Current Applications of Digital PCR in Veterinary Parasitology: An Overview PDF

See discussions, stats, and author profiles for this publication at: https://www.researchgate.net/publication/373690766 Current Applications of Digital PCR in Veterinary Parasitology: An Overview Article in Parasitologia · September 2023 DOI: 10.3390/parasitologia3030028 CITATIONS READS 2 155 5 authors, including: Constantina Tsokana Georgios Sioutas University of Thessaly Aristotle University of Thessaloniki 57 PUBLICATIONS 366 CITATIONS 34 PUBLICATIONS 93 CITATIONS SEE PROFILE SEE PROFILE Athanasios I Gelasakis Elias Papadopoulos Agricultural University of Athens Aristotle University of Thessaloniki 135 PUBLICATIONS 1,310 CITATIONS 256 PUBLICATIONS 4,667 CITATIONS SEE PROFILE SEE PROFILE All content following this page was uploaded by Athanasios I Gelasakis on 06 September 2023. The user has requested enhancement of the downloaded file. Review Current Applications of Digital PCR in Veterinary Parasitology: An Overview Constantina N. Tsokana 1 , Isaia Symeonidou 1, * , Georgios Sioutas 1 , Athanasios I. Gelasakis 2 and Elias Papadopoulos 1 1 Laboratory of Parasitology and Parasitic Diseases, School of Veterinary Medicine, Faculty of Health Sciences, Aristotle University of Thessaloniki, 54124 Thessaloniki, Greece; [email protected] (C.N.T.); [email protected] (G.S.); [email protected] (E.P.) 2 Laboratory of Anatomy and Physiology of Farm Animals, Department of Animal Science, School of Animal Biosciences, Agricultural University of Athens, 11855 Athens, Greece; [email protected] * Correspondence: [email protected]; Tel.: +30-69-38008589 Abstract: Digital PCR (dPCR) is an emerging technology that enables the absolute quantification of the targeted nucleic acids. The body of research on the potential applications of this novel tool is growing in human and veterinary medicine. Most of the research on dPCR applications in veterinary parasitology is concentrated on developing and validating new assays to detect and quantify parasites of great financial impact in the food-producing animal industry. Several studies describe the utility of dPCR for individualized medicine in companion animals. Most frequently, dPCR performance is assessed compared to quantitative PCR or Next Generation Sequencing platforms, while others also compare the accuracy of dPCR with traditional parasitological techniques considered gold standard methods. Other researchers describe dPCR assays for surveillance purposes, species identification, and quantification in mixed parasitic infections, the detection of mutations indicative of anthelmintic resistance, and the identification of new targets for drug development. This review provides an overview of the studies that employed dPCR in investigating animal parasites and parasitic diseases from a veterinary perspective and discusses how this novel technology could advance and facilitate diagnosis, surveillance, and the monitoring of response to treatment, or shed light on current gaps in Citation: Tsokana, C.N.; our knowledge of the epidemiology of significant veterinary parasitic diseases. Symeonidou, I.; Sioutas, G.; Gelasakis, A.I.; Papadopoulos, E. Keywords: digital PCR; Dirofilaria immitis; Echinococcus multilocularis; gastrointestinal nematodes; Current Applications of Digital PCR poultry; protozoa; ruminants; Schistosoma japonicum; veterinary parasitology in Veterinary Parasitology: An Overview. Parasitologia 2023, 3, 269–283. https://doi.org/10.3390/ parasitologia3030028 1. Introduction Academic Editor: Geoff Hide The advent of molecular methods has been a game changer and deepened our un- derstanding of veterinary parasitology. The invention and application of DNA-based Received: 31 July 2023 molecular tools, such as Polymerase Chain Reaction (PCR) and quantitative PCR (qPCR), Revised: 25 August 2023 followed by high-throughput sequencing technologies, gave new insights into molecular Accepted: 4 September 2023 diagnostics and research in this field. Published: 6 September 2023 Digital PCR (dPCR) is an emerging technology that enables the absolute quantification of the targeted nucleic acids. It is regarded as a vastly improved version of conventional PCR and qPCR. For the time being, most studies on parasitic diseases of veterinary Copyright: © 2023 by the authors. importance involve developing and validating dPCR assays and evaluating their perfor- Licensee MDPI, Basel, Switzerland. mance compared to qPCR or Next Generation Sequencing (NGS) platforms. Several studies This article is an open access article also compare the sensitivity of dPCR with traditional parasitological techniques that are distributed under the terms and considered gold standard methods [3–6]. Other researchers described dPCR assays for conditions of the Creative Commons surveillance purposes, species identification, and quantification in mixed infections, the Attribution (CC BY) license (https:// detection of mutations indicative of anthelmintic resistance, as well as the identification of creativecommons.org/licenses/by/ new targets for drug development [5,7–9]. 4.0/). Parasitologia 2023, 3, 269–283. https://doi.org/10.3390/parasitologia3030028 https://www.mdpi.com/journal/parasitologia Parasitologia 2023, 3, FOR PEER REVIEW Parasitologia 2023, 3 infections, the detection of mutations indicative of anthelmintic resistance, 270 as well identification of new targets for drug development [5,7–9]. This novel technology is based on endpoint quantification after sample divisi This novel technology isinformation also provides on the precise based on endpoint analyte after quantification concentrations in the original sample division. It sa expressed inon also provides information DNAthe copies preciseper microliter, analyte along withinconfidence concentrations the original interval sample, estimation expressed in DNAThe dPCR copiesassays usually combine per microliter, along withprobe-based confidencePCR (typically interval TaqMan estimations probes) w. The dPCR assays microfluidics usually combineanalysisprobe-based platform. One PCRof the major advantages (typically of dPCR TaqMan probes) compared with a to is that itplatform. microfluidics analysis does not One require reference of the samples andofa dPCR major advantages standard curve for compared to the qPCR quantificat the require is that it does not parasiticreference burden. Moreover, samples and athe assay’scurve standard performance is not aﬀected by PCR i for the quantification itors, as the sample partitioning has a dilution eﬀect of the parasitic burden. Moreover, the assay’s performance is not affected for the inhibitors. Howeve by PCR cost inhibitors, as the per sample sample is still has partitioning significantly a dilutionhigher effect than conventional for the inhibitors.andHowever, qPCR, and it lack potential the cost per sample is stilltosignificantly perform DNA sequencing higher to confirm than conventional a positive and qPCR, and result duethe it lacks to the extre low number potential to perform of amplicons DNA sequencing per droplet to confirm (Tableresult a positive 1) [10,11]. due to the extremely low number of amplicons per droplet (Table 1) [10,11]. Table 1. Advantages and disadvantages of the dPCR technology. Table 1. Advantages and disadvantages of the dPCR technology. Advantages Disadvantages AdvantagesAbsolute quantification Disadvantages High cost No reference samples required Absolute quantification Inability to sequence the PCR amplic High cost No standard No reference samples requiredcurve requiredInability to sequence the PCR amplicons No standard curve requiredin the presence $$$$$$of Better performance Better performance in the presence inhibitors of inhibitors High sensitivity High sensitivity Among the diﬀerent dPCR forms, the droplet dPCR (ddPCR) is the most comm Among the different dPCR forms, used in veterinary the droplet parasitology dPCR [4,7,12]. (ddPCR) The general isprinciples the most and commonly technical advan used in veterinary have been described in detail elsewhere and are beyond the scope advan- parasitology [4,7,12]. The general principles and technical of this review a tages have been described [2,13,14]. in detailthe Concisely, elsewhere and are PCR reaction is beyond the into subdivided scopethousands of this review of small part article [2,13,14].(droplets), Concisely,uniform the PCRinreaction volume,is by subdivided into thousands various available methods. of small These parti- droplets opti tions (droplets),contain uniform in volume, only a single by various or no available template DNAmethods. molecule.These Afterdroplets optimally a specia PCR amplification, contain only a single or no template DNA molecule. After PCR amplification, a specialized reader measures the number of fluorescent droplets that corresponds to the numb reader measures the number template of fluorescent molecules droplets with a particular that corresponds fluorescence (Figureto1) the.number of template molecules with a particular fluorescence (Figure 1). Figure 1. Visualized workflow of the ddPCR assay illustrating the subdivision of a single sample containing the target sequence (A) into thousands of droplets, (B) the PCR amplification in each Figure droplet, and (C) the 1. Visualized measurement workflow of the numberofofthe ddPCR assay fluorescent illustrating droplets (D) that the subdivision corresponds of a single s to the containing the target sequence (A) into thousands of droplets, (B) the PCR amplification number of template molecules with a particular fluorescence leading to absolute quantification (E). in This review provides an overview of the studies that employed dPCR in investigating animal parasites and parasitic diseases from a veterinary perspective. We also discuss how this novel technology could provide added value, aid and benefit diagnosis, surveillance, Parasitologia 2023, 3 271 and the monitoring of response to treatment, or could shed light on current gaps in our knowledge of the epidemiology of important veterinary parasitic diseases. 2. Protozoa 2.1. Eimeria spp. Traditionally, the description and differentiation of Eimeria spp. are based on the oocysts’ shape, size, and features. Precise species identification is essential for coccidio- sis control since it reveals the degree of drug or vaccine resistance. However, species identification based on oocyst morphology is challenging due to the variations within and between oocyst morphometrics. Consequently, several molecular tools have been employed for discriminating at the species level and others, such as qPCR, for quantifying the parasitic burden [17–19]. Snyder et al. developed a highly specific ddPCR to discriminate seven Eimeria species- E. acervulina, E. brunetti, E. maxima, E. mitis, E. necatrix, E. tenella, and E. praecox. The researchers used a single PCR amplicon labeled with genus-specific and species-specific probes targeting conserved and specific regions. The targeted cytochrome c oxidase subunit III gene in the mitochondrial genome (mtCOIII) allowed accurate species differentiation due to its interspecific variability. The specificity was high even in samples containing DNA from more than one species. The relative species quantification obtained from the ddPCR was in agreement with the NGS assay used. The ddPCR assay presented high sensitivity for all the seven described Eimeria spp.; it detected low concentrations of DNA: 0.00001 ng/µL for E. brunetti, E. praecox, and E. tenella; 0.0001 ng/µL for E. maxima and E. mitis; and 0.001 ng/µL for E. acervulina and E. necatrix. One limitation of this assay is that it does not provide quantification data for oocysts. Instead, it provides information on the relative abundance of different Eimeria species in a sample based on the number of copies of DNA for each species. Therefore, the results should be interpreted in combination with the oocysts per gram data. Moreover, non-specific binding was observed between E. necatrix and E. tenella. Nonetheless, the authors suggested that the newly developed ddPCR assay would provide valuable information on coccidiosis, a disease of major financial impact in the poultry sector, and they proposed many potential applications in commercial chicken production systems. 2.2. Haemosporidian Parasites Haemosporidian parasites, transmitted by dipteran blood-sucking insects, are cos- mopolitan in birds [20,21]. Clinical manifestations appear during the acute phase of infection when erythrocytic parasitemia is high, while low-intensity infections do not usually become evident. Some species cause severe disease in avian hosts , and coinfections with different species or genetic lineages, which are often particularly virulent, have been reported worldwide [23,24]. Currently, the identification of avian haemosporid- ian is mainly based on the analysis of blood samples by traditional light microscopy and qPCR. However, both methods present limitations. Microscopy has low sensitivity; it requires high-quality blood smears that are difficult to achieve in field conditions and high infection levels. As for qPCR, although it is more sensitive compared to microscopy, it is difficult to standardize and requires reference samples of absolute known parasite DNA concentrations that limit the inter-laboratory comparisons [23,26]. Huang et al. developed a ddPCR protocol for the detection and absolute quantifi- cation of avian haemosporidians belonging to Plasmodium spp., Haemoproteus spp., and Leucocytozoon spp.. The method’s performance was assessed compared to qPCR, nested PCR, and light microscopy in blood samples from raptors. The newly developed ddPCR assay enabled reliable quantification even in samples with minimum parasitic load, i.e., one parasite copy in 105 host genomes. The ddPCR assay showed equal sensitivity and high agreement with qPCR. Notably, the quantity assessment was more accurate than qPCR, and the assay demonstrated higher consistency among technical duplicates and reactions, especially in low parasitic loads. Unlike nested PCR and light microscopy, ddPCR identified Parasitologia 2023, 3 272 more than 60% and 74% of the negative samples, respectively, as positive. The researchers suggested that despite the higher cost of ddPCR compared to qPCR, it could be a better choice in several cases, such as the comparison of the absolute quantifications reported from different laboratories, when reference samples are not available, as well as in long-term studies where sample storage could negatively affect the DNA integrity. Moreover, they highlighted the potential of ddPCR for investigating abortive infections, which are difficult to identify but may be detected by quantifying very low-intensity infections. In the same context, in a previous study in Australia, ddPCR targeting the mitochon- drial 18S rRNA gene was used to quantify the parasitic load of Leucocytozoon podargii in tissues collected during necropsy from a tawny frogmouth, which exhibited signs consis- tent with a Leucocytozoon infection. Histopathological analysis of the respective tissues revealed significant changes in the lung tissue. This finding was in agreement with the absolute quantification data provided by ddPCR; the infected lung tissue displayed the highest Leucocytozoon load. 2.3. Cytauxzoon felis Recently, a ddPCR assay was designed to detect and quantify Cytauxzoon felis (C. felis) in feline blood samples during early infection and throughout treatment. The re- searchers evaluated the performance of the test in clinical samples from cats suspected of C. felis infection correlated to the traditionally used blood smear microscopy; the two methods showed 100% agreement. They also compared ddPCR to nested PCR and qPCR for C. felis in blood samples from experimentally infected cats pre- and post- antiprotozoal treatment. Although no significant differences in the detection rate were found between the molecular methods in cases of severe cytauxzoonosis—probably due to the high circulating parasite load before treatment—the ddPCR and qPCR assays performed better in samples collected ten days post-treatment. Regarding the quantification of the parasite load, the ddPCR assay detected as low as 0.0000231 ng DNA/reaction in the reference samples from acute cases and 0.00232 ng DNA/reaction in the reference samples from chronic cases. It is also worth mentioning that ddPCR identified infection up to one day prior to the development of clinical signs in experimentally infected cats. Thus, this assay successfully detected the early stages of the disease, even when employed in small sample volumes with low DNA concentrations. This is extremely important in the case of C. felis, as accurately detecting the earliest stages of infection is critical for initiating treatment. In addition, the clinical progression of the disease is rapid, and most cats die or are euthanized within 24 h of presentation in the veterinary clinic. The authors suggested that ddPCR is also useful for monitoring the parasite load throughout treatment by means of the absolute quantification of target DNA copies in samples acquired pre- and post-treatment. 2.4. Cryptosporidium spp. Quantitative molecular methods are increasingly gaining ground in Cryptosporidium spp. diagnostics due to their invaluable advantage of estimating the parasitic load in human, animal, and environmental samples. The low infectious dose (10–100 oocysts) of Cryptosporidium spp., the ability to survive in the environment for long periods, and the inherent resistance to drinking water disinfectants make the quantification of the parasitic load necessary for further diagnostic and management steps. In addition, quantitative molecular methods have a significantly lower limit of detection (LOD) than microscopy, which requires 1 × 104 –5 × 104 oocysts per mL of feces. In a 2014 study, the researchers developed and validated a ddPCR assay for detecting and quantifying Cryptosporidium spp. DNA in samples from sheep, cattle, and humans. They compared the performance of the newly developed assay with qPCR and showed a high degree of linearity and positive correlation between the two tests for the reference and clinical samples examined. The ddPCR was superior in precision and was not affected by the presence of inhibitors. This is especially important when the presence of inhibitors is anticipated in the biological samples examined, like feces. The authors also suggested that Parasitologia 2023, 3 273 ddPCR could be helpful for calibrating qPCR standards to deliver more precise standard curves. Later, when Zahedi et al. investigated the occurrence of Cryptosporidium spp. and Giardia spp. in dam water in sheep farms, they followed this suggestion and quantified the reference samples that they used in Cryptosporidium qPCR with ddPCR. Recently, a study showed how ddPCR coupled with the phenol-chloroform DNA extraction method is a valuable tool for monitoring and detecting Cryptosporidium spp. in wastewater samples. Environmental samples like water are challenging due to the low parasitic load, the complexity of their matrix that involves a higher concentration of PCR inhibitors, and the additional concentration step that is required to obtain sufficient biomass containing oocysts [36,37]. In that study, the researchers developed and evaluated a ddPCR assay for Cryptosporidium spp., which presented high sensitivity and a very low LOD of 5.93 copies, equivalent to less than one oocyst per reaction. The ability to detect such small starting quantities of protozoan parasites is essential in water samples since the infectious dose can be as low as ten oocysts. 2.5. Leishmania infantum Many qPCR assays have been developed for detecting and quantifying Leishmania DNA in clinical samples and provided new insights into the kinetics of the parasitic load. Usually, high burdens are associated with progressive disease, while a marked decrease appears following effective treatment. However, the parasitological cure is not anticipated, and most dogs remain infected for life. On top of the above, even dogs with zero parasitic burdens after treatment may present fluctuations over time [39,40]. Quantitative assays display high sensitivity in detecting Leishmania DNA and, thus, are increasingly popular in diagnosing canine leishmaniosis, as well as monitoring the disease progression following treatment and the potential for relapses. They have also been extensively used for species identification in animal, human, and vector studies. Although sensitive, rapid, and with reduced possibility of contamination, qPCR does not provide absolute quantification and, currently, there is no standardized method [41,42]. In the 2023 study of Pereira et al., a ddPCR assay for Leishmania infantum (L. infantum) DNA detection was developed and validated. The researchers assessed its performance in spleen samples from dogs with confirmed canine leishmaniosis following necropsy compared to qPCR. The two molecular methods presented perfect agreement (100%) and a positive correlation between the number of copies detected by ddPCR and the quantification cycles found in qPCR. No correlation was found between the copy numbers recorded in ddPCR and the morphological changes in the spleen of the dogs included in the study. This finding is in concordance with the study of Vasconcelos et al., which demonstrated that dogs with severe disease, as well as asymptomatic or mildly symptomatic animals with moderate to extensive splenic tissue disorganization, can have high parasitic loads. The authors suggested that ddPCR is advantageous over qPCR as it does not require a standard curve and is easy to standardize; therefore, it should be further used to investigate the relationship between parasitic load and the pathogenesis of the disease in dogs. 2.6. Theileria spp. Currently, the diagnosis of bovine theileriosis is based on clinical signs coupled with detecting the parasites in blood samples with light microscopy. Species identification is pivotal in bovine theileriosis. Unlike the most pathogenic species, Theileria annulata (T. annulata) and Theileria parva (T. parva), the other Theileria spp. are not life-threatening and do not require veterinary intervention. However, microscopy presents several limitations; the identification of the low blood parasite load is complex and may fail to detect early infection status. Furthermore, the presence of morphologically identical parasites like Babesia spp. may be misleading. Thus, employing highly sensitive and specific tools for disease diagnosis at early stages is paramount in bovine theileriosis. The treatment relies on the administration of buparvaquone, and the efficient elimination of the parasite is anticipated when early detection and treatment initiation occur. Additionally, Parasitologia 2023, 3 274 resistance to buparvaquone has been reported, and delayed diagnosis may lead to deadly lymphoproliferative disease. Recently, a multiplex ddPCR assay was developed for identifying and quantifying Theileria spp. and T. annulata in clinical samples. The researchers assessed the efficacy of the ddPCR assay compared to a qPCR assay and showed that they were equally efficient. The ddPCR presented high sensitivity for Theileria spp. (100%) and T. annulata (97.8%) identifying quantities as low as 8.5 copies/µL of T. annulata DNA. Noticeably, the ddPCR assay had higher sensitivity than qPCR at lower parasite burdens and exhibited consider- ably less variability. The method was also performed on DNA samples from treated and untreated Theileria-infected cell lines with buparvaquone to assess the treatment’s efficacy. The study’s findings displayed the ability of this novel tool to track the treatment response in clinical cases of bovine theileriosis, which is considered a critical feature. 2.7. Toxoplasma gondii In a 2022 study, the researchers developed and validated a ddPCR assay for detecting and quantifying Toxoplasma gondii (T. gondii) DNA in meat samples from intermediate hosts. They determined the accuracy of the new assay compared to qPCR and showed an almost perfect agreement between the two methods. The ddPCR presented high sen- sitivity (97.5%) and specificity (100%) and resulted in higher positivity rates in the meat samples (7.6% vs. 1.2% in qPCR), with a detection limit of 8 genomic copies/µL. Increased sensitivity is essential for T. gondii detection in meat samples because of the non- homogeneous distribution of tissue cysts and the small size of the sample that is usually examined. This is why many molecular tools that have been developed up to now present unexpectedly low sensitivity. The authors suggested that ddPCR is a promising tool and should be further tested in food matrices like milk and dairy products, as well as vegetables, to rapidly detect low parasitic loads of T. gondii. Earlier, a dPCR platform was used to investigate the hypothesis that edible fishes can harbor and effectively transmit T. gondii to marine organisms and human consumers. In this context, Marino et al. examined edible fishes using dPCR and qPCR. They showed by dPCR that fish specimens (skin/muscle, intestine, and gills) belonging to 12 different fish species were contaminated with T. gondii DNA to the extent of 1 to 5.7 × 104 copies/mL. The authors suggested that although fishes are not deemed as competent hosts for T. gondii, they could possibly act as mechanical carriers and, thus, be accidentally involved in the transmission cycle of the parasite. 3. Trematodes Schistosoma japonicum Schistosoma japonicum (S. japonicum) causes intravascular disease in humans and is endemic in the People’s Republic of China, the Philippines, and Indonesia. Among several human schistosome species, S. japonicum is zoonotic; it infects domestic and wild animals, thus complicating the national control strategy for the disease in the human population. Although most studies on schistosomiasis focus on humans, as China gets closer to eliminating the disease, it becomes essential to investigate the possible role of other hosts in maintaining low levels of transmission and the contamination of the environment. In a 2017 study, fecal samples from rodents, goats, dogs, cattle, and water buffaloes were collected and examined using traditional parasitological techniques and qPCR to detect and quantify the S. japonicum DNA levels in different hosts. A previously de- scribed ddPCR assay was also performed on the collected goat fecal samples. Goats, cattle, and water buffaloes were more frequently infected. The molecular methods presented in- creased sensitivity more than the traditional parasitological techniques, which significantly underestimated the actual prevalence of infection in all animal species examined. Notably, using ddPCR, a considerably higher prevalence of infection was recorded in goats (46.4%) compared to qPCR (6.9%). This discrepancy is probably due to inhibitors in the fecal sam- Parasitologia 2023, 3 275 ples that negatively affect the performance of qPCR but exhibit no effect on ddPCR. Based on the findings of ddPCR, the authors highlighted the importance of obtaining precise estimates of the prevalence of infection in animal species that could be involved in the transmission cycle as reservoirs or as maintenance hosts. They also suggested the inclusion of goats as targets of control to achieve the aim of eliminating schistosomiasis in China. 4. Cestodes Echinococcus multilocularis In the case of E. multilocularis, infection in intermediate hosts is regularly detected through the macroscopic examination of the target organs, like the liver, for lesions. However, the macroscopic examination may fail to detect exposure to the parasite, thus leading to an underestimation of the true infection prevalence. Consequently, macro- scopic examination is typically followed by histopathology, immunohistochemistry, or molecular tests. Massolo et al. applied a ddPCR assay and assessed its suitability for detecting E. multilocularis DNA in liver samples from intermediate hosts independently of macro- scopic lesions. The ddPCR assay provided the highest positivity rates for E. multilocu- laris DNA (15.09%) compared to qPCR (4.72%) and the presence of macroscopic lesions (1.88%). Applying such high-sensitivity molecular methods in prevalence studies can significantly increase the accuracy of the prevalence estimations. As depicted in the study of Massolo et al., great differences in the prevalence estimates may appear even between highly sensitive tools, as in the case of ddPCR and qPCR. According to the authors, this discrepancy could be related to the presence of bile acids in the liver, which act as inhibitors and negatively affect the performance of qPCR. They also suggested that results from high-sensitivity molecular methods, like ddPCR, should always be interpreted cautiously. Evidence of E. multilocularis DNA does not necessarily correspond to early, successfully developing lesions. It could represent cases of exposure to the parasite, which was eliminated by the immune system, and early or abortive infections, which are not expected to develop into successful infections. Nonetheless, the above study highlighted that sensitive molecular tools like ddPCR could better estimate the exposure rates of intermediate hosts, identify the transmission foci, define the competence of less common intermediate hosts, and refine epidemiological models. 5. Nematodes 5.1. Gastrointestinal Nematodes 5.1.1. Haemonchus contortus Haemonchus contortus (H. contortus) is one of the most pathogenic and abundant gastrointestinal nematodes in small ruminants. Infection may result in anemia, production losses, and mortality, mainly in lambs and pregnant ewes. Effective treatment aims to reduce the worm burden and pasture contamination, thus preventing the establishment of infective-stage larvae (L3). Treatment is based on broad-spectrum anthelmintics of three major drug classes, i.e., benzimidazoles, imidazothiazoles/tetrahydropyrimidines, and macrocyclic lactones. However, anthelmintic resistance has increased globally and has become a significant concern for the sheep industry. The occurrence of H. contortus-resistant field strains in all three most commonly used anthelmintic drug classes is well documented [56–58] and has led to the need for reliable screening and diagnostic techniques in routine settings. The Fecal Egg Count Reduction Test (FECRT) is the gold standard method for identifying clinical anthelmintic resistance in flocks. However, this method provides a rough estimation and lacks sensitivity. In addition, it is negatively affected by several parameters, such as the level of excretion, the aggregation of fecal egg counts (FECs), the sample size, and dilution factors [7,60]. Toward this end, several molecular tools have been developed and validated for screening, detecting, and evaluating resistance to anthelmintic drugs. Until now, the following Parasitologia 2023, 3 276 studies employed ddPCR assays in H. contortus investigation, focusing on identifying molecular markers that could be used to detect resistant field strains. In 2018, Baltrusis et al. validated and optimized a ddPCR assay using single adult H. contortus worms collected from 13 countries to detect and quantify the F200Y mutant allele that is linked to anthelmintic resistance to benzimidazole drugs. They targeted the β-tubulin isotype 1 gene, which is well known to present increased variability within populations of H. contortus and to result in resistance to benzimidazoles. Moreover, to obtain a reference read, they used ovine fecal larval culture samples containing mixed H. contortus strains (wild type and resistant strains) from Swedish sheep farms pre- and post-treatment with albendazole that had been molecularly characterized by an NGS platform (PacBio RSII Sequencing). When comparing the fractional abundance values (the percentage of the variant allele in the sum of background and variant alleles) of the resistance-determining mutant allele between NGS and the newly developed ddPCR assay, the two methods showed an excellent agreement and yielded highly similar fractional abundance values. Interestingly, although the initial FECRTs performed on post-treatment larval culture samples across various farms showed an efficient egg count reduction, NGS and ddPCR characterized the same strains as resistant. This finding suggests that although the resistant strains decreased after treatment, they persisted regardless of the treatment, and underlines the lack of FECRT sensitivity in detecting resistant strains. The authors suggested that ddPCR could be a powerful tool for mutation detection that needs to be further tested before being implemented in routine fecal examinations. In a 2020 study, Baltrušis et al. used pooled samples of mixed larvae cultures containing H. contortus from 67 farms in Sweden in a 6-year period to estimate the presence of the two most frequently observed mutations, F167Y and F200Y, in the isotype 1 β tubulin gene using an in-house ddPCR and pyrosequencing. They also compared the samples collected pre- and post-treatment with ivermectin or albendazole regarding changes in the frequency of the F200Y mutation. Similar to the previous study , the two methods had an excellent agreement concerning the frequency of the mutations. The F167Y mutation frequency was low, but the F200Y was dominant in the samples from most of the farms included in the study, irrespective of the year of sampling. Furthermore, the fractional changes of the mutation F200Y on farms before and after treatment with ivermectin or albendazole provided solid evidence only for the selection of the F200Y mutation after treatment with albendazole. Later, Baltrušis et al. used the previously mentioned ddPCR assay for detecting the F200Y mutation to estimate the frequency of the mutated β tubulin allele in L1 of H. contortus that had been hatched under gradually increasing thiabendazole concentra- tions. In this experimental study, the researchers used two laboratory-maintained strains with distinct resistance statuses, and they showed that F200Y can be used as the main genetic marker to estimate and evaluate the degree of benzimidazole resistance in this parasite species. An earlier study examined the suitability of dyf-7 Single Nucleotide Polymorphisms (SNPs) as a molecular marker for ivermectin resistance in H. contortus strains. The developed and validated ddPCR assay targeted the dyf-7 SNPs of H. contortus, using mixed species larval cultures from sheep feces pre- and post-treatment with ivermectin. The study included a number of Swedish sheep farms where FECRT demonstrated ivermectin failure. The ddPCR assay was robust for detecting mutations of the dyf-7 allele frequency in mixed larval cultures with a low threshold (≈3 copies/µL). However, this study showed that mutations in dyf-7 are not involved in ivermectin resistance because the fractional abundance was not increased in the post-treatment samples. Moreover, the frequency of the mutations was high in the post-treatment samples despite the ivermectin treatment being 100% effective based on the FECRT. Similarly, ddPCR assays have been developed in other studies to detect genetic mark- ers that could be associated with levamisole resistance in small ruminants. To that end, a ddPCR assay targeting the hco-acr-8 L-AchR subunit gene, previously identified as associ- Parasitologia 2023, 3 277 ated with levamisole resistance, was used. That study showed that hco-acr-8 L-AchR is not a predictive marker for levamisole resistance. Although the “resistant” allele was highly prevalent, the researchers did not observe a decrease in levamisole’s efficacy or an increased frequency of surviving animals in the field populations treated with levamisole. On the contrary, in another survey, a non-synonymous mutation in the exon 4 of this gene, resulting in the S168T substitution, was identified as a major determinant of levamisole resistance that could be used as a potential molecular marker in sheep populations. The researchers accomplished the application of ddPCR to define and assess the relative frequency of the S168T mutation. Moreover, following treatment with levamisole, they examined multiple phenotypically distinct H. contortus isolates and field larvae populations from Swedish sheep farms. 5.1.2. Trichuris spp. Lately, a ddPCR assay targeting the Internal Transcribed Spacer (ITS) gene of Trichuris spp. was applied to sheep fecal samples, and its performance was evaluated compared to qPCR. The ddPCR assay demonstrated good reproducibility and consistency even in low parasitic loads. The LOD was lower (less than 3.17 copies per reaction), and the sensitivity was higher than qPCR. Notably, the ddPCR assay detected more positive samples (80.6%) than qPCR (72.4%). At the same time, it presented high specificity without cross-amplification of other relevant gastrointestinal nematodes. This ddPCR assay could be useful for the accurate and early diagnosis of the infection in sheep and a valuable tool for the diagnosis and prevention of the disease. 5.1.3. Mixed Infections with Gastrointestinal Nematodes in Ruminants Although H. contortus has been recognized as a parasite of major concern in small rumi- nants due to its increased pathogenicity and rapidly emerging anthelmintic resistance , pasture-grazing sheep are also exposed to several other nematode species, resulting in multi-species infections. Mixed infections are especially important in cases of low levels of H. contortus infection that are difficult to detect with conventional parasitological techniques. Up to now, a wide variety of DNA-based approaches exist for detecting, quantifying, and discriminating the different gastrointestinal nematode species. In 2018, a ddPCR assay was developed and validated for the absolute quantification and identification of three of the most abundant genera of strongylids in sheep: Haemonchus, Teladorsagia, and Trichostrongylus. This assay employed one universal target for all strongylid gastrointestinal nematodes and three genus-specific targets, thus allowing the estimation of the relative abundance of each parasite species with high precision even in samples containing multiple genera of strongylids. Noticeably, no cross-amplifications were ob- served between the genera, verifying that the ddPCR assay is genus-specific. Moreover, the ddPCR assay presented a good agreement with FECRT. Regarding H. contortus, the researchers found excellent agreement between the Haemonchus-specific ddPCR assay and a well-established qPCR assay. They suggested that ddPCR could be used to evaluate the efficacy of different anthelmintics and could successfully complement FECRT and other routine diagnostic methods. The ddPCR assay developed by Elmahalawy et al. was later used to determine the occurrence and quantify the DNA copies of the three major strongylid genera infecting sheep in the following surveys. Högberg et al. investigated how activity patterns along with standard diagnostic indicators and FEC are influenced in naïve grazing lambs when they are exposed to gastrointestinal nematodes under natural grazing conditions. Höglund et al. provided an overview of the development of anthelmintic resistance in sheep farms in Sweden based on surveillance data. Finally, Högberg et al. investigated the effect of weaning age on animal performance in lambs naturally exposed to nematodes. Later, another ddPCR assay was developed to discriminate gastrointestinal nematodes frequently identified in mixed infections in cattle. In this case, the ddPCR assay targeted Cooperia spp. and Ostertagia spp. Both genera were amplified using the same primer pair, Parasitologia 2023, 3 278 and the discrimination was enabled using different probes in duplex reactions. The assay produced promising results in terms of fractional abundance and LOD for each parasite genus in the presence of the other. It detected Cooperia oncophora (C. oncophora) DNA when it represented only 2.5% of the template and Ostertagia ostertagi (O. ostertagi) DNA, even when it corresponded to only 0.67% of the template. 5.1.4. Dual Infections with Ascaridia galli and Heterakis gallinarum in Poultry As regards poultry nematodes, the flotation technique is sensitive, but the differen- tiation of Ascaridia galli (A. galli) and Heterakis gallinarum (H. gallinarum) is difficult. It requires professional skills and trained personnel due to the morphological similarities between the eggs of the two nematodes. On top of that, in dual infections, A. galli eggs encompass most of the excreted parasite eggs because H. gallinarum produces fewer eggs, thus underestimating the occurrence of mixed infections [74,75]. As for the necropsy, the two species are easily identified based on their substantial differences in size and location. However, it is considered an invasive procedure where healthy animals are sacrificed for diagnostic purposes [5,76]. Heterakis gallinarum may also be involved as an intermediate host in the life cycle of Histomonas meleagridis, the causative agent of histomonosis, which, in the absence of approved drugs for chicken in the EU, can reach up to 20% mortality, with high morbidity in chicken. Thus, the early detection and treatment of the H. gallinarum infection are crucial in flocks with a history of histomonosis as it comprises one of the primary management tools. In a 2021 study, the researchers developed a duplex ddPCR to identify and quantify A. galli and H. gallinarum DNA in chicken feces and evaluated its accuracy compared to the flotation technique. The two methods showed substantial agreement. The ddPCR assay displayed a 6% higher detection rate than the flotation technique. It also enabled the simultaneous detection and differentiation, with no cross-amplification, between these two intestinal nematodes of major importance. It is noteworthy that ddPCR had such a low LOD that enabled the identification of small amounts of H. gallinarum DNA in samples with dual infection with A. galli. In particular, in samples with a constant A. galli concentration, the lowest detection level of H. gallinarum DNA was as low as 0.8%. This critical feature makes ddPCR useful for diagnostics at individual and flock levels and overcomes the limitations of the flotation technique and necropsy, the traditional diagnostic procedures. The authors also emphasized that ddPCR does not rely on the quality and storage conditions of the samples. At the same time, this is not the case for the flotation technique, in which the freshness of the fecal material and the integrity of the parasite eggs strongly affect its sensitivity. This study showed that ddPCR could be a useful monitoring tool for A. galli and H. gallinarum dual infections in commercial chicken flocks. 5.2. Dirofilaria immitis A 2020 study used ddPCR to identify the role of the ecdysone signaling system during the developmental regulation of Dirofilaria immitis (D. immitis) microfilariae in its arthropod host, using an in vitro culture condition that mimics the mosquito host environment. This investigation aimed to give insights into the in vitro development of D. immitis microfilariae and provide data for novel targets for drug development. The ddPCR was employed during the transcript-level study and provided data for the absolute quantification of the target nucleic acids present in the sample. This study displayed that the ecdysone signaling system might play an important role in filarial nematode developmental transitions, and gave another example of the potential applications of ddPCR in veterinary parasitology. Lately, Curry et al. used ddPCR to measure the level of the expression of the D. immitis P-glycoprotein 11 (DimPgp-11) SNP in macrocyclic lactone-susceptible and resistant isolates. This study confirmed that genetic changes in the P-glycoprotein 11 gene, encoding an Parasitologia 2023, 3 279 ATP-binding cassette transporter, are associated with the macrocyclic lactone-resistant phenotypes and could be employed as markers of drug resistance. 6. Conclusions Novel molecular tools have emerged and are widely used even in routine diagnostics. In this context, the body of the literature is growing in human and veterinary medicine for the potential applications of dPCR. Currently, the vast majority of studies on this novel tool in veterinary parasitology focus on developing and validating dPCR assays for detecting and quantifying parasites of great financial impact on the food-producing animal industry. Some steps have been taken to apply dPCR for individualized medicine in companion animals. The dPCR assays developed so far presented high sensitivity and specificity, as well as low levels of detection, comparable to or even higher than qPCR and NGS platforms. This new molecular method accurately detects low parasitic loads in clinical samples, facilitating early diagnosis and treatment initiation at individual and flock levels, even in mixed infections. Regarding the parasitic diseases that species identification is crucial for diagnosis and treatment, dPCR is a promising tool. As for the absolute quantification of the parasitic burden, it will be an invaluable advantage for monitoring disease progression and treatment outcomes. Moreover, the use of dPCR in surveillance and epidemiological studies will increase our knowledge of the prevalence estimates and the role and com- petence of different hosts. Last but not least, dPCR has the potential to be used for the discovery of new molecular markers to identify resistance to parasiticides and new targets for drug development. Author Contributions: Conceptualization, C.N.T. and E.P.; methodology, C.N.T. and I.S.; inves- tigation, C.N.T. and I.S.; resources, I.S. and E.P.; data curation, C.N.T., I.S., G.S., A.I.G. and E.P.; writing—original draft preparation, C.N.T.; writing—review and editing, C.N.T., I.S., G.S., A.I.G. and E.P.; supervision, E.P.; and project administration, E.P. All authors have read and agreed to the published version of the manuscript. Funding: This research received no external funding. Institutional Review Board Statement: Not applicable. Informed Consent Statement: Not applicable. Data Availability Statement: No new data were created or analyzed in this study. Data sharing is not applicable to this article. Conflicts of Interest: The authors declare no conflict of interest. Abbreviations Cytochrome c oxidase subunit III gene in the mitochondrial genome (mtCOIII); deoxyribonu- cleic acid (DNA); digital PCR (dPCR); droplet digital PCR (ddPCR); fecal egg count (FEC); Fecal Egg Count Reduction Test (FECRT); Internal Transcribed Spacer (ITS); limit of detection (LOD); Next Generation Sequencing (NGS); Polymerase Chain Reaction (PCR); quantitative PCR (qPCR); ribonucleic acid (RNA); ribosomal RNA (rRNA); and Single Nucleotide Polymorphisms (SNPs). References 1. Kumar, S.; Gupta, S.; Mohmad, A.; Fular, A.; Parthasarathi, B.C.; Chaubey, A.K. Molecular Tools-Advances, Opportunities and Prospects for the Control of Parasites of Veterinary Importance. Int. J. Trop. Insect Sci. 2021, 41, 33–42. [CrossRef] [PubMed] 2. Baltrušis, P.; Höglund, J. Digital PCR: Modern Solution to Parasite Diagnostics and Population Trait Genetics. Parasites Vectors 2023, 16, 143. [CrossRef] 3. Elmahalawy, S.T.; Halvarsson, P.; Skarin, M.; Höglund, J. Droplet Digital Polymerase Chain Reaction (DdPCR) as a Novel Method for Absolute Quantification of Major Gastrointestinal Nematodes in Sheep. Vet. Parasitol. 2018, 261, 1–8. [CrossRef] Parasitologia 2023, 3 280 4. Snyder, R.P.; Guerin, M.T.; Hargis, B.M.; Imai, R.; Kruth, P.S.; Page, G.; Rejman, E.; Barta, J.R. Exploiting Digital Droplet PCR and Next Generation Sequencing Technologies to Determine the Relative Abundance of Individual Eimeria Species in a DNA Sample. Vet. Parasitol. 2021, 296, 109443. [CrossRef] [PubMed] 5. Tarbiat, B.; Enweji, N.; Baltrusis, P.; Halvarsson, P.; Osterman-Lind, E.; Jansson, D.S.; Höglund, J. A Novel Duplex DdPCR Assay for Detection and Differential Diagnosis of Ascaridia galli and Heterakis gallinarum Eggs from Chickens Feces. Vet. Parasitol. 2021, 296, 109499. [CrossRef] [PubMed] 6. Yu, Z.; Zhao, Z.; Chen, L.; Li, J.; Ju, X. Development of a Droplet Digital PCR for Detection of Trichuriasis in Sheep. J. Parasitol. 2020, 106, 603–610. [CrossRef] 7. Baltrušis, P.; Halvarsson, P.; Höglund, J. Exploring Benzimidazole Resistance in Haemonchus contortus by next Generation Sequencing and Droplet Digital PCR. Int. J. Parasitol. Drugs Drug Resist. 2018, 8, 411–419. [CrossRef] 8. Shang Kuan, T.-C.; Prichard, R.K. Developmental Regulation of Dirofilaria immitis Microfilariae and Evaluation of Ecdysone Signaling Pathway Transcript Level Using Droplet Digital PCR. Parasites Vectors 2020, 13, 614. [CrossRef] 9. Van Dorssen, C.F.; Gordon, C.A.; Li, Y.; Williams, G.M.; Wang, Y.; Luo, Z.; Gobert, G.N.; You, H.; McManus, D.P.; Gray, D.J. Rodents, Goats and Dogs—Their Potential Roles in the Transmission of Schistosomiasis in China. Parasitology 2017, 144, 1633–1642. [CrossRef] 10. Chen, B.; Jiang, Y.; Cao, X.; Liu, C.; Zhang, N.; Shi, D. Droplet Digital PCR as an Emerging Tool in Detecting Pathogens Nucleic Acids in Infectious Diseases. Clin. Chim. Acta 2021, 517, 156–161. [CrossRef] 11. Wichianchot, S.; Hongsrichan, N.; Maneeruttanarungroj, C.; Pinlaor, S.; Iamrod, K.; Purisarn, A.; Donthaisong, P.; Karanis, P.; Nimsuphan, B.; Rucksaken, R. A Newly Developed Droplet Digital PCR for Ehrlichia Canis Detection: Comparisons to Conventional PCR and Blood Smear Techniques. J. Vet. Med. Sci. 2022, 84, 831–840. [CrossRef] [PubMed] 12. Massolo, A.; Gerber, A.; Umhang, G.; Nicholas, C.; Liccioli, S.; Mori, K.; Klein, C. Droplet Digital PCR as a Sensitive Tool to Assess Exposure Pressure from Echinococcus multilocularis in Intermediate Hosts. Acta Trop. 2021, 223, 106078. [CrossRef] [PubMed] 13. Powell, E.A.; Babady, N.E. Digital PCR in the Clinical Microbiology Laboratory: Another Tool on the Molecular Horizon. Clin. Microbiol. Newsl. 2018, 40, 27–32. [CrossRef] 14. Salipante, S.J.; Jerome, K.R. Digital PCR—An Emerging Technology with Broad Applications in Microbiology. Clin. Chem. 2020, 66, 117–123. [CrossRef] 15. Fatoba, A.J.; Adeleke, M.A. Diagnosis and Control of Chicken Coccidiosis: A Recent Update. J. Parasit. Dis. 2018, 42, 483–493. [CrossRef] 16. Long, P.L.; Joyner, L.P. Problems in the Identification of Species of Eimeria. J. Protozool. 1984, 31, 535–541. [CrossRef] 17. Kawahara, F.; Taira, K.; Nagai, S.; Onaga, H.; Onuma, M.; Nunoya, T. Detection of Five Avian Eimeria Species by Species-Specific Real-Time Polymerase Chain Reaction Assay. Avian Dis. 2008, 52, 652–656. [CrossRef] 18. Kirkpatrick, N.C.; Blacker, H.P.; Woods, W.G.; Gasser, R.B.; Noormohammadi, A.H. A Polymerase Chain Reaction-Coupled High-Resolution Melting Curve Analytical Approach for the Monitoring of Monospecificity of Avian Eimeria Species. Avian Pathol. 2009, 38, 13–19. [CrossRef] 19. Lalonde, L.F.; Gajadhar, A.A. Detection and Differentiation of Coccidian Oocysts by Real-Time PCR and Melting Curve Analysis. J. Parasitol. 2011, 97, 725–730. [CrossRef] 20. Perkins, S.L. Malaria’s Many Mates: Past, Present, and Future of the Systematics of the Order Haemosporida. J. Parasitol. 2014, 100, 11–25. [CrossRef] 21. Valkiūnas, G.; Iezhova, T.A. Keys to the Avian Haemoproteus Parasites (Haemosporida, Haemoproteidae). Malar. J. 2022, 21, 269. [CrossRef] [PubMed] 22. Atkinson, C.T.; Thomas, N.J.; Hunter, D.B. (Eds.) Parasitic Diseases of Wild Birds; Wiley-Blackwell: Ames, IA, USA, 2008; ISBN 978-0-8138-2081-1. 23. Bernotienė, R.; Palinauskas, V.; Iezhova, T.; Murauskaitė, D.; Valkiūnas, G. Avian Haemosporidian Parasites (Haemosporida): A Comparative Analysis of Different Polymerase Chain Reaction Assays in Detection of Mixed Infections. Exp. Parasitol. 2016, 163, 31–37. [CrossRef] [PubMed] 24. Valkiŭnas, G.; Bensch, S.; Iezhova, T.A.; Krizanauskiené, A.; Hellgren, O.; Bolshakov, C.V. Nested Cytochrome b Polymerase Chain Reaction Diagnostics Underestimate Mixed Infections of Avian Blood Haemosporidian Parasites: Microscopy Is Still Essential. J. Parasitol. 2006, 92, 418–422. [CrossRef] [PubMed] 25. Bensch, S.; Hellgren, O. The Use of Molecular Methods in Studies of Avian Haemosporidians. In Avian Malaria and Related Parasites in the Tropics; Santiago-Alarcon, D., Marzal, A., Eds.; Springer International Publishing: Cham, Switzerland, 2020; pp. 113–135; ISBN 978-3-030-51632-1. 26. Huang, X. Assessment of Associations between Malaria Parasites and Avian Hosts-A Combination of Classic System and Modern Molecular Approach. Biology 2021, 10, 636. [CrossRef] 27. Jiang, Y.; Brice, B.; Nguyen, M.; Loh, R.; Greay, T.; Adlard, R.; Ryan, U.; Yang, R. Further Characterisation of Leucocytozoon Podargii in Wild Tawny Frogmouths (Podargus strigoides) in Western Australia. Parasitol. Res. 2019, 118, 1833–1840. [CrossRef] 28. Kao, Y.-F.; Peake, B.; Madden, R.; Cowan, S.R.; Scimeca, R.C.; Thomas, J.E.; Reichard, M.V.; Ramachandran, A.; Miller, C.A. A Probe-Based Droplet Digital Polymerase Chain Reaction Assay for Early Detection of Feline Acute Cytauxzoonosis. Vet. Parasitol. 2021, 292, 109413. [CrossRef] Parasitologia 2023, 3 281 29. Lloret, A.; Addie, D.D.; Boucraut-Baralon, C.; Egberink, H.; Frymus, T.; Gruffydd-Jones, T.; Hartmann, K.; Horzinek, M.C.; Hosie, M.J.; Lutz, H.; et al. Cytauxzoonosis in Cats: ABCD Guidelines on Prevention and Management. J. Feline Med. Surg. 2015, 17, 637–641. [CrossRef] 30. O’Leary, J.K.; Sleator, R.D.; Lucey, B. Cryptosporidium spp. Diagnosis and Research in the 21st Century. Food Waterborne Parasitol. 2021, 24, e00131. [CrossRef] 31. Fayer, R. Cryptosporidium: A Water-Borne Zoonotic Parasite. Vet. Parasitol. 2004, 126, 37–56. [CrossRef] 32. Khurana, S.; Chaudhary, P. Laboratory Diagnosis of Cryptosporidiosis. Trop. Parasitol. 2018, 8, 2. [CrossRef] 33. Yang, R.; Paparini, A.; Monis, P.; Ryan, U. Comparison of Next-Generation Droplet Digital PCR (DdPCR) with Quantitative PCR (QPCR) for Enumeration of Cryptosporidium Oocysts in Faecal Samples. Int. J. Parasitol. 2014, 44, 1105–1113. [CrossRef] [PubMed] 34. Zahedi, A.; Ryan, U.; Rawlings, V.; Greay, T.; Hancock, S.; Bruce, M.; Jacobson, C. Cryptosporidium and Giardia in Dam Water on Sheep Farms—An Important Source of Transmission? Vet. Parasitol. 2020, 288, 109281. [CrossRef] 35. Mthethwa, N.P.; Amoah, I.D.; Reddy, P.; Bux, F.; Kumari, S. Development and Evaluation of a Molecular Based Protocol for Detection and Quantification of Cryptosporidium spp. in Wastewater. Exp. Parasitol. 2022, 234, 108216. [CrossRef] [PubMed] 36. Hawash, Y. DNA Extraction from Protozoan Oocysts/Cysts in Feces for Diagnostic PCR. Korean J. Parasitol. 2014, 52, 263–271. [CrossRef] 37. Schrader, C.; Schielke, A.; Ellerbroek, L.; Johne, R. PCR Inhibitors—Occurrence, Properties and Removal. J. Appl. Microbiol. 2012, 113, 1014–1026. [CrossRef] [PubMed] 38. Zacharia, A.; Ahmada, W.; Outwater, A.H.; Ngasala, B.; Van Deun, R. Evaluation of Occurrence, Concentration, and Removal of Pathogenic Parasites and Fecal Coliforms in Three Waste Stabilization Pond Systems in Tanzania. Sci. World J. 2019, 2019, 3415617. [CrossRef] 39. Bruno, B.; Romano, A.; Zanatta, R.; Spina, S.; Mignone, W.; Ingravalle, F.; Barzanti, P.; Ceccarelli, L.; Goria, M. Serum Indirect Immunofluorescence Assay and Real-Time PCR Results in Dogs Affected by Leishmania infantum: Evaluation before and after Treatment at Different Clinical Stages. J. Vet. Diagn. Investig. 2019, 31, 222–227. [CrossRef] 40. Francino, O.; Altet, L.; Sánchez-Robert, E.; Rodriguez, A.; Solano-Gallego, L.; Alberola, J.; Ferrer, L.; Sánchez, A.; Roura, X. Advantages of Real-Time PCR Assay for Diagnosis and Monitoring of Canine Leishmaniosis. Vet. Parasitol. 2006, 137, 214–221. [CrossRef] 41. Akhoundi, M.; Downing, T.; Votýpka, J.; Kuhls, K.; Lukeš, J.; Cannet, A.; Ravel, C.; Marty, P.; Delaunay, P.; Kasbari, M.; et al. Leishmania Infections: Molecular Targets and Diagnosis. Mol. Asp. Med. 2017, 57, 1–29. [CrossRef] 42. Tsokana, C.N.; Athanasiou, L.V.; Valiakos, G.; Spyrou, V.; Manolakou, K.; Billinis, C. Molecular Diagnosis of Leishmaniasis, Species Identification and Phylogenetic Analysis. In Leishmaniasis—Trends in Epidemiology, Diagnosis and Treatment; Claborn, D., Ed.; InTech: London, UK, 2014; ISBN 978-953-51-1232-7. 43. Pereira, D.C.A.; Teixeira-Neto, R.G.; Lopes, V.V.; Pena, H.P.; Paz, G.F.; Custodio, C.H.X.; Belo, V.S.; Da Fonseca Júnior, A.A.; Da Silva, E.S. Development of Quantitative PCR and Digital PCR for the Quantification of Leishmania infantum in Dogs. Mol. Cell Biochem. 2023. [CrossRef] 44. De Vasconcelos, T.C.B.; Bruno, S.F.; de Miranda, L.H.M.; Conceição-Silva, F.; Belo, V.S.; Figueiredo, F.B. Parasite Load, INOS and Cytokine Profiles, and Histopathological Aspects of Leishmania infantum Infection in Dogs with Different Clinical Presentations. Cienc. Rural. 2019, 49, e20180984. [CrossRef] 45. Murthy, S.; Suresh, A.; Dandasena, D.; Singh, S.; Subudhi, M.; Bhandari, V.; Bhanot, V.; Arora, J.S.; Sharma, P. Multiplex DdPCR: A Promising Diagnostic Assay for Early Detection and Drug Monitoring in Bovine Theileriosis. Pathogens 2023, 12, 296. [CrossRef] 46. Mans, B.J.; Pienaar, R.; Latif, A.A. A Review of Theileria Diagnostics and Epidemiology. Int. J. Parasitol. Parasites Wildl. 2015, 4, 104–118. [CrossRef] [PubMed] 47. Mhadhbi, M.; Naouach, A.; Boumiza, A.; Chaabani, M.F.; BenAbderazzak, S.; Darghouth, M.A. In Vivo Evidence for the Resistance of Theileria annulata to Buparvaquone. Vet. Parasitol. 2010, 169, 241–247. [CrossRef] [PubMed] 48. Mancusi, A.; Giordano, A.; Bosco, A.; Girardi, S.; Proroga, Y.T.R.; Morena, L.; Pinto, R.; Sarnelli, P.; Cringoli, G.; Rinaldi, L.; et al. Development of a Droplet Digital Polymerase Chain Reaction Tool for the Detection of Toxoplasma Gondii in Meat Samples. Parasitol. Res. 2022, 121, 1467–1473. [CrossRef] [PubMed] 49. Opsteegh, M.; Langelaar, M.; Sprong, H.; Den Hartog, L.; De Craeye, S.; Bokken, G.; Ajzenberg, D.; Kijlstra, A.; Der Giessen, J.V. Direct Detection and Genotyping of Toxoplasma Gondii in Meat Samples Using Magnetic Capture and PCR. Int. J. Food Microbiol. 2010, 139, 193–201. [CrossRef] 50. Marino, A.M.F.; Giunta, R.P.; Salvaggio, A.; Castello, A.; Alfonzetti, T.; Barbagallo, A.; Aparo, A.; Scalzo, F.; Reale, S.; Buffolano, W.; et al. Toxoplasma Gondii in Edible Fishes Captured in the Mediterranean Basin. Zoonoses Public. Health 2019, 66, 826–834. [CrossRef] 51. Gray, D.J.; Li, Y.-S.; Williams, G.M.; Zhao, Z.-Y.; Harn, D.A.; Li, S.-M.; Ren, M.-Y.; Feng, Z.; Guo, F.-Y.; Guo, J.-G.; et al. A Multi-Component Integrated Approach for the Elimination of Schistosomiasis in the People’s Republic of China: Design and Baseline Results of a 4-Year Cluster-Randomised Intervention Trial. Int. J. Parasitol. 2014, 44, 659–668. [CrossRef] Parasitologia 2023, 3 282 52. Wang, T.-P.; Vang Johansen, M.; Zhang, S.-Q.; Wang, F.-F.; Wu, W.-D.; Zhang, G.-H.; Pan, X.-P.; Ju, Y.; Ørnbjerg, N. Transmission of Schistosoma japonicum by Humans and Domestic Animals in the Yangtze River Valley, Anhui Province, China. Acta Trop. 2005, 96, 198–204. [CrossRef] 53. Liccioli, S.; Duignan, P.J.; Lejeune, M.; Deunk, J.; Majid, S.; Massolo, A. A New Intermediate Host for Echinococcus multilocularis: The Southern Red-Backed Vole (Myodes gapperi) in Urban Landscape in Calgary, Canada. Parasitol. Int. 2013, 62, 355–357. [CrossRef] 54. Besier, R.B.; Kahn, L.P.; Sargison, N.D.; Van Wyk, J.A. The Pathophysiology, Ecology and Epidemiology of Haemonchus contortus Infection in Small Ruminants. In Advances in Parasitology; Elsevier: Amsterdam, The Netherlands, 2016; Volume 93, pp. 95–143; ISBN 978-0-12-810395-1. 55. Sargison, N.D. Pharmaceutical Control of Endoparasitic Helminth Infections in Sheep. Vet. Clin. North. Am. Food Anim. Pract. 2011, 27, 139–156. [CrossRef] 56. Playford, M.; Smith, A.; Love, S.; Besier, R.; Kluver, P.; Bailey, J. Prevalence and Severity of Anthelmintic Resistance in Ovine Gastrointestinal Nematodes in Australia (2009–2012). Aust. Vet. J. 2014, 92, 464–471. [CrossRef] [PubMed] 57. Rose, H.; Rinaldi, L.; Bosco, A.; Mavrot, F.; De Waal, T.; Skuce, P.; Charlier, J.; Torgerson, P.R.; Hertzberg, H.; Hendrickx, G.; et al. Widespread Anthelmintic Resistance in European Farmed Ruminants: A Systematic Review. Vet. Rec. 2015, 176, 546-546. [CrossRef] 58. Tsotetsi, A.M.; Njiro, S.; Katsande, T.C.; Moyo, G.; Baloyi, F.; Mpofu, J. Prevalence of Gastrointestinal Helminths and Anthelmintic Resistance on Small-Scale Farms in Gauteng Province, South Africa. Trop. Anim. Health Prod. 2013, 45, 751–761. [CrossRef] 59. Várady, M.; Papadopoulos, E.; Dolinská, M.; Königová, A. Anthelmintic Resistance in Parasites of Small Ruminants: Sheep versus Goats. Helminthologia 2011, 48, 137–144. [CrossRef] 60. Höglund, J.; Gustafsson, K.; Ljungström, B.-L.; Engström, A.; Donnan, A.; Skuce, P. Anthelmintic Resistance in Swedish Sheep Flocks Based on a Comparison of the Results from the Faecal Egg Count Reduction Test and Resistant Allele Frequencies of the β-Tubulin Gene. Vet. Parasitol. 2009, 161, 60–68. [CrossRef] 61. Von Samson-Himmelstjerna, G.; Walsh, T.K.; Donnan, A.A.; Carrière, S.; Jackson, F.; Skuce, P.J.; Rohn, K.; Wolstenholme, A.J. Molecular Detection of Benzimidazole Resistance in Haemonchus contortus Using Real-Time PCR and Pyrosequencing. Parasitology 2009, 136, 349–358. [CrossRef] [PubMed] 62. Baltrušis, P.; Halvarsson, P.; Höglund, J. Utilization of Droplet Digital PCR to Survey Resistance Associated Polymorphisms in the β Tubulin Gene of Haemonchus contortus in Sheep Flocks in Sweden. Vet. Parasitol. 2020, 288, 109278. [CrossRef] [PubMed] 63. Baltrušis, P.; Komáromyová, M.; Várady, M.; Von Samson-Himmelstjerna, G.; Höglund, J. Assessment of the F200Y Muta- tion Frequency in the β Tubulin Gene of Haemonchus contortus Following the Exposure to a Discriminating Concentration of Thiabendazole in the Egg Hatch Test. Exp. Parasitol. 2020, 217, 107957. [CrossRef] 64. Elmahalawy, S.T.; Halvarsson, P.; Skarin, M.; Höglund, J. Genetic Variants in Dyf-7 Validated by Droplet Digital PCR Are Not Drivers for Ivermectin Resistance in Haemonchus contortus. Int. J. Parasitol. Drugs Drug Resist. 2018, 8, 278–286. [CrossRef] 65. Baltrušis, P.; Charvet, C.L.; Halvarsson, P.; Mikko, S.; Höglund, J. Using Droplet Digital PCR for the Detection of Hco-Acr-8b Levamisole Resistance Marker in H. contortus. Int. J. Parasitol. Drugs Drug Resist. 2021, 15, 168–176. [CrossRef] [PubMed] 66. Baltrušis, P.; Halvarsson, P.; Charvet, C.L.; Höglund, J. The Presence and Relative Frequency Detection of the Levamisole- Resistance-Associated S168T Substitution in Hco-Acr-8 in Haemonchus contortus. Int. J. Parasitol. Drugs Drug Resist. 2023, 21, 91–95. [CrossRef] [PubMed] 67. Waller, P.J.; Chandrawathani, P. Haemonchus Contortus: Parasite Problem No. 1 from Tropics—Polar Circle. Problems and Prospects for Control Based on Epidemiology. Trop. Biomed. 2005, 22, 131–137. 68. Ljungström, S.; Melville, L.; Skuce, P.J.; Höglund, J. Comparison of Four Diagnostic Methods for Detection and Relative Quantification of Haemonchus contortus Eggs in Feces Samples. Front. Vet. Sci. 2018, 4, 239. [CrossRef] 69. Zarlenga, D.S.; Hoberg, E.P.; Tuo, W. The Identification of Haemonchus Species and Diagnosis of Haemonchosis. In Advances in Parasitology; Elsevier: Amsterdam, The Netherlands, 2016; Volume 93, pp. 145–180. ISBN 978-0-12-810395-1. 70. Högberg, N.; Hessle, A.; Lidfors, L.; Enweji, N.; Höglund, J. Nematode Parasitism Affects Lying Time and Overall Activity Patterns in Lambs Following Pasture Exposure around Weaning. Vet. Parasitol. 2021, 296, 109500. [CrossRef] [PubMed] 71. Höglund, J.; Baltrušis, P.; Enweji, N.; Gustafsson, K. Signs of Multiple Anthelmintic Resistance in Sheep Gastrointestinal Nematodes in Sweden. Vet. Parasitol. Reg. Stud. Rep. 2022, 36, 100789. [CrossRef] 72. Högberg, N.; Hessle, A.; Lidfors, L.; Höglund, J. The Effect of Weaning Age on Animal Performance in Lambs Exposed to Naturally Acquired Nematode Infections. Vet. Parasitol. 2023, 316, 109900. [CrossRef] 73. Baltrušis, P.; Halvarsson, P.; Höglund, J. Molecular Detection of Two Major Gastrointestinal Parasite Genera in Cattle Using a Novel Droplet Digital PCR Approach. Parasitol. Res. 2019, 118, 2901–2907. [CrossRef] 74. Daş, G.; Abel, H.; Savaş, T.; Sohnrey, B.; Gauly, M. Egg Production Dynamics and Fecundity of Heterakis gallinarum Residing in Different Caecal Environments of Chickens Induced by Fibre-Rich Diets. Vet. Parasitol. 2014, 205, 606–618. [CrossRef] 75. Wongrak, K.; Gauly, M.; Daş, G. Diurnal Fluctuations in Nematode Egg Excretion in Naturally and in Experimentally Infected Chickens. Vet. Parasitol. 2015, 208, 195–203. [CrossRef] Parasitologia 2023, 3 283 76. Luna-Olivares, L.A.; Ferdushy, T.; Kyvsgaard, N.C.; Nejsum, P.; Thamsborg, S.M.; Roepstorff, A.; Iburg, T.M. Localization of Ascaridia Galli Larvae in the Jejunum of Chickens 3 Days Post Infection. Vet. Parasitol. 2012, 185, 186–193. [CrossRef] 77. McDougald, L.R. Blackhead Disease (Histomoniasis) in Poultry: A Critical Review. Avian Dis. 2005, 49, 462–476. [CrossRef] 78. Curry, E.; Prichard, R.; Lespine, A. Genetic Polymorphism, Constitutive Expression and Tissue Localization of Dirofilaria immitis P-Glycoprotein 11: A Putative Marker of Macrocyclic Lactone Resistance. Parasit. Vectors 2022, 15, 482. [CrossRef] Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content. View publication stats

Current Applications of Digital PCR in Veterinary Parasitology: An Overview PDF

Document Details

Tags

Related

Summary

Full Transcript

Upgrade to continue