antimicrobial Declaration: Authors declare no off‐label use of antimicrobials.
Consensus Statements of the American College of Veterinary Internal Medicine (ACVIM) provide the veterinary community with up‐to‐date information on the pathophysiology, diagnosis, and treatment of clinically important animal diseases. The ACVIM Board of Regents oversees selection of relevant topics, identification of panel members with the expertise to draft the statements, and other aspects of assuring the integrity of the process. The statements are derived from evidence‐based medicine whenever possible and the panel offers interpretive comments when such evidence is inadequate or contradictory. A draft is prepared by the panel, followed by solicitation of input by the ACVIM membership which may be incorporated into the statement. It is then submitted to the Journal of Veterinary Internal Medicine, where it is edited before publication. The authors are solely responsible for the content of the statements.
References
- 1. Rooney JR, Prickett ME, Delaney FM, et al. Focal myelitis‐encephalitis in horses. Cornell Vet 1970;60:494–501. [PubMed] [Google Scholar]
- 2. Prickett ME. Equine spinal ataxia. In: 14th Annual Convention of the American Association of Equine Practitioners, Philadelphia, PA 1968;147–148.
- 3. Cusick PK, Sells DM, Hamilton DP, et al. Toxoplasmosis in two horses. J Am Vet Med Assoc 1974;164:77–80. [PubMed] [Google Scholar]
- 4. Beech J, Dodd DC. Toxoplasma‐like encephalomyelitis in the horse. Vet Pathol 1974;11:87–96. [DOI] [PubMed] [Google Scholar]
- 5. Mayhew IG, De Lahunta A, Whitlock RH, et al. Equine protozoal myeloencephalitis. Proc Annu Conv Am Assoc Equine Pract 1977;22d:107–114. [Google Scholar]
- 6. Dubey JP, Davis SW, Speer CA, et al. Sarcocystis neurona n. sp. (Protozoa: Apicomplexa), the etiologic agent of equine protozoal myeloencephalitis. J Parasitol 1991;77:212–218. [PubMed] [Google Scholar]
- 7. Cheadle MA, Lindsay DS, Rowe S, et al. Prevalence of antibodies to Neospora sp. in horses from Alabama and characterisation of an isolate recovered from a naturally infected horse [corrected]. Int J Parasitol 1999;29:1537–1543. [DOI] [PubMed] [Google Scholar]
- 8. Dubey JP, Liddell S, Mattson D, et al. Characterization of the Oregon isolate of Neospora hughesi from a horse. J Parasitol 2001;87:345–353. [DOI] [PubMed] [Google Scholar]
- 9. Hamir AN, Tornquist SJ, Gerros TC, et al. Neospora caninum‐associated equine protozoal myeloencephalitis. Vet Parasitol 1998;79:269–274. [DOI] [PubMed] [Google Scholar]
- 10. Marsh AE, Barr BC, Madigan J, et al. Neosporosis as a cause of equine protozoal myeloencephalitis. J Am Vet Med Assoc 1996;209:1907–1913. [PubMed] [Google Scholar]
- 11. Lindsay DS, Steinberg H, Dubielzig RR, et al. Central nervous system neosporosis in a foal. J Vet Diagn Invest 1996;8:507–510. [DOI] [PubMed] [Google Scholar]
- 12. Fenger CK, Granstrom DE, Langemeier JL, et al. Identification of opossums (Didelphis virginiana) as the putative definitive host of Sarcocystis neurona . J Parasitol 1995;81:916–919. [PubMed] [Google Scholar]
- 13. Dubey JP, Lindsay DS, Kerber CE, et al. First isolation of Sarcocystis neurona from the South American opossum, Didelphis albiventris, from Brazil. Vet Parasitol 2001;95:295–304. [DOI] [PubMed] [Google Scholar]
- 14. Cheadle MA, Yowell CA, Sellon DC, et al. The striped skunk (Mephitis mephitis) is an intermediate host for Sarcocystis neurona . Int J Parasitol 2001;31:843–849. [DOI] [PubMed] [Google Scholar]
- 15. Dubey JP, Saville WJ, Stanek JF, et al. Sarcocystis neurona infections in raccoons (Procyon lotor): evidence for natural infection with sarcocysts, transmission of infection to opossums (Didelphis virginiana), and experimental induction of neurologic disease in raccoons. Vet Parasitol 2001;100:117–129. [DOI] [PubMed] [Google Scholar]
- 16. Cheadle MA, Tanhauser SM, Dame JB, et al. The nine‐banded armadillo (Dasypus novemcinctus) is an intermediate host for Sarcocystis neurona . Int J Parasitol 2001;31:330–335. [DOI] [PubMed] [Google Scholar]
- 17. Dubey JP, Saville WJ, Lindsay DS, et al. Completion of the life cycle of Sarcocystis neurona . J Parasitol 2000;86:1276–1280. [DOI] [PubMed] [Google Scholar]
- 18. Dubey JP. Prevalence of Sarcocystis species sporocysts in wild‐caught opossums (Didelphis virginiana). J Parasitol 2000;86:705–710. [DOI] [PubMed] [Google Scholar]
- 19. Mullaney T, Murphy AJ, Kiupel M, et al. Evidence to support horses as natural intermediate hosts for Sarcocystis neurona . Vet Parasitol 2005;133:27–36. [DOI] [PubMed] [Google Scholar]
- 20. Pivoto FL, de Macedo AG Jr, da Silva MV, et al. Serological status of mares in parturition and the levels of antibodies (IgG) against protozoan family Sarcocystidae from their pre colostral foals. Vet Parasitol 2014;199:107–111. [DOI] [PubMed] [Google Scholar]
- 21. Pusterla N, Mackie S, Packham A, et al. Serological investigation of transplacental infection with Neospora hughesi and Sarcocystis neurona in broodmares. Vet J 2014;202:649–650. [DOI] [PubMed] [Google Scholar]
- 22. Ellison SP, Greiner E, Brown KK, et al. Experimental infection of horses with culture‐derived Sarcocystis neurona merozoites as a model for equine protozoal myeloencephalitis. Int J Appl Res Vet Med 2004;2:79–89. [Google Scholar]
- 23. Lindsay DS, Mitchell SM, Yang J, et al. Penetration of equine leukocytes by merozoites of Sarcocystis neurona . Vet Parasitol 2006;138:371–376. [DOI] [PubMed] [Google Scholar]
- 24. Speer CA, Dubey JP, Mattson DE. Comparative development and merozoite production of two isolates of Sarcocystis neurona and Sarcocystis falcatula in cultured cells. J Parasitol 2000;86:25–32. [DOI] [PubMed] [Google Scholar]
- 25. Lewis S, Ellison S, Dascanio J, et al. Effects of experimental Sarcocystis neurona‐induced infection on immunity in an equine model. J Vet Med 2014; doi: 10.1155/2014/239495 (16 pages). [DOI] [PMC free article] [PubMed] [Google Scholar]
- 26. McAllister MM, Dubey JP, Lindsay DS, et al. Dogs are definitive hosts of Neospora caninum . Int J Parasitol 1998;28:1473–1478. [PubMed] [Google Scholar]
- 27. Antonello AM, Pivoto FL, Camillo G, et al. The importance of vertical transmission of Neospora sp. in naturally infected horses. Vet Parasitol 2012;187:367–370. [DOI] [PubMed] [Google Scholar]
- 28. Pusterla N, Conrad PA, Packham AE, et al. Endogenous transplacental transmission of Neospora hughesi in naturally infected horses. J Parasitol 2011;97:281–285. [DOI] [PubMed] [Google Scholar]
- 29. Dubey JP. Migration and development of Sarcocystis neurona in tissues of interferon gamma knockout mice fed sporocysts from a naturally infected opossum. Vet Parasitol 2001;95:341–351. [DOI] [PubMed] [Google Scholar]
- 30. Witonsky SG, Gogal RM Jr, Duncan RB, et al. Immunopathologic effects associated with Sarcocystis neurona‐infected interferon‐gamma knockout mice. J Parasitol 2003;89:932–940. [DOI] [PubMed] [Google Scholar]
- 31. Witonsky SG, Gogal RM Jr, Duncan RB, et al. Protective immune response to experimental infection with Sarcocystis neurona in 57BL/6 mice. J Parasitol 2003;89:924–931. [DOI] [PubMed] [Google Scholar]
- 32. Witonsky SG, Gogal RM Jr, Duncan RB Jr, et al. Prevention of meningo/encephalomyelitis due to Sarcocystis neurona infection in mice is mediated by CD8 cells. Int J Parasitol 2005;35:113–123. [DOI] [PubMed] [Google Scholar]
- 33. Furr M, Pontzer C. Transforming growth factor beta concentrations and interferon gamma responses in cerebrospinal fluid of horses with equine protozoal myeloencephalitis. Equine Vet J 2001;33:721–725. [DOI] [PubMed] [Google Scholar]
- 34. Tornquist SJ, Boeder LJ, Mattson DE, et al. Lymphocyte responses and immunophenotypes in horses with Sarcocystis neurona infection. Equine Vet J 2001;33:726–729. [DOI] [PubMed] [Google Scholar]
- 35. Yang J, Ellison S, Gogal R, et al. Immune response to Sarcocystis neurona infection in naturally infected horses with equine protozoal myeloencephalitis. Vet Parasitol 2006;138:200–210. [DOI] [PubMed] [Google Scholar]
- 36. Saville WJ, Morley PS, Reed SM, et al. Evaluation of risk factors associated with clinical improvement and survival of horses with equine protozoal myeloencephalitis. J Am Vet Med Assoc 2000;217:1181–1185. [DOI] [PubMed] [Google Scholar]
- 37. Saville WJ, Stich RW, Reed SM, et al. Utilization of stress in the development of an equine model for equine protozoal myeloencephalitis. Vet Parasitol 2001;95:211–222. [DOI] [PubMed] [Google Scholar]
- 38. Sofaly CD, Reed SM, Gordon JC, et al. Experimental induction of equine protozoan myeloencephalitis (EPM) in the horse: effect of Sarcocystis neurona sporocyst inoculation dose on the development of clinical neurologic disease. J Parasitol 2002;88:1164–1170. [DOI] [PubMed] [Google Scholar]
- 39. Cutler TJ, MacKay RJ, Ginn PE, et al. Immunoconversion against Sarcocystis neurona in normal and dexamethasone‐treated horses challenged with S. neurona sporocysts. Vet Parasitol 2001;95:197–210. [DOI] [PubMed] [Google Scholar]
- 40. Saville WJ, Sofaly CD, Reed SM, et al. An equine protozoal myeloencephalitis challenge model testing a second transport after inoculation with Sarcocystis neurona sporocysts. J Parasitol 2004;90:1406–1410. [DOI] [PubMed] [Google Scholar]
- 41. Asmundsson IM, Dubey JP, Rosenthal BM. A genetically diverse but distinct North American population of Sarcocystis neurona includes an overrepresented clone described by 12 microsatellite alleles. Infect Genet Evol 2006;6:352–360. [DOI] [PubMed] [Google Scholar]
- 42. Elsheikha HM, Schott HC 2nd, Mansfield LS. Genetic variation among isolates of Sarcocystis neurona, the agent of protozoal myeloencephalitis, as revealed by amplified fragment length polymorphism markers. Infect Immun 2006;74:3448–3454. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 43. Howe DK, Gaji RY, Marsh AE, et al. Strains of Sarcocystis neurona exhibit differences in their surface antigens, including the absence of the major surface antigen SnSAG1. Int J Parasitol 2008;38:623–631. [DOI] [PubMed] [Google Scholar]
- 44. Wendte JM, Miller MA, Lambourn DM, et al. Self‐mating in the definitive host potentiates clonal outbreaks of the apicomplexan parasites Sarcocystis neurona and Toxoplasma gondii . PLoS Genet 2010;6:e1001261. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 45. Fayer R, Mayhew IG, Baird JD, et al. Epidemiology of equine protozoal myeloencephalitis in North America based on histologically confirmed cases. J Vet Intern Med 1990;4:54–57. [DOI] [PubMed] [Google Scholar]
- 46. Boy MG, Galligan DT, Divers TJ. Protozoal encephalomyelitis in horses: 82 cases (1972‐1986). J Am Vet Med Assoc 1990;196:632–634. [PubMed] [Google Scholar]
- 47. Bentz BG, Granstrom DE, Stamper S. Seroprevalence of antibodies to Sarcocystis neurona in horses residing in a county of southeastern Pennsylvania. J Am Vet Med Assoc 1997;210:517–518. [PubMed] [Google Scholar]
- 48. Bentz BG, Ealey KA, Morrow J, et al. Seroprevalence of antibodies to Sarcocystis neurona in equids residing in Oklahoma. J Vet Diagn Invest 2003;15:597–600. [DOI] [PubMed] [Google Scholar]
- 49. Blythe LL, Granstrom DE, Hansen DE, et al. Seroprevalence of antibodies to Sarcocystis neurona in horses residing in Oregon. J Am Vet Med Assoc 1997;210:525–527. [PubMed] [Google Scholar]
- 50. Saville WJ, Reed SM, Granstrom DE, et al. Seroprevalence of antibodies to Sarcocystis neurona in horses residing in Ohio. J Am Vet Med Assoc 1997;210:519–524. [PubMed] [Google Scholar]
- 51. Tillotson K, McCue PM, Granstrom DE, et al. Seroprevalence of antibodies to Sarcocystis neurona in horses residing in northern Colorado. J Equine Vet Sci 1999;19:122–126. [Google Scholar]
- 52. Dubey JP, Kerber CE, Granstrom DE. Serologic prevalence of Sarcocystis neurona, Toxoplasma gondii, and Neospora caninum in horses in Brazil. J Am Vet Med Assoc 1999;215:970–972. [PubMed] [Google Scholar]
- 53. Dubey JP, Venturini MC, Venturini L, et al. Prevalence of antibodies to Sarcocystis neurona, Toxoplasma gondii and Neospora caninum in horses from Argentina. Vet Parasitol 1999;86:59–62. [DOI] [PubMed] [Google Scholar]
- 54. Bartova E, Sedlak K, Syrova M, et al. Neospora spp. and Toxoplasma gondii antibodies in horses in the Czech Republic. Parasitol Res 2010;107:783–785. [DOI] [PubMed] [Google Scholar]
- 55. Dubey JP, Mitchell SM, Morrow JK, et al. Prevalence of antibodies to Neospora caninum, Sarcocystis neurona, and Toxoplasma gondii in wild horses from central Wyoming. J Parasitol 2003;89:716–720. [DOI] [PubMed] [Google Scholar]
- 56. Pitel PH, Pronost S, Romand S, et al. Prevalence of antibodies to Neospora caninum in horses in France. Equine Vet J 2001;33:205–207. [DOI] [PubMed] [Google Scholar]
- 57. Vardeleon D, Marsh AE, Thorne JG, et al. Prevalence of Neospora hughesi and Sarcocystis neurona antibodies in horses from various geographical locations. Vet Parasitol 2001;95:273–282. [DOI] [PubMed] [Google Scholar]
- 58. Villalobos EM, Furman KE, Lara Mdo C, et al. Detection of Neospora sp. antibodies in cart horses from urban areas of Curitiba, Southern Brazil. Rev Bras Parasitol Vet 2012;21:68–70. [DOI] [PubMed] [Google Scholar]
- 59. Dangoudoubiyam S, Oliveira JB, Viquez C, et al. Detection of antibodies against Sarcocystis neurona, Neospora spp., and Toxoplasma gondii in horses from Costa Rica. J Parasitol 2011;97:522–524. [DOI] [PubMed] [Google Scholar]
- 60. Gupta GD, Lakritz J, Kim JH, et al. Seroprevalence of Neospora, Toxoplasma gondii and Sarcocystis neurona antibodies in horses from Jeju island, South Korea. Vet Parasitol 2002;106:193–201. [DOI] [PubMed] [Google Scholar]
- 61. Hoane JS, Gennari SM, Dubey JP, et al. Prevalence of Sarcocystis neurona and Neospora spp. infection in horses from Brazil based on presence of serum antibodies to parasite surface antigen. Vet Parasitol 2006;136:155–159. [DOI] [PubMed] [Google Scholar]
- 62. Hoane JS, Yeargan MR, Stamper S, et al. Recombinant NhSAG1 ELISA: a sensitive and specific assay for detecting antibodies against Neospora hughesi in equine serum. J Parasitol 2005;91:446–452. [DOI] [PubMed] [Google Scholar]
- 63. NAHMS . Equine Protozoal Myeloencephalitis (EPM) in the U.S In: USDA:APHIS:VS , ed. Centers for Epidemiology and Animal Health. Fort Collins, Colorado: NAHMS; 2001:1–46. [Google Scholar]
- 64. MacKay RJ, Davis SW, Dubey JP. Equine protozoal myeloencephalitis. Compend Contin Educ Pract Vet 1992;14:1359–1367. [Google Scholar]
- 65. Fenger CK, Granstrom DE, Langemeier JL, et al. Epizootic of equine protozoal myeloencephalitis on a farm. J Am Vet Med Assoc 1997;210:923–927. [PubMed] [Google Scholar]
- 66. Granstrom DE, Alvarez O Jr, Dubey JP, et al. Equine protozoal myelitis in Panamanian horses and isolation of Sarcocystis neurona . J Parasitol 1992;78:909–912. [PubMed] [Google Scholar]
- 67. Saville WJ, Reed SM, Morley PS, et al. Analysis of risk factors for the development of equine protozoal myeloencephalitis in horses. J Am Vet Med Assoc 2000;217:1174–1180. [DOI] [PubMed] [Google Scholar]
- 68. Dunigan CE, Oglesbee MJ, Podell M, et al. Seizure activity associated with equine Protozoal Myeloencephalitis. Prog Vet Neurol 1995;6:50–54. [Google Scholar]
- 69. Reed SM, Granstrom DE. Equine protozoal encephalomyelitis. In: 13th Annual Veterinary Medical Forum of the American College of Veteinary Internal Medicine 1993;591–592.
- 70. Hamir AN, Moser G, Galligan DT, et al. Immunohistochemical study to demonstrate Sarcocystis neurona in equine protozoal myeloencephalitis. J Vet Diagn Invest 1993;5:418–422. [DOI] [PubMed] [Google Scholar]
- 71. Johnson AL, Morrow JK, Sweeney RW. Indirect fluorescent antibody test and surface antigen ELISAs for antemortem diagnosis of equine protozoal myeloencephalitis. J Vet Intern Med 2013;27:596–599. [DOI] [PubMed] [Google Scholar]
- 72. Reed SM, Howe DK, Morrow JK, et al. Accurate antemortem diagnosis of equine protozoal myeloencephalitis (EPM) based on detecting intrathecal antibodies against Sarcocystis neurona using the SnSAG2 and SnSAG4/3 ELISAs. J Vet Intern Med 2013;27:1193–1200. [DOI] [PubMed] [Google Scholar]
- 73. Furr M. Antigen‐specific antibodies in cerebrospinal fluid after intramuscular injection of ovalbumin in horses. J Vet Intern Med 2002;16:588–592. [DOI] [PubMed] [Google Scholar]
- 74. Finno CJ, Packham AE, David Wilson W, et al. Effects of blood contamination of cerebrospinal fluid on results of indirect fluorescent antibody tests for detection of antibodies against Sarcocystis neurona and Neospora hughesi . J Vet Diagn Invest 2007;19:286–289. [DOI] [PubMed] [Google Scholar]
- 75. Furr M, Howe D, Reed S, et al. Antibody coefficients for the diagnosis of equine protozoal myeloencephalitis. J Vet Intern Med 2011;25:138–142. [DOI] [PubMed] [Google Scholar]
- 76. Miller MM, Sweeney CR, Russell GE, et al. Effects of blood contamination of cerebrospinal fluid on western blot analysis for detection of antibodies against Sarcocystis neurona and on albumin quotient and immunoglobulin G index in horses. J Am Vet Med Assoc 1999;215:67–71. [PubMed] [Google Scholar]
- 77. Tumani H, Nolker G, Reiber H. Relevance of cerebrospinal fluid variables for early diagnosis of neuroborreliosis. Neurology 1995;45:1663–1670. [DOI] [PubMed] [Google Scholar]
- 78. Dorta‐Contreras AJ, Reiber H. Intrathecal synthesis of immunoglobulins in eosinophilic meningoencephalitis due to Angiostrongylus cantonensis . Clin Diagn Lab Immunol 1998;5:452–455. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 79. Lejon V, Reiber H, Legros D, et al. Intrathecal immune response pattern for improved diagnosis of central nervous system involvement in trypanosomiasis. J Infect Dis 2003;187:1475–1483. [DOI] [PubMed] [Google Scholar]
- 80. Contini C, Fainardi E, Cultrera R, et al. Advanced laboratory techniques for diagnosing Toxoplasma gondii encephalitis in AIDS patients: significance of intrathecal production and comparison with PCR and ECL‐western blotting. J Neuroimmunol 1998;92:29–37. [DOI] [PubMed] [Google Scholar]
- 81. Potasman I, Resnick L, Luft BJ, et al. Intrathecal production of antibodies against Toxoplasma gondii in patients with toxoplasmic encephalitis and the acquired immunodeficiency syndrome (AIDS). Ann Intern Med 1988;108:49–51. [DOI] [PubMed] [Google Scholar]
- 82. Daft BM, Barr BC, Gardner IA, et al. Sensitivity and specificity of western blot testing of cerebrospinal fluid and serum for diagnosis of equine protozoal myeloencephalitis in horses with and without neurologic abnormalities. J Am Vet Med Assoc 2002;221:1007–1013. [DOI] [PubMed] [Google Scholar]
- 83. Duarte PC, Daft BM, Conrad PA, et al. Comparison of serum indirect fluorescent antibody test with two Western blot tests for the diagnosis of equine protozoal myeloencephalitis. J Vet Diagn Invest 2003;15:8–13. [DOI] [PubMed] [Google Scholar]
- 84. Duarte PC, Daft BM, Conrad PA, et al. Evaluation and comparison of an indirect fluorescent antibody test for detection of antibodies to Sarcocystis neurona, using serum and cerebrospinal fluid of naturally and experimentally infected, and vaccinated horses. J Parasitol 2004;90:379–386. [DOI] [PubMed] [Google Scholar]
- 85. Duarte PC, Ebel ED, Traub‐Dargatz J, et al. Indirect fluorescent antibody testing of cerebrospinal fluid for diagnosis of equine protozoal myeloencephalitis. Am J Vet Res 2006;67:869–876. [DOI] [PubMed] [Google Scholar]
- 86. Ellison SP, Kennedy TJ, Brown KK. Development of an ELISA to detect antibodies to rSAG1 in the horse. Int J App Res Vet Med 2003;1:318–327. [Google Scholar]
- 87. Granstrom DE, Dubey JP, Davis SW, et al. Equine protozoal myeloencephalitis: antigen analysis of cultured Sarcocystis neurona merozoites. J Vet Diagn Invest 1993;5:88–90. [DOI] [PubMed] [Google Scholar]
- 88. Hoane JS, Morrow JK, Saville WJ, et al. Enzyme‐linked immunosorbent assays for the detection of equine antibodies specific to Sarcocystis neurona surface antigens. Clin Diagn Lab Immunol 2005;12:1050–1056. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 89. Johnson AL, Burton AJ, Sweeney RW. Utility of 2 immunological tests for antemortem diagnosis of equine protozoal myeloencephalitis (Sarcocystis neurona Infection) in naturally occurring cases. J Vet Intern Med 2010;24:1184–1189. [DOI] [PubMed] [Google Scholar]
- 90. Rossano MG, Mansfield LS, Kaneene JB, et al. Improvement of western blot test specificity for detecting equine serum antibodies to Sarcocystis neurona . J Vet Diagn Invest 2000;12:28–32. [DOI] [PubMed] [Google Scholar]
- 91. Yeargan MR, Howe DK. Improved detection of equine antibodies against Sarcocystis neurona using polyvalent ELISAs based on the parasite SnSAG surface antigens. Vet Parasitol 2011;176:16–22. [DOI] [PubMed] [Google Scholar]
- 92. Ellison SP, Lindsay DS. Decoquinate combined with levamisole reduce the clinical signs and Serum SAG 1, 5, 6 antibodies in horses with suspected equine protozoal myeloencephalitis. Int J Appl Res Vet Med 2012;10:1–7. [Google Scholar]
- 93. Granstrom D. Equine protozoal myeloencephalitis: Parasite biology, experimental disease, and laboratory diagnosis. In: International Equine Neurology Conference, Ithaca, NY 1997.
- 94. Ellison SP, Omara‐Opyene AL, Yowell CA, et al. Molecular characterisation of a major 29 kDa surface antigen of Sarcocystis neurona . Int J Parasitol 2002;32:217–225. [DOI] [PubMed] [Google Scholar]
- 95. Howe DK, Gaji RY, Mroz‐Barrett M, et al. Sarcocystis neurona merozoites express a family of immunogenic surface antigens that are orthologues of the Toxoplasma gondii surface antigens (SAGs) and SAG‐related sequences. Infect Immun 2005;73:1023–1033. [DOI] [PMC free article] [PubMed] [Google Scholar]
- 96. Marsh AE, Howe DK, Wang G, et al. Differentiation of Neospora hughesi from Neospora caninum based on their immunodominant surface antigen, SAG1 and SRS2. Int J Parasitol 1999;29:1575–1582. [DOI] [PubMed] [Google Scholar]
- 97. Reed SM, Howe DK, Yeargan MR, et al. New quantitative assays for the differential diagnosis of equine protozoal myeloencephalitis (EPM). In: ACVIM Forum 2010.
- 98. Renier AC, Morrow JK, Graves A, et al. Diagnosis of equine protozoal myeloencephalitis using indirect fluorescent antibody testing and enzyme‐linked immunosorbent assay titer ratios for Sarcocystis neurona and Neospora hughesi. In: ACVIM Forum, EPM SIG 2012.
- 99. Saville WJ. Comparison of diagnostic tests for EPM run on blinded sera at four different laboratories. In: ACVIM Forum, EPM SIG 2007.
- 100. Packham AE, Conrad PA, Wilson WD, et al. Qualitative evaluation of selective tests for detection of Neospora hughesi antibodies in serum and cerebrospinal fluid of experimentally infected horses. J Parasitol 2002;88:1239–1246. [DOI] [PubMed] [Google Scholar]
- 101. Bogan JA, Galbraith A, Baxter P, et al. Effect of feeding on the fate of orally administered phenylbutazone, trimethoprim and sulphadiazine in the horse. Vet Rec 1984;115:599–600. [DOI] [PubMed] [Google Scholar]
- 102. Clarke CR, MacAllister CG, Burrows GE, et al. Pharmacokinetics, penetration into cerebrospinal fluid, and hematologic effects after multiple oral administrations of pyrimethamine to horses. Am J Vet Res 1992;53:2296–2299. [PubMed] [Google Scholar]
- 103. Cavallito JC, Nichol CA, Brenckman WD Jr, et al. Lipid‐soluble inhibitors of dihydrofolate reductase. I. Kinetics, tissue distribution, and extent of metabolism of pyrimethamine, metoprine, and etoprine in the rat, dog, and man. Drug Metab Dispos 1978;6:329–337. [PubMed] [Google Scholar]
- 104. Green SL, Mayhew IG, Brown MP, et al. Concentrations of trimethoprim and sulfamethoxazole in cerebrospinal fluid and serum in mares with and without a dimethyl sulfoxide pretreatment. Can J Vet Res 1990;54:215–222. [PMC free article] [PubMed] [Google Scholar]
- 105. Reed S, Saville WJ. Equine Protozoal Myeloencephalitis. In: 42nd Annual Meeting of the American Association of Equine Practitioners 1996;75–79.
- 106. Welsch BB. Treatment of equine protozoal myeloencephalitis. Compend Contin Educ Pract Vet 1991;13:1599–1602. [Google Scholar]
- 107. Chung MK, Han SS, Roh JK. Synergistic embryotoxicity of combination pyrimethamine and folic acid in rats. Reprod Toxicol 1993;7:463–468. [DOI] [PubMed] [Google Scholar]
- 108. Toribio RE, Bain FT, Mrad DR, et al. Congenital defects in newborn foals of mares treated for equine protozoal myeloencephalitis during pregnancy. J Am Vet Med Assoc 1998;212:697–701. [PubMed] [Google Scholar]
- 109. Castles TR, Kintner LD, Lee CC. The effects of folic or folinic acid on the toxicity of pyrimethamine in dogs. Toxicol Appl Pharmacol 1971;20:447–459. [DOI] [PubMed] [Google Scholar]
- 110. Hackstein JH, Mackenstedt U, Mehlhorn H, et al. Parasitic apicomplexans harbor a chlorophyll a‐D1 complex, the potential target for therapeutic triazines. Parasitol Res 1995;81:207–216. [DOI] [PubMed] [Google Scholar]
- 111. Lindsay DS, Dubey JP. Determination of the activity of diclazuril against Sarcocystis neurona and Sarcocystis falcatula in cell cultures. J Parasitol 2000;86:164–166. [DOI] [PubMed] [Google Scholar]
- 112. Lindsay DS, Dubey JP, Kennedy TJ. Determination of the activity of ponazuril against Sarcocystis neurona in cell cultures. Vet Parasitol 2000;92:165–169. [DOI] [PubMed] [Google Scholar]
- 113. Lindsay DS, Rippey NS, Cole RA, et al. Examination of the activities of 43 chemotherapeutic agents against Neospora caninum tachyzoites in cultured cells. Am J Vet Res 1994;55:976–981. [PubMed] [Google Scholar]
- 114. Dirikolu L, Lehner F, Nattrass C, et al. Diclazuril in the horse: its identification and detection and preliminary pharmacokinetics. J Vet Pharmacol Ther 1999;22:374–379. [DOI] [PubMed] [Google Scholar]
- 115. Furr M, Kennedy T. Cerebrospinal fluid and serum concentrations of ponazuril in horses. Vet Ther 2001;2:232–237. [PubMed] [Google Scholar]
- 116. Hunyadi L, Papich MG, Pusterla N. Pharmacokinetics of a low dose and FDA‐labeled dose of diclazuril administered orally as a pelleted topdressing in adult horses. J Vet Pharmacol Ther 2015;38:243–248. [DOI] [PubMed] [Google Scholar]
- 117. Reed SM, Wendel M, King S, et al. Pharmacokinetics of Ponazuril in Horses. In: 58th Annual Convention of the American Association of Equine Practitioners, Anaheim, CA 2012;572.
- 118. Furr M, Kennedy T, MacKay R, et al. Efficacy of ponazuril 15% oral paste as a treatment for equine protozoal myeloencephalitis. Vet Ther 2001;2:215–222. [PubMed] [Google Scholar]
- 119. Bentz BG, Dirikolu L, Carter WG, et al. Equine protozoal myeloencephalitis (EPM): a clinical report. Equine Vet Educ 2000;16:258–263. [Google Scholar]
- 120. Furr M, McKenzie H, Saville WJ, et al. Prophylactic administration of ponazuril reduces clinical signs and delays seroconversion in horses challenged with Sarcocystis neurona . J Parasitol 2006;92:637–643. [DOI] [PubMed] [Google Scholar]
- 121. Mackay RJ, Tanhauser ST, Gillis KD, et al. Effect of intermittent oral administration of ponazuril on experimental Sarcocystis neurona infection of horses. Am J Vet Res 2008;69:396–402. [DOI] [PubMed] [Google Scholar]
- 122. Pusterla N, Packham A, Mackie S, et al. Daily feeding of diclazuril top dress pellets in foals reduces seroconversion to Sarcocystis neurona . Vet J 2015;206:236–238. 10.1016/j.tvjl.2015.07.018 [DOI] [PubMed] [Google Scholar]