Veterinary Medicine International

Veterinary Medicine International / 2020 / Article

Research Article | Open Access

Volume 2020 |Article ID 8821324 |

Daniel W. Wanja, Paul G. Mbuthia, Robert M. Waruiru, Lilly C. Bebora, Helena A. Ngowi, "Natural Concurrent Infections with Black Spot Disease and Multiple Bacteriosis in Farmed Nile Tilapia in Central Kenya", Veterinary Medicine International, vol. 2020, Article ID 8821324, 8 pages, 2020.

Natural Concurrent Infections with Black Spot Disease and Multiple Bacteriosis in Farmed Nile Tilapia in Central Kenya

Academic Editor: Francesca Mancianti
Received05 May 2020
Revised29 Jun 2020
Accepted03 Jul 2020
Published30 Jul 2020


Nile tilapia (Oreochromis niloticus) is the most cultured and available fish for Kenyan consumers, and therefore, any tilapine disease deprives them the valuable source of protein. Nile tilapia farm was diagnosed with severe concurrent black spot disease and multiple bacteriosis using gross lesions and parasitological, histopathology, and standard bacteriological procedures. A total of 25 fish were sampled and inspected, and all of them had raised, macroscopic 1 mm-sized black spot lesions. The mean intensity of black spots per fish was 728 with an abundance of 2–1740 metacercariae cysts per fish. A high intensity of black spot infestation was observed in the fins (43.9%), skin and underlying muscles (18.3%), and gills (18%). In addition, histopathological data confirmed presence of a metacercaria of Neascus spp. as the aetiological agent of black spot disease. Furthermore, a thick fibrous capsule around the metacercaria, black pigment melanomacrophages, and moderate muscle atrophy were observed. The most prevalent bacteria isolated were Aeromonas, Enterobacter cloacae, Klebsiella pneumoniae, and Micrococcus luteus. Physicochemical parameters of pond water were temperature (28.2°C), dissolved oxygen (4.2 mgl−1), pH (8.5), ammonia free nitrogen (15.8 mgl−1), alkalinity (112 mgl−1), hardness (68 mgl−1), nitrites (0.058 mgl−1), nitrates (58 mgl−1), and phosphates (0.046 mgl−1). However, the levels of nitrates, nitrites, alkalinity, and ammonia free nitrogen exceeded the recommended limits. In conclusion, these findings suggest that coinfections by these organisms coupled by water quality-related stress can be associated with low-grade mortality observed in postfingerling tilapia as well as reduced growth. The authors recommended immediate destocking, thorough disinfection, and control of piscivorous birds. Moreover, attention ought to be geared towards prevention of parasitic infestations in fish so as to minimize fish deaths related to secondary bacteriosis. Further experimental studies should be carried out to elucidate the relationship of these pathogens.

1. Introduction

Nile tilapia (Oreochromis niloticus) is a resilient species, which grows in a diverse range of aquatic environment, enduring extreme limits of dissolved oxygen, temperature, and contaminants [1]. Nile tilapia possesses advantageous characteristics for pisciculture, including ability to grow rapidly [2], excellent feed conversion efficiency [3], high resistance to disease [4], and ability to reproduce in captivity [5]. This justifies the dominance of Nile tilapia in global-scale production. The roughness and/or resilient nature and disease resistance make it an ideal aquatic “zebu”. However, recent epidemics such as tilapia lake virus have threatened the species and consequently have outlined the importance of protecting the species through increased disease surveillance [6].

Farmed tilapine fish are exposed to single or multiple pathogens such as parasitic, bacterial, or mixed infections leading to diseases and mortalities [7]. Even though multiple or concurrent infections are common naturally, most studies on tilapia diseases focus on isolation of single pathogen [8]. Poor understanding of coinfections may explain this observation [9].

Bacterial diseases constitute the most important infections threatening sustainability of intensively farmed tilapia [10, 11]. Common bacterial diseases with an enormous economic effect on farmed Nile tilapia in Kenya include motile aeromonads septicaemia, streptococcosis, and pseudomonads septicaemia [1214]. On the other hand, parasites are the basis of all fish epidemics that are associated with secondary invasion with bacteria [15, 16] and can act as a vector to transmit bacterial pathogens [15, 17]. Parasites affecting Nile tilapia under Kenyan aquaculture include myxozoans, monogeneans, nematodes, digenean trematodes, acanthocephalans, and cestodes [18, 19].

Black spot disease or black grub disease is caused by the metacercarial stage of several genera of digenean flukes among the families Heterophyidae and Diplostomatidae [20]. Species of the genera Apophallus, Crassiphiala, Uvulifer [21], Bolbophorus [22], and more generally as Neascus-type trematodes [23, 24] have been documented in many freshwater and saltwater fish. The pathogenesis of black spot disease follows penetration of larvae forms (cercariae) of the parasites into the skin of a fish, where they encyst and develop into metacercariae [25]. The metacercariae provokes the host to form a fibrous capsule around the parasite. The host immune and/or inflammatory response results into infiltration of melanomacrophages through the fibrous wall of the cysts, hence causing the typical appearance of black spots [26]. The black spot lesions are usually visible grossly.

The objective of this study was to describe the occurrence of natural coinfection of black spot disease with multiple bacteriosis in Nile tilapia (Oreochromis niloticus) in a small-scale farm in Central Kenya that was experiencing mortality and aesthetic rejection of fish.

2. Materials and Methods

2.1. Study Area and Case History

The study was conducted between the months of February and November 2018, in a farm located in Kibingo, Kirinyaga Central subcounty, Central Kenya, on longitude 37°15.256E and latitude 00°29.085S and at an altitude of 1652 m above sea level. The farm owns a single 336 m2 sized ultraviolet-treated plastic-lined pond, stocked with mixed sex Nile tilapia. The disease history was obtained from the owner. The initial fish stocking density was 1000 fingerlings; however, current stocking density was unknown due to inbreeding, partial harvests, and mortalities. The disease was surmised when the owner noted raised black skin lesions on fish with low mortality (especially the postfingerlings) and high morbidity and harvested fish rejected by consumers.

2.2. Water Quality Assessment

Water parameters such as temperature, dissolved oxygen, and pH were measured in situ using waterproof handheld HANNA Multiprobe meters 9142 and 98127, respectively (Hanna Instruments Inc., USA), at three different sites on the pond. Water samples were collected and analysed for ammonia free nitrogen, alkalinity, hardness, nitrites, nitrates, and phosphates following standard methods for examination of water and wastewater developed by Boyd and Tucker [27].

2.3. Fish Sampling, Necropsy, and Parasitological Examination

Following owner’s consent, twenty-five fish were harvested using a seine net. These were then transported alive in buckets with source water to County Veterinary Laboratory, Kerugoya, for necropsy and analysis.

Postmortem examination was performed using standard procedures as described by Noga [28] and Roberts [29]. The fish were stunned with a single blow to the back of the head and pithed to separate the central nervous system from the spinal cord. An external examination of individual fish was performed to check for occurrence of ectoparasites and gross lesions. Prior to dissection, individual fish weight (g) and total length were recorded for calculation of the condition factor. The condition factor was calculated by a formula given by Froese [30]: , where “K” is Fulton’s condition factor, “W” is the wet weight in grams, and “L” is the total body length in centimetres. The sex of the fish was also recorded.

2.4. Histopathological Examination

Tissue specimens were taken from the skin and underneath muscle from the flanks of few O. niloticus that were heavily infested with black spot lesions. The samples were fixed in 10% buffered formalin overnight. The tissue sections were then gradually dehydrated in 70–100% ethanol, cleared in xylene, and finally embedded in paraffin wax through standard procedures [31, 32]. Tissue specimens were sectioned at 3–5 µm and stained with haematoxylin and eosin (H&E). Slides were then observed under a light microscope.

2.5. Bacteriological Examination

Out of the 25 fish collected, 10 fish were randomly selected for bacteriological isolation, which was done on aseptically collected kidney swab from individual fish. These swabs were streaked separately and aseptically onto plates containing nutrient agar, 10% sheep blood agar, and MacConkey agar. The inoculated plates were incubated aerobically at room temperature (24°C–26°C), in an inverted position. After 24–48 hours of incubation, the plates were examined, and colony morphology on the plates was recorded. The isolates were identified using colony morphology, Gram staining characteristics, conventional biochemical tests (catalase reaction, cytochrome oxidase, methyl red, citrate utilization, urea degradation, sulphur-indole-motility, and sugars fermentation) following Austin and Austin [11], Bergey’s Manual of determinative bacteriology [33], and Markey et al. [34]. Further characterization of Gram-negative lactose fermenters was conducted using the Analytic Profile Index 20E (API 20E) microbial identification strips according to manufacturer’s protocol (BioMérieux Marcy-l’Étoile, France).

2.6. Data Analysis

The disease prevalence, mean abundance (average number of black spot lesions seen in all the fish), and mean intensity (mean number of black spot lesions per fish infested) were calculated as described by Bush et al. [35]. The collected data were validated, entered, and stored in Microsoft Excel® spreadsheet, which was also used to calculate means and proportions. Inferential statistics were performed using Statistical Package for the Social Sciences (SPSS®), version 22.0. The chi square test was used to compare proportions. Pearson correlation matrix was used to check for association. All tests were tested at a level of 0.05 for significance.

3. Results

3.1. Physicochemical Parameters of Pond Water and on Farm Observations

The pond water colour was dark green, an indication of overfertilization. The average values of other parameters measured are summarized in Table 1. From the table, the pond water temperature, pH, dissolved oxygen, water hardness, and phosphates levels measured were within the recommended/desired range for rearing tilapia. However, levels of nitrates, nitrites, alkalinity, and ammonia free nitrogen were above the recommended limits.

Physicochemical parameters of waterRecorded pond value

(1) Temperature (°C)28.2c
(2) Dissolved oxygen (mgl−1)4.2c
(3) pH8.5c
(4) Total ammonia free nitrogen (mgl−1)15.8a
(5) Alkalinity (mgl−1)112a
(6) Hardness (mgl−1)68c
(7) Nitrites (mgl−1)0.058a
(8) Nitrates (mgl−1)58a
(9) Phosphates (mgl−1)0.046c

Note. The recommended range of physicochemical parameters of water for culturing Nile tilapia in ponds are temperature = 22–32°C; dissolved oxygen = 5–7 mgl−1; pH = 6.5–8.5; ammonia 0.3–2 mgl−1; alkalinity 20–100 mgl−1; hardness 10–100 mgl−1; nitrite = <0.02 mgl−1; nitrates = 0.1–4.5 mgl−1, and phosphorous = 0.01–3 mgl−1 [3638]. Key: a = pond value was above the recommended range; b = pond value was below the recommended range; and c = pond value was within the recommended range.
3.2. Fish Samples and Their Biodata

Of the 25 fish sampled, 16 were females and the rest were males. The mean weight, standard, and total lengths of the fish samples were 119 ± 4.7 g, 15.2 ± 0.2 mm, and 19 ± 0.3 mm, respectively. The mean condition factor (K) of fish was 1.73 ± 0.03, with no significant difference between males and females.

3.3. Macroscopic and Necropsy Findings

On macroscopic examination, all the 25 fish examined were infested with macroscopic 1 mm raised black spot lesions, with no other apparent clinical signs (behavioural) of parasitism or bacteriosis. The lesions were extensively distributed throughout the body surface including the fins, operculum, mouth, skin, gills, and eyes (Figure 1(a)). On dissecting the fish, more conspicuous black spots were also observed on the epidermis, dermis, and musculature and on the gill rakers and filaments of fish (Figures 1(b) and 1(c)). There were lesions in the vertebral bone; however, no skeletal deformity was observed. There were no significant findings seen in other visceral organs.

Table 2 shows distribution of lesions in various organs and their corresponding percentage. The fins were the most infested. The mean intensity of black spots per fish was 728.48 3 with an abundance range of 2–1740 metacercariae cysts per fish. There was a significant negative correlation between intensity and body condition (R2 = −0.49).

OrganTotal number of black spot lesionsDistribution (%)

Skin and muscles333418.3
Buccal cavity4782.6

3.4. Histopathological Findings

Histopathological findings revealed that the aetiological agent causing this disease was a metacercaria of Neascus spp., a digenean trematode. The parasite localized in the stratified epithelial tissue and musculature (Figure 2(a)). Histopathological analysis further revealed a thick fibrous capsule around the encysted metacercariae with the periphery of the cyst containing black pigment due to melanomacrophages responsible for the formation of dark spots (Figure 2(b)). Moderate muscle atrophy was also observed.

3.5. Bacteriological Findings

The results of bacteriological examination revealed 4 bacteria taxa, which were identified by colonial morphology, Gram stain reaction, and by use of conventional biochemical tests (Figure 3). The predominant bacteria were Aeromonas spp. (30%, n = 3), Enterobacter cloacae (20%, n = 2), Klebsiella pneumoniae (10%, n = 1), and Micrococcus luteus (10%, n = 1), while 30% (n = 3) of the kidney swabs yielded no bacterial growth with respect to isolation procedures used.

4. Discussion

Although black spot disease (BSD) does not cause much pathological effect, it affects the aesthetic appeal of fish, therefore causing rejection at market level [25]. However, the black spots can be quite pathogenic if they are located in sensitive areas such as gills. Gill infestation leads to respiratory distress [39], while fish with eye infestation may be blind.

Coinfections occur when hosts are infected by two or more different pathogens either concurrently or as secondary invaders, so that two or more pathogenic agents are active together in the same host [40]. This study confirmed such coinfections of metacercarial stages of Neascus spp. causing “black spot” disease with several bacteria genera including Aeromonas, Enterobacter, Klebsiella, and Micrococcus in farmed Nile tilapia collected from Kirinyaga County. The results are contrary to a previous study in Winam Gulf of Lake Victoria, Kenya, by Thon et al. [41] who reported a prevalence of 0.7% in wild Nile tilapia. The differences in prevalence rate may be due to the fact that parasitic infestations might be annihilating in farmed fish compared to wild fish [42]. This is so because farmed fish is associated with stressful culture conditions including overcrowding and poor water quality, thus making them more susceptible to diseases [42, 43]. Moreover, Thon et al. [41] focused on parasitological isolation of endohelminths of wild Nile tilapia, and therefore, the bacteriological status of the sampled fish was not investigated. The findings are, however, partially in line with a previous study in Pacific Northwest by Arkoosh et al. [23] who reported coinfection of black spot disease and Renibacterium salmoninarum in juvenile salmon (Oncorhynchus species). In this study, several bacteria taxa including Aeromonas spp., Klebsiella pneumoniae, Enterobacter cloacae, and Micrococcus luteus were isolated from the kidney of examined fish. The discrepancy in bacteria taxa in the current study and that of Arkoosh et al. [23] could be due to culture environment of the fish species; tilapia is a warm water species, while salmon is a cold water fish. The bacteria isolated in this study are ubiquitous in aquatic environments and have been reported previously in Kenya [13, 14]. Some of these including Aeromonas spp. and Klebsiella pneumoniae are pathogenic to fish [11], while Micrococcus luteus have been developed as fish probiotics [44]. Recovery of these bacteria from the kidney is an indication of infection after overcoming the fish defence mechanisms.

In this study, all the sampled fish had a condition factor of more than one. A condition factor value of more than one implies a good fish health condition and proportional growth, which is recommendable in a fish farm [45]. However, histopathological sections revealed moderate muscle atrophy; which explains the negative correlation between parasite intensity and condition factor. This perhaps suggests that this was a case of recent infection, considering that none of the fish had skeletal abnormality.

Physicochemical parameters of the water and nutrients and presence of pollutants have a positive influence on the occurrence of parasitic and bacterial populations and communities in fish cultured environments [4649]. The fish pond recorded slightly high levels of calcium carbonates (alkalinity) and high levels of nitrites, nitrates, and ammonia free nitrogen than the recommended range for rearing tilapia. A study by Ismail et al. [50] demonstrated that presence of Aeromonas hydrophila, Enterobacter cloacae, and Micrococcus spp., among other bacteria was greatly influenced by water temperature, levels of nitrites, phosphates, sulphide, and ammonia. On the other hand, Isyagi et al. [36] reported that consistently high levels of ammonia nitrogen above the recommended limit are associated with trematode infestations such as Neascus spp. As such, poor water quality may reduce fish immunological ability and thus become more susceptible to disease-causing pathogens [48], including bacteria and parasites.

This could be the first report on natural concurrent infection of Neascus spp. and multiple bacteriosis. However, the relationship among these pathogens is not fully understood. In a probably similar pathogenesis cascade as the current study, Sandell et al. [51] reported stunted growth and low survival chances among juvenile salmons due to concurrent infections of Neascus spp. and Renibacterium salmoninarum. Some researchers have postulated that coinfections of some ectoparasites simultaneously with ubiquitous bacteria have a mutual benefit relationship [52, 53], unlike in this case where there were mortalities. A number of studies have shown synergetic interaction of parasitic and bacterial coinfections [54, 55]. These studies have shown higher mortality rates in concurrent bacterial-parasitic infections. This synergistic effect has been explained as a result of stress caused by parasites that lowers fish immunity to other infections including secondary bacterial infections [56], as well as the damaging effects caused by the parasite that provide portal of entry for the secondary invaders including bacteria.

Due to lack of prior studies on coinfections in fish, particularly in farmed Nile tilapia, we can compare with findings from other systems on parasite species from the same fish in Kenya and beyond. For instance, Florio et al. [57] reported a slightly higher parasitic infestation of 86.5% in pond-cultured tilapia compared to wild or caged fish in Kenya. Florio et al. [57] reported 23 different parasite genera in Kenya, 15 in Uganda, and 13 in Ethiopia under different aquatic systems. Trichodina spp. Trichodinella spp., Myxobolus spp., Dactylogyrus spp., Gyrodactylus spp., diplostomatid and clinostomid metacercariae, Neascus spp., cestodes, and larval nematodes were reported in all the three countries. Florio et al.’ [57] work shows that parasitic infestation in fish vary greatly from one system to another, and this may be influenced by physicochemical properties of culture water and occurrence of intermediate hosts. Moreover, climatic/topographical conditions of the region, seasonality, and host parasite relationship may also play a role in the epidemiology of parasites of fish.

5. Conclusion

In conclusion, our findings show that synergistic coinfections by metacercariae of Neascus spp. and multiple bacteria taxa coupled with poor water quality were responsible for the reported mortality in postfingerling Nile tilapia. The findings of this study may be of significance to aquaculture, especially at a time of scanty information on diseases of farmed fish in developing countries, including Kenya.

6. Recommendations

It ought to be noted that presence of snails and piscivorous birds is one of the risk factors that propagate the life cycle of the Neascus spp. While there are no practical means to treat BSD, the authors recommend immediate destocking, thorough disinfection (including use of molluscicides), and controlling piscivorous birds. Moreover, attention ought to be given towards prevention of parasitic infestations in fish so as to minimize fish deaths related to secondary bacteriosis and economic loss due to aesthetic reasons. Further experimental infection challenge studies are recommended in order to evaluate the associations of these organisms so as to comprehend their significance on fish.

Data Availability

Data associated with this paper are retrievable from the online repository at

Conflicts of Interest

The authors have no conflicts of interest regarding publication of this paper.


The authors acknowledge the Norwegian Agency for Development Cooperation (NORAD) for financing this work under the capacity building for the Training and Research in Aquatic and Environmental Health in Eastern and Southern Africa (TRAHESA) project (Grant TAN 13/0027).


  1. Z. Beyruth, C. Mainardes-Pinto, S. Fusco, F. Faria, and A. Silva, “Utilizacao de alimentos naturais por Oreochromis niloticus em tanques de terra com arracoamento (use of natural food by Oreochromis niloticus in earthen ponds with feeding),” Boletim Do Instituto De Pesca, vol. 30, no. 1, pp. 9–24, 2018. View at: Google Scholar
  2. H. A. Hassanien, M. Elnady, A. Obeida, and H. Itriby, “Genetic diversity of Nile tilapia populations revealed by randomly amplified polymorphic DNA (RAPD),” Aquaculture Research, vol. 35, no. 6, pp. 587–593, 2004. View at: Publisher Site | Google Scholar
  3. F. Kubitza, Tilapia: Tecnologia e Planejamento na Producao Comercial (Tilapia: Technology Planning and in Commercial Production), Degaspari Publisher, Jundiai, Sao Paulo, Brazil, 2000.
  4. I. Ardjosoediro and I. W. Ramnarine, “The influence of turbidity on growth, feed conversion and survivorship of the Jamaica red tilapia strain,” Aquaculture, vol. 212, no. 1–4, pp. 159–165, 2002. View at: Publisher Site | Google Scholar
  5. A. P. Shoko, S. M. Limbu, H. D. J. Mrosso, and Y. D. Mgaya, “Reproductive biology of female Nile tilapia Oreochromis niloticus (Linnaeus) reared in monoculture and polyculture with African sharptooth catfish Clarias gariepinus (Burchell),” SpringerPlus, vol. 4, no. 1, p. 275, 2015. View at: Publisher Site | Google Scholar
  6. M. D. Jansen, H. T. Dong, and C. V. Mohan, “Tilapia lake virus: a threat to the global tilapia industry?” Reviews in Aquaculture, vol. 11, no. 3, pp. 725–739, 2019. View at: Publisher Site | Google Scholar
  7. C. A. Shoemaker, D.-H. Xu, P. H. Klesius, and J. J. Evans, “Concurrent infections (parasitism and bacterial disease) in tilapia,” in Proceedings of the 8th International Symposium on Tilapia in Aquaculture, pp. 1365–1375, Cairo, Egypt, January 2008. View at: Google Scholar
  8. H. M. Abdel‐Latif, M. A. O. Dawood, S. Menanteau‐Ledouble, and M. El‐Matbouli, “The nature and consequences of coinfections in tilapia: a review,” Journal of Fish Diseases, vol. 43, no. 6, pp. 651–664, 2020. View at: Publisher Site | Google Scholar
  9. H. T. Dong, V. V. Nguyen, H. D. Le et al., “Naturally concurrent infections of bacterial and viral pathogens in disease outbreaks in cultured Nile tilapia (Oreochromis niloticus) farms,” Aquaculture, vol. 448, pp. 427–435, 2015. View at: Publisher Site | Google Scholar
  10. A.-F. M. El-Sayed, Tilapia Culture, CABI Publishing, Cambridge, USA, 2006.
  11. B. Austin and D. A. Austin, Bacterial Fish Pathogens: Disease of Farmed and Wild Fish, Springer, New York, NY, USA, 6th edition, 2016.
  12. P. Akoll and W. W. Mwanja, “Fish health status, research and management in East Africa: past and present,” African Journal of Aquatic Science, vol. 37, no. 2, pp. 117–129, 2012. View at: Publisher Site | Google Scholar
  13. R. D. Karimi, “The bacterial flora of tilapia (Oreochromis niloticus) and catfish (Clarias gariepinus) from earthen ponds in Sagana fish farm and Masinga dam,” Thesis for Award of MSc Degree at Kenyatta University, Nairobi, Kenya, 2015, M. Sc thesis. View at: Google Scholar
  14. D. W. Wanja, P. G. Mbuthia, R. M. Waruiru et al., “Bacterial pathogens isolated from farmed fish and source pond water in Kirinyaga County, Kenya,” International Journal of Fisheries and Aquatic Studies, vol. 7, no. 2, pp. 295–301, 2019. View at: Google Scholar
  15. H. M. Abdel‐Latif and A. F. Khafaga, “Natural coinfection of cultured Nile tilapia Oreochromis niloticus with Aeromonas hydrophila and Gyrodactylus cichlidarum experiencing high mortality during summer,” Aquaculture Research, vol. 51, no. 5, pp. 1880–1892, 2020. View at: Publisher Site | Google Scholar
  16. I. Taghreed, “Diseases of Nile tilapia with special emphasis on water pollution,” Journal of Environmental Science and Technology, vol. 13, no. 1, pp. 29–56, 2019. View at: Publisher Site | Google Scholar
  17. A. S. Holzer, C. Sommerville, and R. Wootten, “Molecular studies on the seasonal occurrence and development of five myxozoans in farmed Salmo trutta L,” Parasitology, vol. 132, no. Pt 2, pp. 193–205, 2006. View at: Publisher Site | Google Scholar
  18. G. C. Mathenge, “Prevalence, intensity and pathological lesions associated with helminth infection in farmed and wild fish in upper Tana River Basin, Kenya,” University of Nairobi, Nairobi, Kenya, 2010, Master’s Dissertation. View at: Google Scholar
  19. S. K. Mavuti, R. M. Waruiru, P. G. Mbuthia, J. G. Maina, J. M. Mbaria, and R. O. Otieno, “Prevalence of ecto- and endoparasitic infections of farmed tilapia and catfish in Nyeri County, Kenya,” Livestock Research for Rural Development, vol. 29, no. 6, pp. 55–59, 2017. View at: Google Scholar
  20. A. Happel, “A volunteer-populated online database provides evidence for a geographic pattern in symptoms of black spot infections,” International Journal for Parasitology: Parasites and Wildlife, vol. 10, pp. 156–163, 2019. View at: Publisher Site | Google Scholar
  21. G. L. Hoffman, Parasites of North American Freshwater Fishes, Cornell University Press, Ithaca, NY, USA, 2019.
  22. R. M. Overstreet, S. S. Curran, L. M. Pote, D. T. King, C. K. Blend, and W. D. Grater, “Bolbophorus damnificus n. sp. (Digenea: Bolbophoridae) from the channel catfish Ictalurus punctatus and American white pelican Pelecanus erythrorhynchos in the USA based on life-cycle and molecular data,” Systematic Parasitology, vol. 52, no. 2, pp. 81–96, 2002. View at: Publisher Site | Google Scholar
  23. M. R. Arkoosh, E. Clemons, A. N. Kagley et al., “Survey of pathogens in juvenile Salmon oncorhynchus spp. Migrating through Pacific Northwest estuaries,” Journal of Aquatic Animal Health, vol. 16, no. 4, pp. 186–196, 2004. View at: Publisher Site | Google Scholar
  24. M. A. Cairns, J. L. Ebersole, J. P. Baker, P. J. Wigington, H. R. Lavigne, and S. M. Davis, “Influence of summer stream temperatures on black spot infestation of juvenile coho salmon in the Oregon coast range,” Transactions of the American Fisheries Society, vol. 134, no. 6, pp. 1471–1479, 2005. View at: Publisher Site | Google Scholar
  25. R. L. Lane and J. E. Morris, Biology, Prevention, and Effects of Common Grubs (Digenetic Trematodes) in Freshwater Fish, NCRAC Technical Bulletins, Iowa State University, Ames, IA, USA, 2010.
  26. A. O. Bush, J. C. Fernandez, G. W. Esch, and J. R. Seed, Parasitism: The Diversity and Ecology of Animal Parasites, Cambridge University Press, Cambridge, United Kingdom, 2001.
  27. C. E. Boyd and C. S. Tucker, Pond Aquaculture Water Quality Management, Springer Science & Business Media, Berlin, Germany, 2012.
  28. E. J. Noga, Fish Disease: Diagnosis and Treatment, Wiley Blackwell, Hoboken, NJ, USA, 2nd edition, 2010.
  29. R. J. Roberts, Fish Pathology, Wiley-Blackwell, Ames, Iowa, USA, 4th edition, 2012.
  30. R. Froese, “Cube law, condition factor and weight-length relationships: history, meta-analysis, and recommendations,” Journal of Applied Ichthyology, vol. 22, no. 4, pp. 241–253, 2006. View at: Publisher Site | Google Scholar
  31. B. Oidtmann, P. Steinbauer, S. Geiger, and W. R. Hoffmann, “Experimental infection and detection of Aphanomyces invadans in European catfish, rainbow trout and European eel,” Diseases of Aquatic Organisms, vol. 82, no. 3, pp. 195–207, 2008. View at: Publisher Site | Google Scholar
  32. M. N. A. Amal, C. B. Koh, M. Nurliyana et al., “A case of natural coinfection of Tilapia lake virus and Aeromonas veronii in a Malaysian red hybrid tilapia (Oreochromis niloticus × O. mossambicus) farm experiencing high mortality,” Aquaculture, vol. 485, pp. 12–16, 2018. View at: Publisher Site | Google Scholar
  33. D. H. Bergey, G. H. Holt, N. R. Krieg, and H. A. S. Peter, Bergey’s Manual of Determinative Bacteriology, Lippincott Williams and Wilkins, Philadelphia. PA. USA, 9th edition, 1994.
  34. B. Markey, F. Leonard, M. Archambault, A. Cullinane, and D. Maguire, Clinical Veterinary Microbiology, Oxford University Press, New York, NY, USA, 2nd edition, 2013.
  35. A. O. Bush, K. D. Lafferty, J. M. Lotz, and A. W. Shostak, “Parasitology meets ecology on its own terms: Margolis et al. revisited,” The Journal of Parasitology, vol. 83, no. 4, pp. 575–583, 1997. View at: Publisher Site | Google Scholar
  36. N. A. Isyagi, K. L. Veverica, R. Asiimwe, and W. H. Daniels, Manual for the Commercial Pond Production of the African Catfish in Uganda, Walimi Fish Co-op Society, Kampala, Uganda, 2009.
  37. F. C. Ikeogu, C. I. Nsofor, and O. O. Ikpeze, “A review of risk factors for fish diseases in aquatic environments,” in Proceedings of the 6th National Conference of the Society for Occupational Safety and Environmental Health (SOSEH), pp. 199–204, University of Nigeria Nsukka, Nsukka, EN, Nigeria, January 2010. View at: Google Scholar
  38. A. Bhatnagar and P. Devi, “Water quality guidelines for the management of pond fish culture,” International Journal of Environmental Sciences, vol. 3, no. 6, pp. 1980–2009, 2013. View at: Publisher Site | Google Scholar
  39. D. Hoole, D. Bucke, P. Burgess, and I. Wellby, Diseases of Carps and other Cyprinid Fishes, Wiley-Blackwell, Oxford, England, 2001.
  40. M. H. Kotob, S. Menanteau-Ledouble, G. Kumar, M. Abdelzaher, and M. El-Matbouli, “The impact of coinfections on fish: a review,” Veterinary Research, vol. 47, no. 1, p. 98, 2016. View at: Publisher Site | Google Scholar
  41. C. C. Thon, O. E. Otachi, and A. A. Oldewage, “Endo-helminths infestation in Nile perch, Lates niloticus, (L.,) and Nile tilapia, Oreochromis niloticus (L.,) in Winam Gulf of Lake Victoria, Kenya,” Egerton Journal of Science and Technology, vol. 16, no. 1–139, 2019. View at: Google Scholar
  42. M. G. Bondad-Reantaso, R. P. Subasinghe, J. R. Arthur et al., “Disease and health management in Asian aquaculture,” Veterinary Parasitology, vol. 132, no. 3-4, pp. 249–272, 2005. View at: Publisher Site | Google Scholar
  43. D. W. Wanja, P. G. Mbuthia, R. M. Waruiru et al., “Fish husbandry practices and water quality in central Kenya: potential risk factors for fish mortality and infectious diseases,” Veterinary Medicine International, vol. 2020, Article ID 6839354, 10 pages, 2020. View at: Publisher Site | Google Scholar
  44. A. M. A. El-Rhman, Y. A. E. Khattab, and A. M. E. Shalaby, “Micrococcus luteus and Pseudomonas species as probiotics for promoting the growth performance and health of Nile tilapia, Oreochromis niloticus,” Fish Shellfish Immunology, vol. 27, no. 2, pp. 175–180, 2009. View at: Publisher Site | Google Scholar
  45. A. A. Ayode, “Length-weight relationship and diet of African carp Labeo ogunensis (Boulenger, 1910) in Asejire Lake Southwestern Nigeria,” Journal of Fisheries and Aquatic Sciences, vol. 6, no. 4, pp. 472–478, 2011. View at: Google Scholar
  46. U. R. Zargar, A. R. Yousuf, M. Z. Chishti, F. Ahmed, H. Bashir, and F. Ahmed, “Effects of water quality and trophic status on helminth infections in the cyprinid fish, Schizothorax Niger Heckel, 1838 from three lakes in the Kashmir Himalayas,” Journal of Helminthology, vol. 86, no. 1, pp. 70–76, 2012. View at: Publisher Site | Google Scholar
  47. K. Gorlach-Lira, C. Pacheco, L. C. T. Carvalho, H. N. Melo Júnior, and M. C. Crispim, “The influence of fish culture in floating net cages on microbial indicators of water quality,” Brazilian Journal of Biology, vol. 73, no. 3, pp. 457–463, 2013. View at: Publisher Site | Google Scholar
  48. J. Biswas and S. Pramanik, “Assessment of aquatic environmental quality using Gyrodactylus sp. as a living probe: parasitic biomonitoring of ecosystem health,” Journal of Advances in Environmental Health Research, vol. 4, no. 4, pp. 219–226, 2016. View at: Google Scholar
  49. R. A. Ojwala, E. O. Otachi, and N. K. Kitaka, “Effect of water quality on the parasite assemblages infecting Nile tilapia in selected fish farms in Nakuru County, Kenya,” Parasitology Research, vol. 117, no. 11, pp. 3459–3471, 2018. View at: Publisher Site | Google Scholar
  50. N. I. A. Ismail, M. N. A. Amal, S. Shohaimi, M. Z. Saad, and S. Z. Abdullah, “Associations of water quality and bacteria presence in cage cultured red hybrid tilapia, Oreochromis niloticus × O. mossambicus,” Aquaculture Reports, vol. 4, pp. 57–65, 2016. View at: Publisher Site | Google Scholar
  51. T. A. Sandell, D. J. Teel, J. Fisher, B. Beckman, and K. C. Jacobson, “Infections by Renibacterium salmoninarum and Nanophyetus salmincola Chapin are associated with reduced growth of juvenile Chinook salmon, Oncorhynchus tshawytscha (Walbaum), in the Northeast Pacific Ocean,” Journal of Fish Diseases, vol. 38, no. 4, pp. 365–378, 2015. View at: Publisher Site | Google Scholar
  52. A. E. Eissa, M. M. Zaki, and A. A. Aziz, “Flavobacterium columnare/Myxobolus tilapiae concurrent infection in the earthen pond reared Nile tilapia (Oreochromis niloticus) during the early summer,” Interdisciplinary Bio Central, vol. 2, no. 2, pp. 5.1–5.9, 2010. View at: Publisher Site | Google Scholar
  53. D.-H. Xu, C. A. Shoemaker, and P. H. Klesius, “Evaluation of the link between gyrodactylosis and streptococcosis of Nile tilapia, Oreochromis niloticus (L.),” Journal of Fish Diseases, vol. 30, no. 4, pp. 233–238, 2007. View at: Publisher Site | Google Scholar
  54. M. Bandilla, E. Valtonen, L. Suomalainen, P. Aphalo, and T. Hakalahti, “A link between ectoparasite infection and susceptibility to bacterial disease in rainbow trout,” International Journal for Parasitology, vol. 36, no. 9, pp. 987–991, 2006. View at: Publisher Site | Google Scholar
  55. P. Pylkkö, L.-R. Suomalainen, M. Tiirola, and E. T. Valtonen, “Evidence of enhanced bacterial invasion during Diplostomum spathaceum infection in European grayling, Thymallus thymallus (L.),” Journal of Fish Diseases, vol. 29, no. 2, pp. 79–86, 2006. View at: Publisher Site | Google Scholar
  56. J. M. Bowers, A. Mustafa, D. J. Speare et al., “The physiological response of Atlantic salmon, Salmo salar L., to a single experimental challenge with sea lice, Lepeophtheirus salmonis,” Journal of Fish Diseases, vol. 23, no. 3, pp. 165–172, 2000. View at: Publisher Site | Google Scholar
  57. D. Florio, A. Gustinelli, M. Caffara et al., “Veterinary and public health aspects in tilapia (Oreochromis niloticus niloticus) aquaculture in Kenya, Uganda and Ethiopia,” Ittiopatologia, vol. 6, no. 12, pp. 51–93, 2009. View at: Google Scholar

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