Rumen fluke (Paramphistomatidae spp.) are trematode parasites infecting ruminants worldwide. Traditionally rumen flukes were regarded as parasites mainly confined to tropical and sub-tropical areas. However, within European livestock, the presence in recent decades of high levels of rumen fluke, in particularly the species Calicophoron daubneyi, is of potential concern. Calicophoron daubneyi was first recorded infecting cattle in Kenya in the 1950s (Dinnik, Reference Dinnik1962), with confirmation of its occurrence in Europe from the 1970s (Sey, Reference Sey1980) and the UK in 2012 (Gordon et al. Reference Gordon, Zadoks, Skuce and Sargison2012). In recent years, the UK has experienced an apparent sudden increase in the prevalence of rumen fluke, with the proportion of rumen fluke detected in ruminant submissions by passive veterinary surveillance increasing on average by 57% annually between 2010 and 2015 (VIDA, 2016a ). High prevalence has been observed across Western Europe, with abattoir studies recording cattle prevalence levels of 29% in the UK (Sargison et al. Reference Sargison, Francis, Davison, Bronsvoort, Handel and Mazeri2016), 44·7% in France (Mage et al. Reference Mage, Bourgne, Toullieu, Rondelaud and Dreyfuss2002), 18·8% in Spain (Gonzalez-Warleta et al. Reference Gonzalez-Warleta, Lladosa, Castro-Hermida, Martinez-Ibeas, Conesa, Munoz, Lopez-Quilez, Manga-Gonzalez and Mezo2013), 28% in Belgium (Malrait et al. Reference Malrait, Verschave, Skuce, Van Loo, Vercruysse and Charlier2015) and 52% in Ireland (Toolan et al. Reference Toolan, Mitchell, Searle, Sheehan, Skuce and Zadoks2015). Paramphistomosis (rumen fluke disease) has been reported in both cattle (Millar et al. Reference Millar, Colloff and Scholes2012) and sheep (Mason et al. Reference Mason, Stevenson, Cox and Dick2012) in the UK, however, UK passive veterinary surveillance has been detecting rumen fluke in larger proportions of cattle submissions compared with sheep submissions (VIDA, 2016a ), while in Ireland prevalence levels have been shown to be lower in sheep compared with cattle (Toolan et al. Reference Toolan, Mitchell, Searle, Sheehan, Skuce and Zadoks2015). In all cases of paramphistomosis, a heavy burden of juvenile fluke in the intestine has been attributed as the cause of the disease, with adult C. daubneyi believed to be well tolerated (Zintl et al. Reference Zintl, Garcia-Campos, Trudgett, Chryssafidis, Talavera-Arce, Fu, Egan, Lawlor, Negredo, Brennan, Hanna, De Waal and Mulcahy2014). Nevertheless, adult C. daubneyi are known to induce inflammatory reactions in the rumen and reticulum (Fuertes et al. Reference Fuertes, Pérez, Benavides, González-Lanza, Mezo, González-Warleta, Giráldez, Fernández, Manga-González and Ferreras2015), and in some instances may cause symptoms including bloat, loss of condition and the softening of feces in infected cattle (Alzieu and Dorchies, Reference Alzieu and Dorchies2007). The potential threat of these symptoms to the UK livestock industry is heightened due to limited anthelmintic options for treatment, with oxyclozanide the only anthelmintic regarded as an effective paramphistomicide (Malrait et al. Reference Malrait, Verschave, Skuce, Van Loo, Vercruysse and Charlier2015). All published molecular level studies highlight C. daubneyi as the dominant and potentially the only Paramphistomatidae species present in UK livestock (Gordon et al. Reference Gordon, Roberts, Lean, Zadoks, Sargison and Skuce2013; Huson et al. Reference Huson, Brophy, Morphew and Mackintosh2015), while earlier reports of Paramphistomum cervi in British livestock were only based on morphological identification (Pillers, Reference Pillers1922; Craig and Davies, Reference Craig and Davies1937). Recent molecular analyses have also identified Paramphistomum leydeni infecting reindeer in south west England (VIDA, 2016b ) and fallow deer in Ireland (O'Toole et al. Reference O'Toole, Browne, Hogan, Bassiere, DeWaal, Mulcahy and Zintl2014), leading to the possibility of alternative Paramphistomatidae spp. infecting UK livestock.
As with other trematode species, rumen fluke requires an intermediate snail host to complete its lifecycle, a process which sees the parasite exploit this host to develop and multiply rapidly. The prominent host of C. daubneyi is Galba truncatula (Dinnik, Reference Dinnik1962; Degueurce et al. Reference Degueurce, Abrous, Dreyfuss, Rondelaud and Gevrey1999; Martinez-Ibeas et al. Reference Martinez-Ibeas, Gonzalez-Warleta, Martinez-Valladares, Castro-Hermida, Gonzalez-Lanza, Minambres, Ferreras, Mezo and Manga-Gonzalez2013), a snail species, which thrives in the UKs consistently wet and mild climate. Galba truncatula is also the prominent intermediate host of the highly pathogenic liver fluke (Fasciola hepatica), a parasite which has been endemic in the UK for centuries (Dalton, Reference Dalton1998). As G. truncatula has recently been shown to host C. daubneyi in the UK (Jones et al. Reference Jones, Williams, Dalesman and Brophy2015), the potential epidemiological range of this parasite is also likely to be widespread.
Numerous predictive models of F. hepatica based on key climatic drivers for G. truncatula activity, including rainfall and temperature have been created over the past 60 years. The most prominent model, the Ollerenshaw index (Ollerenshaw and Rowlands, Reference Ollerenshaw and Rowlands1959), is widely used commercially as a regional fasciolosis risk guide for farmers (NADIS, 2016). In recent years, further climatic F. hepatica models have been created with the inclusion of either or both environmental factors (McCann et al. Reference McCann, Baylis and Williams2010) and farm management factors (Howell et al. Reference Howell, Baylis, Smith, Pinchbeck and Williams2015) in an attempt to predict fasciolosis occurrence at a finer scale. As well as increasing the accuracy of models, any farm management practices identified as risk factors for F. hepatica may inform veterinarians and farmers of best practices to negate fasciolosis risk. However, despite their similar reliance on G. truncatula, it remains to be resolved whether these models can accurately predict the occurrence of C. daubneyi due to differences in their epidemiology including, different egg hatching stimulus (Chryssafidis et al. Reference Chryssafidis, Fu, De Waal and Mulcahy2015), timeframe of development within the snail (Dreyfuss, Reference Dreyfuss2015), sensitivity to temperature at shedding (Abrous et al. Reference Abrous, Rondelaud and Dreyfuss1999) and geotropism of cercariae (Dreyfuss et al. Reference Dreyfuss, Abrous, Vignoles and Rondelaud2004). These epidemiological differences mean risk factors for C. daubneyi presence may vary significantly from F. hepatica, although risk factors for G. truncatula occurrence are likely to be confounding risk factors for both parasites. Calicophoron daubneyi models are currently scarce compared with models for F. hepatica. A Galician model identified decreasing rainfall and temperature, and increasing cattle density and slope as predictors of C. daubneyi prevalence in cattle (Gonzalez-Warleta et al. Reference Gonzalez-Warleta, Lladosa, Castro-Hermida, Martinez-Ibeas, Conesa, Munoz, Lopez-Quilez, Manga-Gonzalez and Mezo2013), while an Italian Apennines model identified the presence of streams, springs or brooks, heathland and moorland as positive predictors of C. daubneyi (Cringoli et al. Reference Cringoli, Taddei, Rinaldi, Veneziano, Musella, Cascone, Sibilio and Malone2004). In these countries, the climate, environment and agricultural systems are very different to the UK, and risk factors associated with C. daubneyi prevalence is therefore likely to vary within each country. There are also unanswered questions regarding the potential interaction between C. daubneyi and F. hepatica at intermediate host level in the UK (Jones et al. Reference Jones, Williams, Dalesman and Brophy2015), which could influence each parasite's distribution in the presence of the other. This consequence could be positive, due to a synergistic effect in infecting alternative snail species (Abrous et al. Reference Abrous, Rondelaud, Dreyfuss and Cabaret1998), or negative, due to within-snail predation and competition for nutrients (Rondelaud et al. Reference Rondelaud, Vignoles and Dreyfuss2007).
In this case study, the prevalence of C. daubneyi on participating Welsh farms was recorded along with climatic, environmental and farm management factors for each farm. The aim was to create models explaining the presence of C. daubneyi on Welsh farms and to identify associated risk factors. Fasciola hepatica prevalence was also recorded with the aim of comparing the prevalence, infection intensity and risk factors of both parasites.
MATERIALS AND METHODS
During 2015 farmers were invited to participate in the study through Young Farmers Clubs Wales, on social media and at various agricultural events. From September 2015 participants were instructed to fill an online questionnaire (Schmitz, Reference Schmitz2015) containing 36 questions regarding the number and type of livestock on their farm, the presence of liver fluke and rumen fluke on their farm, their farms environmental features and management factors. Twenty-nine questions were closed, and seven were open ended. Open ended questions included months when cattle were housed, months of liver fluke and rumen fluke treatment, and which anthelmintics were used to treat against each parasite. In the case of anthelmintic use, answers given as the product brand name were transformed into the active drug class for that particular product. Participants were also asked to provide their full postal address and the postcode district location of each of their major holdings along with their proportional size. In total of 128 farmers completed the survey, all of which indicated their willingness to test their livestock for fluke. The project was approved by the Aberystwyth University Research Ethics Panel (project number 496).
Fecal sampling and testing
A total of 128 packages containing gloves, 25 mL measuring apparatus, 50 mL tubes, question sheet and a prepaid return envelope were dispatched, and 100 were returned with appropriate samples between November 2015 and February 2016. Participants were instructed to collect 25 mL of feces from 20 individual cattle or sheep using a supplied measuring apparatus, before thoroughly mixing the samples and using the same apparatus to place 25 mL of feces in a supplied tube for posting to the laboratory. Farmers with both cattle and sheep were requested to repeat the process for both species and return separate 25 mL samples. The amount of feces requested for submission was selected to ensure return packages conformed to UN3373 biological sample postage regulations. Participants were also invited to submit details of sampled animals including, their age and most recent anthelmintic treatment against fluke species. Samples were stored at 4 °C and processed within 48 h of arrival at the laboratory. Fecal samples were tested for fluke infection using a sedimentation fecal egg count (FEC) technique. Approximately 20 g of feces were mixed thoroughly with water and washed through 300, 150 and 45 µm mesh sieves. Materials including any fluke eggs collected on the 45 µm sieves were washed into a 1 L measuring cylinders and allowed to sediment for 7 min. The supernatant was removed via aspiration, with the process repeated 3–4 times until the sample was sufficiently clear. The samples were then stained with two drops of 1% methylene blue, placed in a 5 cm petri dish and viewed under a stereo microscope to count fluke eggs. Fluke eggs were differentiated via the golden and clear colour of F. hepatica and C. daubneyi eggs, respectively (Kajugu et al. Reference Kajugu, Hanna, Edgar, McMahon, Cooper, Gordon, Barley, Malone, Brennan and Fairweather2015), before the numbers of eggs counted were divided with the weight of feces tested to calculate the eggs per gram (EPG) values.
Identification of C. daubneyi in rumen fluke positive cases
DNA from rumen fluke eggs that were isolated from feces via FEC were used to confirm the presence of C. daubneyi in each positive sample. Eggs and debris were resedimented until concentrated into a 0·5 mL centrifuge tube. If very low levels of eggs were observed during the FEC, the eggs were pipetted from the final FEC sedimentation to a 0·5 mL centrifuge tube. Four 0·1–0·5 mm zirconia beads and 100 µL of 5% Chelex® 100 (Bio-Rad, Hercules, USA) was added to the mixture and vortexed for 2 min, prior to incubation firstly at 56 °C for 60 min, and secondly at 95 °C for 10 min. Samples were centrifuged at 15 000 rpm for 7 min with the supernatant diluted to the required concentration with nuclease free water (1/10 or 1/100). Each DNA extraction sample was subjected to an in-house polymerase chain reaction (PCR) protocol using C. daubneyi specific primers (F:5′-GTTTGTGTGGTTTGCCACGG-3′; R:5′-CTACCCCAAGCAGCCACTAC-3′) that amplifies 169 bp strands from the C. daubneyi cytochrome c oxidase subunit 1 (cox1) gene (GenBank JQ815200). Primers were designed using Geneious software (Kearse et al. Reference Kearse, Moir, Wilson, Stones-Havas, Cheung, Sturrock, Buxton, Cooper, Markowitz, Duran, Thierer, Ashton, Mentjies and Drummond2012) and were based on regions of the cox1 gene unique to C. daubneyi in comparison with other Paramphistomatidae spp. and F. hepatica. Designed primer sequences were cross-referenced with NCBI sequences via primer-BLAST to ensure species specificity for its amplified sequences. For each sample, a 25 µL master mix was created containing 12·5 µL of MyTaq™ red mix (Bioline, London, UK), 50 µ m of primer, 1 µL of the extracted DNA and nuclease free water. Each sample was subjected to PCR amplification consisting of an initial denaturation at 95 °C for 2 min followed by 35 cycles consisting of stages of denaturation (30 s at 95 °C) annealing (30 s at 65 °C) and extension (30 s at 72 °C), before a final 10 min extension phase at 72 °C. PCR products were visualized in 1% agarose gel stained with GelRed (Biotium, Hayward, USA) along with positive and negative controls, with 169 bp band visualized in a well under UV light signifying a positive species identification for C. daubneyi. The presence or absence of other Paramphistomatidae spp. in sampled animals was not confirmed.
Rumen fluke and liver fluke prevalence
All statistical tests described in this section were performed in SPSS (v. 22). Prevalence data at farm, flock and herd level were attained by calculating the proportion of samples with EPG levels greater than zero at each respective level. To calculate the prevalence of C. daubneyi in participating farms from different regional areas, farms were categorized into six regions (north west, north east, Ceredigion, Montgomery, south west, south east) created using ordnance survey boundary line data (Ordnance Survey, 2016) in ArcMap (v 10.2.2). A chi-square test was performed to compare C. daubneyi prevalence levels on farms in western regions (north west, Ceredigion, south west) and eastern regions (north east, Montgomery, south east) of Wales. Differences in the prevalence of both C. daubneyi and F. hepatica between cattle herds and sheep flocks were analysed using a chi-square test. A Mann–Whitney U-test used to analyse differences in EPG levels of both parasites between cattle herds and sheep flocks for all cases where EPG levels were >0. As numerous farms in this study only had one livestock species present on their holding, the results of the two latter analyses could be skewed due to potential differences in the type of land seen on sheep only farms compared with cattle only farms. To combat this issue, parasite prevalence and intensity data from farms submitting samples for both livestock species were also analysed using paired difference tests (referred to as ‘paired’ samples hereafter). This allowed the prevalence and infection intensity of each parasite to be compared between cattle and sheep on each individual farm. This was analysed using a McNemar test (McNemar, Reference McNemar1947) for positive/negative cases, and a Wilcoxon ranked signed test for EPG values. The intensity of F. hepatica and C. daubneyi infections within herds, flocks and farms was also compared using spearman rank correlation (rho). Only herds and flocks, which were positive for either or both parasites were included in the analyses.
Variables regarding farm structure, management and observed environmental features were extracted from questionnaire answers in Microsoft Excel. In instances where questions were directed at a specific species (cattle or sheep), answers were also adapted to be representative of farm level. For example, on farms where both cattle and sheep were present, the mean number of yearly F. hepatica treatments was calculated. Further variables were calculated using data from the questionnaire, including cattle grazing season length, grazing density (LSU/ha) and timing of F. hepatica treatment. Questionnaire postcode data were also used to geo-reference participating farms using ArcGIS (v 10.2.2). A full postcode for each farms address, or their largest holdings where applicable, was derived from the questionnaire and converted into geographical coordinates.
Observed climate data were sourced from the Met Office at 5 km2 resolution (Perry and Hollis, Reference Perry and Hollis2005). A detailed literature review was performed to identify potential climate factors on the C. daubneyi lifecycle, with each identified factor calculated from monthly observed data. For each variable, a value for the year 2015 and a value sourced from 2011 to 2015 (2012–2015 in the instance of sunshine hours due to changes in data format) were calculated. Climatic data were also used alongside extra-terrestrial radiation data (Duffie and Beckman, Reference Duffie and Beckman2013) to calculate 5 km2 resolution Ollerenshaw index values (Mt) (Ollerenshaw and Rowlands, Reference Ollerenshaw and Rowlands1959) during the last 12 months and between 2011 and 2015.
Data regarding soil type, pH and moisture levels at 1 km2 resolution were sourced from the Centre for Ecology and Hydrology (CEH) (Henrys et al. Reference Henrys, Keith, Robinson and Emmett2012; Henrys et al. Reference Henrys, Keith, Robinson and Emmett2014), and soil mineral levels were sourced from the British geological survey (BGS) (Rawlins et al. Reference Rawlins, McGrath, Scheib, Breward, Cave, Lister, Ingham, Gowing and Carter2012). A literature review of minerals shown to either have been included in predictive models for F. hepatica or known to have an effect on Lymnaeidae snail biology determined the choice of soil minerals to analyse. ArcMap (v 10.2.2) was used to extract all climate and environmental data using the raster to point function.
Statistical analysis of C. daubneyi and F. hepatica presence
Presence data for C. daubneyi and F. hepatica along with the data sourced above was statistically analysed with the aim of creating models to explain the presence and absence of the parasites on the study farms, cattle herds and sheep flocks.
Variables regarded as being potential predictor values for C. daubneyi and F. hepatica were selected for inclusion as potential model variables via univariate analysis. Univariate analysis was performed using the Pearson chi-square test for binary variables and the Mann–Whitney U-test for numerical variables in SPSS (v 22·0). For each test, a significance value of P < 0·10 was required for each variable to be selected for the next stage of analysis.
Binary logistic regression was performed on the data from the univariate analysis to create candidate models explaining the presence or absence of C. daubneyi. Farms with C. daubneyi EPG values >0 for either or both cattle and sheep samples were considered as C. daubneyi positive, while farms with C. daubneyi EPG of 0 from all samples were considered negative. Forward Wald and backward Wald logistic regression with a probability for stepwise of P < 0·05 for entry and P > 0·10 for removal was performed in SPSS (v.22) to create candidate models. Odds ratios and their respective 95% confidence intervals were calculated to quantify the strength of each variable's association with C. daubneyi prevalence within each model. However, when prevalence is above 10%, odds ratios can overestimate risk (Zhang and Yu, Reference Zhang and Yu1998) and thus any interpretation of odds ratios in these instances must be made cautiously. This process was repeated to create cattle herd (n = 76) and sheep flock (n = 90) C. daubneyi models. The above process was also repeated to create a farm level F. hepatica model. However, as 14 farms had recently treated all sampled animals with flukicide prior to submission of their FEC samples, only 86 farms were used to create this model.
Multi-model selection and fitting
Each candidate model was tested for goodness of fit via the Hosmer–Lemeshow test with non-significant chi-square statistic values (P > 0·05) indicating a model with goodness of fit. The small sample corrected Akaike information criterion (AICc) (Burnham and Anderson, Reference Burnham and Anderson2002) was calculated with the SAM (v4.0) (Rangel et al. Reference Rangel, Diniz-Filho and Bini2010) software for candidate models identified by stepwise model building. The model with the lowest AICc values were considered the models with the most empirical support (Burnham and Anderson, Reference Burnham and Anderson2002) and chosen for further predictive testing.
Model predictive testing
Interpreting the predictive performance of logistic regression models through metrics such as the area under the curve (AUC) is an important part of their evaluation (Fielding and Bell, Reference Fielding and Bell1997), but one fraught with dangers such as the inflation of metrics by spatial patterns in the data leading to inflated Type I errors (Lobo et al. Reference Lobo, Jiménez-Valverde and Real2008). Consequently, the AUC values of the chosen models were compared against appropriate null models using the method proposed by Beale et al. (Reference Beale, Lennon and Gimona2008) and adapted by Williams et al. (Reference Williams, Cross, Crump, Drost and Thomas2015). For each selected model, 99 null models were created and these null models retained the spatial patterns in the observed distribution of C. daubneyi on farms. In each instance, models were randomly split 1000 times into training and testing points at a ratio of 60:40, respectively. The median AUC of each test model across 1000 splits were then calculated. The chosen models were adjudged to have identified a prediction greater than expected by chance if their median AUC were higher than the median AUC values of 95 of accompanying null models. See Williams et al. (Reference Williams, Cross, Crump, Drost and Thomas2015) for full details of the methodology used.
One hundred farms submitted samples for testing the presence or absence of C. daubneyi. Details on the number of herd types and flocks along with the average size of each can be seen in Table 1.
Forty-nine per cent of participants were aware of rumen fluke prior to this study, with 10% indicating rumen fluke was or had been present on their farms. There was no significant relationship between a participants prior knowledge of rumen fluke and its presence on their farm (χ2 = 0·749, P = 0·387). Six per cent of participating farmers had recently treated directly against rumen fluke with an oxyclozanide product, with 5% using the anthelmintic to treat against F. hepatica over the past 12 months.
Rumen fluke species ID
DNA from 81 rumen fluke egg samples (44 cattle; 37 sheep) were extracted and screened for C. daubneyi DNA. All 81 samples (100%) were positive for C. daubneyi.
Sixty-one per cent of farms were positive for C. daubneyi, while 68% were positive for F. hepatica, with only 17% of farms negative for both. Co-infection of both C. daubneyi and F. hepatica was seen on 46% of farms. The prevalence of C. daubneyi across six regional areas of Wales can be seen in Fig. 1. Calicophoron daubneyi prevalence was significantly higher in western regions (NW, C, SW) of Wales compared with eastern regions (NE, M, SE) (χ2 = 7·507. P = 0·006).
The prevalence of C. daubneyi and F. hepatica in herds and flocks are presented in Table 2. Fifty-nine per cent of cattle herds sampled in this study were positive for C. daubneyi, compared with a significantly lower prevalence level of 42% in sampled sheep flocks (P = 0·029). The prevalence levels of C. daubneyi in paired cattle herds (59%) was significantly higher compared with their sheep flock counterparts (42%) when using a paired difference test (P = 0·035) on individual farms, which had submitted both cattle and sheep samples. There was no significant difference between the EPG levels of C. daubneyi within positive sheep flocks and cattle herds in either normal (P = 0·596) or paired (P = 0·131) analysis (Table 3).
EPG, eggs per gram.
There was no significant difference between prevalence levels of F. hepatica in cattle herds and sheep flocks in the total submitted samples (P = 0·916) and paired (P = 0·851) samples (Table 2). Fasciola hepatica EPG level were however, significantly higher in positive sheep flocks compared with positive cattle herds for total samples (P < 0·001) and paired samples (P = 0·004) (Table 3).
Fluke species correlation
A significant negative correlation between EPG levels of C. daubneyi and F. hepatica was recorded for herds (rho = −0·358, P = 0·007), with a non-significant (rho = −0·199, P = 0·11) negative correlation recorded for flocks.
Logistic regression models of C. daubneyi and F. hepatica presence or absence
Univariate analysis selected 20, 24 and 14 variables as potential predictors of C. daubneyi at farm, herd and flock level, respectively, for input into logistic regression analysis (Supplementary Table 1). The final models explaining the prevalence of C. daubneyi on Welsh farms, in cattle herds and sheep flocks are seen in Table 4. The farm model identified four positive predictors for C. daubneyi on Welsh farms; the cattle model identified five positive predictors for C. daubneyi in cattle herds, while the sheep model identified two positive predictors for C. daubneyi in sheep flocks. Univariate analysis selected 17 variables as potential predictors of F. hepatica at farm level, and four significant predictors were selected in the final model (Table 4). All final models AICc values were at least two points lower than the AICc values of other candidate models, including models created using only climate variables.
AIC, Akaike information criterion; AUC, area under the curve; CI, confidence interval; HL, Hosmer–Lemeshow; NMR, Null Model Rank; s.e., standard error; MJJ; May –July.
This study is the first to record the on-farm prevalence of C. daubneyi in any area within the UK. This initial estimate of C. daubneyi prevalence (61%) indicates that it is established in Wales, a finding which is supported by the increasing prevalence of rumen fluke observed by passive veterinary surveillance across the UK since 2010 (VIDA, 2016a ). The logistic regression models created are also the first models explaining the prevalence of C. daubneyi in an area of the UK. Each final model created included both climate and environmental/management factors, and were superior to climate only models at the model selection stage. This indicates the importance of using environmental and management factors alongside climate variables when modelling C. daubneyi prevalence at farm level, as is the case with F. hepatica (Bennema et al. Reference Bennema, Ducheyne, Vercruysse, Claerebout, Hendrickx and Charlier2011).
Despite our finding that C. daubneyi may be very common in Wales; it is not universally known within the Welsh agricultural community. Calicophoron daubneyi prevalence was shown to be lower than F. hepatica despite the fact that most farms in the study treated against F. hepatica and not C. daubneyi. Calicophoron daubneyi may therefore be in the process of spreading and colonizing farms and regions in Wales. The high proportion of farms harbouring co-infection of C. daubneyi and F. hepatica within their livestock (46%) suggests the parasites share a similar geographic range in Wales. Similarities were also observed between C. daubneyi and F. hepatica risk factors, with environmental features linked to G. truncatula presence such as presence/density of boggy habitats, soil factors and water sources important variables in models for both parasites. In contrast to the C .daubneyi models, climate variables were absent from the F. hepatica model, which may be explained by the importance of environmental factors in previous F. hepatica predictive models (McCann et al. Reference McCann, Baylis and Williams2010; Bennema et al. Reference Bennema, Ducheyne, Vercruysse, Claerebout, Hendrickx and Charlier2011).
A negative correlation was recorded between the intensity of infection of each parasite in both cattle herds and sheep flocks. The high levels of C. daubneyi and low levels of F. hepatica seen in numerous cases could be explained by Welsh farmers treating against F. hepatica with anthelmintics not active against C. daubneyi. Yet treatment regimen alone does not explain the decreasing EPG levels of C. daubneyi seen in the presence of increasing F. hepatica as none of the small proportion of participating farms in this study that had recently used oxyclozanide in their livestock had higher EPG levels of F. hepatica. This raises potential intriguing questions regarding the epidemiology of each parasite. Despite their apparent preference for the same intermediate snail host, it is unclear whether each parasite's different epidemiology leads to farms being more suited to one fluke species than the other, or whether potential competition between each parasite at the intermediate snail stage occurs. C. daubneyi and F. hepatica are known to eliminate each other when dually infecting G. truncatula (Rondelaud et al. Reference Rondelaud, Vignoles and Dreyfuss2007) while the presence of other trematode have been shown to suppress F. hepatica levels within snail populations (Gordon and Boray, Reference Gordon and Boray1970; Whitelaw and Fawcett, Reference Whitelaw and Fawcett1982; Goumghar et al. Reference Goumghar, Abrous, Ferdonnet, Dreyfuss and Rondelaud2000). If competition does occur, it could explain the reason for variables regarding treatment against F. hepatica being a positive predictor for C. daubneyi in final models. By treating against F. hepatica regularly, especially during spring (a positive predictor for C. daubneyi presence in the cattle model), the number of F. hepatica eggs shed onto pasture may be reduced, potentially freeing G. truncatula snails to be infected with C. daubneyi. However, caution must be maintained when interpreting these results, as treatment regularity may be partly determined by historic F. hepatica issues, which in turn may be partly determined by the density of G. truncatula habitats. Despite this, an increasing efficacy of treatment for F. hepatica in France has been suggested as a reason for their recorded increase in paramphistomosis over the past 25 years (Mage et al. Reference Mage, Bourgne, Toullieu, Rondelaud and Dreyfuss2002; Rieu et al. Reference Rieu, Recca, Bénet, Saana, Dorchies and Guillot2007). In the UK, the growing threat of triclabendazole resistance (Gordon et al. Reference Gordon, Zadoks, Skuce and Sargison2012) is causing major issues with F. hepatica treatment efficacy (Sargison et al. Reference Sargison, Francis, Davison, Bronsvoort, Handel and Mazeri2016). Thus, it is hypothesized that the varying efficacy of a farm's treatment regimen against F. hepatica could determine, which parasite prevails in a competition to dominate a farm's endogenous G. truncatula populations and therefore be capable of infecting livestock at high intensities. Furthermore, in an instance where C. daubneyi could suppress F. hepatica through competition, farms could in theory benefit from the presence of C. daubneyi. For example, it is currently believed that a heavy burden of juvenile C. daubneyi is required to cause clinical disease in livestock (Mason et al. Reference Mason, Stevenson, Cox and Dick2012; Millar et al. Reference Millar, Colloff and Scholes2012), with adult paramphistomes well tolerated (Zintl et al. Reference Zintl, Garcia-Campos, Trudgett, Chryssafidis, Talavera-Arce, Fu, Egan, Lawlor, Negredo, Brennan, Hanna, De Waal and Mulcahy2014). In comparison, heavy infections of both juvenile and adult F. hepatica are known to cause severe losses in livestock (Dargie, Reference Dargie1987), with production losses also associated with lighter burdens (Schweizer et al. Reference Schweizer, Braun, Deplazes and Torgerson2005). However, further research would be required on both the dynamics of this potential competition, as well as the pathogenicity of both juvenile and adult C. daubneyi prior to any implementation of strategies to take advantage of this potential phenomenon.
Differences in the prevalence of C. daubneyi between cattle herds and sheep flocks were also observed, with prevalence higher in cattle compared with sheep. This coincides with UK passive veterinary surveillance data (VIDA, 2016a ) and data from Irish abattoirs and veterinary surveillance (Toolan et al. Reference Toolan, Mitchell, Searle, Sheehan, Skuce and Zadoks2015). One suggested reason for the latter finding in Ireland was that sheep graze rougher pasture compared with cattle; however, this seems to be an unlikely factor in our results as there was no significant difference between F. hepatica prevalence in cattle and sheep, which indicates a similar exposure to G. truncatula habitats for each ruminant species. It has been shown that another Paramphistomum species, C. microbothrium, is better suited to infecting cattle compared with sheep, with the parasite having an increased lifespan, and is known to migrate quicker and exhibit increased growth and egg laying ability when infecting cattle (Horak, Reference Horak1967). Calicophoron daubneyi may similarly be better suited to infecting cattle compared with sheep, however, there was no significant difference in the EPG levels seen in positive herds and flocks, in fact the highest EPG levels for C. daubneyi in this study was seen in a sheep flock. Ovine paramphistomosis has also been reported in the UK (Mason et al. Reference Mason, Stevenson, Cox and Dick2012), which indicates that C. daubneyi should not be disregarded as a pathogenic parasite of sheep. The importance of cattle in the epidemiology of C. daubneyi was further emphasised in each model, where either the total number of cattle or number of heifers or steers present on a farm were selected as positive predictors for C. daubneyi. An increasing herd size may increase the sources of C. daubneyi eggs shedding onto pasture and thus parasite spread within a farm, but may also lead to an increased risk of buying in the parasite with increasing herd size a potential proxy for herd turnover rate (Reilly and Courtenay, Reference Reilly and Courtenay2007). This was highlighted in the questionnaire data where farms buying in cattle had significantly larger herd sizes. This also highlights the role of biosecurity in disease prevention; with C. daubneyi seemingly well-established less than a decade since significant reports of its occurrence in the UK began.
Other variables which could have biosecurity implications that were included as positive predictors in the best performing models were the ‘presence of livestock accessible streams or drainage ditches’ and ‘water flowing from other farms’. The inclusion of these variables may be a measure of the presence of intermediate host snail habitats, with muddy areas surrounding streams and ditches a common habitat for G. truncatula similarly to boggy pastures, which was also a positive predictor for C. daubneyi in two of the final models. However, streams are also potential movement corridors for G. truncatula snails, with data from France suggesting G. truncatula snails can travel upstream and contaminate pasture free from livestock with F. hepatica metacercariae (Rondelaud et al. Reference Rondelaud, Hourdin, Vignoles and Dreyfuss2005). The role of streams in the spread of C. daubneyi and potentially TCBZ resistant strains of F. hepatica in the UK is therefore worthy of further investigation.
The only direct climate variable to be included in all of the final C. daubneyi models was sunshine hours. The exact reason for this inclusion is unclear; however, C. daubneyi eggs are known to be more dependent on light as a hatching stimulus compared with F. hepatica eggs (Chryssafidis et al. Reference Chryssafidis, Fu, De Waal and Mulcahy2015). If this is the reason for sunshine's inclusion in each model it may suggest that eggs in areas receiving longer levels of sunshine may have higher hatching success rates, leading to increasing lifecycle opportunities. A calculated Ollerenshaw index value for the summer of 2015 was also a positive predictor of C. daubneyi in the cattle model. Although its effect on the model was small, potentially due to the limited impact of between-year weather variation on between-farm fluke prevalence (McCann et al. Reference McCann, Baylis and Williams2010), its inclusion may unsurprisingly suggests that climate predictors of fasciolosis may also have predictive power regarding C. daubneyi. This may partly explain the higher prevalence of C. daubneyi seen in participating farms from western regions of Wales, with western Wales shown to be one area of the UK at most risk of fasciolosis both historically and in future forecasts when using the Ollerenshaw model (Fox et al. Reference Fox, White, McClean, Marion, Evans and Hutchings2011). A westerly trend of increased rumen fluke detection in passive veterinary surveillance has similarly been observed in Wales and throughout the UK (VIDA, 2016a ), which would also suggest that the traditional climate drivers of F. hepatica prevalence are also important factors for C. daubneyi. To enhance our understanding of the relationship between climatic variables and C. daubneyi prevalence, it would be necessary to analyse a dataset on a wider scale.
It remains unclear how and why C. daubneyi has apparently become so prevalent in the UK in recent years, and questions remain regarding its origins. It is possible that low levels of C. daubneyi in the UK may have been overlooked previously due to the perceived presence of P. cervi as the dominant Paramphistomatidae sp. in UK livestock (Gordon et al. Reference Gordon, Roberts, Lean, Zadoks, Sargison and Skuce2013), and its non-pathogenicity at low levels (Zintl et al. Reference Zintl, Garcia-Campos, Trudgett, Chryssafidis, Talavera-Arce, Fu, Egan, Lawlor, Negredo, Brennan, Hanna, De Waal and Mulcahy2014). In this instance, it could be suggested that a decrease in the popularity of ‘old’ anthelmintic products, including oxyclozanide, following the licencing of TCBZ in the mid 80s would have allowed C. daubneyi to ultimately increase its prevalence in UK livestock. There is also a possibility that C. daubneyi parasites may have recently been imported into the UK in infected animals, with cattle imports to the UK increasing substantially in the aftermath of the 2001 foot and mouth disease outbreak (Mitchell et al. Reference Mitchell, Bourn, Mawdsley, Wint, Clifton-Hadley and Gilbert2005), which coincides with a period where C. daubneyi levels in France had just increased significantly (Mage et al. Reference Mage, Bourgne, Toullieu, Rondelaud and Dreyfuss2002). In either or both instances, it is likely that climate change will have played a role in the recent establishment of C. daubneyi in the UK. Since 1970, increasing rainfall and temperatures have seen the UK climate become more suitable for G. truncatula populations (Fox et al. Reference Fox, White, McClean, Marion, Evans and Hutchings2011), a factor which has seen increasing reports of fasciolosis (Pritchard et al. Reference Pritchard, Forbes, Williams, Salimi-Bejestani and Daniel2005) and may have had a similar positive effect on C. daubneyi. Increasing annual hours of sunshine have also been observed in the UK over the past 50 years (Met-Office, 2016), which may have also contributed to C. daubneyi establishment if indeed sunshine duration is a driver for its prevalence. Climate change could also lead to future increases in C. daubneyi prevalence due to further climate change forecast of increases in climate suitability for G. truncatula (Fox et al. Reference Fox, White, McClean, Marion, Evans and Hutchings2011).
This study was the first farm level survey for C. daubneyi in any area of the UK, with the results indicating C. daubneyi is endemic in Wales. The study has also raised important questions regarding differing prevalence levels between ruminant species, and potential competition between C. daubneyi and F. hepatica. To answer these questions further research on the epidemiology of C. daubneyi at a finer and broader scale will be required. Finally, this study produced the first model for C. daubneyi in an area of the UK. The predictors identified may be used in future as a basis to further study C. daubneyi epidemiology and to develop models of further value to farmers and veterinarians in predicting and combating C. daubneyi occurrence and paramphistomosis risk.
The supplementary material for this article can be found at https://doi.org/10.1017/S0031182016001797
The authors would like to thank all farmers participating in this project; the staff at YFC Wales; Dr Martin Vickers for assistance in creating project website; Dan Hollis of the UK Met Office for assistance in providing observed climate data; farmers and veterinarians who have contributed to the VIDA dataset; and two anonymous reviewers for their constructive comments, which greatly improved the manuscript.
Rhys Aled Jones gratefully acknowledges the Dr Owen Price scholarship for funding his Ph.D. The project was funded by the Coleg Cymraeg Cenedlaethol (to H. W. W.).