Introduction
Infectious disease has been a major cause of mortality, with early outbreaks referred to as plagues and blamed on unrelated factors, such as climate and religious beliefs (Bazin, Reference Bazin2003). By the late 19th century, these early explanations of contagious illness were replaced with germ theory (Valent et al., Reference Valent, Groner, Schumacher, Superti-Furga, Busslinger, Kralovics, Zielinski, Penninger, Kerjaschki, Stingl, Smolen, Valenta, Lassmann, Kovar, Jäger, Kornek, Müller and Sörgel2016). In 1910, Paul Ehrlich synthesized the first antibiotic agent, arsphenamine (Salvarsan®; Valent et al., Reference Valent, Groner, Schumacher, Superti-Furga, Busslinger, Kralovics, Zielinski, Penninger, Kerjaschki, Stingl, Smolen, Valenta, Lassmann, Kovar, Jäger, Kornek, Müller and Sörgel2016; Vernon, Reference Vernon2019). Salvarsan® was an organoarsenic compound that was a popular treatment for syphilis (Vernon, Reference Vernon2019). It would take Alexander Fleming a further 18 years to identify penicillin and more than 20 years after that for the Golden Age of Antibiotic Discovery to peak (Table 1; Hutchings et al., Reference Hutchings, Truman and Wilkinson2019). Since Fleming's game-changing discovery, antibiotics have become a cornerstone of human medical treatment and have extended the average life expectancy by an average of 23 years (Hutchings et al., Reference Hutchings, Truman and Wilkinson2019). Veterinary medicine and livestock farming have also greatly benefited from the advent of antibiotic treatment, with routine antibiotic therapy preventing the dissemination of zoonotic diseases amongst large herds of livestock (Landers et al., Reference Landers, Cohen, Wittum and Larson2012).
Table 1. Excerpt of the parallel timelines of antibiotic discovery and the development of antibiotic resistance
a Golden age of antibiotic discovery.
Source: Adapted from Fair and Tor (Reference Fair and Tor2014) and Hutchings et al. (Reference Hutchings, Truman and Wilkinson2019).
However, we are now facing the concerning rise in antibiotic resistance (AR), which is the result of prolonged exposure of bacteria to antibiotic agents, usually as a consequence of failed medical treatment or, in the case of livestock farming, routine administration of antibiotics to pre-empt potential infections (Palma et al., Reference Palma, Tilocca and Roncada2020). AR is now one of the most concerning threats against human and veterinary health, and it is predicted that by 2050, human deaths resulting from AR infections will outnumber those by cancer and result in major economic losses globally (Dadgostar, Reference Dadgostar2019). These losses include the farming sector, due to a reduction in breeding and trading of livestock, as well as animal death and culling due to resistant infection (Bengtsson and Greko, Reference Bengtsson and Greko2014; Dadgostar, Reference Dadgostar2019). For this reason, it is not only important to adapt human medicine in accordance with increased incidence of AR infections but also veterinary medicine.
A brief history of veterinary medicine
Veterinary medicine likely dates back to 9000 BC when the Neolithic man first began domesticating animals (Hunter, Reference Hunter2018). Archaeological evidence supports this, as instances of cranial surgery have been identified in animal skulls dating from that period (Ramirez Rozzi and Froment, Reference Ramirez Rozzi and Froment2018). As agriculture developed, a king of ancient Babylon incorporated laws pertaining to the payment and responsibilities of veterinary surgeons into what is now known as ‘The Code of Hammurabi’ (Samad, Reference Samad2016).
The advent of what can be considered as ‘modern’ veterinary medicine, which is scientifically informed and consistent, occurred much more recently. In 1761, the first veterinary school was established in Lyon, France, by Cladude Bourgelat (Cáceres, Reference Cáceres2011; Samad, Reference Samad2016). During the 18th century, rinderpest (cattle plague) was a major concern for cattle health, and a physician named Giovanni Maria Lancisi had proposed very effective control measures (e.g. separating sick and healthy animals; Mourant et al., Reference Mourant, Fenimore, Manore and Mcmahon2018). It was Bourgelat's goal to train veterinarians in Lancisi's methods of maintaining animal health (Cáceres, Reference Cáceres2011).
Today, there are more than 650 veterinary colleges across the globe (Gyles, Reference Gyles2015; Samad, Reference Samad2016). There is also a new approach to medicine known as ‘One Health’, which was developed after the emergence of severe acute respiratory disease and recognizes the link between human and animal health, as well as the threat to food security and agricultural economies posed by zoonoses and animal illness (Samad, Reference Samad2016; Mackenzie and Jeggo, Reference Mackenzie and Jeggo2019). One aspect of the One Health concept of medicine is understanding the connection between antibiotic use (and misuse) in human and animal medicine and the rise in AR (Collignon and McEwen, Reference Collignon and Mcewen2019; Mackenzie and Jeggo, Reference Mackenzie and Jeggo2019; More, Reference More2020; Palma et al., Reference Palma, Tilocca and Roncada2020).
Antibiotic use in veterinary medicine
As new antibiotic classes were discovered, and new products were rolled out to human medicine, they were also introduced to veterinary therapies (Economou and Gousia, Reference Economou and Gousia2015). Unlike human medicine, antibiotics are employed more extensively within veterinary health (e.g. in 2014, 8927 tons of antibiotics were used in veterinary medicine in the EU versus 3821 tons in human medicine), as they also serve nontherapeutic functions in agriculture, such as prophylactic supplements and growth promoters (Cuong et al., Reference Cuong, Padungtod, Thwaites and Carrique-Mas2018; Collignon and McEwen, Reference Collignon and Mcewen2019).
These additional functions of antibiotic treatment in livestock animals serve to prevent the transmission of potential infections (such as mastitis in dairy cattle), as well as marginally promote weight gain (Economou and Gousia, Reference Economou and Gousia2015; Collignon and McEwen, Reference Collignon and Mcewen2019). While the use of antibiotic agents as growth promoters has been banned in the European Union since 2006, ionophores (nutrient-utilization-promoting antibiotics) are still heavily employed in European feedlots (Economou and Gousia, Reference Economou and Gousia2015; More, Reference More2020).
Similarly, the US frequently uses tylosin, a macrolide used exclusively in veterinary medicine, in 88% of pigs and 42% of beef calves to promote growth (Landers et al., Reference Landers, Cohen, Wittum and Larson2012). In 2014, the agriculture sector was responsible for approximately 70% of total antibiotic consumption in the US (interestingly, the 8927 tons of antibiotic used in animal medicine in the EU, also equates to approximately 70% of total antibiotic consumption in 2014; Cuong et al., Reference Cuong, Padungtod, Thwaites and Carrique-Mas2018).
Unfortunately, reliable quantitative data regarding antibiotic usage in agriculture are not readily available, in part as there is a general lack of infrastructure to support the documentation of antibiotic use. This is to change, as the EU Veterinary Medicines Regulations shall require EU members to report antibiotic use in food animals in national databases from 2027 (Martin et al., Reference Martin, Manzanilla, More, O'neill, Bradford, Carty, Collins and Mcaloon2020). Currently, however, the data surrounding antibiotic use in livestock are relatively limited, and there is no clear distinction between therapeutic and nontherapeutic use (Collignon and McEwen, Reference Collignon and Mcewen2019; More, Reference More2020). What is far more evident is the risk posed by excessive and/or long-term antibiotic exposure to zoonotic and environmental bacteria (Manyi-Loh et al., Reference Manyi-Loh, Mamphweli, Meyer and Okoh2018).
Antibiotic resistance associated with veterinary disease
AR infections, such as methicillin-resistant Staphylococcus aureus, were once largely associated with hospitals, where organisms were likely to be subjected to selective pressure caused by exposure to residual antibiotics (Duerden et al., Reference Duerden, Fry, Johnson and Wilcox2015). Increasingly, community-acquired infections and environmental isolates are displaying AR (Whittaker et al., Reference Whittaker, Lohm, Lemoh, Cheng and Davis2019; Hua et al., Reference Hua, Huang, Chen, Rehmet, Jin and Huang2020; Donner et al., Reference Donner, Staley Zachery, Petali, Sangster, Li, Mathews, Snow, Howe, Soupir, Bartelt-Hunt and Auchtung Jennifer2022). There is considerable evidence that supports the over-use of antibiotics in agriculture contributing to the increase in non-hospital associated AR, with specific respect to food animals shedding subclinical levels of antibiotics into the environment and introducing AR-organisms into the food chain (Martin et al., Reference Martin, Thottathil and Newman2015; Manyi-Loh et al., Reference Manyi-Loh, Mamphweli, Meyer and Okoh2018; Hua et al., Reference Hua, Huang, Chen, Rehmet, Jin and Huang2020). Of particular concern is the apparently high prevalence of AR (33–67%) to commonly used veterinary antibiotics, such as tetracycline, chloramphenicol, and beta-lactams, associated with food isolates (Manyi-Loh et al., Reference Manyi-Loh, Mamphweli, Meyer and Okoh2018).
As AR associated with community infections and foodborne illness is a major concern for human health, it stands to reason that it is also a major consideration in treating animal illness (Bengtsson and Greko, Reference Bengtsson and Greko2014; Palma et al., Reference Palma, Tilocca and Roncada2020). By treating livestock prophylactically, it may lead to treatment failure should an animal acquire an infection that is typically treated with the same or similar antibiotic (Bengtsson and Greko, Reference Bengtsson and Greko2014). For example, penicillin was previously a first-line antibiotic treating mastitis in dairy animals, but it is now not an advised therapy due to widespread resistance (Bengtsson and Greko, Reference Bengtsson and Greko2014; Käppeli et al., Reference Käppeli, Morach, Zurfluh, Corti, Nüesch-Inderbinen and Stephan2019).
Unfortunately, literature relating to AR originating from agriculture is biased toward discussing the impact on human health, as opposed to the risk that animals may contract AR infections that exclusively affect their species (Bengtsson and Greko, Reference Bengtsson and Greko2014). This bias needs to be addressed, not only to ensure animal welfare in general, but to avoid an unfair and unrealistic distribution of therapeutic resources within the One Health concept. Similarly, alternatives to antibiotics should be extensively examined for potential applications in veterinary medicine. This will not only increase the arsenal for treating animal illness but will in turn reduce the burden of AR in human infection by limiting the evolution of AR in food isolates.
Alternatives to antibiotics in veterinary medicine
Within the EU, only ionophores are used as feed additives and several countries, such as France, Sweden, and the Netherlands, have implemented further controls to reduce the prescription of antibiotics by veterinarians (Economou and Gousia, Reference Economou and Gousia2015; Wong, Reference Wong2019; Nowakiewicz et al., Reference Nowakiewicz, Zięba, Gnat and Matuszewski2020). While limiting the prescribing of antibiotics may help reduce the incidence of AR in animal illness, it begs the question – how else will animal health be managed? A possible answer is developing novel prophylactics which could offer some protection against disease to healthy animals. Novel prophylactics would not only improve and maintain animal health but would remove the perceived necessity of dosing animals with subclinical levels of antibiotics.
Pre- and probiotics in animal health
Prebiotics are nondigestible dietary fiber compounds which support the growth of beneficial gut bacteria, which have been shown to aid digestion, improve weight gain, and reduce levels of potentially pathogenic bacteria in several species (Arowolo and He, Reference Arowolo and He2018; Markowiak and Śliżewska, Reference Markowiak and Śliżewska2018; Asha and Khalil, Reference Asha and Khalil2020). Probiotics are live microbes that confer health benefits when consumed in adequate quantities (Asha and Khalil, Reference Asha and Khalil2020). Several studies have found that the inclusion of probiotic yeast strains in dairy cattle feed aids rumen digestion and reduces oxidative stress (respectively improving gut health and reducing seasonal variation in milk yield; Pinloche et al., Reference Pinloche, Mcewan, Marden, Bayourthe, Auclair and Newbold2013; Mirzad et al., Reference Mirzad, Goto, Endo, Ano, Kobayashi, Yamauchi and Katamoto2019). Similarly, bacterial probiotics have been shown to positively affect the rumen and improve weight gain in livestock, with several feed types including lactic acid bacteria, such as Lactobacillus (Arowolo and He, Reference Arowolo and He2018; Alayande et al., Reference Alayande, Aiyegoro and Ateba2020; Direkvandi et al., Reference Direkvandi, Mohammadabadi and Salem2020; Bhogoju and Nahashon, Reference Bhogoju and Nahashon2022).
Despite the benefits, several limitations exist which prevent the widespread application of pre- and probiotics in animal feed, including inconsistent effects, difficulties registering novel feed additives, and a lack of regulation surrounding probiotic usage (Cheng et al., Reference Cheng, Hao, Xie, Wang, Dai, Huang and Yuan2014; Markowiak and Śliżewska, Reference Markowiak and Śliżewska2018; Direkvandi et al., Reference Direkvandi, Mohammadabadi and Salem2020). For example, China has formally approved 12 probiotics, but up to 50 are in use (Cheng et al., Reference Cheng, Hao, Xie, Wang, Dai, Huang and Yuan2014). Until these issues are addressed, particularly the inconsistent outcomes, it's unlikely that pre- and probiotics will be ushered into a new generation feed additives.
Vaccination
Preventative vaccination could be a cost-effective alternative to prophylactic antibiotics. The goal of vaccination is to stimulate an antibody-mediated immune response to a pathogen without exposure to a virulent organism, usually by injection of dead/attenuated pathogen or immunogenic elements of the pathogen (Meeusen et al., Reference Meeusen, Walker, Peters, Pastoret and Jungersen2007; McVey and Shi, Reference Mcvey and Shi2010). Vaccines are highly regarded for their proven effectiveness and are widely employed in veterinary medicine (e.g. vaccines against rabies and S. aureus-mediated bovine mastitis; McVey and Shi, Reference Mcvey and Shi2010; Cheng et al., Reference Cheng, Hao, Xie, Wang, Dai, Huang and Yuan2014). Vaccination has also demonstrated positive results beyond disease prevention, for instance, a vaccine against the etiological agent of ileitis in pigs improved mortality rates and weight gain of the animals (Bak and Rathkjen, Reference Bak and Rathkjen2009). Encouragingly, the efficacy of this vaccine-reduced antibiotic treatment for ileitis by 80% in pigs and in a larger study, most farms noted reduced antibiotic usage and associated costs (Bak and Rathkjen, Reference Bak and Rathkjen2009; Hoelzer et al., Reference Hoelzer, Bielke, Blake, Cox, Cutting, Devriendt, Erlacher-Vindel, Goossens, Karaca, Lemiere, Metzner, Raicek, Collell Suriñach, Wong, Gay and Van Immerseel2018). Unfortunately, vaccination remains a neglected means of disease control in animals, as many smallholder farmers and poor rural populations do not have access to appropriate vaccines, and it is difficult to demonstrate the value of vaccination, as many vaccines are against zoonoses which have little to no clinical effect on the animals (Donadeu et al., Reference Donadeu, Nwankpa, Abela-Ridder and Dungu2019). Alongside the issues surrounding accessibility and understanding of vaccines, the regrettable state of the art is that there are many diseases, which currently lack an approved vaccine.
Other alternatives
Prophylactic alternatives aside, what remains to be reviewed are alternatives to antibiotic therapy. One-third of antibiotics used in agriculture are employed for therapeutic purposes, i.e. actively treating illness (Martin et al., Reference Martin, Thottathil and Newman2015; Nowakiewicz et al., Reference Nowakiewicz, Zięba, Gnat and Matuszewski2020). This highlights their importance in maintaining animal health, and consequently their use cannot be entirely erased without the provision of a therapeutic alternative. One such alternative to therapeutic antibiotic use, which has garnered renewed interest in medicine, is bacteriophage (phage) therapy (PT).
A brief history of phage therapy
Remarkably, while PT is under much investigation in the current century as an alternative to antibiotics, it actually predates the discovery of penicillin (McCallin et al., Reference Mccallin, Sacher, Zheng and Chan2019). By 1917, the phage phenomenon had been described twice in independent reports, including one by Félix d'Herelle, who is considered the founder of PT (Wittebole et al., Reference Wittebole, De Roock and Opal2014; McCallin et al., Reference Mccallin, Sacher, Zheng and Chan2019).
d'Herelle proposed the name ‘bacteriophage,’ by combining ‘bacteria’ and ‘phagein’, from the Greek for ‘to devour’, as the phage appeared to devour cells (Sulakvelidze et al., Reference Sulakvelidze, Alavidze and Morris2001; Dublanchet and Bourne, Reference Dublanchet and Bourne2007; Wittebole et al., Reference Wittebole, De Roock and Opal2014). It is now understood that it is the lytic cycle of phage (i.e. phage infection resulting in bacterial lysis) that causes the collapse of the culture (Fig. 1; Lin et al., Reference Lin, Koskella and Lin2017; Furfaro et al., Reference Furfaro, Payne and Chang2018). d'Herelle determined that phage-targeted specific bacterial hosts, and he commonly isolated disease-specific phage from the filtered stool of convalescents (Dublanchet and Bourne, Reference Dublanchet and Bourne2007; Wittebole et al., Reference Wittebole, De Roock and Opal2014). PT involving strictly lytic phages became a popular treatment in the pre-antibiotic decades, particularly in the former USSR (Summers, Reference Summers2012; Wittebole et al., Reference Wittebole, De Roock and Opal2014; Furfaro et al., Reference Furfaro, Payne and Chang2018; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021).
Figure 1. Lytic cycle of phage. Attachment/infection. The phage particle (blue) recognizes specific receptors on the surface of the bacterium (red) via binding proteins in its tail fibers and injects its genetic material into the cell. (Replication) A combination of host and phage factors allows the phage particles to replicate to high numbers within the host cell. (Bacterial lysis/Phage release) Newly synthesized phage particles are released during bacterial lysis caused by phage endolysins rupturing the cell wall and are free to restart the attachment/infection phase with neighboring bacteria. Created with BioRender.com.
In the post-antibiotic era, PT fell out of favor, partly because the highly specific nature of phage was perceived as a limitation when compared to broad-spectrum antibiotics (Sulakvelidze et al., Reference Sulakvelidze, Alavidze and Morris2001; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). There was also controversy surrounding the variable success rates/regulation of treatment and limited understanding of phage biology (Lin et al., Reference Lin, Koskella and Lin2017). Nowadays, PT, or ‘compassionate PT,’ is a last-resort option for patients whose infection has evaded all attempts at antibiotic treatment (e.g. multi-drug resistant Acinetobacter baumanii and Pseudomonas aeruginosa; Furfaro et al., Reference Furfaro, Payne and Chang2018; McCallin et al., Reference Mccallin, Sacher, Zheng and Chan2019; Anomaly, Reference Anomaly2020; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). Using that same logic, it's reasonable to presume PT could be employed in compassionate circumstances in veterinary medicine, particularly diarrheal diseases (which might display AR). There could also be an opportunity for PT to entirely replace certain therapeutic antibiotics in agriculture, as the global call to reduce their usage in this sector may support the routine use of PT in livestock.
Bacteriophage in veterinary medicine
Currently, there is no United States Food and Drug Administration (USFDA) approved PT for use in veterinary medicine, though several have approval for use in food processing, such as the use of phage against Listeria monocytogenes to decontaminate surfaces (Kahn et al., Reference Kahn, Bergeron, Bourassa, De Vegt, Gill, Gomes, Malouin, Opengart, Ritter, Singer, Storrs and Topp2019; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). This lack of approved PT for use in animals is liable to change as more evidence is presented regarding their safety and efficacy.
Many studies investigating PT have involved animal models, e.g. murine models of Escherichia coli (E. coli) infections, which have generally returned positive results and suggest the potential for PT to be used against similar animal illnesses (Atterbury, Reference Atterbury2009). This has been practically demonstrated during investigations of PT in food animals. Huff et al. (Reference Huff, Huff, Rath and Donoghue2006) found that treating E. coli-challenged chickens with either phage DAF6 or SPR02 reduced mortality associated with colibacillosis by 41%. Similar poultry studies have shown that PT generates significant reductions in Salmonella and Campylobacter colonization (Atterbury, Reference Atterbury2009). Larger livestock, such as calves, piglets, and lambs, have also undergone PT trials that demonstrated phage were capable of reducing the burden of verotoxigenic and enterotoxigenic E. coli, with one study demonstrating both effective prophylactic use and remission after the onset of clinical signs (Smith and Huggins, Reference Smith and Huggins1983; Atterbury, Reference Atterbury2009). Interestingly, during the PT trials conducted by Smith and Huggins (Reference Smith and Huggins1983), 11 out of 13 calves treated with phage after the onset of diarrhea recovered, while the entire control group died. This drastic contrast between the control and test groups very clearly illustrates how animal death-related profit losses can be reduced by employing PT.
While the therapeutic application of phage is not yet standard practice in veterinary health, Smith and Huggins (Reference Smith and Huggins1983) have also indirectly revealed that the compassionate application of PT may be ideal for use in the terminal stage of a (potentially AR) diarrheal disease, such as Johne's disease (JD), which shall become the focus of this review.
Johne's disease
JD is a chronic gastrointestinal illness of ruminants that features granulomatous enteritis, diarrhea, and nutrient malabsorption, with subsequent weight loss and muscle wasting (Fig. 2; Rathnaiah et al., Reference Rathnaiah, Zinniel, Bannantine, Stabel, Gröhn, Collins and Barletta2017; Stinson et al., Reference Stinson, Baquero and Plattner2018; Field et al., Reference Field, Mcaloon, Gavey and Mee2022). The signs of JD in cattle were first described in the early 19th century and were likened to ‘consumption’, i.e. tuberculosis (TB; Skellett, Reference Skellett1807; Dziedzinska and Slana, Reference Dziedzinska and Slana2017; Moonan, Reference Moonan2018). It was presumed that Mycobacterium tuberculosis (the causative agent of TB) was the causative agent of JD until 1895, when veterinary pathologists Dr Heinrich Johne and Dr Langdon Frothingham identified Mycobacterium pseudotuberculosis, later termed Mycobacterium avium subsp. paratuberculosis (MAP; Harris and Barletta, Reference Harris and Barletta2001; Sechi and Dow, Reference Sechi and Dow2015; Davis et al., Reference Davis, Kuenstner and Singh2017; Dziedzinska and Slana, Reference Dziedzinska and Slana2017).
Figure 2. Ruminant animals suffering from clinical Johne's disease. (a) Cow. (b) Goat. (c) Sheep. (d) Deer. Images adapted from https://johnes.org/.
Mycobacterium avium subsp. paratuberculosis
In veterinary medicine, non-tuberculosis mycobacteria (NTM) infections present more frequently than TB (non-primates rarely develop active TB; Hlokwe et al., Reference Hlokwe, Said and Gcebe2017). One such NTM infection is paratuberculosis, or JD, caused by MAP. MAP is an obligate intracellular pathogen that belongs to the Mycobacterium avium complex (Garvey, Reference Garvey2020; Matthews et al., Reference Matthews, Cotter and O'Mahony2021). It differs from other species in this complex by its ability to infect non-immunocompromised ruminants, its exceptionally slow cultivation (up to 16 weeks or more), its inability to produce the iron-chelator mycobactin and the presence of multiple copies of insertion element IS900 in its genome (Harris and Barletta, Reference Harris and Barletta2001; Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006; Robertson et al., Reference Robertson, Cerf, Condron, Donaghy, Heggum and Jordan2017; Cunha et al., Reference Cunha, Rosalino, Leão, Bandeira, Fonseca, Botelho and Reis2020; Okuni et al., Reference Okuni, Hansen, Eltom, Eltayeb, Amanzada, Omega, Czerny, Abd El Wahed and Ojok2020). It appears that MAP is more heat stable than other mycobacteria, as previous research has demonstrated its ability to survive pasteurization (Rathnaiah et al., Reference Rathnaiah, Zinniel, Bannantine, Stabel, Gröhn, Collins and Barletta2017; Gerrard et al., Reference Gerrard, Swift, Botsaris, Davidson, Hutchings, Huxley and Rees2018). Therefore, a test for its rapid detection would therefore not only be extremely useful in veterinary medicine but also in dairy processing.
There is an apparently cyclical relationship between the environmental distribution of MAP and the incidence of JD, as the infected animals shed MAP into the soil, and slurry/run-off introduces MAP to water sources (Salgado et al., Reference Salgado, Alfaro, Salazar, Badilla, Troncoso, Zambrano, González, Mitchell and Collins2015; Garvey, Reference Garvey2018). Broadly speaking, the extra-intestinal lifecycle of MAP is not well understood, though it has been suggested that free-living amoebae may act as a non-mammalian host that contributes to their environmental persistence, with one study practically demonstrating the survival of MAP in Acanthamoeba castellani in vitro (Salgado et al., Reference Salgado, Alfaro, Salazar, Badilla, Troncoso, Zambrano, González, Mitchell and Collins2015; Samba-Louaka et al., Reference Samba-Louaka, Robino, Cochard, Branger, Delafont, Aucher, Wambeke, Bannantine, Biet and Héchard2018; Okuni et al., Reference Okuni, Hansen, Eltom, Eltayeb, Amanzada, Omega, Czerny, Abd El Wahed and Ojok2020). The thick, waxy cell wall is also considered to be a major factor in the persistence of MAP in the environment, where it appears to contribute to its stability under various heat, UV, and low pH conditions (Okuni et al., Reference Okuni, Hansen, Eltom, Eltayeb, Amanzada, Omega, Czerny, Abd El Wahed and Ojok2020). Previous studies have found that MAP can remain viable for several months to a year in manure, soil, and/or water, with shaded pastures and troughs proving the most permissible to MAP survival (Whittington et al., Reference Whittington, Marshall, Nicholls, Marsh and Reddacliff2004; Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019). Considering its environmental distribution, an important consideration for designing novel detection assays would be whether the assay can be applied to a wide range of sample types (e.g. blood, soil, or water) to maximize usefulness.
The mycolic acid-rich cell wall and the intracellular lifecycle of MAP also explain the worryingly intrinsic AR of this species to certain antibiotics (e.g. isoniazid; Brown-Elliott et al., Reference Brown-Elliott, Nash and Wallace2012; Franco-Paredes et al., Reference Franco-Paredes, Marcos, Henao-Martínez, Rodríguez-Morales, Villamil-Gómez, Gotuzzo and Bonifaz2018). This emphasizes the need for alternative therapies and control strategies to be found to combat JD, as the intrinsic AR of MAP already limits treatment options. What would be a great benefit, is a clinical treatment and/or detection method that is not unhindered by the mycolic acid-rich cell wall but exploits it. By closely monitoring the farm environment in tandem with animal testing, it should be possible to actively sever routes of transmission, which are discussed below in the context of dairy herds.
Transmission of Mycobacterium avium subsp. paratuberculosis
Vertical transmission of MAP involves the prenatal exposure of unborn calves by MAP-positive cows/heifers through transplacental infection (Park et al., Reference Park, Park, Cho, Kim, Jung, Shin, Lee, Kim and Yoo2017; Garvey, Reference Garvey2020). The possibility that susceptibility to MAP infection is inheritable has been analyzed to be low to moderate, so it is likely that the prevalence of vertical transmission is in some way related to the prevalence of MAP within the herd (Park et al., Reference Park, Park, Cho, Kim, Jung, Shin, Lee, Kim and Yoo2017). An issue inherent to analyses of vertical transmission is difficulty in differentiating vertical from horizontal transmission (Judge et al., Reference Judge, Kyriazakis, Greig, Davidson and Hutchings2006; Park et al., Reference Park, Park, Cho, Kim, Jung, Shin, Lee, Kim and Yoo2017; Mitchell et al., Reference Mitchell, Beaver, Knupfer, Pradhan, Fyock, Whitlock and Schukken2019).
Horizontal transmission occurs postnatally (pseudo-vertically), often within the first month of life when calves consume contaminated colostrum/milk or are exposed to the fecal matter from the infected mother or other calves (Wolf et al., Reference Wolf, Orsel, De Buck and Barkema2015; Al-Mamun et al., Reference Al-mamun, Smith, Schukken and Gröhn2017; Field et al., Reference Field, Mcaloon, Gavey and Mee2022). Horizontal transmission has been occasionally observed in older cattle, primarily through the fecal–oral route, whereby MAP-infected animals shed the bacteria and thereby contaminate the environment, as described in a previous section (Garvey, Reference Garvey2020). This draws attention to the necessity for a highly effective diagnostic test. An ideal test would also have a rapid turnaround time in order to quickly detect and isolate animals who may be shedding MAP and actively infecting other livestock in the herd.
Interestingly, MAP infection does not guarantee progression to JD, as additional factors such as herd size, animal age, and milk production contribute to disease prognosis (Wolf et al., Reference Wolf, Orsel, De Buck and Barkema2015; Garvey, Reference Garvey2018; Garvey, Reference Garvey2020). Overall, it is understood that calves are the most at risk of infection due to their underdeveloped immune system (Windsor and Whittington, Reference Windsor and Whittington2010; Wolf et al., Reference Wolf, Orsel, De Buck and Barkema2015; Facciuolo et al., Reference Facciuolo, Gonzalez-Cano, Napper, Griebel and Mutharia2016; Garvey, Reference Garvey2020).
Pathogenesis of Johne's disease
Progression to JD involves MAP cells breaching the mucosal defences of the small intestine and establishing a niche resulting in granulomatous lesions along the wall of the ileum (Weiss et al., Reference Weiss, Evanson and Souza2006; Martcheva et al., Reference Martcheva, Lenhart, Eda, Klinkenberg, Momotani and Stabel2015; DeKuiper and Coussens, Reference Dekuiper and Coussens2019). MAP transverse the epithelium by exploiting fibronectin receptors on the surface of microfold (M) cells. M cells are specialized epithelial cells responsible for ‘sampling’ the lumen contents and transporting potential antigens, including live bacteria, to the underlying lymphoid follicles (Dillon and Lo, Reference Dillon and Lo2019; Kobayashi et al., Reference Kobayashi, Takahashi, Takano, Kimura and Hase2019). The lymphoid follicles, termed Peyer's patches, are home to macrophages, which phagocytose the MAP at the basal side of the M cells (Fig. 3; Patel et al., Reference Patel, Danelishvili, Yamazaki, Alonso, Paustian, Bannantine, Meunier-Goddik and Bermudez2006; Wagner et al., Reference Wagner, Bonnardel, Da Silva, Martens, Gorvel and Lelouard2018; Garvey, Reference Garvey2020). Infected macrophages enter the lymphatic system, which further disseminates the MAP infection (Patel et al., Reference Patel, Danelishvili, Yamazaki, Alonso, Paustian, Bannantine, Meunier-Goddik and Bermudez2006; Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006).
Figure 3. Schematic of MAP uptake by M cells. The MAP (red) interacts with the fibronectin receptors on the surface of the M cell (blue), triggering endocytosis. MAP is released from the endosome at the basal side of the M cell and is presented to macrophages (purple) resident in Peyer's patches (green). The macrophages phagocytose the MAP and will eventually aggregate into granulomas. MAP-infected macrophages may also enter the lymphatic system through the Peyer's patch, which creates a systemic infection and secondary sites of infection, such as in the mammary glands. Created with BioRender.com.
During early infection, some MAP survives within the phagosome by preventing lysosome fusion (Broxmeyer et al., Reference Broxmeyer, Sosnowska, Miltner, Chacón, Wagner, Mcgarvey, Barletta and Bermudez2002). This poses an additional problem in terms of developing novel treatments and rapid diagnostic tests, as the pathogens effectively have a mammalian cell shield preventing the drug or the probe accessing its target. This becomes a greater issue as the infection progresses, as infected macrophages eventually differentiate into epithelioid cells, which aggregate to form granulomas to suppress bacterial growth (Martcheva et al., Reference Martcheva, Lenhart, Eda, Klinkenberg, Momotani and Stabel2015; Rice et al., Reference Rice, Mcdaniel, Holland and Eda2019). Within the granuloma, MAP enters a dormant state and can gradually reactivate in later stages of infection, resulting in intermittent shedding of MAP in mid-stage disease (Martcheva et al., Reference Martcheva, Lenhart, Eda, Klinkenberg, Momotani and Stabel2015; Rice et al., Reference Rice, Mcdaniel, Holland and Eda2019; Garvey, Reference Garvey2020). The granulomas attract T lymphocytes to the site of infection, which release inflammatory cytokines that contribute to the pathology of JD (DeKuiper and Coussens, Reference Dekuiper and Coussens2019; Rice et al., Reference Rice, Mcdaniel, Holland and Eda2019). For clarity, JD is typically described in four stages based on the severity of signs and likelihood of a positive result from a serological diagnostic test (Table 2; Whitlock and Buergelt, Reference Whitlock and Buergelt1996).
Table 2. Stages of Johne's disease
Source: Adapted from the National Research Council Committee on and Control of Johne's Disease (2003) and Tiwari et al. (Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006).
Stage I is the preclinical phase and does not display any noticeable pathologies and only post-mortem tissue culture to recover MAP returns a positive diagnosis (Whittington et al., Reference Whittington, Begg, De Silva, Purdie, Dhand and Plain2017). Similarly, Stage II is the subclinical phase and features no clinical signs, but animals may intermittently shed MAP (Wright et al., Reference Wright, Plain, Purdie, Saunders and De Silva2019; Garvey, Reference Garvey2020). Dairy cows may yield less milk during Stage II which can lead to culling prior to diagnosis (Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006). Diagnostic testing at this stage can be difficult, due to the intermittent nature of shedding causing fecal culture to be unreliable and anti-MAP antibodies are usually only detectable shortly before progression to Stage III (Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006; Berry et al., Reference Berry, Wu, Venturino and Talaat2018). Due to the slow growth rate of MAP and potential for the bacteria to enter a dormant phase within granulomas, infected animals remain in Stages I–II for prolonged incubation periods of 2–5 years (Garvey, Reference Garvey2020; Elsohaby et al., Reference Elsohaby, Fayez, Alkafafy, Refaat, Al-Marri, Alaql, Al Amer, Abdallah and Elmoslemany2021). Clinical signs develop at Stage III, at which point illness is apparent, with the hallmarks of JD (major diarrhea and weight loss) evident while vital signs remain normal (e.g. heart rate; Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006; Berry et al., Reference Berry, Wu, Venturino and Talaat2018). At this stage, both fecal culture and serological testing will return a positive result for MAP infection (Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006). Stage IV is considered advanced clinical disease and is fatal (Künzler et al., Reference Künzler, Torgerson, Keller, Wittenbrink, Stephan, Knubben-Schweizer, Berchtold and Meylan2014; Whittington et al., Reference Whittington, Begg, De Silva, Purdie, Dhand and Plain2017). The clinical of Stage III worsen, and animals become too weak to stand, anemic, and very skeletal in appearance (Fig. 1a; Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006; Garvey, Reference Garvey2020). Diagnostic tests will return positive results but relatively few animals reach this stage due to culling in Stage II or III, typically as an outcome of test-and-cull policies (Forde et al., Reference Forde, Pruvot, De Buck and Orsel2015). While test-and-cull may appear to be a quick and logical process of disease control, the sad truth is that these policies are fundamentally flawed, as a result of the unreliability of existing testing methods.
Test-and-cull to limit the transmission of Johne's disease
Culling is believed to be an important control measure for JD (Al-Mamun et al., Reference Al-mamun, Smith, Schukken and Gröhn2017; Garvey, Reference Garvey2020). Adult cows are typically culled once their milk yield reduces enough to affect overall productivity of the farm, potentially prior to any testing to diagnose subclinical JD (Tiwari et al., Reference Tiwari, Vanleeuwen, Mckenna, Keefe and Barkema2006; Lavers et al., Reference Lavers, Mckenna, Dohoo, Barkema and Keefe2013). As a result of more targeted efforts at reducing the impact of JD, test-based culling has become the standard, with newly bought calves and heifers undergoing testing for MAP infection. A negative result allows the new purchase to be integrated into the wider herd, while a positive result leads to culling (Jordan et al., Reference Jordan, Citer, Mcaloon, Graham, Sergeant and More2020). An inherent issue with test-and-cull methods is that no testing method is both 100% specific and 100% sensitive and existing programs are expensive and limited by the ability of farmers and veterinarians to recognize JD (Windsor and Whittington, Reference Windsor and Whittington2010). The three main methods of MAP detection are fecal culture, polymerase chain reaction (PCR)-based assays, and serological tests (Fig. 4).
Figure 4. Venn diagram illustrating the types of tests performed on various samples to diagnose JD.
Fecal culture
Fecal culture is a diagnostic test that determines the cause of diarrhea resulting from a presumed bacterial infection (Hewison et al., Reference Hewison, Heath and Ingram2012). While fecal culture to recover MAP offers a 100% specific result, it is usually only 30% sensitive and, in the context of large-scale testing on dairy farms, its cost outweighs the benefits (Lavers et al., Reference Lavers, Mckenna, Dohoo, Barkema and Keefe2013; Al-Mamun et al., Reference Al-mamun, Smith, Schukken and Gröhn2017). This method of testing is also inefficient for diagnosing JD in a timely manner, due to the long cultivation periods associated with MAP, even when using optimized conditions (Wolf et al., Reference Wolf, Orsel, De Buck and Barkema2015; Al-Mamun et al., Reference Al-mamun, Smith, Schukken and Gröhn2017; Okuni et al., Reference Okuni, Hansen, Eltom, Eltayeb, Amanzada, Omega, Czerny, Abd El Wahed and Ojok2020; Dane et al., Reference Dane, Koidis, Stewart and Grant2022). Likewise, fecal culture is an unreliable test for JD, due to the intermittent nature of MAP shedding in the subclinical stage and the potential for ingested MAP to be passively shed (i.e. no true infection), leading to incorrect diagnoses (Corbett et al., Reference Corbett, De Jong, Orsel, De Buck and Barkema2019; Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019). Fecal culture may also not be widely available in certain parts of the world, such as Saudi Arabia (Elsohaby et al., Reference Elsohaby, Fayez, Alkafafy, Refaat, Al-Marri, Alaql, Al Amer, Abdallah and Elmoslemany2021).
Polymerase chain reaction
Feces-based PCR tests are rapid and comparably sensitive to fecal culture, and the MAP-specific genetic elements, such as the insertion element IS900 (gold standard), f57, and open reading frame MAP0865, provide prime targets for analysis (Semret et al., Reference Semret, Turenne and Behr2006; Imirzalioglu et al., Reference Imirzalioglu, Dahmen, Hain, Billion, Kuenne, Chakraborty and Domann2011; Cunha et al., Reference Cunha, Rosalino, Leão, Bandeira, Fonseca, Botelho and Reis2020; Ramovic et al., Reference Ramovic, Madigan, Mcdonnell, Griffin, Bracken, Nighallchoir, Quinless, Galligan, Egan and Prendergast2020; Elsohaby et al., Reference Elsohaby, Fayez, Alkafafy, Refaat, Al-Marri, Alaql, Al Amer, Abdallah and Elmoslemany2021). Quantitative real-time PCR (qPCR) methods for IS900 detection have improved MAP sensitivity compared to conventional PCR (Sonawane and Tripathi, Reference Sonawane and Tripathi2013; Albuquerque et al., Reference Albuquerque, Santos, Souza Neto, Kim, Cavalcanti, Oliveira, Mota and Júnior2017; Beinhauerova et al., Reference Beinhauerova, Beinhauerova, Mccallum, Sellal, Ricchi, O'brien, Blanchard, Slana, Babak and Kralik2021) and Acharya et al. (Reference Acharya, Dhand, Whittington and Plain2017) have provided solutions to PCR inhibition that improved qPCR sensitivity to 80% compared to fecal culture. qPCR has also been shown to be highly effective at detecting infective MAP in environmental samples (Albuquerque et al., Reference Albuquerque, Santos, Souza Neto, Kim, Cavalcanti, Oliveira, Mota and Júnior2017; Ramovic et al., Reference Ramovic, Madigan, Mcdonnell, Griffin, Bracken, Nighallchoir, Quinless, Galligan, Egan and Prendergast2020). However, fecal-qPCR tests can be liable to return false positives due to passive MAP shedding, which can lead to premature culling (Forde et al., Reference Forde, Pruvot, De Buck and Orsel2015; Corbett et al., Reference Corbett, De Jong, Orsel, De Buck and Barkema2019; Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019; Beinhauerova et al., Reference Beinhauerova, Beinhauerova, Mccallum, Sellal, Ricchi, O'brien, Blanchard, Slana, Babak and Kralik2021).
Enzyme-linked absorbance assays
Enzyme-linked absorbance assays (ELISA) have been developed to detect MAP-related antigens, anti-MAP antibodies and elevated interferon-γ (an inflammatory cytokine associated with JD; Harris and Barletta, Reference Harris and Barletta2001; Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019). ELISA is a quick and cost-effective method and several user-friendly kits have been created to aid veterinary risk assessments and management plans (Kennedy et al., Reference Kennedy, Byrne, Garcia, O'Mahony and Sayers2016; Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019; Jordan et al., Reference Jordan, Citer, Mcaloon, Graham, Sergeant and More2020). Unlike PCR, ELISA is highly effective at detecting MAP in bulk milk samples (Beaver et al., Reference Beaver, Sweeney, Hovingh, Wolfgang, Gröhn and Schukken2017). Unfortunately, though the most economically favorable, ELISA is the least sensitive, with testing complicated by common antigens between MAP and other mycobacteria, such as Mycobacterium bovis, and the fact that the immune response in the early stages of JD are cellular (i.e. phagocyte mediated) as opposed to humoral (i.e. antibody mediated; Harris and Barletta, Reference Harris and Barletta2001; Beaver et al., Reference Beaver, Sweeney, Hovingh, Wolfgang, Gröhn and Schukken2017; Elsohaby et al., Reference Elsohaby, Fayez, Alkafafy, Refaat, Al-Marri, Alaql, Al Amer, Abdallah and Elmoslemany2021). Consequently, current strategies rely on using ELISA to determine the overall JD status of herd and ELISA-positive cattle undergo further testing, usually fecal culture, to confirm the diagnosis. However, a positive ELISA does not necessarily predict a positive fecal culture (due to intermittent shedding of MAP; Beaver et al., Reference Beaver, Sweeney, Hovingh, Wolfgang, Gröhn and Schukken2017; Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019; Ramovic et al., Reference Ramovic, Madigan, Mcdonnell, Griffin, Bracken, Nighallchoir, Quinless, Galligan, Egan and Prendergast2020). Research also suggests that veterinarians are not appropriately advised on the handling of serum samples prior to testing, which can affect the outcome of the ELISA (Alinovi et al., Reference Alinovi, Ward, Lin and Wu2009).
The future of test-and-cull methods
Evidently, vast improvements must be made upon the existing testing methods before test-and-cull becomes a truly efficient method of JD control. Similarly, veterinarians will likely require further education and training regarding JD and associated testing to ensure tests are carried out correctly and in a timely manner. Consequently, an ideal novel diagnostic assay should not only be highly sensitive and specific, but easy to use with clear sample handling guidelines and have a rapid turnaround time to benefit animals whose clinical signs were recognized late. Ideally, a novel test will also be capable of detecting the antibiotic susceptibilities of MAP.
However, until such novel diagnostics are developed and marketed, the unfortunate reality is that the combination of inefficient diagnostics tests, intermittent MAP shedding, and the slow prognosis of JD will inevitably lead to high global prevalence of the disease and subsequent economic losses associated with culling and replacing cattle.
Prevalence and economic impact of Johne's disease
JD is a global issue, though disease prevalence varies between countries and appears to be correlated to whether an informed control program is in available/complied with, and the accessibility/quality of diagnostics (Whittington et al., Reference Whittington, Donat, Weber, Kelton, Nielsen, Eisenberg, Arrigoni, Juste, Sáez, Dhand, Santi, Michel, Barkema, Kralik, Kostoulas, Citer, Griffin, Barwell, Moreira, Slana, Koehler, Singh, Yoo, Chávez-Gris, Goodridge, Ocepek, Garrido, Stevenson, Collins, Alonso, Cirone, Paolicchi, Gavey, Rahman, De Marchin, Van Praet, Bauman, Fecteau, Mckenna, Salgado, Fernández-Silva, Dziedzinska, Echeverría, Seppänen, Thibault, Fridriksdottir, Derakhshandeh, Haghkhah, Ruocco, Kawaji, Momotani, Heuer, Norton, Cadmus, Agdestein, Kampen, Szteyn, Frössling, Schwan, Caldow, Strain, Carter, Wells, Munyeme, Wolf, Gurung, Verdugo, Fourichon, Yamamoto, Thapaliya, Di Labio, Ekgatat, Gil, Alesandre, Piaggio, Suanes and De Waard2019; Jordan et al., Reference Jordan, Citer, Mcaloon, Graham, Sergeant and More2020; Klopfstein et al., Reference Klopfstein, Leyer, Berchtold, Torgerson and Meylan2021). The unreliability of the diagnostic tests described in the previous section makes accurately determining prevalence difficult (Windsor and Whittington, Reference Windsor and Whittington2010; Beaver et al., Reference Beaver, Sweeney, Hovingh, Wolfgang, Gröhn and Schukken2017; Mitchell et al., Reference Mitchell, Beaver, Knupfer, Pradhan, Fyock, Whitlock and Schukken2019; Garvey, Reference Garvey2020). This is reflected in a retrospective analysis undertaken by Lombard et al. (Reference Lombard, Gardner, Jafarzadeh, Fossler, Harris, Capsel, Wagner and Johnson2013) that determined the apparent prevalence of JD to be 70.4% in 2007, while the apparent prevalence for that year was 91.1%. The discrepancy between the apparent and true prevalence is important to address in terms of disease control but also in relation to economic losses.
According to Lombard et al. (Reference Lombard, Gardner, Jafarzadeh, Fossler, Harris, Capsel, Wagner and Johnson2013), in 1996 the US prevalence of JD was 21.6%, and for the same year Losinger (Reference Losinger2005) reports losses of $200 million ± $160 million to the US economy. By 2010, the global economic losses tied to JD were more than US$ 1.5 billion, correlating to the increase in MAP prevalence in the US and Europe in the intervening years (Johnston et al., Reference Johnston, Coffey, O'Mahony and Sleator2010; Lombard et al., Reference Lombard, Gardner, Jafarzadeh, Fossler, Harris, Capsel, Wagner and Johnson2013; Garvey, Reference Garvey2020). The economic impact associated with JD is largely related to the reduction in milk production and the culling of infected animals further reducing the productivity of dairy farms (Harris and Barletta, Reference Harris and Barletta2001; Johnston et al., Reference Johnston, Coffey, O'Mahony and Sleator2010; Wolf et al., Reference Wolf, Orsel, De Buck and Barkema2015; Rasmussen et al., Reference Rasmussen, Barkema, Mason, Beaulieu and Hall2021). For instance, MAP-positive dairy farms in Germany lose approximately 1.41% of gross milk revenue and 34–41% of total losses incurred by the Irish dairy industry are attributed to premature culling and decreased slaughter value (Rasmussen et al., Reference Rasmussen, Barkema, Mason, Beaulieu and Hall2021). There are also additional veterinary costs related to treating MAP-associated mastitis, diagnostic testing, and implementing other control measures (such as routine testing; Garvey, Reference Garvey2020; Jordan et al., Reference Jordan, Citer, Mcaloon, Graham, Sergeant and More2020). Fewer costs are associated with treatment of JD, as most guidelines promote test-and-cull, but actively treating MAP infection could provide a solution to culling-related losses and expenses (i.e. diagnostic testing and purchasing replacement cattle). It is therefore important to consider how to effectively treat JD, while abiding by the legislation surrounding antibiotic use in food animals and limiting the risk of AR development.
Treatment of Johne's disease and the risk of antibiotic resistance
Presently, clinical JD is considered untreatable, and there is no recommended drug therapy or preventive vaccine (Garvey, Reference Garvey2020), although Australian researchers have recently published optimistic data from a large-scale vaccination trial, in which herd immunity (~70% immunity) was achieved amongst sheep against ovine JD (Links et al., Reference Links, Denholm, Evers, Kingham and Greenstein2021). Some available treatments include anti-inflammatory drugs, steroids, and monoclonal antibodies, but these are only partially effective, and relapse is common (Click, Reference Click2011b). Proposed antibiotic treatments for MAP infection involve a multi-drug approach over several months, as is the case for human TB infection (Slocombe, Reference Slocombe1982; St-Jean and Jernigan, Reference St-Jean and Jernigan1991; Davis et al., Reference Davis, Kuenstner and Singh2017).
AR, and the potential development of AR, is an important consideration when designing antibiotic regimens to treat JD. Ramovic et al. (Reference Ramovic, Madigan, Mcdonnell, Griffin, Bracken, Nighallchoir, Quinless, Galligan, Egan and Prendergast2020) observed during a pilot study that MAP and AR Gram-negative bacteria can co-exist within the same herd, thus posing a threat that a reservoir of AR genes is accessible to MAP. Similar to other mycobacteria, MAP has intrinsic resistance to certain antibiotics, such as isoniazid (Harris and Barletta, Reference Harris and Barletta2001; Garvey, Reference Garvey2020). Notably, macrolide resistance in MAP may be aided or even mediated by a ‘reluctant’ dimethyl-transferase, Erm (38), which has been identified in the M. tuberculosis complex (Madsen et al., Reference Madsen, Jakobsen and Douthwaite2005; Brown-Elliott et al., Reference Brown-Elliott, Nash and Wallace2012). As traditional culture-based antibiotic susceptibility testing is inefficient in the context of slow-growing MAP (i.e. it can several months to confidently determine susceptibility), the ability for a rapid diagnostic test to not only determine infection status, but the AR status of a positive result, would be a major advantage.
Considering the potential for MAP to become resistant to typical anti-mycobacterial drugs, other approaches have been considered. Forbes et al. (Reference Forbes, Ebsworth-Mojica, Didone, Li, Freundlich, Connell, Dunman and Krysan2015) have developed a high-throughput screening method to identify small molecules with anti-mycobacterial potential. Probiotics have also shown promise, with the bacterium Dietzia demonstrating the ability to prevent JD development following in utero or neonatal MAP infection, as well as the ability to improve the signs of Stage IV JD to a point of clinical remission (Click, Reference Click2011a, Reference Click2011b).
At the time of writing this review, PT has yet to be practically employed as a treatment for JD. However, interest in phage that infect mycobacteria or mycobacteriophage (MP), has been renewed in recent years as incidence of AR associated with human mycobacterial infections (including NTM infections) has increased (Azimi et al., Reference Azimi, Mosadegh, Nasiri, Sabour, Karimaei and Nasser2019). Similarly, as the global prevalence of JD has increased over recent decades, MP has been explored in lab settings as a potential control measure in the management of JD.
Mycobacteriophage
The first isolated MP targeted Mycobacterium smegmatis (M. smegmatis) and was identified in 1947. To date, approximately 12,000 MP have been isolated according to the Actinobacteriophage Database (https://phagesdb.org/hosts/genera/1/; accessed 25 July 2022) (Gardner and Weiser, Reference Gardner and Weiser1947; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). Most MP was discovered during large screening efforts involving programs aimed at second- and third-level students. For instance, the Phage Hunters Integrating Research and Education (PHIRE) program was developed in the early 2000s and has identified more than 300 novel MP (Hatfull, Reference Hatfull2018). Later, the University of Pittsburgh collaborated with the Science Education Alliance to create the Science Education Alliance Phage Hunters Advancing Genomics and Evolutionary Science (SEA-PHAGES) program, which has discovered thousands of MP, over 2000 of which have been sequenced (Jacob et al., Reference Jacob, Alvarez, Carney, Castro, Alvarez and Connors2020; Hatfull, Reference Hatfull2022).
The sequenced MP revealed extensive genetic diversity. It became apparent that MP genomes are architectural mosaics (meaning specific regions have evident evolutionary lineages, as opposed to the complete genome) with largely conserved gene organizations, featuring structural operons to one end of the genome and the genes required for infection and the lytic/lysogenic lifecycles to the other (Lima-Junior et al., Reference Lima-Junior, Viana-Niero, Conde Oliveira, Machado, Rabello, Martins-Junior, Martins, Digiampietri, Da Silva, Setubal, Russell, Jacobs-Sera, Pope, Hatfull and Leão2016; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). As a consequence of their mosaic architectures, it is exceedingly difficult to describe the evolution of MP in terms of biological relatedness. Therefore, the phage are grouped into ‘clusters’ and ‘subclusters’ according to overall nucleotide sequence similarity (Hatfull, Reference Hatfull2018; Sinha et al., Reference Sinha, Eniyan, Manohar, Ramesh and Bajpai2020). Each cluster is composed of phage which shares a minimum of 35% of their genes and members of subclusters share 90% (Pope et al., Reference Pope, Mavrich, Garlena, Guerrero-Bustamante, Jacobs-Sera, Montgomery, Russell, Warner and Hatfull2017; Hatfull, Reference Hatfull2018). MP which does not meet the minimum sequence homology required for inclusion in a cluster is termed ‘singletons’ (Suarez et al., Reference Suarez, Franceschelli, Tasselli and Morbidoni2020). For a comprehensive review of the MP clusters and genomics, please see Hatfull et al. (Hatfull, Reference Hatfull2022).
All MP described to date is double-stranded DNA viruses with icosahedral capsids and tails (Fig. 5; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). The tail proteins are important factors which determine the host specificity and infectability of MP (Hatfull, Reference Hatfull2018). Generally, phage recognize host-specific receptors present on the surface of bacteria, but unfortunately identifying mycobacterial receptors of importance for MP has proven to be a challenge and the basis of MP–host interactions remains elusive (McNerney and Traoré, Reference Mcnerney and Traoré2005; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021).
Figure 5. Electron micrographs of several MP. As the lack of genetic relatedness between MP does not easily lend itself to a systematic naming system, in combination with the fact that students are often responsible for their discovery, MP is not named according to any logical nomenclature. As a result, the monikers of MP range from the seemingly typical, such as TM4, L5, and D29, to the delightfully random, such as Corndog, Barnyard, and Rosebush. Adapted from Pedulla et al. (Reference Pedulla, Ford, Houtz, Karthikeyan, Wadsworth, Lewis, Jacobs-Sera, Falbo, Gross, Pannunzio, Brucker, Kumar, Kandasamy, Keenan, Bardarov, Kriakov, Lawrence, Jacobs, Hendrix and Hatfull2003).
Despite the insufficient understanding of how MP interact with their hosts, it has been noted that MP mutate in order to broaden their host specificity, with a relatively high frequency of 1 in every 100,000 acquiring such a mutation (which results in a single amino acid change in the tail proteins; Jacobs-Sera et al., Reference Jacobs-Sera, Marinelli, Bowman, Broussard, Guerrero Bustamante, Boyle, Petrova, Dedrick, Pope, Modlin, Hendrix and Hatfull2012). This adaptability suggests the potential for MP which infects non-pathogenic strains of M. smegmatis to readily adapt to infect clinical mycobacteria, such as MAP. MAP-sensitive MP could then be used to aid the biocontrol of JD, by detecting and potentially treating MAP infections.
Applications of mycobacteriophage in the biocontrol of Johne's disease
Mycobacteriophage-based detection of Mycobacterium avium subsp. paratuberculosis
MAP-sensitive MP have been applied in novel assays used to detect MAP in herds, bulk milk tanks and the farm environment (Fig. 6; Foddai and Grant, Reference Foddai and Grant2020). The FASTPlaqueTB assay was the first MP-based test to be used to detect viable MAP in milk, when researchers in the UK adapted the TB diagnostic tool. The basis of the test is phage-amplification. Viable mycobacteria present in the sample will allow for amplification or propagation of the MP, resulting in an increase in MP-plaque numbers by the end point of the test (Fig. 6a; Stanley et al., Reference Stanley, Mole, Smith, Glenn, Barer, Mcgowan and Rees2007). This modified assay was then combined with IS900-PCR to determine if the plaques contained MAP DNA to increase the specificity of the assay (Stanley et al., Reference Stanley, Mole, Smith, Glenn, Barer, Mcgowan and Rees2007).
Figure 6. Mycobacterial detection assays. (a) FASTPlaqueTB. A known concentration of phage-forming units (PFU) ml−1 is added to the samples. If there are no mycobacteria present in the sample, the endpoint PFU ml−1 will remain the same as the initial PFU ml−1 the phage is unable to propagate. If there are mycobacteria in the sample, the phage will infect the cells and propagate, resulting in an increase in PFU ml−1 at the endpoint of the assay relative to the initial concentration. (b) Actiphage. Phage is added to a sample to induce the lysis of any mycobacteria that may be present. Released DNA is then isolated and used in PCR-based detection methods to confirm the presence of mycobacteria. (c) Magnetic beads. Phage is attached to magnetic beads and used to bind to mycobacteria on the sample, which is then removed using a second magnet. The beads are subsequently placed in fresh broth to allow for infection and lysis prior to DNA isolation and PCR-based detection methods. (d). Antibiotic resistance detection. A known concentration of PFU ml−1 are added to mycobacterial cultures following the addition of an antibiotic. If the culture is susceptible to that antibiotic, the cells will have been killed prior to phage addition and thus the endpoint PFU ml−1 will remain the same as the initial PFU ml−1. If the culture is resistant to that antibiotic, the cells will still be viable at the point of phage addition and the endpoint PFU ml−1 will be increased relative to the initial PFU ml−1. Created with BioRender.com.
More recently, the same UK research group developed a rapid diagnostic test capable of detecting low levels of MAP in blood samples, called Actiphage®. This assay does not require plaques to form prior to PCR analysis, instead the lytic effect of phage D29 is exploited to release DNA from mycobacterial cells present in a sample prior to IS900-PCR (Fig. 6b; Swift et al., Reference Swift, Meade, Barron, Bennett, Perehenic, Hughes, Stevenson and Rees2020). During validation, Actiphage® was shown to be more sensitive and as specific as earlier phage-amplification-PCR methods, with Actiphage® detecting MAP in 87% of experimentally infected calves (0% in the control group) while the phage-amplification-PCR detected 66% (Swift et al., Reference Swift, Meade, Barron, Bennett, Perehenic, Hughes, Stevenson and Rees2020).
A similar MAP-detection assay was developed by Foddai and Grant (Reference Foddai and Grant2020). This assay resembles Actiphage®, in that it is based on the PCR detection of MAP DNA following phage-related lysis, but its procedure builds on a previous assay developed by this group that involves magnetic beads (Foddai et al., Reference Foddai, Strain, Whitlock, Elliott and Grant2011). The beads are coated with D29, which retain the ability to interact with MAP. An additional magnet is used to remove the bead-phage-MAP complex, which is then resuspended in fresh media to allow for infection and subsequent cell lysis. Once the cells have been lysed, the released DNA undergoes qPCR analysis to identify samples positive for MAP (Fig. 6c; Foddai and Grant, Reference Foddai and Grant2020). A similar phage coated magnetic bead assay also been optimized for detection MAP in milk (Hosseiniporgham et al., Reference Hosseiniporgham, Rebechesu, Pintore, Lollai, Dattena, Russo, Ruiu and Sechi2022)
Something that these assays do not address is AR in MAP. As described in a previous section, MAP possesses intrinsic resistance to certain antibiotics and may have access to a pool of resistance genes present in AR-Gram-negative commensals. There is a TM4-based assay which employs the phage-amplification technique to determine antibiotic sensitivities of M. smegmatis (Fig. 6d; Crowley et al., Reference Crowley, O'Mahony, Coffey, Sayers and Cotter2019). Mycobacterium smegmatis is incubated with the minimum inhibitory concentration of the drug before TM4 is added to the culture (Crowley et al., Reference Crowley, O'Mahony, Coffey, Sayers and Cotter2019). Plaque assays are performed similarly to the FASTPlaqueTB test (Stanley et al., Reference Stanley, Mole, Smith, Glenn, Barer, Mcgowan and Rees2007; Crowley et al., Reference Crowley, O'Mahony, Coffey, Sayers and Cotter2019). An increase in plaque numbers at the end point of the assay suggests the M. smegmatis cells were still viable and therefore resistant to the antibiotic (Crowley et al., Reference Crowley, O'Mahony, Coffey, Sayers and Cotter2019). It is very plausible that this assay can be optimized to determine AR-profiles of other mycobacteria, including MAP. This would likely reduce the turnaround considerably compared to traditional culture-based AR-susceptibility testing, because MP-based assays generally take 48 h to obtain results, while MAP culture can exceed 4 months (Broxmeyer et al., Reference Broxmeyer, Sosnowska, Miltner, Chacón, Wagner, Mcgarvey, Barletta and Bermudez2002; Crowley et al., Reference Crowley, O'Mahony, Coffey, Sayers and Cotter2019). The optimized assay could be modified to resemble the FASTPlaqueTB-IS900-PCR assay, so it could simultaneously determine the AR-profile and have high specificity for MAP (Stanley et al., Reference Stanley, Mole, Smith, Glenn, Barer, Mcgowan and Rees2007). This could aid the design of more effective antibiotic therapies and lead to a reduction in treatment failure, which would thereby reduce culling and economic losses. Similar loss-reductions could also be achieved, if safe and effective MP therapy (MPT) is developed as an alternative to antibiotic treatment.
Mycobacteriophage-based treatment of Johne's disease
At the time of writing, there have been no published attempts of clinically administering MP in an effort to treat JD. It appears the majority of studies involving MP and MAP only investigated the potential for MP to be used as diagnostic/detection tools, but the notion that they can be developed into a viable treatment option has been entertained before (Emery and Whittington, Reference Emery and Whittington2004; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). While exploration into the MPT in veterinary health is lacking, the rising incidence of extensively drug-resistant TB, and the concurrent rise in NTM and AR-NTM infections, has heightened the interest in MPT within human medicine (Azimi et al., Reference Azimi, Mosadegh, Nasiri, Sabour, Karimaei and Nasser2019; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021).
Several MP has been investigated for efficacy in reducing the bacterial burden in TB infections, including the model MP D29 and TM4 (Azimi et al., Reference Azimi, Mosadegh, Nasiri, Sabour, Karimaei and Nasser2019). These studies have largely been conducted in vitro, and to date only two in vivo studies concerning MPT have been performed (Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). While the first in vivo study conducted by Sula et al. (Reference Sula, Sulová and Stolcpartová1981) demonstrated the therapeutic effect of MP DS-6A against disseminated TB infection in guinea pigs (resulting in fewer lesions in the spleen, liver, and lungs), the second study found that MPT was less effective than isoniazid in treating disseminated TB in the same model (however fewer granulomas were observed in the phage treated guinea pigs; Zemskova and Dorozhkova, Reference Zemskova and Dorozhkova1991). Although the curative properties of MP remain hypothetical, the reduction in granuloma formation associated with disseminated TB could mean that combining MPT and traditional antibiotic regimens could improve prognoses and aid recovery. Likewise, there appears to be hope in prophylactic MPT, as a recent investigation found that mice treated with nebulized D29 prior to TB inhalation had a significantly reduced bacterial burden compared to the control group (Carrigy et al., Reference Carrigy, Larsen, Reese, Pecor, Harrison, Kuehl, Hatfull, Sauvageau, Baldwin, Finlay, Coler and Vehring2019). These results suggest that it may be possible to prophylactically treat dairy cattle (and other susceptible ruminants) against MAP infection, and therefore JD.
Compassionate MPT could also be a viable treatment option, should a MAP infection prove resistant to the recommended antibiotic therapies. For example, a recent case study of an AR-NTM infection in a cystic fibrosis patient has demonstrated the efficacy of genetically engineered-MP treatment in resolving AR mycobacterial infections (Dedrick et al., Reference Dedrick, Guerrero-Bustamante, Garlena, Russell, Ford, Harris, Gilmour, Soothill, Jacobs-Sera, Schooley, Hatfull and Spencer2019). While evidence that this success story will translate effectively into bovine JD is lacking, the amazing accomplishments of PT associated with compassionate use in human medicine offers hope that its introduction to veterinary medicine will be similarly effective in treating late-stage JD with MP.
Potential limitations of mycobacteriophage therapy
Aside from the lack of legislation surrounding PT and Western society, PT (and therefore MPT) is still largely regarded as an ‘experimental’ treatment that has little public understanding. For a comprehensive review on the limitations of MPT, please refer to Allué-Guardia et al. (Reference Allué-Guardia, Saranathan, Chan and Torrelles2021).
Briefly, host specificity can limit the applicability of any one phage (which is why PT often involves phage cocktails) and there are several concerns regarding the risks posed by phage to mammals (Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). These include the risk of toxic shock as a consequence of cytotoxic components being released from lysed bacterial cells following phage infection (Henein, Reference Henein2013; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). Similarly, the bacterial debris and the phage themselves could possibly trigger an allergic reaction (although no trials in any mammalian model have observed such a reaction; Cisek et al., Reference Cisek, Dąbrowska, Gregorczyk and Wyżewski2017; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021). Another possible hindrance is anti-phage antibodies, which may clear the phage before the infection is treated (Cisek et al., Reference Cisek, Dąbrowska, Gregorczyk and Wyżewski2017). Additionally, intracellular pathogens, such as MAP, are presumed to be well concealed by the mammalian cell, thus preventing recognition by phage (Azimi et al., Reference Azimi, Mosadegh, Nasiri, Sabour, Karimaei and Nasser2019; Allué-Guardia et al., Reference Allué-Guardia, Saranathan, Chan and Torrelles2021).
Despite this presumption, it has been observed that phage can exploit transcytosis to cross the epithelial barrier and enter the bloodstream and other organs. It is estimated that 31 billion phage transcytose the epithelial barrier in the gut daily (Nguyen et al., Reference Nguyen, Baker, Padman, Patwa, Dunstan, Weston, Schlosser, Bailey, Lithgow, Lazarou, Luque, Rohwer, Blumberg and Barr2017; Otero et al., Reference Otero, García-Rodríguez, Cano-Sarabia, Maspoch, Marcos, Cortés and Llagostera2019). Pathogen-infected phagocytes are also capable of internalizing phage via endocytosis, at which point the endosome and phagosome can merge (as typically only lysosome fusion is inhibited by bacteria), thereby granting phage access to the pathogen (Broxmeyer et al., Reference Broxmeyer, Sosnowska, Miltner, Chacón, Wagner, Mcgarvey, Barletta and Bermudez2002; Jończyk-Matysiak et al., Reference Jończyk-Matysiak, Weber-Dąbrowska, Owczarek, Międzybrodzki, Łusiak-Szelachowska, Łodej and Górski2017). Other investigations have demonstrated the ability of genetically engineered phage to induce endocytosis and kill intracellular bacteria (Bárdy et al., Reference Bárdy, Pantůček, Benešík and Doškař2016; Møller-Olsen et al., Reference Møller-Olsen, Ho, Shukla, Feher and Sagona2018).
Regarding MAP/mycobacterial infections specifically, there is much interest in the use of M. smegmatis or liposomes to facilitate a ‘Trojan horse’ approach (Broxmeyer et al., Reference Broxmeyer, Sosnowska, Miltner, Chacón, Wagner, Mcgarvey, Barletta and Bermudez2002; Nieth et al., Reference Nieth, Verseux, Barnert, Süss and Römer2015; Azimi et al., Reference Azimi, Mosadegh, Nasiri, Sabour, Karimaei and Nasser2019; Otero et al., Reference Otero, García-Rodríguez, Cano-Sarabia, Maspoch, Marcos, Cortés and Llagostera2019). Non-virulent M. smegmatis harboring MP can present antigens to MAP-infected phagocytes and following internalization, can protect the MP from degradation and deliver the phage to the target bacteria (Broxmeyer et al., Reference Broxmeyer, Sosnowska, Miltner, Chacón, Wagner, Mcgarvey, Barletta and Bermudez2002). Similarly, encapsulating MP in liposomes can shield them from undesirable conditions and enable transcytosis of MP by interacting with the lipid membranes of epithelial and phagocytic cells (Otero et al., Reference Otero, García-Rodríguez, Cano-Sarabia, Maspoch, Marcos, Cortés and Llagostera2019).
While yet to be explored in a clinical setting, it appears that the limitations that may arise during the design of MPT have a good chance of being overcome, particularly as understanding of phage-host and phage-mammalian cell interactions advances. However, it is vital that every potential barrier to effective MPT (and PT in general) is addressed in extreme detail, both to quell any concerns held by the agricultural and veterinary sectors and (especially in the case of compassionate MPT) to confirm the safety and efficacy of treatment.
Concluding remarks
Employing JD as a case study, this review has highlighted the negative impact of this disease on both the physical wellbeing of infected ruminants and the profit margin of the dairy industry. The current limitations associated with diagnosing JD and the risk that its etiological agent, MAP, could develop AR have also been addressed. Ergo, developing novel diagnostic approaches and highly targeted treatments would benefit both the agricultural and health sector, by reducing the economic impact of JD and the potentially negative impact of antibiotic use in livestock. The notion that MP may constitute a highly effective basis for rapid MAP-detection assays and possibly phage-based medications, which can greatly aid JD control programs, has been emphasized in this review. While the introduction of MP-based control measures for JD is a relatively novel approach, and currently there is little evidence supporting the in vivo efficacy of MPT, the potential for these simple organisms to transform how JD is managed is considerable.
Acknowledgments
The authors would like to acknowledge the financial contribution of the Risam PhD Scholarship Fund.
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