Next Article in Journal
The Potential of Probiotics to Eradicate Gut Carriage of Pathogenic or Antimicrobial-Resistant Enterobacterales
Next Article in Special Issue
Ethnobotany, Ethnopharmacology, and Phytochemistry of Medicinal Plants Used for Treating Human Diarrheal Cases in Rwanda: A Review
Previous Article in Journal
Microwave-Assisted, One-Pot Synthesis of Doxycycline under Heterogeneous Catalysis in Water
Previous Article in Special Issue
Clinical Outcomes and Safety of Meropenem–Colistin versus Meropenem–Tigecycline in Patients with Carbapenem-Resistant Acinetobacter baumannii Pneumonia
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Antibiotics
Volume 10
Issue 9
10.3390/antibiotics10091085
antibiotics-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Review

Phages for Africa: The Potential Benefit and Challenges of Phage Therapy for the Livestock Sector in Sub-Saharan Africa

by
Angela Makumi
*,
Amos Lucky Mhone
,
Josiah Odaba
,
Linda Guantai
and
Nicholas Svitek
*
Department of Animal and Human Health, International Livestock Research Institute (ILRI), P.O. Box 30709, Nairobi 00100, Kenya
*
Authors to whom correspondence should be addressed.
Antibiotics 2021, 10(9), 1085; https://doi.org/10.3390/antibiotics10091085
Submission received: 6 July 2021 / Revised: 24 August 2021 / Accepted: 25 August 2021 / Published: 8 September 2021
(This article belongs to the Special Issue Alternative Approaches to Treating Antimicrobial Resistant Infections)
Browse Figure
Review Reports Versions Notes

Abstract

:
One of the world’s fastest-growing human populations is in Sub-Saharan Africa (SSA), accounting for more than 950 million people, which is approximately 13% of the global population. Livestock farming is vital to SSA as a source of food supply, employment, and income. With this population increase, meeting this demand and the choice for a greater income and dietary options come at a cost and lead to the spread of zoonotic diseases to humans. To control these diseases, farmers have opted to rely heavily on antibiotics more often to prevent disease than for treatment. The constant use of antibiotics causes a selective pressure to build resistant bacteria resulting in the emergence and spread of multi-drug resistant (MDR) organisms in the environment. This necessitates the use of alternatives such as bacteriophages in curbing zoonotic pathogens. This review covers the underlying problems of antibiotic use and resistance associated with livestock farming in SSA, bacteriophages as a suitable alternative, what attributes contribute to making bacteriophages potentially valuable for SSA and recent research on bacteriophages in Africa. Furthermore, other topics discussed include the creation of phage biobanks and the challenges facing this kind of advancement, and the regulatory aspects of phage development in SSA with a focus on Kenya.

1. Introduction

In Africa, a majority of the population, in a range of 250–300 million, depend on livestock for their income and livelihood, with livestock representing an average of 30% of the agricultural gross domestic product (GDP) and roughly 10% of the total GDP [1]. Animal diseases, including zoonoses, are crucial constraints in the enhancement of livestock-production systems [2] and compromise food-producing animals’ nutritional and economic potential [3]. Facing its own challenges, Africa has been reported to be one of the continents with the highest number of foodborne diseases, with approximately 91 million related diseases and 137,000 death per annum [4]. Unfortunately, on a global scale, the use of antibiotics is largely unregulated, and this is worse in developing countries where the use of antibiotics for food and animal productions to accelerate the growth of animals is rampant. Compared to other continents, Africa produces fewer antibiotics, but unregulated access and inappropriate use worsens antibiotic resistance [4,5]. Other factors, such as the poor regulation on the use of antimicrobials in both human and animals, inaccessibility to appropriate therapy, weak surveillance systems, and a lack of updated use and treatment guidelines of antimicrobials, play a role in the spread of antibiotics resistance [6]. Farmers also play a massive role in the misuse of antibiotics whereby there is a tendency to store drugs and treat animals based on symptoms they are familiar with from past infections, engaging unskilled people to treat animals, and unregulated disposal of waste in dumps. Counterfeit medicines are an additional issue that could jeopardize the fight against antimicrobial resistance [7]. Due to this constant application of antibiotics, whether for prevention, treatment, or growth promotion, this creates a selective pressure on resistant bacteria. Due to this exposure, bacteria have also developed bet-hedging strategies to resist these harsh antibiotics over time; however, this comes at survival cost for the bacteria but propels survival of a population of bacteria from extinction [7,8]. Among the strategies’ that bacteria use to acquire resistance, include the transfer of resistant genes through horizontal gene transfer, mobile genetic elements, and the bacterial toxin–antitoxin system [9].

2. Antibiotic Resistance in Livestock Farming

In Africa, pathogenic bacteria pose a significant challenge due to antibiotic resistance [10]. The World Health Organization (WHO) has listed priority pathogens based on research and development with a higher number of Gram-negative bacteria named as critical AMR-related threats globally [11], including Enterobacteriaceae that are carbapenem-resistant or extended spectrum beta-lactamase (ESBL) producing as indicated in Table 1. In other cases, resistant commensals such as E. coli, which rarely cause disease directly, can act as an AMR gene reservoir. The genes can be transferred to zoonotic pathogens, for example, Salmonella enterica, or other Gram-negative bacteria in the gut [12]. Additionally, most microorganisms are naturally transformable, for example, C. jejuni acquiring antibiotic-resistant genes from other organisms [13]. According to the WHO, antibiotics such as fluoroquinolones used in agricultural animals have resulted in the development of ciprofloxacin-resistant Salmonella, Campylobacter, and E. coli, that contribute to human infections that are difficult to treat. Tetracycline, penicillin, and sulfonamides are among the most abused antimicrobials SSA (Table 1) which has also been reported in other low resource setting countries [14]. Other bacteria species that are relevant in livestock and causes substantial loses include Methicillin-Resistant Staphylococcus aureus. However, it is difficult to estimate the exact prevalence of antimicrobial resistance in SSA due to the low number of antimicrobial resistance surveillance programs and research reports.
Data in Table 1 was collated from several research papers over the last ten years (2011–2021), which includes the country of research, livestock species focused on, and the sample analyzed for presence of bacteria as well as the antibiotic resistance pattern obtained from bacteria isolated. Using the data from the table above, Figure 1 below was tabulated to represent the species of livestock farmed in SSA. Additionally, poultry appears to be a popular livestock species that is commonly farmed (Figure 1) in most SSA countries but also records to be a source of high antibiotic resistance, with some African countries reporting resistance to more than ten antibiotics, as depicted in Table 1.
In comparison to other livestock farmed in SSA, but comparable to other low- and middle-income countries, the high popularity of poultry farming can be attributed to several key factors such as small body size (hence, more birds can be kept in a smaller holding), relatively short life cycle between flocks, high energy uptake efficiency, and robust adaptability to environmental conditions [50,51,52]. Due to these factors, this principally causes a shift from subsistence to intensive farming that also requires routine antimicrobial usage to improve chicken health and results in weight gain while also preventing diseases such as necrotic enteritis caused by Clostridium perfringens [53]. If antibiotic use is absolutely necessary, the withdrawal of antibiotics before slaughtering should be followed as the conventional standard practice; however, it could be difficult to monitor if small-scale rural poultry farmers consistently follow this guideline [54]. For this reason, alternatives need to be sought after as this will drastically decrease the overuse of antibiotics while mitigating antibiotic resistance in SSA.

3. Alternatives to Antibiotics Used in Livestock Farming

Given the fact that bacteria have become resistant to antibiotics and could continue to cause infections, there is a growing need to find alternatives to antibiotics in the prevention and treatment of microbial infections. One of the alternative approaches is the use of naturally occurring botanicals that can be used in place of or together with antibiotics [55]. The conventional curative system has turned its attention to traditional herbs that are rich in compounds such as alkaloids, terpenoids, tannins, steroids, and flavonoids [55]. Most traditional plants have antimicrobials that can operate in synergy with antibiotics or possess compounds that have no intrinsic antibacterial activity but can sensitize the pathogens to previously ineffective antibiotics [56].
As humans produce antibodies to fight against disease, plants also produce primary metabolites such as amino acids, fatty acids, carbohydrates, and organic acids for their survival [57]. Some of the livestock diseases that have been controlled by using alternatives include mastitis, which is the most prevalent diseases in dairy cattle worldwide [58] and with the increasing rise of antibiotic resistance in the fight against mastitis, plant extracts, essential oils, and isolated compounds are used as an alternative in treating this infection [59]. These derivatives are used to disrupt the biofilm formation, thus preventing the bacteria’s ability to adhere and multiply [60]. Other alternatives used in the control of mastitis caused by multi-drug resistant (MDR) Staphylococcus spp. include bacteriocin Nisin combined with dioctadecyldimethylammonium bromide (NS/DDA) nanoparticles that have been shown to be a promising treatment alternative [58]. Minthostachus verticillate is a plant that produces essential oils and limonene, a monoterpene present in the scent and resin of the plant, and these extracts have been used against Escherichai coli, Bacillus pumilus, and Enterococcus faecium. The essential oil from this plant is used to inhibit the growth of the pathogens, while both agents affect the formation of biofilms [61]. There are other alternatives available and currently being used, including prebiotics/probiotics, enzymes, organic acids, and plant extracts [4]; however, this is not the scope of this review.
An alternative that is going through a renaissance is the use of bacteriophages (phages), viruses that infect bacteria, which have been used and administered as pharmaceutical agents even before the discovery of antibiotics [62]. Phages are the most abundant and ubiquitous organisms on earth, and can be found in natural and man-made environments, especially those in which their bacterial host thrives [63,64]. After the discovery of antibiotics by Alexander Fleming in 1928, phage therapy was rapidly abandoned in the West. However, in countries that had witnessed the birth of phage therapy, such as Georgia and Poland, this therapy continued to flourish until modern days [65]. Phages are viruses that have the ability to infect bacteria, replicate within them, and eventually kill their susceptible host releasing progeny virions [66]. Phages use two primary life cycles to replicate, the lytic cycle and the lysogenic cycle, each having significant implications for their therapeutic application [66]. In the lytic cycle, the phage attaches itself to the bacterial cell, allowing the penetration of phage nucleic acid, transcription, translation, assembly, and exit. This exit involves killing the bacteria through the expression of endolysins and releasing multiple, as low as 20 and up to hundreds or thousands of progeny phages, which can infect other bacterial cells, thereby repeating the cycle [67]. The duration from the attachment of a phage particle to a bacterial cell and its subsequent release of new phage particles usually happens within 20–40 min but can take up to 1–2 h [68]. Due to this short life cycle, phages could potentially be used for different applications such as prior slaughter, to treat or control bacteria that may pose harm to the farmer or end user [68]. The lysogenic cycle begins with inclusion its genetic material into the chromosome of the bacterial cell, after which, replication of the phage nucleic acid together with the host genes occurs for numerous generations without major metabolic consequences for the bacterial cell, thus allowing co-existence between the phage and bacteria [69]. This also facilitates the exchange of genetic material between the phage and bacteria. However, the phage may occasionally return to the lytic cycle, leading to the release of phage particles and, in some scenarios, spreading acquired bacterial DNA [70]. Temperate phages are usually not recommended for phage therapy, as during replication they can randomly pick up a wide range of segments of bacterial DNA and transfer them to a new host. This quality makes them undesirable for therapeutic applications since virulence-associated genes, or antibiotic-resistance genes, amongst other examples, could be transferred by this route [71,72]. In some scenarios, when a suitable lytic phage cannot be isolated, it may be necessary to exclude such harmful genes, usually by synthetic biology, to circumvent or eliminate these unfavorable features. Apart from reducing undesirable qualities, other potential benefits of using synthetic biology to alter phage function include modulating the phage host range, reducing phage toxicity and immunogenicity, enhancing phage survival after administration, improving phage activity against biofilms, and enhancing bacterial killing when combined with antibiotics [71]. On the contrary to most antibiotics, phages are highly specific antibacterial agents that have the advantage of causing minor damage to the healthy microbial flora of the treated animal [73]. With the increasing cases of antimicrobial resistance worldwide, phage therapy can be used as an alternative to antibiotics and in the treatment of several bacterial infections [74]. Moreover, phages have been used to combat bacterial infections in animals with the goal of reducing the bacterial load [75].

3.1. Attributes of Phage-Based Products That Could Be Compelling for Livestock Farming

Livestock has been reported to be the sector contributing to resistance to the most clinically relevant antibiotics, and this paves way for the use of phages to control bacterial infections. Phages could potentially be used as additives in feed if legislation approves such products. An example of an additive is with a commercial phage product to prevent or control mastitis, Salmonella enterica [76], Escherichia coli [77], Campylobacter spp. [78], and Listeria monocytogenes [79], which are some of the most prominent foodborne zoonotic pathogens. Previous studies have shown that phages successfully reduce bacterial colonization in the gastrointestinal tract through the oral delivery route. By measuring the colony forming units (CFU), Salmonella phages isolated from abattoirs, chicken farms, and wastewater, administered orally to chicken in antacid suspension, successfully reduced infection by S. Typhimurium and S. Enteritidis by 4.2 log10 CFU and 2.19 log10 CFU, respectively, within 24 h [80]. Campylobacter phage cocktail demonstrated an ability to reduce the titer of both C. coli and C. jejuni by approximately 2 log10 CFU/g when administered orally and in feed for poultry [81]. The use of a broad-spectrum cocktail for phage therapy is cost-effective compared to the use of a single phage [82]. Since the discovery of phages a century ago, they have tremendously transformed modern medicine.
The efficacy of bacteriophages as antimicrobials has fostered the approval and commercialization of several products intended for the reduction of different pathogenic bacterial species [83]. Examples of some phage-related products include SalmoFree and SalmoFresh™, both containing Salmonella enterica phages [82,84], ListShield™ designed with Listeria monocytogenes phages [85], as well as phage-derived enzymes such as Lysins, integrases, and excisionases, have received considerable attention as potential antibacterial agents [86]. Phage and phage related products have advantages over antibiotics in many ways; e.g., some applications may require only a single dose since phages can self-amplify. Moreover, because phages are easy to isolate from the environment, meaning short product development time frames and reduced production costs compared to antibiotics [87], this may make them suitable for SSA. Other beneficial properties of phages include a decreased probability of resistance development if a single phage with a wide host range or a cocktail of phages is used. Additionally, phages are safe (non-toxic) for eukaryotic cells and act as a bactericidal by hijacking many essential cellular processes required by the bacteria [88]. Below, the characteristics mentioned are described in detail and may qualify them to be used in livestock.

3.1.1. Single-Dose Potential

Due to their self-amplification nature and depending on the nature of the host, phages, in most cases, may not need repeated administrations over several days compared to antibiotics that require lengthy prescription doses to maintain the bioavailability of the active ingredient for a more extended period in the system [89,90]. Some studies have demonstrated that only one dose of phages could be required for therapy. A single dose of 200 µL of Avian Pathogenic Escherichia coli (APEC) phage cocktail (TM3, TM1, TM2, and TM4) at 1011 PFU/mL reduced the total viable E. coli count and increased the weight of chickens [91]. Polymer-encapsulated phages wV8, rV5, wV7, and wV11 reduced the shedding of E. coli O157:H7 in cattle feedlot upon a single dose administration [92]. In vivo studies in pigs have demonstrated that S. Typhimurium bacteriophages at 107 PFU/mL and 109 PFU/mL significantly reduced (p < 0.05) S. Typhimurium counts to 1.6 and 2.5 log10 CFU/mL, respectively, with a single dose after 24 h [92]. Likewise, an in vivo reduction of 1.49, 0.65, and 0.58 log10 CFU/mL in Salmonella Enteritidis number was obtained in broilers after a single oral gavage dose of 2.9 × 1010 PFU/mL [93]. Similarly, a single dose of vB_STy-RN5i1 and vB_STy-RN29 phages against Salmonella enterica obtained from market drain water was able to reduce bacterial cells by 3.1 and 2.7 log10 CFU/mL when characterized at 32 °C [94]. The phage cocktail (phiCcoIBB35, phiCcoIBB37, phiCcoIBB120) was able to reduce the titer of both Campylobacter coli and C. jejuni in feces by approximately 2 log10 CFU/g when administered by oral gavage and in feed upon a single dose [81]. The above literature indicates considerable decrease of bacterial load when single doses are used, which could be beneficial for resource-limited countries, especially if the production of large quantities of phages may not be feasible.

3.1.2. Inexpensive Drugs of Infectious Diseases

Phage production is relatively cheap, while research into antibiotic discovery is highly exorbitant due to processes involved in drug discovery. Every year, about 20% of animal production losses are linked to animal infectious diseases [95]. The global animal treatment market estimates that 60–70% of farm animals in developing countries receive basic medicalization. This rate of basic medicalization is projected to increase in the coming years owing to the increase in emerging infectious diseases, antimicrobial resistance, animal welfare initiatives, and the improving regulatory framework. This increase is expected to affect the cost of production for antibiotics and other medications. The estimated cost of production of a single new antibiotic is USD 1.5 billion [96]. This is much higher than the production cost of a phage product which is between USD 8000 and USD 20,000 [97]. In the phage production model, the cost of a single dose of Salmonella Enteritidis is estimated at USD 0.02 [98]. With the increased funding for research and development and the low cost of production of phage-related products, it is estimated that the bacteriophage market will steadily increase in the coming years.

3.1.3. Short Product Development Time Frames

Phage discovery is relatively easy because they are natural entities that are easier to isolate, purify, and characterize within a short time and at a lower cost as compared to antibiotics, which require several years of discovery and clinical trials [99]. The four methods of phages isolation—spot lysis, plaque testing, culture lysis, and routine test dilution (RTD)—have been shown to require only 24 h [100]. Likewise, the isolation of phages from animals and their environment also requires about 24 h, which is less time and effort than antibiotic discovery [100,101]. These former steps are easy to achieve but numerous factors should be taken into account in the context of product development. Bacteriophages that are considered for product development must be produced with an acceptable level of purity and have to be assessed for their efficacy in vivo and the safety of the final product. To ensure the consistency and stability of phages, the procedure for their manufacture, physicochemical and biological quality tests should be defined, as well as stringent production facilities [102]. As livestock farming in SSA is quite dynamic, with farmers rearing multiple livestock species together, this represents a complex ecology between bacteria species from different livestock as well as their interactions with phages. However, this encourages the development and delivery of local phage products that would take into account these farming dynamics.

3.1.4. Decreased Probability of Resistance Development

Bacteria are less likely to develop resistance against phages when the latter are used as therapy as compared to antibiotics. One of the drawbacks to this is the host range of the phages used. The host range describes the breadth of bacteria a phage is capable of infecting [103,104,105,106]. The narrow host range which is exhibited by most phages limits the number of bacterial types with which selection for specific phage-resistance mechanisms can occur [107]. Experimental data has shown that 80% of phage-resistant variants occur mostly in wide host range phages. The use of well-characterized phage cocktails is less likely to cause phage resistance as compared to broad-spectrum antibiotics [81,108,109,110]. The reason for this phenomenon is that phage cocktails generally rely on different receptor-binding proteins during attachment, allowing specific binding of a phage to a specific host through alternate routes of entry. Using single phage preparations rather than a cocktail toward a specific bacterial species only accelerates the process of mutations, thus rendering the phage product inactive [111]. Some examples of phage cocktails that have shown high activity include the SalmoFREE® phage cocktail, which demonstrated massive reduction of Salmonella, at the same time resulting in increased feed conversion, weight gain, homogeneity in chickens, without showing any cocktail resistant Salmonella strains in the course of the treatment [82]. Additionally, SalmoFresh™, which contains six strains of Salmonella phages, has demonstrated the capacity to reduce bacterial counts by an average of 5.34 logs CFU/mL after 5 h at 25 °C [84]. ListShield™ has demonstrated the ability to reduce the bacteria below detection levels (<10 CFU/mL) in pigs [79]. Although these phage products could be tested or used in SSA, there is need for research on local phages and their host range, which might provide more information on specificity of phages isolated in SSA, receptors involved as well as mutation frequencies of bacterial species.

4. Current Phage Research in Africa

Different research groups have been initiated in Africa, some of which are collaborating with Phages for Global Health (PGH). Since 2017, PGH has tasked itself with 2-week hands-on laboratory training course teaching scientists in developing countries how to isolate and characterize phages in their own regions. These countries so far include Kenya, Uganda, Ghana, and Tanzania. Using articles that have been published on different aspects of phage research, data has been collated over the last decade (2011–2021) to summarize the research that has been carried out in Africa. As this section is on the general but current phage research in Africa, the data represented herein (Table 2) include phage research on livestock, human, aquaculture, and the environment. The data in Table 2 show phage research that has been undertaken in Africa including the country, the source of phage isolation, phage host (where applicable), phage family, and the kind of research undertaken. From the table, phage research is gaining interest in Africa, whereby most research entails phage isolation and characterization, sequencing and metavirome studies. However, some gaps still exist despite many groups isolating and characterizing phages; only a few groups have delved into phage product design and development. There is also missing data on in vivo studies to test efficacy and safety of phages, phage bank establishment, and the regulatory aspect of phage products in the African context, such as that tackled in Section 6. Combining these data is important as this can help researchers from different groups across the world, and specifically the African continent, to fill in the gaps on phage research and areas that might need to be focused on. For this reason, phage research still needs to be sensitized and encouraged in Africa and collaborations with countries that have successfully used phages need to be fostered.

5. Hurdles of Phage Research and Regulatory Aspects of Phage Development/Products in SSA with a Focus on Kenya

As phage research in Africa is gaining interest, phages that are pure, well-characterized, sequenced, and have a defined host specificity still need to be documented. Moreover, this information should be publicly available to the different government bodies regulating veterinary practices in Africa. Currently, characterization, purification, sequencing, and storage of one phage can be achieved at a cost of about EUR 500 [162], which is not sustainable for the African continent and may need collaboration between different phage research groups around the world to cut down this cost. It is important to remember that several bacterial strains are often present in an infection; hence, multiple phage types may be needed to treat different strains of one bacterial species [162], making the goal of having a phage bank consisting of characterized phages equitably impossible if support from local governments is not achieved. Hence, our group, and several others, are pleading for the creation of phage banks across Africa to cater to the need for phages that are predicted to grow over the years to come amid the alarming rate at which AMR is progressing in the sub-continent.
Moreover, information on phage banks should become available to the local authorities, and the phage banks need to be able to supply phages for fast amplification and treatment within the shortest time possible. This creates another complication within the African context as the transport infrastructure is not well developed or may be complex within the African countries. Based on this, regional banks within Africa based on the livestock intensity or common disease outbreaks may be necessary to be able to support phage therapy in Africa. Using successful systems, for example, large phage collections already existing in Brussels, Belgium, Tbilisi, Republic of Georgia, Novosibirsk, Russia, Braunschweig, Germany, Zurich, Switzerland, Helsinki, Finland, and the Felix d’Hérelle reference phages bank in Quebec City, Canada could help in understanding the design and data storage of a phage bank [163].
Achieving a suitable phage product requires a good understanding of phage–host biology as well as phage product formulations that do not impact the effectiveness of the phage [163]. Such formulations should be well designed to fit into the African context, enabling a long shelf life, an easy to comprehend method of administration, and mechanisms in place for mass delivery in the shortest period of time [164]. So far, there is no single center in Africa serving as a manufacturing hub for bacteriophage. However, as phage research in livestock is gaining popularity in Africa, veterinary regulatory boards existing in the different countries should be alerted to support both academic and research institutes, as well as private companies, in the process of coming up with phage products. Such combined efforts between local authorities and institutions will hasten interim regulations on phage products as well as reduce stringency on phage product design.
A point to consider during the development of phage therapies for livestock that is often overlooked is the regulatory requirements and legislation aspect that can shape the end product’s design at the early stage of development. Identifying the route of administration and the relevant bacterial pathogen to target can also benefit in developing the strategy. Contrary to antibiotics legislation and regulations that have solid systems in place, phage regulation guidelines are not uniform and readily in place as a grey zone surrounds the classification of phages as biological agents, chemical agents (for enzymes derived from phages such as endolysins), veterinary medicine products, or food additive [165,166]. In the USA, phages were classified as drugs in 2011, whereas in Europe, they have been classified as medicinal products [167]. However, Georgia, one of the few countries that have maintained research and development of phage products for use in medicine, considers phages as pharmaceuticals [168]. Even in Poland, which has been a pioneer in phage therapy in Europe, phage therapy is classified as experimental treatment according to Polish law [167].
A problem that scientists and regulators alike are faced with concerning phage therapy is the lack of awareness about phage-based products or clinical data from large studies supporting phage therapy as an alternative to antibiotics. An initial discussion with the Veterinary Medicines Directorate (VMD) of Kenya indicated a great interest from this regulatory body for a phage-based product to tackle AMR in Kenya (Svitek N., personal communication). In Kenya, according to the VMD, a veterinary medicinal product includes pharmaceutical products, vaccines, alternative medicines products as well as biological products, and veterinary feed supplements [169]. Key parameters brought forward by the VMD of Kenya to assess a new product include the stability over a medium- and long-term period of time at different temperatures, efficacy, and safety of the product in the targeted animal population.
One challenge that regulators are likely to encounter is the continuous renewal of phage cocktails with novel phages to counteract the emergence of resistance in bacteria [170]. By doing this, phages need to be tested again to make sure they are lytic, do not contain toxins or AMR genes, and are safe for the animals or humans using by-products of the treated animals [171]. The regulatory framework surrounding phage licensing should be flexible enough to allow slight changes in cocktail formulations for an approved product, unless it is for a hitherto unregistered product. The current regulatory framework used for antibiotics is too long and costly to be used for phages without adapting or adjusting it [172]. Moreover, in veterinary medicine, the compassionate use of phages is not likely to be the strategy of choice, as is the case in human medicine.
In Kenya, a marketing authorization (or “registration/licensing”) is given by the VMD as approval that a veterinary medicines product can be sold and used and includes the specificities of the medicine (ex: the name of the active ingredient), the animal species for which it can be used, the indications for proper use (posology, dosage, and treatment duration) [169]. The product also requires mentioning the conditions of use (for instance, the storage conditions and the shelf life, the withdrawal period before selling the animal’s meat, and the instructions for safe use as well as the instructions for safe disposal of waste) and possible contraindications. Phage-based products would therefore require going through this process at a minimum. Other information that would be needed specifically for phages includes its impact on the environment, which is currently known to be safe, and its potential spread to neighboring farms.
Another challenge with phage products is their lack of patentability potential as is in the USA and Europe, phages cannot be patented [165,173]. However, some phage cocktails have been patented or kept as proprietary by the companies that have developed them [166]. Phage is an active treatment (because it is self-replicating) so different rules apply as the “pharmacology” of phages is different [166]. An additional concern for regulators is the co-evolving property of phages that co-evolve with their host. Furthermore, another level of complexity will be added for regulating genetically modified phages designed to evade immune recognition by the host or reduce the emergence of bacterial-resistant mutants.

6. Conclusions

The control of zoonotic bacteria with antibiotics marks the beginning of the arms race between the discovery of new antibiotics and bacteria. However, winning this fight and mitigating these pathogens requires an intelligent approach of staying ahead of the organisms’ ability to evolve. Using bacteriophages as an alternative contributes to a part of the solution as nature is an almost infinite phage resource. With the constant worry of bacterial evolution towards antibiotics, new phages can be isolated for most kinds of problematic bacteria, as bacteria and their phages constantly co-evolve. Additionally, the use of “cocktails” of multiple phages may reduce the probability of resistant bacteria development. As phage research is being revitalized, there needs to be a practical approach on using phages, creation of phage biobanks, and regulations on phage product development to suit the African context, creating a lasting sustainable solution.

Author Contributions

A.M. and N.S. conceived of the overall topic; A.M., A.L.M., L.G., J.O. and N.S. defined the contents of the manuscript and wrote the text; A.M. and N.S. edited the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

We wish to gratefully acknowledge our funders, the Canadian International Development Research Center (IDRC), in partnership with the UKAID Global AMR Innovation Fund, Department of Health and Social Care (DHSC) [109049], as well as the CGIAR Research Program on Livestock [CRP 3.7], for supporting our work on phages for the replacement of antibiotics in poultry farms in Kenya.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

Not applicable.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Enahoro, D.; Mason-D’Croz, D.; Mul, M.; Rich, K.M.; Robinson, T.P.; Thornton, P.; Staal, S.S. Supporting sustainable expansion of livestock production in South Asia and Sub-Saharan Africa: Scenario analysis of investment options. Glob. Food Secur. 2019, 20, 114–121. [Google Scholar] [CrossRef]
  2. Agriculture Organization of the United Nations; Animal Production, Health Division, Agriculture Organization of the United Nations. Emergency Prevention System for Transboundary Animal, Plant Pests. In Improved Animal Health for Poverty Reduction and Sustainable Livelihoods; Food & Agriculture Organization: Rome, Italy, 2002. [Google Scholar]
  3. Halliday, J.E.; Allan, K.J.; Ekwem, D.; Cleaveland, S.; Kazwala, R.R.; Crump, J.A. Endemic zoonoses in the tropics: A public health problem hiding in plain sight. Vet. Rec. 2015, 176, 220–225. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  4. Andrew Selaledi, L.; Mohammed Hassan, Z.; Manyelo, T.G.; Mabelebele, M. The Current Status of the Alternative Use to Antibiotics in Poultry Production: An African Perspective. Antibiotics 2020, 9, 594. [Google Scholar] [CrossRef]
  5. World Health Organization. Joint FAO/OIE/WHO Expert Workshop on Non-Human Antimicrobial Usage and Antimicrobial Resistance: Scientific Assessment: Geneva, 1–5 December 2003; World Health Organization: Geneva, Switzerland, 2004.
  6. Iskandar, K.; Molinier, L.; Hallit, S.; Sartelli, M.; Hardcastle, T.C.; Haque, M.; Lugova, H.; Dhingra, S.; Sharma, P.; Islam, S. Surveillance of antimicrobial resistance in low-and middle-income countries: A scattered picture. Antimicrob. Resist. Infect. Control 2021, 10, 1–19. [Google Scholar] [CrossRef] [PubMed]
  7. Appiah, B. US Pharmacopeia fighting counterfeit medicines in Africa. Can. Med. Assoc. J. 2013, 185, E666. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  8. Martín, P.V.; Muñoz, M.A.; Pigolotti, S. Bet-hedging strategies in expanding populations. PLoS Comput. Biol. 2019, 15, e1006529. [Google Scholar]
  9. Sultan, I.; Rahman, S.; Jan, A.T.; Siddiqui, M.T.; Mondal, A.H.; Haq, Q.M.R. Antibiotics, resistome and resistance mechanisms: A bacterial perspective. Front. Microbiol. 2018, 9, 2066. [Google Scholar] [CrossRef] [Green Version]
  10. Wangai, F.K.; Masika, M.M.; Lule, G.N.; Karari, E.M.; Maritim, M.C.; Jaoko, W.G.; Museve, B.; Kuria, A. Bridging antimicrobial resistance knowledge gaps: The East African perspective on a global problem. PLoS ONE 2019, 14, e0212131. [Google Scholar] [CrossRef]
  11. World Health Organization. WHO Publishes List of Bacteria for Which New Antibiotics Are Urgently Needed. 2017. Available online: https://www.who.int/ru/news-room/detail/27-02-2017-who-publishes-list-of-bacteria-for-which-new-antibiotics-are-urgently-needed. (accessed on 1 April 2021).
  12. van den Bogaard, A.E.; Stobberingh, E.E. Epidemiology of resistance to antibiotics: Links between animals and humans. Int. J. Antimicrob. Agents 2000, 14, 327–335. [Google Scholar] [CrossRef]
  13. Iovine, N.M. Resistance mechanisms in Campylobacter jejuni. Virulence 2013, 4, 230–240. [Google Scholar] [CrossRef] [Green Version]
  14. Van Boeckel, T.P.; Glennon, E.E.; Chen, D.; Gilbert, M.; Robinson, T.P.; Grenfell, B.T.; Levin, S.A.; Bonhoeffer, S.; Laxminarayan, R. Reducing antimicrobial use in food animals. Science 2017, 357, 1350–1352. [Google Scholar] [CrossRef] [Green Version]
  15. Monistero, V.; Barberio, A.; Biscarini, F.; Cremonesi, P.; Castiglioni, B.; Graber, H.; Bottini, E.; Ceballos-Marquez, A.; Kroemker, V.; Petzer, I. Different distribution of antimicrobial resistance genes and virulence profiles of Staphylococcus aureus strains isolated from clinical mastitis in six countries. J. Dairy Sci. 2020, 103, 3431–3446. [Google Scholar] [CrossRef] [PubMed]
  16. Theobald, S.; Etter, E.M.C.; Gerber, D.; Abolnik, C. Antimicrobial resistance trends in Escherichia coli in South African poultry: 2009–2015. Foodborne Pathog. Dis. 2019, 16, 652–660. [Google Scholar] [CrossRef]
  17. Fri, J.; Njom, H.A.; Ateba, C.N.; Ndip, R.N. Antibiotic resistance and virulence gene characteristics of methicillin-resistant Staphylococcus aureus (MRSA) isolated from healthy Edible Marine Fish. Int. J. Microbiol. 2020, 2020, 9803903. [Google Scholar] [CrossRef] [PubMed]
  18. Pillay, S.; Amoako, D.G.; Abia, A.L.; Somboro, A.M.; Shobo, C.O.; Perrett, K.; Bester, L.A.; Essack, S.Y. Characterisation of Campylobacter spp. isolated from poultry in KwaZulu-Natal, South Africa. Antibiotics 2020, 9, 42. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  19. Langata, L.M.; Maingi, J.M.; Musonye, H.A.; Kiiru, J.; Nyamache, A.K. Antimicrobial resistance genes in Salmonella and Escherichia coli isolates from chicken droppings in Nairobi, Kenya. BMC Res. Notes 2019, 12, 22. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  20. Ahmed, A.O.; Raji, M.A.; Mamman, P.H.; Raufu, I.A.; Aremu, A.; Akorede, G.J.; Kwanashie, C.N. Salmonellosis: Serotypes, prevalence and multi-drug resistant profiles of Salmonella enterica in selected poultry farms, Kwara State, North Central Nigeria. Onderstepoort J. Vet. Res. 2019, 86, 1–8. [Google Scholar] [CrossRef]
  21. Adinortey, C.A.; Aheto, D.W.; Boateng, A.A.; Agbeko, R. Multiple Antibiotic Resistance-Coliform Bacteria in Some Selected Fish Farms of the Central Region of Ghana. Scientifica 2020, 2020, 6641461. [Google Scholar] [CrossRef]
  22. Montso, P.K.; Mlambo, V.; Ateba, C.N. The first isolation and molecular characterization of Shiga Toxin-producing virulent multi-drug resistant atypical enteropathogenic Escherichia coli O177 serogroup from South African Cattle. Front. Cell. Infect. Microbiol. 2019, 9, 333. [Google Scholar] [CrossRef]
  23. Tshitshi, L.; Manganyi, M.C.; Montso, P.K.; Mbewe, M.; Ateba, C.N. Extended Spectrum Beta-Lactamase-Resistant Determinants among Carbapenem-Resistant Enterobacteriaceae from Beef Cattle in the North West Province, South Africa: A Critical Assessment of Their Possible Public Health Implications. Antibiotics 2020, 9, 820. [Google Scholar] [CrossRef]
  24. Hartnack, S.; Odoch, T.; Kratzer, G.; Furrer, R.; Wasteson, Y.; L’Abée-Lund, T.M.; Skjerve, E. Additive Bayesian networks for antimicrobial resistance and potential risk factors in non-typhoidal Salmonella isolates from layer hens in Uganda. BMC Vet. Res. 2019, 15, 212. [Google Scholar] [CrossRef] [PubMed]
  25. Messele, Y.E.; Abdi, R.D.; Tegegne, D.T.; Bora, S.K.; Babura, M.D.; Emeru, B.A.; Werid, G.M. Analysis of milk-derived isolates of E. coli indicating drug resistance in central Ethiopia. Trop. Anim. Health Prod. 2019, 51, 661–667. [Google Scholar] [CrossRef] [PubMed]
  26. Kazibwe, G.; Katami, P.; Alinaitwe, R.; Alafi, S.; Nanteza, A.; Nakavuma, J.L. Bacteriophage activity against and characterisation of avian pathogenic Escherichia coli isolated from colibacillosis cases in Uganda. PLoS ONE 2020, 15, e0239107. [Google Scholar] [CrossRef] [PubMed]
  27. Igbinosa, I.H. Prevalence and detection of antibiotic-resistant determinant in Salmonella isolated from food-producing animals. Trop. Anim. Health Prod. 2015, 47, 37–43. [Google Scholar] [CrossRef]
  28. Ngbede, E.O.; Raji, M.A.; Kwanashie, C.N.; Kwaga, J.K.P. Antimicrobial resistance and virulence profile of enterococci isolated from poultry and cattle sources in Nigeria. Trop. Anim. Health Prod. 2017, 49, 451–458. [Google Scholar] [CrossRef]
  29. Vounba, P.; Rhouma, M.; Arsenault, J.; Alambédji, R.B.; Fravalo, P.; Fairbrother, J.M. Prevalence of colistin resistance and mcr-1/mcr-2 genes in extended-spectrum β-lactamase/AmpC-producing Escherichia coli isolated from chickens in Canada, Senegal and Vietnam. J. Glob. Antimicrob. Resist. 2019, 19, 222–227. [Google Scholar] [CrossRef] [PubMed]
  30. Igbinosa, I.H.; Igbinosa, E.O.; Okoh, A.I. Detection of antibiotic resistance, virulence gene determinants and biofilm formation in Aeromonas species isolated from cattle. Environ. Sci. Pollut. Res. 2015, 22, 17596–17605. [Google Scholar] [CrossRef]
  31. Guetiya Wadoum, R.; Zambou, N.; Anyangwe, F.; Njimou, J.; Coman, M.; Verdenelli, M.; Cecchini, C.; Silvi, S.; Orpianesi, C.; Cresci, A. Abusive use of antibiotics in poultry farming in Cameroon and the public health implications. Br. Poult. Sci. 2016, 57, 483–493. [Google Scholar] [CrossRef]
  32. Iweriebor, B.C.; Obi, L.C.; Okoh, A.I. Macrolide, glycopeptide resistance and virulence genes in Enterococcus species isolates from dairy cattle. J. Med. Microbiol. 2016, 65, 641–648. [Google Scholar] [CrossRef] [Green Version]
  33. Mainda, G.; Bessell, P.R.; Muma, J.B.; McAteer, S.P.; Chase-Topping, M.E.; Gibbons, J.; Stevens, M.P.; Gally, D.L.; Barend, M. Prevalence and patterns of antimicrobial resistance among Escherichia coli isolated from Zambian dairy cattle across different production systems. Sci. Rep. 2015, 5, 12439. [Google Scholar] [CrossRef] [Green Version]
  34. Adegoke, A.A.; Okoh, A.I. Species diversity and antibiotic resistance properties of Staphylococcus of farm animal origin in Nkonkobe Municipality, South Africa. Folia Microbiol. 2014, 59, 133–140. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Chenia, H.Y.; Jacobs, A. Antimicrobial resistance, heavy metal resistance and integron content in bacteria isolated from a South African tilapia aquaculture system. Dis. Aquat. Org. 2017, 126, 199–209. [Google Scholar] [CrossRef]
  36. Raufu, I.A.; Fashae, K.; Ameh, J.A.; Ambali, A.; Ogunsola, F.T.; Coker, A.O.; Hendriksen, R.S. Persistence of fluoroquinolone-resistant Salmonella enterica serovar Kentucky from poultry and poultry sources in Nigeria. J. Infect. Dev. Ctries. 2014, 8, 384–388. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  37. Kemal, J.; Sibhat, B.; Menkir, S.; Beyene, D. Prevalence, assessment, and antimicrobial resistance patterns of Salmonella from raw chicken eggs in Haramaya, Ethiopia. J. Infect. Dev. Ctries. 2016, 10, 1230–1235. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  38. Suleiman, T.; Karimuribo, E.; Mdegela, R. Prevalence of bovine subclinical mastitis and antibiotic susceptibility patterns of major mastitis pathogens isolated in Unguja island of Zanzibar, Tanzania. Trop. Anim. Health Prod. 2018, 50, 259–266. [Google Scholar] [CrossRef] [PubMed]
  39. Katakweba, A.; Møller, K.; Muumba, J.; Muhairwa, A.; Damborg, P.; Rosenkrantz, J.; Minga, U.; Mtambo, M.; Olsen, J. Antimicrobial resistance in faecal samples from buffalo, wildebeest and zebra grazing together with and without cattle in Tanzania. J. Appl. Microbiol. 2015, 118, 966–975. [Google Scholar] [CrossRef]
  40. Rugumisa, B.T.; Call, D.R.; Mwanyika, G.O.; Mrutu, R.I.; Luanda, C.M.; Lyimo, B.M.; Subbiah, M.; Buza, J.J. Prevalence of antibiotic-resistant fecal Escherichia coli isolates from penned broiler and scavenging local chickens in arusha, Tanzania. J. Food Prot. 2016, 79, 1424–1429. [Google Scholar] [CrossRef]
  41. Massot, M.; Couffignal, C.; Clermont, O.; D’Humières, C.; Chatel, J.; Plault, N.; Andremont, A.; Caron, A.; Mentré, F.; Denamur, E. Day-to-day dynamics of commensal Escherichia coli in Zimbabwean cows evidence temporal fluctuations within a host-specific population structure. Appl. Environ. Microbiol. 2017, 83, e00659-17. [Google Scholar] [CrossRef] [Green Version]
  42. Abrahmsén, M.; Persson, Y.; Kanyima, B.M.; Båge, R. Prevalence of subclinical mastitis in dairy farms in urban and peri-urban areas of Kampala, Uganda. Trop. Anim. Health Prod. 2014, 46, 99–105. [Google Scholar] [CrossRef] [Green Version]
  43. Olowe, O.A.; Adewumi, O.; Odewale, G.; Ojurongbe, O.; Adefioye, O.J. Phenotypic and molecular characterisation of extended-spectrum beta-lactamase producing Escherichia coli obtained from animal fecal samples in Ado Ekiti, Nigeria. J. Environ. Public Health 2015, 2015, 497980. [Google Scholar] [CrossRef] [Green Version]
  44. Nworie, A.; Onyema, A.S.; Okekpa, S.I.; Elom, M.O.; Umoh, N.O.; Usanga, V.U.; Ibiam, G.A.; Ukwah, B.N.; Nwadi, L.C.; Ezeruigbo, C. A novel methicillin-resistant Staphylococcus aureus t11469 and a poultry endemic strain t002 (ST5) are present in chicken in Ebonyi State, Nigeria. BioMed Res. Int. 2017, 2017, 2936461. [Google Scholar] [CrossRef] [Green Version]
  45. Saidi, B.; Mafirakureva, P.; Mbanga, J. Antimicrobial resistance of Escherichia coli isolated from chickens with colibacillosis in and around Harare, Zimbabwe. Avian Dis. 2013, 57, 152–154. [Google Scholar] [CrossRef] [PubMed]
  46. Gitau, G.K.; Bundi, R.M.; Mulei, C.M.; Vanleeuwen, J. Mastitogenic bacteria isolated from dairy cows in Kenya and their antimicrobial sensitivity. J. S. Afr. Vet. Assoc. 2014, 85, 1–8. [Google Scholar] [CrossRef]
  47. van den Honert, M.S.; Gouws, P.A.; Hoffman, L.C. Escherichia coli Antibiotic Resistance Patterns from Co-Grazing and Non-Co-Grazing Livestock and Wildlife Species from Two Farms in the Western Cape, South Africa. Antibiotics 2021, 10, 618. [Google Scholar] [CrossRef] [PubMed]
  48. Perreten, V.; Strauss, C.; Collaud, A.; Gerber, D. Colistin resistance gene mcr-1 in avian-pathogenic Escherichia coli in South Africa. Antimicrob. Agents Chemother. 2016, 60, 4414–4415. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  49. Haftu, R.; Taddele, H.; Gugsa, G.; Kalayou, S. Prevalence, bacterial causes, and antimicrobial susceptibility profile of mastitis isolates from cows in large-scale dairy farms of Northern Ethiopia. Trop. Anim. Health Prod. 2012, 44, 1765–1771. [Google Scholar] [CrossRef]
  50. Alders, R.; Pym, R. Village poultry: Still important to millions, eight thousand years after domestication. World’s Poult. Sci. J. 2009, 65, 181–190. [Google Scholar] [CrossRef]
  51. Mapiye, C.; Mwale, M.; Mupangwa, J.; Chimonyo, M.; Foti, R.; Mutenje, M. A research review of village chicken production constraints and opportunities in Zimbabwe. Asian-Australas. J. Anim. Sci. 2008, 21, 1680–1688. [Google Scholar] [CrossRef]
  52. Vaarst, M.; Steenfeldt, S.; Horsted, K. Sustainable development perspectives of poultry production. World’s Poult. Sci. J. 2015, 71, 609–620. [Google Scholar] [CrossRef] [Green Version]
  53. Caly, D.L.; D’Inca, R.; Auclair, E.; Drider, D. Alternatives to antibiotics to prevent necrotic enteritis in broiler chickens: A microbiologist’s perspective. Front. Microbiol. 2015, 6, 1336. [Google Scholar] [CrossRef] [Green Version]
  54. Cardinal, K.M.; Kipper, M.; Andretta, I.; Ribeiro, A.M.L. Withdrawal of antibiotic growth promoters from broiler diets: Performance indexes and economic impact. Poult. Sci. 2019, 98, 6659–6667. [Google Scholar] [CrossRef]
  55. AlSheikh, H.M.A.; Sultan, I.; Kumar, V.; Rather, I.A.; Al-Sheikh, H.; Tasleem Jan, A.; Haq, Q.M.R. Plant-based phytochemicals as possible alternative to antibiotics in combating bacterial drug resistance. Antibiotics 2020, 9, 480. [Google Scholar] [CrossRef]
  56. Aiyegoro, O.; Okoh, A. Use of bioactive plant products in combination with standard antibiotics: Implications in antimicrobial chemotherapy. J. Med. Plants Res. 2009, 3, 1147–1152. [Google Scholar]
  57. Tian, M.; Xu, X.; Liu, F.; Fan, X.; Pan, S. Untargeted metabolomics reveals predominant alterations in primary metabolites of broccoli sprouts in response to pre-harvest selenium treatment. Food Res. Int. 2018, 111, 205–211. [Google Scholar] [CrossRef] [PubMed]
  58. Castelani, L.; Arcaro, J.; Braga, J.; Bosso, A.; Moura, Q.; Esposito, F.; Sauter, I.; Cortez, M.; Lincopan, N. Activity of nisin, lipid bilayer fragments and cationic nisin-lipid nanoparticles against multidrug-resistant Staphylococcus spp. isolated from bovine mastitis. J. Dairy Sci. 2019, 102, 678–683. [Google Scholar] [CrossRef] [Green Version]
  59. Dal Pozzo, M.; Santurio, D.; Rossatto, L.; Vargas, A.; Alves, S.; Loreto, E.; Viegas, J. Activity of essential oils from spices against Staphylococcus spp. isolated from bovine mastitis. Arq. Bras. Med. Vet. Zootec. 2011, 63, 1229–1232. [Google Scholar] [CrossRef] [Green Version]
  60. Budri, P.E.; Silva, N.C.; Bonsaglia, E.C.; Júnior, A.F.; Júnior, J.A.; Doyama, J.T.; Gonçalves, J.L.; Santos, M.; Fitzgerald-Hughes, D.; Rall, V.L. Effect of essential oils of Syzygium aromaticum and Cinnamomum zeylanicum and their major components on biofilm production in Staphylococcus aureus strains isolated from milk of cows with mastitis. J. Dairy Sci. 2015, 98, 5899–5904. [Google Scholar] [CrossRef] [PubMed]
  61. Cerioli, M.F.; Moliva, M.V.; Cariddi, L.N.; Reinoso, E.B. Effect of the essential oil of minthostachys verticillata (Griseb.) epling and limonene on biofilm production in pathogens causing bovine mastitis. Front. Vet. Sci. 2018, 5, 146. [Google Scholar] [CrossRef] [Green Version]
  62. Golkar, Z.; Bagasra, O.; Pace, D.G. Bacteriophage therapy: A potential solution for the antibiotic resistance crisis. J. Infect. Dev. Ctries. 2014, 8, 129–136. [Google Scholar] [CrossRef]
  63. Chibani-Chennoufi, S.; Bruttin, A.; Dillmann, M.-L.; Brüssow, H. Phage-host interaction: An ecological perspective. J. Bacteriol. 2004, 186, 3677–3686. [Google Scholar] [CrossRef] [Green Version]
  64. de Melo, A.G.; Levesque, S.; Moineau, S. Phages as friends and enemies in food processing. Curr. Opin. Biotechnol. 2018, 49, 185–190. [Google Scholar] [CrossRef] [PubMed]
  65. Viertel, T.M.; Ritter, K.; Horz, H.-P. Viruses versus bacteria—Novel approaches to phage therapy as a tool against multidrug-resistant pathogens. J. Antimicrob. Chemother. 2014, 69, 2326–2336. [Google Scholar] [CrossRef]
  66. Clokie, M.R.; Millard, A.D.; Letarov, A.V.; Heaphy, S. Phages in nature. Bacteriophage 2011, 1, 31–45. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  67. Huff, G.; Huff, W.; Rath, N.; Donoghue, A. Critical evaluation of bacteriophage to prevent and treat colibacillosis in poultry. J. Ark. Acad. Sci. 2009, 63, 93–98. [Google Scholar]
  68. Żbikowska, K.; Michalczuk, M.; Dolka, B. The use of bacteriophages in the poultry industry. Animals 2020, 10, 872. [Google Scholar] [CrossRef]
  69. Gopalaiah, H. Bacteriophage as Antimicrobial Agents: A Milestone. J. Indian Acad. Oral Med. Radiol. 2013, 25, 40. [Google Scholar] [CrossRef]
  70. Fortier, L.-C.; Sekulovic, O. Importance of prophages to evolution and virulence of bacterial pathogens. Virulence 2013, 4, 354–365. [Google Scholar] [CrossRef]
  71. Monteiro, R.; Pires, D.P.; Costa, A.R.; Azeredo, J. Phage therapy: Going temperate? Trends Microbiol. 2019, 27, 368–378. [Google Scholar] [CrossRef] [Green Version]
  72. Harper, D.R. Criteria for selecting suitable infectious diseases for phage therapy. Viruses 2018, 10, 177. [Google Scholar] [CrossRef] [Green Version]
  73. Petrovic Fabijan, A.; Khalid, A.; Maddocks, S.; Ho, J.; Gilbey, T.; Sandaradura, I.; Lin, R.C.; Ben Zakour, N.; Venturini, C.; Bowring, B. Phage therapy for severe bacterial infections: A narrative review. Med. J. Aust. 2020, 212, 279–285. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  74. Nagel, T.E.; Chan, B.K.; De Vos, D.; El-Shibiny, A.; Kang’ethe, E.K.; Makumi, A.; Pirnay, J.-P. The developing world urgently needs phages to combat pathogenic bacteria. Front. Microbiol. 2016, 7, 882. [Google Scholar] [CrossRef] [PubMed]
  75. Adebayo, O.; Gabriel-Ajobiewe, R.; Taiwo, M.; Kayode, S. Phage therapy: A potential alternative in the treatment of multi-drug resistant bacterial infections. J. Microbiol. Exp. 2017, 5, 00173. [Google Scholar]
  76. Islam, M.S.; Zhou, Y.; Liang, L.; Nime, I.; Liu, K.; Yan, T.; Wang, X.; Li, J. Application of a Phage Cocktail for Control of Salmonella in Foods and Reducing Biofilms. Viruses 2019, 11, 841. [Google Scholar] [CrossRef] [Green Version]
  77. Abdelsattar, A.S.; Abdelrahman, F.; Dawoud, A.; Connerton, I.F.; El-Shibiny, A. Encapsulation of E. coli phage ZCEC5 in chitosan-alginate beads as a delivery system in phage therapy. AMB Express 2019, 9, 87. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  78. Janež, N.; Kokošin, A.; Zaletel, E.; Vranac, T.; Kovač, J.; Vučković, D.; Smole Možina, S.; Curin Šerbec, V.; Zhang, Q.; Accetto, T.; et al. Identification and characterisation of new Campylobacter group III phages of animal origin. FEMS Microbiol. Lett. 2014, 359, 64–71. [Google Scholar] [CrossRef] [PubMed]
  79. Gutiérrez, D.; Rodríguez-Rubio, L.; Fernández, L.; Martínez, B.; Rodríguez, A.; García, P. Applicability of commercial phage-based products against Listeria monocytogenes for improvement of food safety in Spanish dry-cured ham and food contact surfaces. Food Control 2017, 73, 1474–1482. [Google Scholar] [CrossRef]
  80. Atterbury, R.J.; Van Bergen, M.A.; Ortiz, F.; Lovell, M.A.; Harris, J.A.; De Boer, A.; Wagenaar, J.A.; Allen, V.M.; Barrow, P.A. Bacteriophage therapy to reduce salmonella colonization of broiler chickens. Appl. Environ. Microbiol. 2007, 73, 4543–4549. [Google Scholar] [CrossRef] [Green Version]
  81. Carvalho, C.M.; Gannon, B.W.; Halfhide, D.E.; Santos, S.B.; Hayes, C.M.; Roe, J.M.; Azeredo, J. The in vivo efficacy of two administration routes of a phage cocktail to reduce numbers of Campylobacter coli and Campylobacter jejuni in chickens. BMC Microbiol. 2010, 10, 232. [Google Scholar] [CrossRef] [Green Version]
  82. Clavijo, V.; Baquero, D.; Hernandez, S.; Farfan, J.C.; Arias, J.; Arévalo, A.; Donado-Godoy, P.; Vives-Flores, M. Phage cocktail SalmoFREE® reduces Salmonella on a commercial broiler farm. Poult. Sci. 2019, 98, 5054–5063. [Google Scholar] [CrossRef]
  83. Kawacka, I.; Olejnik-Schmidt, A.; Schmidt, M.; Sip, A. Effectiveness of Phage-Based Inhibition of Listeria monocytogenes in Food Products and Food Processing Environments. Microorganisms 2020, 8, 1764. [Google Scholar] [CrossRef]
  84. Zhang, X.; Niu, Y.D.; Nan, Y.; Stanford, K.; Holley, R.; McAllister, T.; Narváez-Bravo, C. SalmoFresh™ effectiveness in controlling Salmonella on romaine lettuce, mung bean sprouts and seeds. Int. J. Food Microbiol. 2019, 305, 108250. [Google Scholar] [CrossRef] [PubMed]
  85. Vikram, A.; Woolston, J.; Sulakvelidze, A. Phage Biocontrol Applications in Food Production and Processing. Curr. Issues Mol. Biol. 2021, 40, 267–302. [Google Scholar] [CrossRef] [PubMed]
  86. Maciejewska, B.; Olszak, T.; Drulis-Kawa, Z. Applications of bacteriophages versus phage enzymes to combat and cure bacterial infections: An ambitious and also a realistic application? Appl. Microbiol. Biotechnol. 2018, 102, 2563–2581. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  87. Luong, T.; Salabarria, A.-C.; Roach, D.R. Phage therapy in the resistance era: Where do we stand and where are we going? Clin. Ther. 2020, 42, 1659–1680. [Google Scholar] [CrossRef]
  88. Kortright, K.E.; Chan, B.K.; Koff, J.L.; Turner, P.E. Phage therapy: A renewed approach to combat antibiotic-resistant bacteria. Cell Host Microbe 2019, 25, 219–232. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  89. Ma, Y.H.; Islam, G.S.; Wu, Y.; Sabour, P.M.; Chambers, J.R.; Wang, Q.; Wu, S.X.; Griffiths, M.W. Temporal distribution of encapsulated bacteriophages during passage through the chick gastrointestinal tract. Poult. Sci. 2016, 95, 2911–2920. [Google Scholar] [CrossRef]
  90. Malik, D.J.; Sokolov, I.J.; Vinner, G.K.; Mancuso, F.; Cinquerrui, S.; Vladisavljevic, G.T.; Clokie, M.R.J.; Garton, N.J.; Stapley, A.G.F.; Kirpichnikova, A. Formulation, stabilisation and encapsulation of bacteriophage for phage therapy. Adv. Colloid Interface Sci. 2017, 249, 100–133. [Google Scholar] [CrossRef] [Green Version]
  91. Naghizadeh, M.; Karimi Torshizi, M.A.; Rahimi, S.; Engberg, R.M.; Sørensen Dalgaard, T. Effect of serum anti-phage activity on colibacillosis control by repeated phage therapy in broilers. Vet. Microbiol. 2019, 234, 61–71. [Google Scholar] [CrossRef]
  92. Stanford, K.; McAllister, T.A.; Niu, Y.D.; Stephens, T.P.; Mazzocco, A.; Waddell, T.E.; Johnson, R.P. Oral delivery systems for encapsulated bacteriophages targeted at Escherichia coli O157:H7 in feedlot cattle. J. Food Prot. 2010, 73, 1304–1312. [Google Scholar] [CrossRef]
  93. Vaz, C.S.L.; Voss-Rech, D.; Alves, L.; Coldebella, A.; Brentano, L.; Trevisol, I.M. Effect of time of therapy with wild-type lytic bacteriophages on the reduction of Salmonella Enteritidis in broiler chickens. Vet. Microbiol. 2020, 240, 108527. [Google Scholar] [CrossRef]
  94. Imklin, N.; Nasanit, R. Characterization of Salmonella bacteriophages and their potential use in dishwashing materials. J. Appl. Microbiol. 2020, 129, 266–277. [Google Scholar] [CrossRef]
  95. Iannetti, L.; Neri, D.; Santarelli, G.A.; Cotturone, G.; Vulpiani, M.P.; Salini, R.; Antoci, S.; Di Serafino, G.; Di Giannatale, E.; Pomilio, F. Animal welfare and microbiological safety of poultry meat: Impact of different at-farm animal welfare levels on at-slaughterhouse Campylobacter and Salmonella contamination. Food Control 2020, 109, 106921. [Google Scholar] [CrossRef]
  96. Plackett, B. Why big pharma has abandoned antibiotics. Nature 2020, 586, S50–S52. [Google Scholar] [CrossRef]
  97. Parfitt, T. Georgia: An unlikely stronghold for bacteriophage therapy. Lancet 2005, 365, 2166–2167. [Google Scholar] [CrossRef]
  98. Torres-Acosta, M.A.; Clavijo, V.; Vaglio, C.; González-Barrios, A.F.; Vives-Flórez, M.J.; Rito-Palomares, M. Economic evaluation of the development of a phage therapy product for the control of Salmonella in poultry. Biotechnol. Prog. 2019, 35, e2852. [Google Scholar] [CrossRef]
  99. Hughes, D.; Karlén, A. Discovery and preclinical development of new antibiotics. Upsala J. Med. Sci. 2014, 119, 162–169. [Google Scholar] [CrossRef] [Green Version]
  100. Hyman, P. Phages for Phage Therapy: Isolation, Characterization, and Host Range Breadth. Pharmaceuticals 2019, 12, 35. [Google Scholar] [CrossRef] [Green Version]
  101. Cross, T.; Schoff, C.; Chudoff, D.; Graves, L.; Broomell, H.; Terry, K.; Farina, J.; Correa, A.; Shade, D.; Dunbar, D. An optimized enrichment technique for the isolation of Arthrobacter bacteriophage species from soil sample isolates. JoVE (J. Vis. Exp.) 2015, e52781. [Google Scholar] [CrossRef] [Green Version]
  102. Patey, O.; McCallin, S.; Mazure, H.; Liddle, M.; Smithyman, A.; Dublanchet, A. Clinical indications and compassionate use of phage therapy: Personal experience and literature review with a focus on osteoarticular infections. Viruses 2019, 11, 18. [Google Scholar] [CrossRef] [Green Version]
  103. Li, P.; Zhang, X.; Xie, X.; Tu, Z.; Gu, J.; Zhang, A. Characterization and whole-genome sequencing of broad-host-range Salmonella-specific bacteriophages for bio-control. Microb. Pathog. 2020, 143, 104119. [Google Scholar] [CrossRef]
  104. Ross, A.; Ward, S.; Hyman, P. More Is Better: Selecting for Broad Host Range Bacteriophages. Front. Microbiol. 2016, 7, 1352. [Google Scholar] [CrossRef] [Green Version]
  105. de Jonge, P.A.; Nobrega, F.L.; Brouns, S.J.J.; Dutilh, B.E. Molecular and Evolutionary Determinants of Bacteriophage Host Range. Trends Microbiol. 2019, 27, 51–63. [Google Scholar] [CrossRef]
  106. Li, M.; Lin, H.; Jing, Y.; Wang, J. Broad-host-range Salmonella bacteriophage STP4-a and its potential application evaluation in poultry industry. Poult. Sci. 2020, 99, 3643–3654. [Google Scholar] [CrossRef] [PubMed]
  107. Liu, A.; Liu, Y.; Peng, L.; Cai, X.; Shen, L.; Duan, M.; Ning, Y.; Liu, S.; Li, C.; Liu, Y. Characterization of the narrow-spectrum bacteriophage LSE7621 towards Salmonella Enteritidis and its biocontrol potential on lettuce and tofu. LWT 2020, 118, 108791. [Google Scholar] [CrossRef]
  108. Alves, D.; Cerqueira, M.A.; Pastrana, L.M.; Sillankorva, S. Entrapment of a phage cocktail and cinnamaldehyde on sodium alginate emulsion-based films to fight food contamination by Escherichia coli and Salmonella Enteritidis. Food Res. Int. 2020, 128, 108791. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  109. Zaczek-Moczydłowska, M.A.; Young, G.K.; Trudgett, J.; Plahe, C.; Fleming, C.C.; Campbell, K.; Hanlon, R.O. Phage cocktail containing Podoviridae and Myoviridae bacteriophages inhibits the growth of Pectobacterium spp. under in vitro and in vivo conditions. PLoS ONE 2020, 15, e0230842. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  110. Naghizadeh, M.; Karimi Torshizi, M.A.; Rahimi, S.; Dalgaard, T.S. Synergistic effect of phage therapy using a cocktail rather than a single phage in the control of severe colibacillosis in quails. Poult. Sci. 2019, 98, 653–663. [Google Scholar] [CrossRef] [PubMed]
  111. Chadha, P.; Katare, O.P.; Chhibber, S. In vivo efficacy of single phage versus phage cocktail in resolving burn wound infection in BALB/c mice. Microb. Pathog. 2016, 99, 68–77. [Google Scholar] [CrossRef]
  112. Al-Shayeb, B.; Sachdeva, R.; Chen, L.-X.; Ward, F.; Munk, P.; Devoto, A.; Castelle, C.J.; Olm, M.R.; Bouma-Gregson, K.; Amano, Y. Clades of huge phages from across Earth’s ecosystems. Nature 2020, 578, 425–431. [Google Scholar] [CrossRef] [Green Version]
  113. Bumunang, E.W.; McAllister, T.A.; Stanford, K.; Anany, H.; Niu, Y.D.; Ateba, C.N. Characterization of Non-O157 STEC infecting bacteriophages isolated from cattle faeces in North-West South Africa. Microorganisms 2019, 7, 615. [Google Scholar] [CrossRef] [Green Version]
  114. Kering, K.K.; Zhang, X.; Nyaruaba, R.; Yu, J.; Wei, H. Application of adaptive evolution to improve the stability of bacteriophages during storage. Viruses 2020, 12, 423. [Google Scholar] [CrossRef] [Green Version]
  115. Akhwale, J.K.; Rohde, M.; Rohde, C.; Bunk, B.; Spröer, C.; Boga, H.I.; Klenk, H.-P.; Wittmann, J. Isolation, characterization and analysis of bacteriophages from the haloalkaline lake Elmenteita, Kenya. PLoS ONE 2019, 14, e0215734. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  116. Akhwale, J.K.; Rohde, M.; Rohde, C.; Bunk, B.; Spröer, C.; Klenk, H.-P.; Boga, H.I.; Wittmann, J. Comparative genomic analysis of eight novel haloalkaliphilic bacteriophages from Lake Elmenteita, Kenya. PLoS ONE 2019, 14, e0212102. [Google Scholar] [CrossRef] [PubMed]
  117. van Zyl, L.J.; Abrahams, Y.; Stander, E.A.; Kirby-McCollough, B.; Jourdain, R.; Clavaud, C.; Breton, L.; Trindade, M. Novel phages of healthy skin metaviromes from South Africa. Sci. Rep. 2018, 8, 12265. [Google Scholar] [CrossRef] [PubMed]
  118. Yahya, M.; Hmaied, F.; Jebri, S.; Jofre, J.; Hamdi, M. Bacteriophages as indicators of human and animal faecal contamination in raw and treated wastewaters from Tunisia. J. Appl. Microbiol. 2015, 118, 1217–1225. [Google Scholar] [CrossRef] [PubMed]
  119. Maje, M.D.; Kaptchouang Tchatchouang, C.D.; Manganyi, M.C.; Fri, J.; Ateba, C.N. Characterisation of vibrio species from surface and drinking water sources and assessment of biocontrol potentials of their bacteriophages. Int. J. Microbiol. 2020, 2020, 8863370. [Google Scholar] [CrossRef]
  120. Hassim, A.; Lekota, K.E.; Van Dyk, D.S.; Dekker, E.H.; Van Heerden, H. A Unique Isolation of a Lytic Bacteriophage Infected Bacillus anthracis Isolate from Pafuri, South Africa. Microorganisms 2020, 8, 932. [Google Scholar] [CrossRef]
  121. Bumunang, E.W.; Ateba, C.N.; Stanford, K.; Niu, Y.D.; Wang, Y.; McAllister, T.A. Activity of bacteriophage and complex tannins against biofilm-forming shiga toxin-producing Escherichia coli from Canada and South Africa. Antibiotics 2020, 9, 257. [Google Scholar] [CrossRef]
  122. Van Zyl, L.J.; Nemavhulani, S.; Cass, J.; Cowan, D.A.; Trindade, M. Three novel bacteriophages isolated from the East African Rift Valley soda lakes. Virol. J. 2016, 13, 204. [Google Scholar] [CrossRef] [Green Version]
  123. Montso, P.K.; Mlambo, V.; Ateba, C.N. Characterization of lytic bacteriophages infecting multidrug-resistant shiga toxigenic atypical Escherichia coli O177 strains isolated from cattle feces. Front. Public Health 2019, 7, 355. [Google Scholar] [CrossRef]
  124. Damelin, L.H.; Paximadis, M.; Mavri-Damelin, D.; Birkhead, M.; Lewis, D.A.; Tiemessen, C.T. Identification of predominant culturable vaginal Lactobacillus species and associated bacteriophages from women with and without vaginal discharge syndrome in South Africa. J. Med. Microbiol. 2011, 60, 180–183. [Google Scholar] [CrossRef] [Green Version]
  125. Kakabadze, E.; Makalatia, K.; Grdzelishvili, N.; Bakuradze, N.; Goderdzishvili, M.; Kusradze, I.; Phoba, M.-F.; Lunguya, O.; Lood, C.; Lavigne, R. Selection of potential therapeutic bacteriophages that lyse a CTX-M-15 extended spectrum β-lactamase producing Salmonella enterica serovar typhi strain from the democratic republic of the Congo. Viruses 2018, 10, 172. [Google Scholar] [CrossRef] [Green Version]
  126. Akindolire, M.A.; Aremu, B.R.; Ateba, C.N. Complete genome sequence of Escherichia coli O157: H7 phage PhiG17. Microbiol. Resour. Announc. 2019, 8, e01296-18. [Google Scholar] [CrossRef] [Green Version]
  127. Essoh, C.; Vernadet, J.-P.; Vergnaud, G.; Coulibaly, A.; Kakou-N’Douba, A.; Assavo, S.-P.G.; Ouassa, T.; Pourcel, C. Characterization of sixteen Achromobacter xylosoxidans phages from Abidjan, Côte d’Ivoire, isolated on a single clinical strain. Arch. Virol. 2020, 165, 725–730. [Google Scholar] [CrossRef]
  128. Mahmoud, M.; Askora, A.; Barakat, A.B.; Rabie, O.E.-F.; Hassan, S.E. Isolation and characterization of polyvalent bacteriophages infecting multi drug resistant Salmonella serovars isolated from broilers in Egypt. Int. J. Food Microbiol. 2018, 266, 8–13. [Google Scholar] [CrossRef]
  129. Brown, B.P.; Chopera, D.; Havyarimana, E.; Wendoh, J.; Jaumdally, S.; Nyangahu, D.D.; Gray, C.M.; Martin, D.P.; Varsani, A.; Jaspan, H.B. crAssphage genomes identified in fecal samples of an adult and infants with evidence of positive genomic selective pressure within tail protein genes. Virus Res. 2021, 292, 198219. [Google Scholar] [CrossRef]
  130. Maina, A.N.; Mwaura, F.B.; Oyugi, J.; Goulding, D.; Toribio, A.L.; Kariuki, S. Characterization of Vibrio cholerae bacteriophages isolated from the environmental waters of the Lake Victoria region of Kenya. Curr. Microbiol. 2014, 68, 64–70. [Google Scholar] [CrossRef] [Green Version]
  131. Montso, P.K.; Mlambo, V.; Ateba, C.N. Efficacy of novel phages for control of multi-drug resistant Escherichia coli O177 on artificially contaminated beef and their potential to disrupt biofilm formation. Food Microbiol. 2021, 94, 103647. [Google Scholar] [CrossRef] [PubMed]
  132. Essoh, C.; Latino, L.; Midoux, C.; Blouin, Y.; Loukou, G.; Nguetta, S.-P.A.; Lathro, S.; Cablanmian, A.; Kouassi, A.K.; Vergnaud, G. Investigation of a large collection of Pseudomonas aeruginosa bacteriophages collected from a single environmental source in Abidjan, Côte d’Ivoire. PLoS ONE 2015, 10, e0130548. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  133. Marie, V.; Lin, J. Viruses in the environment–presence and diversity of bacteriophage and enteric virus populations in the Umhlangane River, Durban, South Africa. J. Water Health 2017, 15, 966–981. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  134. Ndongmo Teytsa, H.; Tsanou, B.; Bowong, S.; Lubuma, J.M. Bifurcation analysis of a phage-bacteria interaction model with prophage induction. Math. Med. Biol. J. IMA 2021, 38, 28–58. [Google Scholar] [CrossRef] [PubMed]
  135. Bettarel, Y.; Combe, M.; Adingra, A.; Ndiaye, A.; Bouvier, T.; Panfili, J.; Durand, J.-D. Hordes of Phages in the Gut of the Tilapia Sarotherodon melanotheron. Sci. Rep. 2018, 8, 11311. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  136. Mtimka, S.; Pillay, P.; Rashamuse, K.; Gildenhuys, S.; Tsekoa, T.L. Functional screening of a soil metagenome for DNA endonucleases by acquired resistance to bacteriophage infection. Mol. Biol. Rep. 2020, 47, 353–361. [Google Scholar] [CrossRef] [PubMed]
  137. Ezemokwe, C.G.; Agwom, F.M.; Okoliegbe, I.; Okonkwo, F.O.; Ngene, A.C.; Gimba, N.; Morenikeji, O.R.; Egwuenu, A.; Okonkwo, C.H.; Aguiyi, J.C. Complete Genome Sequence of Pseudomonas Phage Zikora. Microbiol. Resour. Announc. 2021, 10, e00489-21. [Google Scholar] [CrossRef]
  138. Cinek, O.; Mazankova, K.; Kramna, L.; Odeh, R.; Alassaf, A.; Ibekwe, M.U.; Ahmadov, G.; Mekki, H.; Abdullah, M.A.; Elmahi, B.M. Quantitative CrAssphage real--time PCR assay derived from data of multiple geographically distant populations. J. Med. Virol. 2018, 90, 767–771. [Google Scholar] [CrossRef]
  139. Rodwell, E.V.; Wenner, N.; Pulford, C.V.; Cai, Y.; Bowers-Barnard, A.; Beckett, A.; Rigby, J.; Picton, D.M.; Blower, T.R.; Feasey, N.A. Isolation and characterisation of bacteriophages with activity against invasive non-typhoidal Salmonella causing bloodstream infection in Malawi. Viruses 2021, 13, 478. [Google Scholar] [CrossRef]
  140. El Didamony, G.; Askora, A.; Shehata, A.A. Isolation and characterization of T7-like lytic bacteriophages infecting multidrug resistant Pseudomonas aeruginosa isolated from Egypt. Curr. Microbiol. 2015, 70, 786–791. [Google Scholar] [CrossRef]
  141. El--Shibiny, A.; El--Sahhar, S.; Adel, M. Phage applications for improving food safety and infection control in Egypt. J. Appl. Microbiol. 2017, 123, 556–567. [Google Scholar] [CrossRef] [PubMed]
  142. Ahmad, A.A.; Elhalag, K.M.; Addy, H.S.; Nasr-Eldin, M.A.; Hussien, A.S.; Huang, Q. Sequencing, genome analysis and host range of a novel Ralstonia phage, RsoP1EGY, isolated in Egypt. Arch. Virol. 2018, 163, 2271–2274. [Google Scholar] [CrossRef]
  143. Adriaenssens, E.M.; Van Zyl, L.; De Maayer, P.; Rubagotti, E.; Rybicki, E.; Tuffin, M.; Cowan, D.A. Metagenomic analysis of the viral community in N amib D esert hypoliths. Environ. Microbiol. 2015, 17, 480–495. [Google Scholar] [CrossRef] [Green Version]
  144. Ganz, H.H.; Law, C.; Schmuki, M.; Eichenseher, F.; Calendar, R.; Loessner, M.J.; Getz, W.M.; Korlach, J.; Beyer, W.; Klumpp, J. Novel giant siphovirus from Bacillus anthracis features unusual genome characteristics. PLoS ONE 2014, 9, e85972. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  145. Elhalag, K.; Nasr--Eldin, M.; Hussien, A.; Ahmad, A. Potential use of soilborne lytic Podoviridae phage as a biocontrol agent against Ralstonia solanacearum. J. Basic Microbiol. 2018, 58, 658–669. [Google Scholar] [CrossRef] [PubMed]
  146. Zablocki, O.; Van Zyl, L.J.; Kirby, B.; Trindade, M. Diversity of dsDNA viruses in a South African hot spring assessed by metagenomics and microscopy. Viruses 2017, 9, 348. [Google Scholar] [CrossRef] [Green Version]
  147. Sharaf, A.; Mercati, F.; Elmaghraby, I.; Elbaz, R.; Marei, E. Functional and comparative genome analysis of novel virulent actinophages belonging to Streptomyces flavovirens. BMC Microbiol. 2017, 17, 51. [Google Scholar] [CrossRef] [Green Version]
  148. Ochieng’Oduor, J.M.; Onkoba, N.; Maloba, F.; Arodi, W.O.; Nyachieo, A. Efficacy of lytic Staphylococcus aureus bacteriophage against multidrug-resistant Staphylococcus aureus in mice. J. Infect. Dev. Ctries. 2016, 10, 1208–1213. [Google Scholar]
  149. D’arc, M.; Furtado, C.; Siqueira, J.D.; Seuánez, H.N.; Ayouba, A.; Peeters, M.; Soares, M.A. Assessment of the gorilla gut virome in association with natural simian immunodeficiency virus infection. Retrovirology 2018, 15, 19. [Google Scholar] [CrossRef]
  150. Pope, W.H.; Jacobs-Sera, D.; Russell, D.A.; Rubin, D.H.; Kajee, A.; Msibi, Z.N.; Larsen, M.H.; Jacobs, W.R., Jr.; Lawrence, J.G.; Hendrix, R.W. Genomics and proteomics of mycobacteriophage patience, an accidental tourist in the Mycobacterium neighborhood. mBio 2014, 5, e02145-14. [Google Scholar] [CrossRef] [Green Version]
  151. Zablocki, O.; van Zyl, L.; Adriaenssens, E.M.; Rubagotti, E.; Tuffin, M.; Cary, S.C.; Cowan, D. High-level diversity of tailed phages, eukaryote-associated viruses, and virophage-like elements in the metaviromes of antarctic soils. Appl. Environ. Microbiol. 2014, 80, 6888–6897. [Google Scholar] [CrossRef] [Green Version]
  152. Safwat Mohamed, D.; Farouk Ahmed, E.; Mohamed Mahmoud, A.; Abd El-Baky, R.M.; John, J. Isolation and evaluation of cocktail phages for the control of multidrug-resistant Escherichia coli serotype O104: H4 and E. coli O157: H7 isolates causing diarrhea. FEMS Microbiol. Lett. 2018, 365, fnx275. [Google Scholar] [CrossRef]
  153. Montso, P.K.; Mnisi, C.M.; Ateba, C.N.; Mlambo, V. An Assessment of the Viability of Lytic Phages and Their Potency against Multidrug Resistant Escherichia coli O177 Strains under Simulated Rumen Fermentation Conditions. Antibiotics 2021, 10, 265. [Google Scholar] [CrossRef]
  154. Jebri, S.; Jofre, J.; Barkallah, I.; Saidi, M.; Hmaied, F. Presence and fate of coliphages and enteric viruses in three wastewater treatment plants effluents and activated sludge from Tunisia. Environ. Sci. Pollut. Res. 2012, 19, 2195–2201. [Google Scholar] [CrossRef] [PubMed]
  155. Fancello, L.; Trape, S.; Robert, C.; Boyer, M.; Popgeorgiev, N.; Raoult, D.; Desnues, C. Viruses in the desert: A metagenomic survey of viral communities in four perennial ponds of the Mauritanian Sahara. ISME J. 2013, 7, 359–369. [Google Scholar] [CrossRef]
  156. Eckstein, S.; Stender, J.; Mzoughi, S.; Vogele, K.; Kühn, J.; Friese, D.; Bugert, C.; Handrick, S.; Ferjani, M.; Wölfel, R. Isolation and characterization of lytic phage TUN1 specific for Klebsiella pneumoniae K64 clinical isolates from Tunisia. BMC Microbiol. 2021, 21, 186. [Google Scholar] [CrossRef] [PubMed]
  157. Peduzzi, P.; Gruber, M.; Gruber, M.; Schagerl, M. The virus’s tooth: Cyanophages affect an African flamingo population in a bottom-up cascade. ISME J. 2014, 8, 1346–1351. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  158. Carrigy, N.; Liang, L.; Wang, H.; Kariuki, S.; Nagel, T.; Connerton, I.; Vehring, R. Mechanistic modeling expedites the development of spray dried biologics. In Proceedings of the IDS 2018, 21st International Drying Symposium Proceedings, Editorial Universitat Politècnica de València, Valencia, Spain, 11–14 September 2018. [Google Scholar]
  159. Carrigy, N.B.; Liang, L.; Wang, H.; Kariuki, S.; Nagel, T.E.; Connerton, I.F.; Vehring, R. Spray-dried anti-Campylobacter bacteriophage CP30A powder suitable for global distribution without cold chain infrastructure. Int. J. Pharm. 2019, 569, 118601. [Google Scholar] [CrossRef]
  160. Carrigy, N.B.; Liang, L.; Wang, H.; Kariuki, S.; Nagel, T.E.; Connerton, I.F.; Vehring, R. Trileucine and pullulan improve anti-campylobacter bacteriophage stability in engineered spray-dried microparticles. Ann. Biomed. Eng. 2019, 48, 1169–1180. [Google Scholar] [CrossRef]
  161. Liang, L.; Carrigy, N.B.; Kariuki, S.; Muturi, P.; Onsare, R.; Nagel, T.; Vehring, R.; Connerton, P.L.; Connerton, I.F. Development of a lyophilization process for campylobacter bacteriophage storage and transport. Microorganisms 2020, 8, 282. [Google Scholar] [CrossRef] [Green Version]
  162. Moelling, K.; Broecker, F.; Willy, C. A wake-up call: We need phage therapy now. Viruses 2018, 10, 688. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  163. Kassa, T. Bacteriophages Against Pathogenic Bacteria and Possibilities for Future Application in Africa. Infect. Drug Resist. 2021, 14, 17. [Google Scholar] [CrossRef]
  164. García, R.; Latz, S.; Romero, J.; Higuera, G.; García, K.; Bastías, R. Bacteriophage production models: An overview. Front. Microbiol. 2019, 10, 1187. [Google Scholar] [CrossRef]
  165. Cooper, C.J.; Khan Mirzaei, M.; Nilsson, A.S. Adapting Drug Approval Pathways for Bacteriophage-Based Therapeutics. Front. Microbiol. 2016, 7, 1209. [Google Scholar] [CrossRef]
  166. Fauconnier, A. Phage Therapy Regulation: From Night to Dawn. Viruses 2019, 11, 352. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  167. Naureen, Z.; Malacarne, D.; Anpilogov, K.; Dautaj, A.; Camilleri, G.; Cecchin, S.; Bressan, S.; Casadei, A.; Albion, E.; Sorrentino, E.; et al. Comparison between American and European legislation in the therapeutical and alimentary bacteriophage usage. Acta Bio-Med. Atenei Parm. 2020, 91, e2020023. [Google Scholar] [CrossRef]
  168. Kwiatek, M.; Parasion, S.; Nakonieczna, A. Therapeutic bacteriophages as a rescue treatment for drug--resistant infections—An in vivo studies overview. J. Appl. Microbiol. 2020, 128, 985–1002. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  169. Kenya, Veterinary Medicines Directorate. In Guidelines on Submission of Documentations for Marketing Authorization for Veterinary Medicines; Draft, Doc No. VMD/GUID/O1; Veterinary Medicines Directorate: Nairobi, Kenya; 108p.
  170. Huys, I.; Pirnay, J.P.; Lavigne, R.; Jennes, S.; De Vos, D.; Casteels, M.; Verbeken, G. Paving a regulatory pathway for phage therapy. Europe should muster the resources to financially, technically and legally support the introduction of phage therapy. EMBO Rep. 2013, 14, 951–954. [Google Scholar] [CrossRef] [Green Version]
  171. Loponte, R.; Pagnini, U.; Iovane, G.; Pisanelli, G. Phage Therapy in Veterinary Medicine. Antibiotics 2021, 10, 421. [Google Scholar] [CrossRef]
  172. Verbeken, G.; Huys, I.; De Vos, D.; De Coninck, A.; Roseeuw, D.; Kets, E.; Vanderkelen, A.; Draye, J.P.; Rose, T.; Jennes, S.; et al. Access to bacteriophage therapy: Discouraging experiences from the human cell and tissue legal framework. FEMS Microbiol. Lett. 2016, 363, fnv241. [Google Scholar] [CrossRef] [Green Version]
  173. Verbeken, G.; Pirnay, J.P.; Lavigne, R.; Jennes, S.; De Vos, D.; Casteels, M.; Huys, I. Call for a dedicated European legal framework for bacteriophage therapy. Arch. Immunol. Ther. Exp. 2014, 62, 117–129. [Google Scholar] [CrossRef] [Green Version]
Antibiotics 10 01085 g001 550
Figure 1. A map representing antibiotic resistance in different livestock species from the different countries, according to research studies carried out in the last decade.
Figure 1. A map representing antibiotic resistance in different livestock species from the different countries, according to research studies carried out in the last decade.
Antibiotics 10 01085 g001
Table
Table 1. Description of antibiotic resistance in different types of bacteria isolated from livestock in SSA.
Table 1. Description of antibiotic resistance in different types of bacteria isolated from livestock in SSA.
CountryAnimal Sample Organism Antibiotic Resistance Data Reference
South Africa Cattle Milk S. aureusSPN, ERY[15]
South Africa PoultryFecal SamplesE. coliCST, FLO, TRS, SPE, FOS, AMX[16]
South Africa Fish Bacterial isolatesS. aureusRIF(82%), CLI(82%), ERY(67%), AMP(67%), TET(27%), VAN (30%)[17]
South Africa Poultry Fecal SamplesC. jejuniERY (79%), CLI (75%), AMP(54%), NAL(48%), CTR(48%), CIP(33%), GEN (15%), TET(16%)[18]
South Africa Poultry Fecal SamplesC. coliERY (60%), CLI (56%),AMP (36%), NAL(26%), CTR(28%), CIP(15%), GEN (8%), TET(7%)[18]
KenyaPoultryFecal SamplesSalmonellaSTR (6%), AMP (50%), TRS (28%), TET (11%)[19]
Kenya Poultry Fecal SamplesE. coliSTR (9%), CHL (2%), NAL(2%), AMO (54%), TRS (26%), TET (12%)[19]
Nigeria Poultry Feces, feed, waterS. EntericaAMP(100%), CHL(100%), CTV(100%), CIP(100%), GEN (100%), CTA(100%), NEO(100%), NAL(100%), CPDS (100%),STR (100%), TET (100%)[20]
Ghana Fish Water and cultured fish speciesColiform BacteriaAMP(98.4%),CUR(88.9%), TET(66.7%), CTA(52.4%), TRS (56.0%), GEN (6.4%)[21]
South Africa Cattle Fecal SamplesE. coliERY(63.84%),AMP(21.54%), TET(13.37%), STR(17.01%), KAN (2.42%), CHL(1.97%),NOR (1.40%)[22]
South Africa Cattle Fecal Samples EnterobacteriaceaeCAA: IMI (42%), ERT (35%), DOR (30%), MER (28%)[23]
UgandaPoultry fecal samplesSalmonellaCIP(46.5%), SULFA(24.4%), TET(15.1%), TRI(7.0%), TRS(7.0%), CHL(4.6%), AMP(4.6%) [24]
Ethiopia Cattle Milk E. coliAMP (68.7%), TRS (50%), STR (25%)[25]
Uganda Poultrypost-mortem samples E. coliPEN G(100%), TRS(87.5%), TET(83.9%), AMP(80.4%), AMX(69.6%), STR(67.9%), NAL(60.7%), CHL (35.7%),GEN (10.7%)[26]
South Africa Cattle Fecal Samples SalmonellaPEN(79%), CTA(28%), NAL(7%), CLT(24%),GEN (1%), CHL(20%), TET(62%), ERY (42%), MIN (46%), VAN (100%), OXA(100%), OFL(9%), AMP(82%), TRS(62%), STR(40%)[27]
South Africa GoatsFecal samples SalmonellaPEN(88%), CTA(54%), NAL(6%), CLT(37%), GEN (24%), CHL(29%), TET(32%), ERY(57%), MIN (15%), VAN(100%), OXA(100%), AMP(25%), TRS (71%), STR (29%)[27]
Nigeria Cattle, Poultry Rectal and cloacol SwabsEnterococcus TET (61.0%), ERY (61.0%), QUD (4.4%), CHL (8.0%)[28]
Senegal PoultryFecal samples E. coliCST(2.2%)[29]
South Africa Cattle Fecal samples Aeromonas AMX (100%, 92%), CHL (7%; 2%), PEN (100%; 95%), PLB (50%; 32%)[30]
Cameroon Poultry muscle, liver, heart, kidney and gizzardsVarious bacteria TET (63%), KAN(45%), AMC(63%), AMP(54%), TRS (36%), ERY(81%),CTF (45%),CHL (36%), ENR (45%), GEN (54%) VAN (63%)[31]
South Africa CattleFecal SamplesEnterococcusVAN (100%), CLO (100%), AMI(74%), CLT (88%), STR (94%), PEN G (91%), CLI (97%), NEO (91%), ERY (99%), IMI (0.6%), AMC (8%), CIP (12%)[32]
ZambiaCattle Fecal SamplesE. coliCPO, CIP, AMP, TRS, TET, GEN[33]
South Africa Pigs/piglets, Cattle, Goats, Poultrynasal, mouth wash, and ear swabsStaphylococcusPEN G (75%),MER (2.3%),VAN (12%),CTA (13%),CTV (40%), OXA(38%), MIN (16%),TET (83%),ERY (12%),CLI (16%),NAL (100%),CIP (3%),OFL (5%),LEV (2%)[34]
South Africa Fish Water Gram-negative bacteriaERY (100%), AMP (85%), TRI (78%)[35]
Nigeria Poultry Fecal SamplesSalmonellaAMP, AMC, CIP, GEN, NAL, NEO; SPE, STR, SME, TET, TRI[36]
Ethiopia Poultry Eggs SalmonellaCLI (100%), ERY (63%), AMP (38%), AMX (38%), TET (25%) [37]
TanzaniaCattle Milk Staphylococcus aureus and other bacteriaAMX, CPX, GEN, KAN, NEO, TET[38]
Tanzania Cattle Fecal Samples E. coliAMP (40%), TET (20%), CTA (10%),TRS (15%) [39]
TanzaniaPoultryfecal SamplesE. coliAMP, AMX, CHL, CIP, STR, SME, TET, TRI[40]
ZimbabweCattleFecal samplesE. coli TET, PEN, TRS[41]
UgandaCattle Milk Streptococci spp. and Staphylococci spp.TET (100%)[42]
Nigeria Cattle and Pigs Fecal samplesE. coliPEN (96%),AMX (88%), AMP (89%), AUG (96%), CTV (58%),CTA (92%), CIX (39%), CUR (83%), CPO(58%), TET (88%), ERY (82%), STR (79%), GEN (49%), CIP(5%), OFL (5%), CLO (84%), TRS (90%), CHL (92%)[43]
Nigeria PoultryCloacae and nasal samplesStaphylococcus aureusAUG(0.8%), CXI (6.1%), CUR (5.3%), CHL (12.1%),DOX (7.7%), ERY (19.4%), GEN (5.3%), LEV (0.8%), TET (45.7%),TRS (40.9%)[44]
ZimbabwePoultryFecal samplesE. coli TET (100%), BCN (100%), CLO (100%) AMP (94.1%)[45]
KenyaCattleMilk Staphylococcus aureus and Streptococcus agalactiae and other bacteriaTRS (76%), AMP (57%)[46]
South AfricaCattle Fecal samplesE. coliAMP, SFZ, TET, STR[47]
South Africa Poultry Isolates E. coliCST (13.5%)[48]
Ethiopia Cattle Milk Staphylococcus species and coliformsAMP, ERY, NAL, CLI, TRS, CHL[49]
South AfricaCattle Milk BacteriaPEN (47.8), OXA (1.1%), CLT (1.1%), STR (16.7%), NEO (5.6%), TET (11.1%), TRS (1.1%), ENR (1.1%), TLS (2.2%)[49]
The antibiotic codes are as follows: CST: Colistin, TET: Tetracycline, AMX: Amoxicillin, PEN: Penicillin, AMP: Ampicillin, ERY: Erythromycin, RIF: Rifampicin, CLI: Clindamycin, AMC: Amoxicillin/Clavulanate, CIP: Ciprofloxacin, VAN: Vancomycin, AMO: Amoxicillin, NAL: Nalidixic acid, CTR: Ceftriaxone, GEN: Gentamycin, STR: Streptomycin, TRS: Trimethoprin/sulphamethoxazole, TRI: Trimethoprin, SME: Sulphamethoxazole, CHL: Chloramphenicol, CTA: Cefotaxime, KAN: Kanamycin, IMI: Imipenem, LEV: Levofloxacin, SPE: Spectinomycin, OXA: Oxacillin, AUG: Augementin, ERT: Ertapenem, MER: Meropenem, DOR: Doripenem, CAA: Carbapenem antimicrobial agents, CPDS: Compound Sulphonamindes, CUR: Cefuroxime, MIN: Minocycline, CLT: Cephalothin, ENR: Enrofloxacin, CTV: Ceftazidime, CLO: Cloxacillin, AMI: Amikacin, CIX: Cefixime, CPO: Cefpodoxime, OFL: Oflocacin, NOR: Norfloxacin, CPX: Cephalexin, NEO: Neomycin, CXI: Cefoxitin, DOX: Doxycline, FLO: Flofenicol, FOS: Fosomycin, SPN: Spiramycin, QUD: Quinupristin-dalfopristin, SFZ: Sulphufurazole, BCN: Bacitracin, PMB: PolymycinB, CTF: Ceftiofur, TLS: Tylosin, SULFA: Sulfanomide. Percentages (%) of isolates resistant to antibiotics were included where data was available. Where two different percentages are included, two different groups of isolates belonging to the same species were tested for antibiotic resistance.
Table
Table 2. Representation of phage research in Africa over a decade (2011–2021).
Table 2. Representation of phage research in Africa over a decade (2011–2021).
CountrySource of SampleHostPhagePurpose of Research Ref.
Tanzania Hadza fecal samplesFirmicutes*N. ISequenced DNA from diverse
ecosystems for phage genomes		[112]
KenyaBaboon fecal samplesActinobacteria,
Proteobacteria,
Firmicutes		*N. ISequenced DNA from diverse
ecosystems for phage genomes		[112]
South AfricaThiocyanate bioreactorProteobacteria*N. ISequenced DNA from diverse
ecosystems for phage genomes		[112]
South AfricaCattle fecesNon-O157 Shiga toxin-producing Escherichia coli (STEC)Myoviridae,
Siphoviridae		Isolation and
characterization		[113]
KenyaEnvironmental water samplesRalstonia
solanacearum strain GIM1.74.		PodoviridaeEvolution experiments
for phage
stability/storage		[114]
Kenya Lake Elmentaita sediment samplesVibrio metschnikovii, Bacillus pseudofirmus, Bacillus bogoriensis, Bacillus horikoshii, Bacillus cohnii, bacillus psedolcaliphilus, Bacillus halmapalus, Exiguobacterium
aurantiacum, Exiguobacterium
alkaliphilum		Myoviridae,
Siphoviridae,
Podoviridae		Isolation,
characterization, comparative
genomics		[115,116]
South AfricaSkinStaphylococcus capitis, PseudomonasMyoviridae,
Siphoviridae,
Podoviridae		Metaviriome
analysis		[117]
TunisiaRaw and treated wastewaters of human and animal originEscherichia coli, Salmonella Typhimurium, Bact. fragilis, Bact. thetaiotaomicronSomatic coliphages (SOMCPH), F-specific RNA bacteriophages (F-RNA), Bact. fragilis phages (RYC2056) and Bact.
thetaiotaomicron phages		Monitor the
microbial quality of water		[118]
South AfricaWater samples collected from taps, boreholes, and damsV. harveyi, V. parahaemolyticus, V. cholerae, V. mimicus, V. vulnificusMyoviridaeIsolation and characterization[119]
South AfricaCarcass remnantsBacillus anthracisMyoviridaeIsolation and characterization[120]
South AfricaCattle fecesShiga toxin-producing Escherichia coli (STEC)*N. IIsolation and characterization[121]
KenyaLake Magadi soil sedimentsBacillus- and Paracoccus speciesMyoviridaeIsolation and characterization[122]
EthiopiaLake Chala soil sedimentsBacillus- and Paracoccus speciesMyoviridae,
Siphoviridae		Isolation and characterization[122]
South AfricaCattle fecesEscherichia coli O177MyoviridaeIsolation and characterization[123]
South AfricaVaginal swabsLactobacillus jensenii, Lactobacillus crispatus, Lactobacillus iners, Lactobacillus gasseri and Lactobacillus vaginalisMyoviridae,
Siphoviridae,
Podoviridae		Isolation and characterization[124]
Democratic Republic of Congo*N. ISalmonella TyphiMyoviridae,
Siphoviridae,
Podoviridae		Testing of 14 Salmonella phages from the Eliava collection and commercial phage cocktail “INTESTI phage”[125]
South AfricaCattle fecesEscherichia coli O157:H7PodoviridaeGenome sequence[126]
Côte d’IvoireSewage waterAchromobacter xylosoxidansSiphoviridae,
Podoviridae		Isolation and characterization[127]
EgyptChicken fecesSalmonella Serovars, Citrobacter freundii, Enterobacter cloacae, Escherichia coli.Siphoviridae,
Myoviridae		Isolation and characterization[128]
South AfricaHuman stool samples*N. IcrAssphageSequencing[129]
KenyaLake Victoria water samples Vibrio choleraeMyoviridaeIsolation and characterization[130]
UgandaChicken postmortem samplesAvian Pathogenic Escherichia coli*N. IIsolation and characterization[26]
South AfricaCattle fecesEscherichia coli O177 MyoviridaeEfficacy of beef decontamination and biofilm disruption[131]
Côte d’IvoireSewage samplesPseudomonas aeruginosaMyoviridae,
Siphoviridae,
Podoviridae		Characterization and sequencing[132]
South AfricaUmhlangane River water sample*N. IMyoviridae,
Siphoviridae,
Podoviridae		Diversity of bacteriophage population[133]
South Africa*N. I*N. I*N. IA predator–prey model to analyze phage–bacteria interactions [134]
SenegalGut and water samples of Tilapia
Sarotherodon
melanotheron		*N. IMyoviridae,
Siphoviridae,
Podoviridae		Viriome analysis[135]
South AfricaSoil samples*N. IEscherichia coli bacteriophage Lambda W60Isolating new endonucleases using functional metagenomic techniques[136]
South AfricaSoil samples*N. ISiphoviridaeMetaviromic techniques for viral diversity[136]
NigeriaSewage waterPseudomonas aeruginosaMyoviridaeGenome sequencing[137]
NigeriaHuman stool samples*N. IcrAssphageQuantitative CrAssphage analysis from multiple geographically distant populations[138]
SudanHuman stool samples*N. IcrAssphageQuantitative CrAssphage analysis from multiple geographically distant populations[138]
MalawiWater samplesS. Typhimurium,
S. Enteritidis		Ackermannviridae,
Siphoviridae		Isolation and characterization[139]
EgyptSewage samples Pseudomonas aeruginosaSiphoviridaeIsolation and characterization[140]
EgyptSewage samplesSalmonella enterica, Escherichia coliSiphoviridae,
Myoviridae		Applications in food safety[141]
EgyptSoil samplesRalstonia solanacearumPodoviridaeSequencing[142]
South AfricaSoil samples*N. IMyoviridae,
Siphoviridae,
Podoviridae		Metagenomic analysis of the viral community[143]
NamibiaWildlife carcassBacillus anthracisSiphoviridaeDissecting novel giant Siphovirus[144]
EgyptSoil samplesRalstonia solanacearumPodoviridaeBiocontrol[145]
South AfricaWater samples from hot springs*N. IMyoviridae,
Siphoviridae,
Podoviridae,
Fuselloviridae		Metavirome analysis[146]
EgyptSoil samplesStreptomyces flavovirensSiphoviridaeSequencing[147]
Kenya Sewage and wastewaterStaphylococcus aureusN. IEfficacy of lysis[148]
CameroonGorilla fecal samples*N. IMyoviridae,
Siphoviridae		Microbiome analysis[149]
South AfricaEnvironmental samples Mycobacterium smegmatisSiphoviridaeGenomics and proteomics of mycobacteriophage[150]
South AfricaSoil samples*N. IMyoviridae,
Siphoviridae,
Podoviridae,
Mimiviridae,
Phycodnaviridae		Metaviromes of Antarctic soils[151]
EgyptWater samples from sewage systemsEscherichia coli O104: H4 Escherichia coli O157: H7Siphoviridae,
Podoviridae		Isolation and characterization[152]
South AfricaRumen fluidEscherichia coli O177MyoviridaeViability of lytic phages under simulated rumen fermentation conditions[153]
TunisiaSewage and waste-water treatment ColiphagesPresence of viruses in wastewater treatment[154]
MauritaniaSoil and water samplesProchlorococcus and Synechococcus sp.MyoviridaeMetagenomics of viruses in the desert[155]
TunisiaWastewater samplesKlebsiella pneumoniaePodoviridaeIsolation and characterization[156]
South AfricaWater samples*N. ISomatic and F-RNA PhagesPhages as an indicator of fecal contamination
KenyaWater samples Arthrospira fusiformiscyanophagesCyanophages affecting an African flamingo population[157]
KenyaPoultry fecesCampylobacter jejuniMyoviridaeDevelopment of spray-dried biologics[158]
KenyaPoultry fecesCampylobacter jejuni
Campylobacter coli		MyoviridaeSpray-dried anti-campylobacter powder suitable for global distribution[159]
KenyaPoultry fecesCampylobacter jejuniMyoviridaeUse of Trileucine and pullulan to improve anti-campylobacter bacteriophage stability[160]
KenyaPoultry fecesCampylobacter jejuniMyoviridaeLyophilization process for campylobacter bacteriophage[161]
*N. I mean not indicated.
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Makumi, A.; Mhone, A.L.; Odaba, J.; Guantai, L.; Svitek, N. Phages for Africa: The Potential Benefit and Challenges of Phage Therapy for the Livestock Sector in Sub-Saharan Africa. Antibiotics 2021, 10, 1085. https://doi.org/10.3390/antibiotics10091085

AMA Style

Makumi A, Mhone AL, Odaba J, Guantai L, Svitek N. Phages for Africa: The Potential Benefit and Challenges of Phage Therapy for the Livestock Sector in Sub-Saharan Africa. Antibiotics. 2021; 10(9):1085. https://doi.org/10.3390/antibiotics10091085

Chicago/Turabian Style

Makumi, Angela, Amos Lucky Mhone, Josiah Odaba, Linda Guantai, and Nicholas Svitek. 2021. "Phages for Africa: The Potential Benefit and Challenges of Phage Therapy for the Livestock Sector in Sub-Saharan Africa" Antibiotics 10, no. 9: 1085. https://doi.org/10.3390/antibiotics10091085

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop