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Nematode infection in liver of the fish Gymnotus inaequilabiatus (Gymnotiformes: Gymnotidae) from the Pantanal Region in Brazil: pathobiology and inflammatory response
Parasites & Vectors volume 9, Article number: 473 (2016)
A survey on endoparasitic helminths from freshwater fishes in the Pantanal Region (Mato Grosso do Sul, Brazil) revealed the occurrence of third-larval stage of the nematode Brevimulticaecum sp. (Heterocheilidae) in most organs of Gymnotus inaequilabiatus (Gymnotidae) also known by the local name tuvira. The aim of the present study was to examine Brevimulticaecum sp.-infected tuvira liver at the ultrastructural level and clarify the nature of granulomas and the cellular elements involved in the immune response to nematode larvae.
Thirty-eight adult specimens of tuvira from Porto Morrinho, were acquired in January and March 2016. Infected and uninfected liver tissues were fixed and prepared for histological and ultrastructure investigations.
The prevalence of infection of tuvira liver by the nematode larvae was 95 %, with an intensity of infection ranging from 4 to 343 larvae (mean ± SD: 55.31 ± 73.94 larvae per liver). In livers with high numbers of nematode larvae, almost entire hepatic tissue was occupied by the parasites. Hepatocytes showed slight to mild degenerative changes and accumulation of pigments. Parasite larvae were surrounded by round to oval granulomas, the result of focal host tissue response to the infection. Each granuloma was typically formed by three concentric layers: an outer layer of fibrous connective tissue with thin elongated fibroblasts; a middle layer of mast cells entrapped in a thin fibroblast-connective mesh; and an inner layer of densely packed epithelioid cells, displaying numerous desmosomes between each other. Numerous macrophage aggregates occurred in the granulomas and in the parenchyma.
Our results in tuvira showed that the larvae were efficiently sequestered within the granulomas, most of the inflammatory components were confined within the thickness of the granuloma, and the parenchyma was relatively free of immune cells and without fibrosis. Presumably this focal encapsulation of the parasites permits uninfected portions of liver to maintain its functions and allows the survival of the host.
Ten species of the genus Brevimulticaecum (Nematoda: Heterocheilidae) have been reported from different parts of the world, of which six species are exclusively distributed in the Americas . Species of this genus have an indirect and complex life-cycle, which involves intermediate, paratenic and definitive hosts. Some macroinvertebrates (e.g. aquatic insects such as members of Odonata and Ephemeroptera) are intermediate hosts of Brevimulticaecum sp.  and amphibians, snakes and freshwater fish have a role as paratenic hosts while crocodilians are definitive hosts [3–7].
Encapsulated third-stage larvae of several species of nematodes are commonly found in the organs of marine [8–12] and freshwater fish [13–16]. A survey on endoparasitic helminths from freshwater fishes in the Pantanal Region (Mato Grosso do Sul, Brazil) revealed the occurrence of third-stage larvae of Brevimulticaecum sp. in most organs of Gymnotus inaequilabiatus [1, 2, 17]. Gymnotus inaequalabiatus, also known by the local name tuvira, is of great importance in southern Brazil as it is used for live-bait to collect other fish species of commercial value. Tuvira is a preferred prey for the Pantanal caiman, Caiman yacare  and adult specimens of Brevimulticaecum sp. were recorded from the intestine of this reptile .
In intestine and visceral organs of most fish species, larvae of helminths often become encapsulated by a host tissue response [13, 19, 20], with the walls of the capsule consisting of thick connective tissue and epithelioid cells [21, 22]. The basic immune response mechanisms in vertebrates against helminths are poorly understood . In response to infection, a variety of cells become activated and cooperate in an effort to control and eliminate the invading pathogens . In fish, the innate defences responding to helminth infection commonly involve mast cells (MCs) [20, 25–27], macrophage aggregates (MAs) or melano-macrophage centres [22, 27, 28], neutrophils [29, 30] and rodlet cells (RCs) [27, 31].
In a recent study on the histopathology of tuvira liver infected with Brevimulticaecum sp. Ventura et al.  stated that “The lack of acute inflammatory process indicates that the parasite is not causing to the host a reaction with inflammatory cells …”. However their study was based on light microscopy which is not sufficient for an accurate determination of liver infection by Brevimulticaecum sp. While histopathology can be used to assess the health impact of parasitism , it is well established that ultrastructural observation analysis of the liver is a superior tool for determining health status . The aim of the present study was to examine Brevimulticaecum sp.-infected tuvira liver at the ultrastructural level and clarify the nature of granulomas as well as the cellular elements involved in the immune response to nematode larvae.
Adult specimens (n = 38) of Gymnotus inaequilabiatus, from Porto Morrinho (21°41′56″S, 57°52′57″W), municipality of Corumbá, Brazil, were collected in January and March 2016. The specimens were transported in oxygenated polyethylene bags to the Laboratory of Pathology, Federal University of Mato Grosso do Sul, Brazil, where fishes were stocked for two hours in aquariua supplied with artificial aeration at constant temperature (25 °C) until euthanasia (2-Fenoxiethanol, 2 ml/l). Euthanized fish were then weighed (total weight in grams) and measured (total length in centimeters). After dissection stomach, intestine, liver, heart, gonads, spleen, and kidney were screened microscopically for endoparasites. The liver was removed from the coelomic cavity and although cysts were visible with a naked eye, a more accurate assessment was made by examining the organ surface under a stereomicroscope. From each infected liver, several 10 × 10 mm pieces were excised and fixed in 10 % neutral buffered formalin for 24 h, then processed routinely for paraffin embedding, sectioned (5 μm thick) and then stained with either Hematoxylin and Eosin, alcian blue 8 GX pH 2.5 and periodic acid Schiff’s (AB/PAS), Perls’ Prussian Blue stain for ferric iron, Giemsa and/or Masson’s Trichrome. Multiple histological sections were taken from each tissue block, examined and photographed using an optical microscope (Nikon Eclipse 80i; Nikon, Tokyo, Japan).
For transmission electron microscopy (TEM), 7 × 7 mm pieces of infected liver tissues were fixed in chilled 2.5 % glutaraldehyde in 0.1 M sodium cacodylate buffer for 3 h. The fixed tissues were then post-fixed in 1 % osmium tetroxide for 2 h and then rinsed and stored in 0.1 M sodium cacodylate buffer containing 6 % sucrose for 12 h. Thereafter, the tissue pieces were dehydrated through a graded acetone series and embedded in epoxy resin (Durcupan ACM, Fluka, Buchs, Switzerland). Semi-thin sections (1.5 μm) were cut on a Reichert Om U 2 ultramicrotome and stained with toluidine blue. Ultra-thin sections (90 nm) were stained with 4 % uranyl acetate solution in 50 % ethanol and Reynold’s lead citrate and then examined using an Hitachi H-800 transmission electron microscope.
For both light and transmission electron microscopy corresponding pieces of uninfected liver were also processed so that a direct comparison with the infected material could be made. From ten livers, over 40 encysted larvae were isolated and fixed in acetic acid and stored in ethanol 70 % and then cleared in lactophenol for species identification.
Thirty-eight specimens of G. inaequilabiatus (mean total length ± standard deviation, SD: 32.36 ± 2.89 cm) were sampled and examined. Nematode larvae were encountered in almost all of the visceral organs of G. inaequilabiatus, but liver appeared to be the most infected organ (Fig. 1a, b). Ninety-five per cent of livers (36 of 38) were infected with nematode larvae (Fig. 1a, b). Based on morphological examinations of a sub-population of larvae isolated/removed from the liver, all specimens were identified as third-stage larvae of Brevimulticaecum sp. based on key features provided in Moravec & Kaiser  and Moravec et al. . The range in intensity of infection was 4–343 larvae per fish (mean ± SD: 55.31 ± 73.94 larvae per liver). Figure 1c shows a small piece of uninfected liver. In infected liver, the vast majority of the larvae was located either singly or as an aggregation of white cysts beneath the serosa of the liver (Fig. 1b, d, e) and within the hepatic parenchyma. Large cysts containing white Brevimulticaecum sp. larvae were noticeable by naked eye during necropsy examination (Fig. 1a, b). In many instances, single larvae or clusters of larvae were observed to be attached to the liver surface by a kind of peduncle of host peritoneal origin (Fig. 1e).
In cases of heavy infection, the vast majority of liver surface was occupied by larvae (Fig. 2a). Brevimulticaecum sp. larvae were encircled by focal host tissue reaction, forming round-oval shaped granulomas (Fig. 2a-c). In most granulomas, especially in those with larger larvae, exfoliation of the inner layer of epithelioid cells resulted in accumulation of amorphous necrotic tissue (Fig. 2b). This necrotic accumulation was slightly to strongly basophilic and PAS positive. Where this exfoliation and related necrosis were absent or moderately present, the cysts were enlarged by means of a faintly eosinophilic, Alcian Blue positive fluid (Fig. 2c). Granulomas were formed by three concentric layers: an outer layer of fibrous connective tissue and thin elongated fibroblasts (Fig. 2d); a middle layer of MCs (Fig. 2d) entrapped in a thin fibroblastic-connective mesh, usually spongiotic in appearance; and an inner layer of densely-packed epithelioid cells (Fig. 2d). The thickness of each layer varied considerably among granulomas (Fig. 2b). MCs showed intense PAS and slightly Alcian Blue pH 2.5 positive granules. Degranulation of MCs was frequent (Fig. 2e).
A net separation was clearly visible between the fibrous connective layer and the remnant tissue; moreover, fibrous connective branches within liver septa were seen in larger granulomas. Nevertheless, there was no evidence of true liver fibrosis. Infected liver had numerous MAs (Fig. 2f). MAs occurred as focal and large accumulation of macrophages (see further) laden with brownish pigments (melanin, chromolipoids, hemosiderin) within the thickness of the granulomas as well as scattered in the parenchyma (Fig. 2e, f). Furthermore, the presence of amorphous proteinaceous amphoterous faintly PAS-positive material, was detected among the connective fibres. Sinusoids dilation, liver hydropic degeneration, and occurrence of brownish pigments (mainly hemosiderin and, to a lesser extent, lipofuscin) were visible inside hepatocytes in parasitized liver (Fig. 2g).
Ultrastructural observations revealed the features of the cell types in each layer of the granuloma (Fig. 3a). The inner layer appeared darker (Fig. 3b, c) than the middle and outer layer of granulomas. The innermost layer of cells surrounding the nematode larvae was composed of elongated transformed macrophages, namely epithelioid cells (Fig. 3a-d). Their nuclei were rich in euchromatin and their cytoplasm contained many filaments, free ribosomes and swollen mitochondria. Numerous desmosomes between epithelioid cells (Fig. 3c, d) and some interdigitations between these cells were noted (Fig. 3d). In some instances, the epithelioid cells displayed a foamy appearance (Fig. 3b).
Figure 4a shows the outer layer of the granuloma with numerous collagenous fibres and some fibroblasts. In the middle layer, numerous granular cells were noticed (Fig. 4b) encircling the epithelioid corona. They contained numerous polymorphic dense granules that displaced the nucleus to the periphery (Fig. 4c) and were identified as MCs. The cytoplasm typically contained two to three mitochondria as well as several electron-dense granules (Fig. 4b, c). Frequently high numbers of MCs increased the thickness of the middle layer (Fig. 4b). Degranulation of the MCs was observed in many granulomas near the nematode larva. Consistent with this degranulation, the matrix of the granules had an extensively reticulated aspect (not shown). Another type of a granular cell, the neutrophil, was found scattered among the blood cells in sinusoid lumen (Fig. 4d), as well as in the parenchymal interstitium. The neutrophils contained smaller granules than those of MCs. These granules were rod-shaped and possessed an elongated, electron dense, lamellar core (not shown).
With reference to the rodlet cells (RCs), their number was low and they were occasionally observed in the epithelium of the biliary ducts and rarely associated with sinusoids. In a few infected livers RCs also occurred in the parenchymal interstitium, near the encysted larva. MAs associated with the nematode larvae consisted of groups of large oval to round cells (Fig. 4e) with eccentric polar nuclei with marked peripheral accumulations of chromatin. The cytoplasm of these cells at low magnification appeared partially vacuolated and foamy, and contained inclusions of differing electron-densities (not shown).
In infected livers, hepatocytes appeared as large polyhedral cells (Fig. 4f), with large and pale euchromatic nuclei, prominent nucleoli, partial enlargement of the rough endoplasmic reticulum cisternae, mitochondria dilation and focal vacuolisation (not shown). Focal cytoplasm rarefaction was also appreciable. The histological and ultrastructural liver pattern was suggestive of slight to mild hepatocyte hydropic degeneration.
The nematode Brevimulticaecum sp. has been reported in several freshwater fish species (e.g. G. inaequalabiatus) in the Pantanal wetland in Barzil . All internal organs of tuvira were infected with third larval stage of Brevimulticaecum sp. However the very high intensity of nematode infection in liver induced us to focus on this organ in order to accurately assess the damage to hepatic tissue.
Nematode parasites harm their host in different ways, such as causing mechanical injury [35, 36], atrophy of tissues, impairment of host fecundity , and pathogenecity of liver [9, 13, 17]. Parasitic helminths in natural habitats can drastically reduce their host fitness, and accordingly the hosts have evolved powerful counter-measures to control infection . It is reasonable to concur with the statement of Secombes & Chappell  and Franke et al.  that the successful infection of helminths largely depends on their capacity to evade and/or manipulate the generally efficient immune system of hosts. In recent years there has been a renaissance in the study of fish immune responses [27, 41–43], which significantly expanded our knowledge of the evolution and diversification of the vertebrate immune system [44, 45]. Innate immunity in teleosts relies on a range of cell types . Below we will examine in turn each immune cell type involved in the response of tuvira liver to Brevimulticaecum sp. larvae.
MCs exist in all classes of vertebrates, sharing both a similar morphology and, most likely, function . MCs are motile [25, 48] and are often strategically positioned at perivascular sites to regulate inflammation, to encounter invading organisms and to orchestrate a response [27, 42, 48–51]. MCs degranulate in response to a variety of pathogens [50, 52] and known degranulating agents [42, 53]. Degranulation of fish MCs close to the tegument of helminths in intestine and other organs was reported in Dezfuli et al. [50, 54]. In the present study degranulation of MCs in close proximity to the cuticle of Brevimulticaecum sp. was observed in numerous granulomas. MCs play an important role in responding to inflammation  and their numbers increase as a consequence of helminth infection in fish intestine [20, 27, 55] as well as in parasitized liver [13, 22, 56]. Numerous MCs were noticed to be in close contact with capillaries and the outer layer of the endothelia as well as within the lumen of the blood vessels in an infected organ [27, 57, 58]. Similar findings were found in liver and pancreas of Phoxinus phoxinus infected with larvae of the nematode Raphidascaris acus , consistent with G. inaequilabiatus liver harbouring Brevimulticaecum sp. larvae observed here. MCs are involved in the fibrotic process and in tissue remodelling [22, 55, 59]. The results of the current study suggest that Brevimulticaecum sp. larva in the tuvira liver preferentially induces the recruitment of MCs, fibroblasts and other immune cells (e.g. macrophages and epithelioid cells) to sites of infection. Moreover, we believe that MCs association with fibroblasts and macrophages may mediate liver remodelling/repair after extensive tissue injury caused by the nematode larva.
Phagocytosis is a well-conserved innate defense mechanism with phagocytes contributing to both pro-inflammatory and anti-inflammatory (resolution) responses at infectious foci [52, 60, 61]. Two major professional phagocyte populations have been described in fish: granulocytes (particularly neutrophils) and mononuclear phagocytes (circulating monocytes and tissue macrophages) [46, 62]. Neutrophils have an important role in the inflammatory process, especially during the period of initial pathogen challenge, migrating from the blood to accumulate at the site of injury or parasitic infection [20, 29, 30, 46, 54]. As mentioned in the previous section, neutrophils were observed in the parenchyma, hepatic sinusoid lumen, and/or interstitium around the capillary in infected tuvira liver. Surprisingly, no neutrophils were observed within the thickness of the granuloma nor in close proximity to the Brevimulticaecum sp. cuticle. In contrast, neutrophils were observed within the capsule surrounding the larva of R. acus that had infected P. phoxinus liver .
Macrophages have emerged as an essential cell type in all vertebrates, endowed with a panoply of capacities [63, 64]. Within an inflammatory site, macrophages are exposed to both pro-inflammatory stimuli and dying cells . Fish macrophages contain different types of pigments including melanin, chromolipoids and hemosiderin [46, 65], consequently, these groups of cells are named macrophage aggregates (MAs) or melano-macrophage centres [28, 66]. MAs may be found within tissue encapsulating many foreign bodies and parasites [20, 66, 67]. MAs functions have been reported to include the focal destruction, detoxification and recycling of endogenous and exogenous materials [68, 69]. Accordingly, MAs are involved against helminth infection [20, 22, 28, 65]. In infected liver of tuvira where numerous MAs were observed there was no recognizable distribution pattern, and in several cases MAs were found within the thickness of the granuloma wall and occasionally within the inner layer and very close to the larval body. Despite the occurrence of numerous neutrophils and MAs in parasitized liver we do not have direct evidence that these phagocytes killed the larva.
The inner layer of the capsule which surrounds Brevimulticaecum sp. larva was formed by epithelioid cells. These cells are so-named because of their morphological similarity to epithelial cells, and indeed are considered differentiated, transformed macrophages that form with persistent inflammatory stimulation [70, 71]. The formation of epithelioid cells in fish is known to occur from a variety of insults and their origin from macrophages was observed in vitro . The transition from metabolically active cells (i.e. macrophages and, to a lesser extent, epithelioid cells) appears to be very interesting aspect of liver response to form a structural sequestering element.
Only occasional RCs were present within the epithelium of the bile ducts of tuvira liver infected with nematode larvae. Data on numerous fish-helminth systems suggest that RCs represent an inflammatory cell type closely linked to other piscine immune cells (e.g. MCs and epithelioid cells) [13, 20, 25, 27, 31].
Some studies on cod liver from the Baltic Sea revealed a remarkable increase of up to 100 % in the prevalence of infection with nematodes [11, 73]. It was suggested that high infection of cod livers by parasites is associated with the successful re-introduction of grey seals (definitive hosts) in the Baltic Sea . The present study also noted a high prevalence of infection (95 %) with Brevimulticaecum sp. larva in the liver of tuvira. This fish is one of the most preferred preys for Caiman yacare in the study area. This crocodilian acts as a definitive host for several helminth species (e.g. Brevimulticaecum sp.)  and in the past was extensively harvested for its skin, illegally through direct hunting, and legally through ranching and collecting wild eggs , but in the last decade is considered a protected species . Similarly to the grey seals of the Baltic Sea, it is reasonable to presume that high numbers of C. yacare in the Pantanal Region ensure to keep very high the prevalence of Brevimulticaecum sp. in the liver of fish paratenic host (e.g. tuvira).
The present study utilized histopathological and ultrastructural assays to provide evidence that pathobiology relies entirely on a focal encapsulating reaction. In heavily infected livers most of the organ is occupied by the encysted parasites and associated enveloping granulomas. However the less extensive regions of uninfected parenchyma were relatively free of immune cells, without fibrosis and showed only slight to mild structural damage to hepatocytes. In other host-nematode systems, the encircling reaction closely resembled that described above for tuvira, although the liver status may differ particularly close to the inflammatory foci (see [13, 76]). Despite the high prevalence and intensity of infection of Brevimulticaecum sp. in tuvira there appears to be little risk of decline of the fish population, presumably thanks to the balance between parasite damage, host defence response and liver compensatory properties.
Alcian blue/periodic acid Schiff
Periodic acid Schiff
Transmission electron microscopy
Vieira KRI, Vicentin W, Paiva F, Pozo CF, Borges FA, Adriano EA, et al. Brevimulticaecum sp. (Nematoda: Heterocheilidae) larvae parasitic in freshwater fish in the Pantanal wetland, Brazil. Vet Parasitol. 2010;172:350–4.
Isaac A, Guidelli GM, Franca JG, Pavanelli GC. Composicao e estrutura das infracomunidades endoparasitarias de Gymnotus spp. (Pisces: Gymnotidae) do rio Baia, Mato Grosso do Sul, Brasil. Acta Scient Biol Sci. 2004;26:453–62.
Catto JB, Amato FFR. Helminth community structure of the Caiman crocodilus yacare in the Brazilian Pantanal. Rev Bras Parasitol Vet. 1994;3:109–18.
Moravec F, Kaiser H. Brevimulticaecum sp. larvae (Nematoda: Anisakidae) from the frog Hyla minuta Peters in Trinidad. J Parasitol. 1994;80:154–6.
Goldberg SR, Bursey CR. Helminths of two species of frogs, Lithobates taylori and Lithobates vaillanti (Ranidae), from Costa Rica. Car J Sci. 2007;43:65–72.
Cardoso AM, de Souza AJ, Menezes RC, Pereira WL, Tortelly R. Gastric lesions in free-ranging black caimans (Melanosuchus niger) associated with Brevimulticaecum species. Vet Pathol. 2012;50:582–4.
Moravec F. Parasitic nematodes of Freshwater Fishes of Europe. 2nd ed. Prague: Academia; 2013.
Abollo E, Gestal C, Pascual S. Anisakis infestation in marine fish and cephalopods from Galician waters: an updated perspective. Parasitol Res. 2001;87:492–9.
Dezfuli BS, Pironi F, Shinn AP, Manera M, Giari L. Histopathology and ultrastructure of Platichthys flesus naturally infected with Anisakis simplex s.l. larvae (Nematoda: Anisakidae). J Parasitol. 2007;93:1416–23.
Skov J, Kania PW, Olsen MM, Lauridsen JH, Buchmann K. Nematode infections of maricultured and wild fishes in Danish waters. A comparative study. Aquaculture. 2009;298:24–8.
Mehrdana F, Bahlool QZ, Skov J, Marana MH, Sindberg D, Mundeling M, et al. Occurrence of zoonotic nematodes Pseudoterranova decipiens, Contracaecum osculatum and Anisakis simplex in cod (Gadus morhua) from the Baltic Sea. Vet Parasitol. 2014;205:581–7.
Horbowy J, Podolska M, Nadolna-Altyn K. Increasing occurrence of anisakid nematodes in the liver of cod (Gadus morhua) from the Baltic Sea: Does infection affect the condition and mortality of fish. Fisheries Res. 2016;179:98–103.
Dezfuli BS, Manera M, Giari L. Immune response to nematode larvae in the liver and pancreas of minnow, Phoxinus phoxinus (L.). J Fish Dis. 2009;32:383–90.
Dezfuli BS, Manera M, Lorenzoni M, Pironi F, Shinn AP, Giari L. Histopathology and the inflammatory response of European perch, Perca fluviatilis muscle infected with Eustrongylides sp. (Nematoda). Parasit Vectors. 2015;8:227.
Fujimoto RY, dos Anjos ECS, Ramos FM, Martins ML. Seasonality of nematode larvae in Iguanodectes spilurus (Characidae) an ornamental fish from northeastern Para, Brazil. Acta Amazon. 2013;43:511–6.
Emde S, Rueckert S, Kochmann J, Knopf K, Sures B, Klimpel S. Nematode eel parasite found inside acanthocephalan cysts - a “Trojan horse” strategy? Parasit Vectors. 2014;7:504.
Ventura AS, Ishikawa MM, de Araujo Gabriel AM, Silbiger HLN, Cavichiolo F, Takemoto RM. Histopathology from liver of tuvira (Gymnotus spp.) parasitized by larvae of nematodes. Ciênc Rural. 2016;46:1233–9.
Farias IP, Marioni B, Verdade LM, Bassetti L, Coutinho ME, de Mendonça SHST, et al. Avaliação do risco de extinção do jacaré-do-pantanal Caiman yacare (Daudin, 1802) no Brasil. Biodiversid Brasil. 2013;3:21–30.
Brinker A, Hamers R. Evidence for negative impact of plerocercoid infection of Triaenophorus nodulosus on Perca fluviatilis L. stock in Upper Lake Constance, a water body undergoing rapid reoligotrophication. J Fish Biol. 2007;71:129–47.
Dezfuli BS, Lui A, Pironi F, Manera M, Shinn AP, Lorenzoni M. Cell types and structures involved in tench, Tinca tinca (L.), defence mechanisms against a systemic digenean infection. J Fish Dis. 2013;36:577–85.
Hoffmann RW, Meder J, Klein M, Osterkorn K, Negele RD. Studies on lesions caused by plerocercoids of Triaenophorus nodulosus in some fish of an alpine lake, the Koenigssee. J Fish Biol. 1986;28:701–12.
Dezfuli BS, Manera M, Giari L. Ultrastructural assessment of granulomas in the liver of perch (Perca fluviatilis) infected by tapeworm. J Comp Pathol. 2015;152:97–102.
Haarder S, Kania PW, Galatius A, Buchmann K. Increased Contracaecum osculatum infection in Baltic cod (Gadus morhua) livers (1982–2012) associated with increasing grey seal (Halichoerus gryphus) populations. J Wildlife Dis. 2013;50:537–43.
Makepeace BL, Martin C, Turner JD, Specht S. Granulocytes in helminth infection - who is calling the shots? Curr Med Chem. 2012;19:1567–86.
Reite OB, Evensen Ø. Inflammatory cells of teleostean fish: a review focusing on mast cells/eosinophilic granule cells and rodlet cells. Fish Shellfish Immunol. 2006;20:192–208.
Buchmann K. Evolution of innate immunity: clues from invertebrates via fish to mammals. Front Immun. 2014;5:459.
Dezfuli BS, Bosi G, DePasquale JA, Manera M, Giari L. Fish innate immunity against intestinal helminths. Fish Shellfish Immunol. 2016;50:274–87.
Agius C, Roberts RJ. Melano-macrophage centres and their role in fish pathology. J Fish Dis. 2003;26:499–509.
Havixbeck JJ, Barreda DR. Neutrophil development, migration, and function in teleost fish. Biology. 2015;4:715–34.
Havixbeck JJ, Rieger AM, Wong ME, Hodgkinson JW, Barreda DR. Neutrophil contributions to the induction and regulation of the acute inflammatory response in teleost fish. J Leukoc Biol. 2016;99:241–52.
Manera M, Dezfuli BS. Rodlet cells in teleosts: a new insight into their nature and functions. J Fish Biol. 2004;65:597–619.
Feist SW, Longshaw M. Histopathology of fish parasite infections - importance for populations. J Fish Biol. 2008;73:2143–60.
Triebskorn R, Bohmer J, Braunbeck T, Honnen W, Kohler H-R, Lehmann R, et al. The project VALIMAR (VALIdation of bioMARkers for the assessment of small stream pollution): objectives, experimental design, summary of results, and recommendations for the application of biomarkers in risk assessment. J Aquat Ecos Stress Recovery. 2001;8:161–78.
Moravec F, Prouza A, Royero R. Some nematodes of freshwater fishes in Venezuela. Folia Parasitol. 1997;44:33–47.
Abdelmonem AA, Metwally MM, Hussein HS, Elsheikha HM. Gross and microscopic pathological changes associated with parasitic infection in European eel (Anguilla anguilla, Linnaeus 1758). Parasitol Res. 2010;106:463–9.
Santoro M, Mattiucci S, Work T, Cimmaruta R, Nardi V, Ciprini P, et al. Parasitic infection by larval helminths in Antarctic fishes: pathological changes and impact on the host body condition index. Dis Aquat Organ. 2013;105:139–48.
Chavez RA, Oliva ME. Philometra chilensis (Nematoda, Philometridae) affects the fecundity of the red cusk-eel, Genypterus chilensis (Guichenot) (Pisces, Ophidiidae) in Chile. Acta Parasitol. 2011;56:236–7.
Summers K, McKeon S, Sellars J, Keusenkothen M, Morris J, Gloeckner D, et al. Parasitic exploitation as an engine of diversity. Biol Rev. 2003;78:639–75.
Secombes CJ, Chappell LH. Fish immune responses to experimental and natural infection with helminth parasites. Annu Rev Fish Dis. 1996;6:167–77.
Franke F, Rahn AK, Dittmar J, Erin N, Rieger JK, Haase D, et al. In vitro leukocyte response of three-spined sticklebacks (Gasterosteus aculeatus) to helminth parasite antigens. Fish Shellfish Immunol. 2014;36:130–40.
Brugman S. The zebrafish as a model to study intestinal inflammation. Dev Comp Immunol. 2016. doi:10.1016/j.dci.2016.02.020.
Galindo-Villegas J, Garcia-Garcia E, Mulero V. Role of histamine in the regulation of intestinal immunity in fish. Dev Comp Immunol. 2016. doi:10.1016/j.dci.2016.02.013.
Tafalla C, Leal E, Yamaguchi T, Fischer U. T cell immunity in the teleost digestive tract. Dev Comp Immunol. 2016. doi:10.1016/j.dci.2016.02.019.
Rauta PR, Nayak B, Das S. Immune system and immune responses in fish and their role in comparative immunity study: a model for higher organisms. Immunol Lett. 2012;148:23–33.
Buchmann K, Kania P. Emerging Pseudoterranova decipiens (Krabbe, 1878) problems in Baltic cod, Gadus morhua L., associated with grey seal colonization of spawning grounds. J Fish Dis. 2012;35:861–6.
Secombes CJ, Ellis AE. The Immunology of Teleosts. In: Roberts RJ, editor. Fish Pathology. 4th ed. Chicester: Blackwell Publishing; 2012. p. 144–66.
Mulero I, Sepulcre MP, Meseguer J, Garcia-Ayala A, Mulero V. Histamine is stored in mast cells of most evolutionarily advanced fish and regulates the fish inflammatory response. Proc Natl Acad Sci U S A. 2007;104:19434–9.
Dezfuli BS, Giari L. Mast cells in the gills and intestines of naturally infected fish: evidence of migration and degranulation. J Fish Dis. 2008;31:845–52.
St. John AL, Abraham SN. Innate immunity and its regulation by mast cells. J Immunol. 2013;190:4458–63.
Dezfuli BS, Bo T, Lorenzoni M, Shinn AP, Giari L. Fine structure and cellular responses at the host-parasite interface in a range of fish-helminth systems. Vet Parasitol. 2015;208:272–9.
Reber LL, Sibilano R, Mukai K, Galli SJ. Potential effector and immunoregulatory functions of mast cells in mucosal immunity. Mucosal Immunol. 2015;8:444–63.
Ellis AE. Innate host defense mechanisms of fish against viruses and bacteria. Dev Comp Immunol. 2001;25:827–39.
Manera M, Giammarino A, Borreca C, Giari L, Dezfuli BS. Degranulation of mast cells due to compound 48/80 induces concentration-dependent intestinal contraction in rainbow trout (Oncorhynchus mykiss Walbaum) ex vivo. J Exp Zool Part A. 2011;315A:447–57.
Dezfuli BS, Giari L, Squerzanti S, Lui A, Lorenzoni M, Sakalli S, Shinn AP. Histological damage and inflammatory response elicited by Monobothrium wageneri (Cestoda) in the intestine of Tinca tinca (Cyprinidae). Parasit Vectors. 2011;4:225.
Dezfuli BS, Giovinazzo G, Lui A, Giari L. Inflammatory response to Dentitruncus truttae (Acanthocephala) in the intestine of brown trout. Fish Shellfish Immunol. 2008;24:724–33.
Dezfuli BS, Giari L, Lorenzoni M, Manera M, Noga EJ. Perch liver reaction to Triaenophorus nodulosus plerocercoids with an emphasis on piscidins 3, 4 and proliferative cell nuclear antigen (PCNA) expression. Vet Parasitol. 2014;200:104–10.
Dezfuli BS, Squerzanti S, Fabbri S, Castaldelli G, Giari L. Cellular response in semi-intensively cultured sea bream gills to Ergasilus sieboldi (Copepoda) with emphasis on the distribution, histochemistry and fine structure of mucous cells. Vet Parasitol. 2010;174:359–65.
Dezfuli BS, Lui A, Giari L, Pironi F, Manera M, Lorenzoni M, Noga EJ. Piscidins in the intestine of European perch, Perca fluviatilis, naturally infected with an enteric worm. Fish Shellfish Immunol. 2013;35:1539–46.
Rocha JS, Chiarini-Garcia H. Mast cell heterogeneity between two different species of Hoplias spp. (Characiformes: Erythrinidae): response to fixatives, anatomical distribution, histochemical contents and ultrastructural features. Fish Shellfish Immunol. 2007;22:218–29.
Rieger AM, Konowalchuk JD, Grayfer L, Katzenback BA, Havixbeck JJ, Kiemele MD, et al. Fish and mammalian phagocytes differentially regulate pro-inflammatory and homeostatic responses in vivo. PLoS One. 2012;7:e47070.
Grayfer L, Hodgkinson JW, Belosevic M. Antimicrobial responses of teleost phagocytes and innate immune evasion strategies of intracellular bacteria. Dev Comp Immunol. 2014;43:223–42.
Esteban MÁ, Cuesta A, Chaves-Pozo E, Meseguer J. Phagocytosis in teleosts. Implications of the new cells involved. Biology. 2015;4:907–22.
Forlenza M, Fink IR, Raes G, Wiegertjes GF. Heterogeneity of macrophage activation in fish. Dev Comp Immunol. 2011;35:1246–55.
Hodgkinson JW, Grayfer L, Belosevic M. Biology of bony fish macrophages. Biology. 2015;4:881–906.
Wolke RE. Piscine macrophage aggregates, a review. Ann Rev Fish Dis. 1992;2:91–108.
Ferguson HW. Systemic pathology of fish: a text and atlas of normal tissues in teleosts and their responses in disease. London: Scotian Press; 2006.
Gregori M, Miragliotta V, Leotta R, Cecchini S, Prearo M, Abramo F. Morphometric evaluation of interrenal gland and kidney macrophages aggregates in normal healthy rainbow trout (Oncorhynchus mykiss) and after bacterial challenge with Yersinia ruckeri. Vet Med Int. 2014;2014:210625.
Ellis AE. Antigen-trapping in the spleen and kidney of the plaice Pleuronectes platessa L. J Fish Dis. 1980;3:413–26.
Vigliano FA, Bermudez R, Quiroga MI, Nieto JM. Evidence for melano-macrophage centres of teleost as evolutionary precursors of germinal centres of higher vertebrates: an immunohistochemical study. Fish Shellfish Immunol. 2006;21:467–71.
Noga EJ, Dykstra MJ, Wright JF. Chronic inflammatory cell with epithelial cell characteristics in teleost fishes. Vet Pathol. 1989;26:429–37.
Gauthier DT, Vogelbein WK, Ottinger CA. Ultrastructure of Mycobacterium marinum granuloma in striped bass Morone saxatilis. Dis Aquat Org. 2004;62:121–32.
Secombes CJ. The nonspecific immune system: cellular defences. In: Iwama G, Nakanishi T, editors. The fish immune system: organism, pathogen, and environment. San Diego: San Diego Academic Press; 1996. p. 63–105.
Haarder S, Kania PW, Bahlool QZM, Buchmann K. Expression of immune relevant genes in rainbow trout following exposure to live Anisakis simplex larvae. Exp Parasitol. 2014;135:564–9.
Buchmann K. Fish immune responses against endoparasitic nematodes - experimental models. J Fish Dis. 2012;35:623–35.
Santos SA, Pinheiro MS, Andreotti R. Efeitos de diferentes dietas as naturais no desenvolvimento inicial de Caiman crocodilus yacare (Crocodilia Alligatoridae). Rev Soc Bras Zoot. 1993;22:406–12.
Dezfuli BS, Simoni E, Rossi R, Manera M. Rodlet cells and other inflammatory cells of Phoxinus phoxinus infected with Raphidascaris acus (Nematoda). Dis Aquat Organ. 2000;43:61–9.
This study was funded by the University of Ferrara to BSD (Grant number FAR 2015).
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The data supporting the conclusions of this article are included within the article.
BSD supervised the laboratory work and wrote the initial draft. CEF and GMG performed the field work. GC, MM, ML, SB and LG performed the laboratory work, collected and analysed the data. JAD intellectually supported the study and corrected the manuscript drafts. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
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Ethics approval and consent to participate
The study was approved by the regional ethical board at Federal University of Mato Grosso do Sul, Campo Grande, Brazil.
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Sayyaf Dezfuli, B., Fernandes, C.E., Galindo, G.M. et al. Nematode infection in liver of the fish Gymnotus inaequilabiatus (Gymnotiformes: Gymnotidae) from the Pantanal Region in Brazil: pathobiology and inflammatory response. Parasites Vectors 9, 473 (2016). https://doi.org/10.1186/s13071-016-1772-2
- Fish immune response
- Nematode larvae
- Hepatic granuloma