Nucleospora cyclopteri n. sp., an intranuclear microsporidian infecting wild lumpfish, Cyclopterus lumpus L., in Icelandic waters
Parasites & Vectors volume 6, Article number: 49 (2013)
Commercial fisheries of lumpfish Cyclopterus lumpus have been carried out in Iceland for centuries. Traditionally the most valuable part is the eggs which are harvested for use as a caviar substitute.
Previously reported parasitic infections from lumpfish include an undescribed intranuclear microsporidian associated with abnormal kidneys and mortalities in captive lumpfish in Canada. During Icelandic lumpfish fisheries in spring 2011, extensive enlargements to the kidneys were observed in some fish during processing. The aim of this study was to identify the pathogen responsible for these abnormalities.
Lumpfish from the Icelandic coast were examined for the causative agent of kidney enlargement. Fish were dissected and used in histological and molecular studies.
Lumpfish, with various grades of clinical signs, were observed at 12 of the 43 sites sampled around Iceland. From a total of 77 fish examined, 18 had clear clinical signs, the most prominent of which was an extensive enlargement and pallor of the kidneys. The histopathology of the most severely affected fish consisted of extensive degeneration and necrosis of kidney tubules and vacuolar degeneration of the haematopoietic tissue. Intranuclear microsporidians were detected in all organs examined in fish with prominent clinical signs and most organs of apparently healthy fish using the new PCR and histological examination. One or multiple uniformly oval shaped spores measuring 3.12 ± 0.15 × 1.30 ± 0.12 μm were observed in the nucleus of affected lymphocytes and lymphocyte precursor cells. DNA sequencing provided a ribosomal DNA sequence that was strongly supported in phylogenetic analyses in a clade containing other microsporidian parasites from the Enterocytozoonidae, showing highest similarity to the intranuclear microsporidian Nucleospora salmonis.
Intranuclear microsporidian infections are common in wild caught lumpfish from around the Icelandic coast. Infections can cause severe clinical signs and extensive histopathological changes, but are also present, at lower levels, in fish that do not show clinical signs. Some common features exist with the intranuclear microsporidian previously reported from captive Canadian lumpfish, but DNA sequence data is required from Canadian fish to confirm conspecificity.
Based on phylogenetic analysis and the intranuclear location of the parasite, the name Nucleospora cyclopteri n. sp. is proposed.
Lumpfish, or lumpsucker, Cyclopterus lumpus, L. 1758, are distributed throughout the North Atlantic Ocean and are a commercially important species in Greenland, Iceland, Norway, and Canada. Female lumpfish are targeted during a coastal spring fishery in Iceland as their valuable eggs are harvested for use as a caviar substitute. Juvenile lumpfish emerge from egg clutches in the spring and spend their first year of life among weed clumps in bays and fjords until they move offshore. Females and males return to the coastal regions during the spring and summer seasons to spawn[1, 2].
Commercial fisheries of lumpfish in Iceland have been carried out for centuries and the average annual catch the last 30 years has been around 6200 t. Until recently, only the lumpfish eggs were harvested due to a lack of markets for the fish muscle. However, over the last two years this has changed due to alterations in fishing regulations that now require fisherman to bring all lumpfish caught to shore for full processing. During the processing of landed lumpfish in spring 2011, it was noticed that some fish had an extensive enlargement of the kidneys.
Captive lumpfish from Eastern Canada have previously been reported with marked pathological changes observed in the kidneys. On that occasion, the pathogen responsible for the condition was an undescribed intranuclear microsporidian parasite that caused the pathology observed and also led to chronic mortalities of the tank-reared fish. Microsporidians were formerly considered protists but are now classified as fungi. They are spore forming organisms known to infect numerous fish species which include species with intranuclear sites of infection and are also found as hyperparasites.
In the present study, we perform histological and molecular studies on Icelandic lumpfish and describe a novel microsporidian, Nucleospora cyclopteri n. sp.
Research material and macroscopic examination
The initial research material was sampled in July 2011 in Haganesvik in Skagafjordur in the northern part of Iceland (66° 4'34.90"N, 19° 9'22.28"W). Three fish with clinical signs in the kidney, observed by local fishermen, were sent for examination to determine an aetiology for the condition. Wet mounts of fresh kidney tissue were examined at 400× and 1000× magnification with a compound microscope and kidney samples fixed in 10% buffered formalin for histological examination and in 95% ethanol for DNA analysis.
For further examination of the nature of the disease, 10 spawning female lumpfish (length 40–48 cm) were sampled from Húnaflói Bay in northern Iceland (66° 3'37. 29"N, 20°28'18. 31"W) aboard a lumpfish vessel in April 2012. Five were selected as they showed clearly visible clinical signs in the kidney and five were selected as they appeared to be healthy with no obvious clinical signs. Immediately post mortem, each fish was dissected using sterile technique and parts of the kidneys, spleen, heart, gills, skin and eggs were fixed in 10% formalin for histological examination and 95% ethanol for molecular analysis.
During the annual Icelandic groundfish survey, performed by the Marine Research Institute in Iceland in late February and early March 2012, 77 lumpfish (68 females; 33–47 cm, 9 males; 26–32 cm) from 43 sites around Iceland were randomly selected and screened for clinical signs in kidneys comparable to those formerly observed. The number of fish examined from each station ranged from a single one to nine fish.
Formalin fixed samples were embedded in paraffin wax, sectioned (4 μm) and prepared for histological examination according to routine protocols. The sections were stained with either Haematoxylin & Eosin (HE) or Giemsa and screened for pathogens and histopathological changes. Furthermore, histological slides were stained with a chitin-specific stain, Calcofluor white M3R (Sigma-Aldrich), to look specifically for microsporidian spores. To evaluate the distribution and intensity of microsporidian spores in the host’s tissues, the slides were examined using a compound microscope at 400× magnification. Infections in each organ were graded as follows: (−ve) = no spores detected; (*) = light infection; less than 10 spores or a cluster of spores (inside the same cell) occasionally seen; (**) = moderate infection; spores seen in most microscopic fields, their number ranging from 10 to 100; (***) = massive infection; more than 100 spores seen in all microscopic fields. To identify with more certainty which cell types were affected, imprints of kidney were taken from fish with extensive clinical signs. These samples were air-dried, fixed in methanol and stained with Calcofluor white M3R and/or Giemsa. All tissue samples were examined at high magnification and photographs taken using a Leica DMLB compound microscope equipped with a digital camera (Leica DC300F).
DNA sequencing and phylogenetic analyses
Dissected ethanol-preserved kidney tissues from three fish suspected to be infected with the microsporidian, and the ten fish for microsporidian screening, were further cut with a scalpel blade and approximately 25 mg of tissue digested at 56°C in tissue lysis buffer containing 100 μg/mL proteinase K until dissolved. DNA was extracted using a GeneMATRIX DNA extraction kit (EURx Poland) following the tissue protocol and 10 ng used as template DNA for PCRs. Small subunit (SSU), internal transcribed spacer (ITS) and partial large subunit (LSU) regions of the rRNA gene were amplified using previously described microsporidian primers[10, 11]. An additional primer 870fwd 5′ tgcggcttaatttgactcaac and its complementary reverse primer 870rev were used with the forward and reverse primers to allow a sufficient overlap for sequence confirmation. PCRs were performed according to the original descriptions with the use of suitable negative controls. PCR products were run alongside a 100 bp DNA ladder on 1% agarose gels, pre-stained with 1× SYBR®-safe (Invitrogen Oregon USA), and visualised with a high performance UV transilluminator (UVP, Cambridge UK). Direct sequencing reactions were done using BigDyeTM Terminator Cycle Sequencing chemistry utilising the same primers. DNA sequencing was performed in both directions on all positive PCR products, of the expected sizes, and compared to sequences available in the GenBank databases using nucleotide-nucleotide BLAST searches to verify a microsporidian origin. The contiguous sequence was obtained manually using CLUSTAL-X and BioEdit. CLUSTAL X was used for the initial sequence alignments, with the settings for gap opening/extension penalties being adjusted manually to achieve optimum alignments, and manually edited using the BioEdit sequence alignment editor. Percentage divergence matrices were constructed in CLUSTAL X using the neighbour-joining method based on the Kimura 2-parameter model. Microsporidia from the Enterocytozoonidae are typically assigned as new species or given generic status partly based on SSU rDNA sequence data. Therefore, alignment files of 16 taxa, representative of microsporidia from the family Enterocytozoonidae and related basal taxa, consisting of 1,269 characters of SSU sequence data were used in the phylogenetic analyses.
Phylogenetic analyses were performed using the maximum likelihood methodology in PhyML with the general time-reversible substitution model selected and 1000 bootstrap repeats, and Bayesian inference (BI) analysis using MrBayes v. 3.0. For the BI analysis, models of nucleotide substitution were first evaluated for the alignment using MrModeltest v. 2.2. The most parameter-rich evolutionary model based on the AIC was the general time-reversible, GTR + I + G model of evolution. Therefore, the settings used for the analysis were nst = 6, with the gamma-distributed rate variation across sites and a proportion of invariable sites (rates = invgamma). The priors on state frequency were left at the default setting (Prset statefreqpr = dirichlet (1, 1, 1, 1). Posterior probability distributions were generated using the Markov Chain Monte Carlo (MCMC) method with four chains being run simultaneously for 1000.000 generations. Burn in was set at 2.500 and trees were sampled every 100 generations making a total of 7.500 trees used to compile the majority rule consensus trees.
Development of nested PCR
DNA extracted from the three fish initially sampled was used to develop the nested PCR. Four controls were used in the assay development to monitor for contamination: a template blank containing no DNA, a negative fish tissue, a positive sample for Desmozoon lepeophtherii, which was to be positive in the first round, but negative in the second round of the nested PCR and a positive control for N. cyclopteri from the initial DNA extractions in this study. The first pair of primers, LN1-fwd 5′ atcctaggatcaaggacgaag and LN1-rev 5′ aatgatatgcttaagttcagg were modified from those used by Freeman et al. and were designed to be semi-specific for microsporidians from the genus Nucleospora amplifying a 950 bp region of the SSU and ITS region. A second specific primer pair LN2-fwd 5′ ctgcttaatttgactcaacgc and LN2-rev 5′ tactgctcctcaaatagtatg targets a 590 bp region, within the first 950 bp amplicon, covering partial SSU and partial ITS regions of the gene, and used 1 μl of the PCR products from round one as a DNA template. Both sets of primers use the same PCR profile: initial denaturing for 4 min at 95°C followed by 35 cycles of: 94°C 30 s, 55°C 45 s, 72°C 1 min, with a terminal extension at 72°C for 7 min. PCR products were run alongside a 100 bp DNA ladder on 1% agarose gels, pre-stained with 1× SYBR®-safe (Invitrogen, Oregon USA), and visualised with a high performance UV transilluminator (UVP, Cambridge UK). Positive PCR bands from all fish (either first or second round PCR) were purified using a GeneMATRIX PCR clean up kit (EURx Poland) and sent for direct sequencing, in both directions, using the same primers from the positive amplifications.
In accordance with section 8.6 of the ICZN’s International Code of Zoological Nomenclature, details of the new species have been submitted to ZooBank with the life science identifier (LSID) zoobank.org:pub:2659C0D4-ADF1-44E5-A53A-C7507B64D0BC.
Clinical signs, distribution and prevalence of infected fish
The most prominent clinical signs were observed in the kidneys. The extent of clinical signs varied considerably between individual fish. Some had normally sized kidneys which had a patchy pallor compared to smooth and evenly red normal kidney (Figure 1a, b). Other fish had various degree of renomegaly and kidney pallor. In the most severe cases the kidneys were extensively and uniformly enlarged, had a whitish appearance and apparently little or no normal tissue visible (Figure 1c, d). Fish with noticeable renomegaly, occasionally showed other clinical signs such as exophthalmos and small lesions on the skin.
Lumpfish, with various grades of clinical signs in the kidney, were observed at 12 of the 43 sites when fish randomly collected aboard the bottom trawl survey were examined (Figure 2). Furthermore, of all the 77 fish examined, 18 had clinical signs, of which 17 were female and one was male. Mostly there was one fish at each station, however, in some cases, multiple fish from certain sites showed clinical signs, for example four of five fish sampled at one site and two of two sampled fish at another site.
No obvious histopathological changes were observed in fish showing no clinical signs (Figure 3a, b). Moderate to severe tissue changes were, however, observed in all fish showing clinical signs of disease, which were most prominent in the kidney. These changes were dominated by degeneration and necrosis of tubules (Figure 3c) and glomeruli. Many tubules contained protein cast and necrotic cell debris of the epithelial layer (Figure 3d), with subsequent collapse of those tubuli worst affected. Vacuolar degeneration of haematopoietic tissue cells was frequent and necrotic foci were observed with marked lymphocyte infiltration (Figure 4a, b, c). In the most severely infected fish, large areas of the kidney were almost totally necrotised, with massive numbers of microsporidian spores surrounded by necrotic cell debris. An inflammatory response with infiltration of lymphocytes was also evident in other organs such as the heart (Figure 4d).
Nucleospora cyclopteri and affected cells
Examination of the initial three lumpfish sampled from Haganesvik in Skagafjordur in July 2011, confirmed heavy microsporidian infections in their kidneys. Examination of wet mounts, revealed oval shaped microsporidian spores, their length ranging from 2.9–3.5 μm (mean ± stdev = 3.12 ± 0.15) and their width 1.1–1.5 μm (1.30 ± 0.12) (n = 30).
Affected cells had all morphological characteristics of lymphocytes and lymphocyte precursor cells. They were round shaped, 8–12 μm in diameter, had a large nucleus occupying most of the cell, a compact chromatin and a thin rim of basophilic cytoplasm which stained sky blue in Giemsa. The number of microsporidian spores inside a single cell nucleus ranged from 1 – 14 (Figure 5a-f).
The presence of Nucleospora cyclopteri in different host organs
Microsporidian spores were found in nine of the 10 female lumpfish sampled in April 2012 using fluorescence stained histological sections; four of the apparently healthy ones (fish 1–5) and all five that had clinical signs (fish 6–10). Infections were found in all organs examined in the fish with clinical signs; kidneys, spleen, gills and heart being most heavily infected but lighter infections in the skin and the ovary (Table 1). In the kidneys and the spleen the spores were distributed in the parenchyma (Figure 6a). In the heart, the spores were most commonly detected in the myocardium, however, in the heaviest infections they also extended into the epicardium. The gills were usually heavily infected with numerous spores seen; most frequently in the primary lamellae but extending somewhat into the secondary lamellae in severely infected fish (Figure 6b). Relatively few spores were seen in the skin and the ovary but some numbers of spores were normally detected in the dermal and epidermal layers of the skin and also in the ovarian stroma (Figure 6c, d). In the four apparently healthy, but infected fish, the infections were light and spores, or clusters of spores within the same cell nucleus, were occasionally detected in renal tissue, splenic tissue and the myocardium of the heart. No spores were detected in the skin, the gills or the ovary of these fish.
All five fish showing clinical signs of microsporidiosis (fish 6–10) were strongly positive using the first round of the PCR in one or more tissues (Table 1). Tissues that were consistently positive in round one were kidney and heart, followed by skin, gills and spleen. The eggs were not strongly positive in any of the five positive fish in round one. All weakly positive or negative tissues from round one were confirmed as positively infected using the second round PCR, except for the eggs in fish nine which remained negative. Fish with no clinical signs (fish 1–5) of infection were either negative or weakly positive in round one, with the exception of fish 3 that was positive in the heart and kidney tissues. All fish (1–5) were shown to be positive for the microsporidian in the second round of the PCR. Some positive PCR products from all ten fish were purified and sequenced to confirm the correct microsporidian sequence had been amplified.
DNA sequencing and phylogenetic analyses
A contiguous microsporidian DNA sequence of 1869 bp of the rRNA gene, including partial SSU (1182 bp), complete ITS region (361 bp) and partial LSU (326 bp), was generated from the three fish with abnormal kidneys from Haganesvik in Skagafjordur. There was no intraspecific variation found between sequences generated from the three different fish when sequencing the PCR product directly. In addition, partial rRNA gene sequences were obtained for the 10 fish used in the nested PCR. If the fish were positive in the first round of the PCR then those products were sequenced (950 bp), if positive in the second round then those products were sequenced (590 bp). No intraspecific differences between sequences were observed between any fish.
The sequence has been submitted to GenBank with the accession number [KC203457]. A BLAST search of the sequence in the databases revealed a 96% similarity to isolates of Nucleospora salmonis, an intranuclear microsporidian infecting salmonid fishes worldwide.
A percentage identity matrix generated for 11 related taxa within the Enterocytozoonidae demonstrates the genetic distances that might be expected at the species level for this group (Table 2). There is 99.1–99.84% similarity between different isolates of N. salmonis amplified from different host fish species. There is an 86.08% and 91.18% similarity between N. salmonis from Atlantic salmon and two unidentified Nucleospora sp., the similarity between N. cyclopteri and the same two Nucleospora spp. is 85.32 and 90.67% respectively. The genus Desmozoon is 87.32% and 87.13% similar to N. cyclopteri and N. salmonis from Atlantic salmon. Other more basal genera from the group, such as Hepatospora are more distantly related (Table 2).
Phylogenetic analyses, of the Enterocytozoonidae based on 1269 characters of aligned SSU rDNA sequence data, using maximum likelihood Bayesian methodologies produced congruent trees topologies (Figure 7). The sequence for N. cyclopteri was robustly supported in a clade that contained other intranuclear microsporidian parasites of fish from the genus Nucleospora.
Nucleospora cyclopteri is a common microsporidian parasite infecting lumpfish around Iceland. Fish with visible clinical signs, like those infected with N. cyclopteri, were found at 12 of 43 sites around the country. Although all fish were not screened for the microsporidian, the cause of the clinical signs observed is assumed to be N. cyclopteri as all other fish screened with equivalent signs were infected with this microsporidian. Even though the prevalence data are limited to a few fish examined at each sampling site, the geographic distribution is wide. It causes severe clinical signs and extensive histopathological changes.
This is the first report of intranuclear microsporidiosis in wild lumpfish, Cyclopterus lumpus. However, a microsporidian infection has previously been reported from lumpfish reared in a recirculation facility in Canada, which was associated with chronic fish mortalities. That paper describes the clinical, histopathological and ultrastructural features of an intranuclear microsporidian. Mullins et al. suggested that the lumpfish microsporidian they found belonged to the genus Enterocytozoon based on similarities to the previously described species Enterocytozoon bieneusi and E. salmonis (syn. Nucleospora salmonis), both with regard to morphology and the type of immune response, but they did not make a formal species description. The former species is a non-intranuclear intestinal parasite of humans and numerous higher vertebrates[22, 23], the latter is a well documented intranuclear microsporidian pathogen which has been identified in various salmonid species[24, 25] and also from Atlantic halibut, Hippoglossus hippoglossus.
Phylogenetic analyses (Figure 7) and a percentage identity matrix (Table 2) show that N. cyclopteri is most closely related to isolates of N. salmonis with an identity of approximately 96% to all isolates. Intraspecific variation of N. salmonis between four separate isolates, amplified from different host fish, is between 99.1–99.84% (Table 2), indicating that a similarity of 96% would represent a different species and not another isolate of N. salmonis. In addition to this, the spore size of 3.12 × 1.30 μm and evenly oval shape in N. cyclopteri is untypical for the family group that generally have smaller more ovoid to rounded spores with sizes recorded for Nucleospora spp. of 1.6 × 0.8 μm and 2.0 × 1.0 μm; Enterocytozoon spp. of 1.5 × 0.8 μm and 1.1 × 0.7 μm; Enterospora 1.3 × 0.7 μm and Desmozoon 2.84 × 1.83 μm.
Comparing the microsporidian infection described in this paper to the one from Canada, some similarities are evident; macroscopic clinical signs include renomegaly and exophthalmos, lymphocytes and lymphoblasts are the target cells in both cases and infections are detected in all organs examined, via vascular migration of infected cells. Other things are more difficult to compare, such as the histopathology and the morphology and size of the microsporidian spores. The histopathological description made by Mullins et al. is quite brief; mainly describing an infiltration of lymphocyte like cells, morphological features of the target cells and their presence in all organs examined, but no actual tissue damage associated with infections. Histopathological changes observed in the lumpfish in the present paper were in many cases considerable including extensive degeneration and necrosis of kidney tubules and vacuolar degeneration of the haematopoietic tissue. It seems that a lymphocytotsis or lymphoblastosis type of inflammatory reaction, with a subsequent prominent hyperplasia, and affected cells being lymphocytes or lymphocyte precursor cells, is a relatively common feature of intranuclear microsporidiosis[28–31]. Except for one fish, all the 13 fish, which where thoroughly examined in the present study, had either light subclinical infections or severe infection with considerable or extreme clinical signs. As the extent of the clinical signs of the fish examined by Mullins et al., such as renomegaly, is not obvious, it is possible that these fish had lighter infections and hence lacked severe histopathological changes, which might occur at later stages of infection in wild fish. Comparing the spore morphology observed in these two studies, the shape is very similar, i.e. uniformly oval and not tapered at one end, which is a common feature of some microsporidian spores. However, the spore size is considerably different, i.e. 2.1 μm x 1.0 μm in the previous study compared to a mean size of 3.12 μm x 1.30 μm in the present study. Mullins et al. made spore measurements using ultrathin sections on a TEM but fresh spores were used in the present study. Hence, the spores from the Canadian lumpfish had been fixed in glutaraldehyde and processed for TEM and might have shrunk during this procedure. Furthermore, when using ultrathin sections, one cannot be sure that the plane of section is through the entire length and width of the spore. Consequently, the spore size in these two studies is not suitable for direct comparison and fresh spores from Canadian lumpfish should be analysed. Although some similarities are apparent between the microsporidians described in these two studies, DNA sequence data is required from Canadian lumpfish to confirm their conspecificity.
Currently, the life cycle of Nucleospora cyclopteri and its route of infection/transmission is not known. However, many microsporidians infecting fish have a simple direct life cycle and no vector or intermediate host is required. This simple form of direct transmission between fish is known to occur in the congener Nucleospora salmonis, which is the closest known relative to N. cyclopteri in our phylogenetic analyses. Indeed, from our histology and PCR results, we found that the kidney and gills were very common sites of infection, indicating that these organs could be the sites for direct transmission to occur, being excreted from the kidney and entering another fish host via the gills.
Another close relative, and the robustly supported sister taxon in the phylogenetic tree, Desmozoon lepeophtherii, is a hyperparasite of the salmon louse Lepeophtheirus salmonis and also an intranuclear parasite of Atlantic salmon[27, 33, 34]. It is possible that multiple hosts or a complicated life cycle could occur in N. cyclopteri infections in lumpfish. Several things could support this: 1) According to Heuch et al. lumpfish are a preferred host for the parasitic copepod Caligus elongatus and might serve as a reservoir for caligid infections of other fish species. 2) One of the clinical signs detected in our study were small lesions on the skin similar to those caused by parasitic copepods. 3) Histological examination revealed microsporidian spores in the most outer layers of lumpfish skin. At present this remains speculative, and additional studies are needed to examine whether C. elongatus are infected with N. cyclopteri and how transmission of the parasite might take place. In the present study spores of N. cyclopteri were also found in close association with the eggs suggesting that spores may also be vertically transmitted. Some microsporidia that infect crustaceans are known to be transovarially (vertically) transmitted[36, 37] and some pathogens that enter the microphyle of the egg before its shell fully matures are known to cause bacterial infection such as Renibacterium salmoninarum. Screening larval lumpfish soon after hatching, using the nested PCR developed in this study, would be a simple method to check for the presence of vertical transmission as a route of infection for this microsporidian. It will become necessary to evaluate such routes of infection for important pathogens of lumpfish, in order to help limit their spread and impact in captive fish. Lumpfish are becoming increasingly more important for the aquaculture industry, being used as cleaner fish in Atlantic salmon cages for the removal of salmon lice. However, their culture is problematic as they are susceptible to numerous pathogens.
The extreme pathology seen in some fish, which looks highly unlikely to be reversible, raises the question whether infections could have an impact upon lumpfish populations. More complete data on prevalence and severity of infections, with regard to fish age, geographic distribution and time of year, are required to determine any potential mortality rates.
Phylum: Microsporidia (Balbiani, 1882)
Class: Microsporea (Levine & Corliss, 1963)
Order: Microsporida (Balbiani, 1882)
Family: Enterocytozoonidae (Cali & Owen, 1990)
Fresh spores are evenly oval in shape, length 2.9–3.5 μm width 1.1–1.5 μm, with two lines of symmetry being evenly rounded at both ends. Mature spores, numbering between 1–14, are found inside lymphocyte nuclei in haematopoietic and other tissues. SSU rDNA sequence data confirms a close association with other Nucleospora species and robustly places N. cyclopteri within the Enterocytozoonidae.
Type host: Atlantic lumpfish (Cyclopterus lumpus, L. 1758)
Location: Coastal waters of Iceland
Type location: Skagafjordur, northern Iceland (66° 4'34.90"N, 19° 9'22.28"W).
Site of infection: The nucleus of lymphocytes and lymphocyte precursor cells. Infected lymphocytes infiltrate haematopoietic tissues (kidney and spleen), heart myocardium, gills and skin.
Etymology: The specific name cyclopteri refers to the generic assignment of the host fish.
Type material: Two stained wet mount slides and two histological sections have been submitted to the collections of the Natural History Museum, London, and assigned the accession numbers: (kidney tissue) NHMUK 2013.1.15.1, (heart tissue) NHMUK 2013.1.15.2, (kidney imprint) NHMUK 2013.1.15.3, (kidney imprint) NHMUK 2013.1.15.4. DNA sequence data has been submitted to GenBank with the accession number [KC203457].
We have described a novel intranuclear microsporidian, Nucleospora cyclopteri, infecting the nuclei of lymphocyte and lymphocyte precursor cells in lumpfish Cyclopterus lumpus. Gross clinical signs of infection, notably severe inflammation of the kidney, were found at numerous locations around the Icelandic coast with a prevalence of 23% (18/77 fish). However, using the new nested PCR, infection rates were shown to be significantly higher and could reach 100%. Marked histopathological changes were evident in fish with clinical signs that are unlikely to be reversible, indicating that N. cyclopteri may have a negative impact on spawning lumpfish populations. Nucleospora cyclopteri is phylogenetically related to other intranuclear microsporidian parasites infecting marine fish and is robustly placed in the Enterocytozoonidae. Some features common to an intranuclear microsporidian previously reported from captive Canadian lumpfish are evident but DNA sequence data is required from Canadian lumpfish to confirm conspecificity.
Due to the importance of wild lumpfish fisheries in northern Atlantic countries, and their potential use as cleaner fish in Atlantic salmon farms, it is vital to evaluate this pathogen and its potential impact upon wild spawning stocks and captive fish.
Ingolfsson A, Kristjánsson BK: Diet of juvenile lumpsucker Cyclopterus lumpus (cyclopteridae) in floating seaweed: effects of ontogeny and prey availability. Copeia. 2002, 2: 472-476.
Jónsson G: Íslenskir fiskar (Icelandic fishes). 2003, Reykjavik: Fjölvaútgáfan
Thorsteinsson V: The ageing validation of the lumpsucker (Cyclopterus lumpus) and the age composition of the lumpsucker in Icelandic lumpsucker fisheries. [http://www.hafro.is/Bokasafn/Greinar/ices_1981_G58.pdf],
State of stocks 2011/2012 Prospects 2012/2013. 2012, Reykjavik: Marine Research Institute, [http://www.hafro.is/Astand/2012/Astandsskyrsla_hafrannsoknastofnunarinnar_2012_lokaprentun.pdf],
Mullins JE, Powell M, Speare DJ, Cawthorn R: An intranuclear microsporidian in lumpfish Cyclopterus lumpus. Dis Aquat Org. 1994, 20: 7-13.
Capella-Gutiérrez S, Marcet-Houben M, Gabaldón T: Phylogenomics supports microsporidia as the earliest diverging clade of sequenced fungi. BMC Biol. 2012, 10: 47-10.1186/1741-7007-10-47.
Lom J, Dyková I: Microsporidia (Phylum Microspora). Protozoan parasites of fishes. Development in Aquaculture and Fisheries Science. 1992, Amsterdam: Elsevier, 125-157.
Freeman MA, Bell AS, Sommerville C: A hyperparasitic microsporidian infecting the salmon louse, Lepeophtheirus salmonis: an rDNA-based molecular phylogenetic study. J Fish Dis. 2003, 26: 667-676. 10.1046/j.1365-2761.2003.00498.x.
Palsson OK, Schopka SA, Stefansson G, Steinarsson BA: Icelandic groundfish survey data used to improve precision in stock assessments. J Northw Atl Fish Sci. 1989, 9: 53-72.
Vossbrinck CR, Baker MD, Didier ES, Debrunner-Vossbrinck BA, Shadduck JA: Ribosomal DNA sequences of Encephalitozoon hellem and Encephalitozoon cuniculi: species identification and phylogenetic construction. J Euk Microbiol. 1993, 40: 354-362. 10.1111/j.1550-7408.1993.tb04928.x.
Pomport-Castillon C, Romestand B, De Jonckheere JF: Identification and phylogenetic relationship of microsporidia by riboprinting. J Euk Microbiol. 1997, 44: 540-544.
Freeman MA, Yokoyama H, Ogawa K: A microsporidian parasite of the genus Spraguea in the nervous tissues of the Japanese anglerfish Lophius litulon. Folia Parasitol. 2004, 51: 167-176.
Zhang Z, Schwartz S, Wagner L, Miller W: A greedy algorithm for aligning DNA sequences. J Comput Biol. 2000, 7: 203-214. 10.1089/10665270050081478.
Thompson JD, Gibson TJ, Plewniak F, Jeanmougin F, Higgins DG: The CLUSTAL-X windows interface: flexible strategies for multiple sequence alignment aided by quality analysis tools. Nucl Acids Res. 1997, 24: 4876-4882.
Hall TA: BioEdit: a user-friendly biological sequence alignment editor and analysis program for Windows 95/98/NT. Nucleic Acids Symp Ser. 1999, 41: 95-98.
Saitou N, Nei M: The neighbour-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol. 1987, 4: 406-425.
Stentiford GD, Bateman KS, Dubuffet A, Chambers E, Stone DM: Hepatospora eriocheir (Wang and Chen, 2007) gen. et comb. nov. infecting invasive Chinese mitten crabs (Eriocheir sinensis) in Europe. J Invertebr Pathol. 2011, 108: 156-166. 10.1016/j.jip.2011.07.008.
Guindon S, Dufayard JF, Lefort V, Anisimov M, Hordijk W, Gascuel O: New algorithms and methods to estimate maximum-likelihood phylogenies: assessing the performance of PhyML 3.0. Syst Biol. 2010, 59: 307-321. 10.1093/sysbio/syq010.
Ronquist F, Huelsenbeck JP, MrBayes 3: Bayesian phylogenetic inference under mixed models. Bioinformatics. 2003, 19: 1572-1574. 10.1093/bioinformatics/btg180.
Nylander JAA, Ronquist F, Huelsenbeck JP, Nieves-Aldrey JL: Bayesian phylogenetic analysis of combined data. Syst Biol. 2004, 53: 47-67. 10.1080/10635150490264699.
Gresoviac SJ, Khattra JS, Nadler SA, Kent ML, Devlin RH, Vivares CP, De La Fuente E, Hedrick RP: Comparison of small subunit ribosomal RNA gene and internal transcribed spacer sequences among isolates of the intranuclear microsporidian Nucleospora salmonis. J Eukaryot Microbiol. 2000, 47: 379-387. 10.1111/j.1550-7408.2000.tb00064.x.
Desportes I, Le Charpentier Y, Galian A, Bernard F, Cochand-Priollet B, Lavergne A, Ravisse P, Modigliani R: Occurrence of a new microsporidian: Enterocytozoon bieneusi n. g. n. sp. in the enterocytes of human patients with AIDS. J Protozool. 1985, 32: 250-254.
Sestak K, Aye PP, Buckholt M, Mansfield KG, Lackner AA, Tzipori S: Quantitative evaluation of Enterocytozoon bieneusi infection in simian immunodeficiency virus-infected rhesus monkeys. J Med Primatol. 2003, 32: 74-81. 10.1034/j.1600-0684.2003.00006.x.
Chilmonczyk S, Cox WT, Hedrick RP: Enterocytozoon salmonis n. sp.: an intranuclear microsporidium from salmonid fish. J Protozool. 1991, 38: 254-259.
Hedrick RP, Groff JM, Baxa DV: Experimental infections with Enterocytozoon salmonis Chilmonczyk, Cox, Hedrick (Microsporea): an intranuclear microsporidium from Chinook salmon Oncorhynchus tshawytscha. Dis Aquat Org. 1991, 10: 103-108.
Nilsen F, Ness A, Nylund A: Observations on an intranuclear microsporidian in lymphoblast from farmed Atlantic halibut larvae (Hippoglossus hippoglossus L.). J Eukaryot Microbiol. 1995, 42: 131-135. 10.1111/j.1550-7408.1995.tb01553.x.
Freeman MA, Sommerville C: Desmozoon lepeophtherii n. gen., n. sp., (Microsporidia: Enterocytozoonidae) infecting the salmon louse Lepeophtheirus salmonis (Copepoda: Caligidae). Parasit Vectors. 2009, 2: 58-10.1186/1756-3305-2-58.
El Alaoui H, Grésoviac SJ, Vivarés C: Ocurrence of the microsporidian parasite Nucleospora salmonis in four species of salmonids from Massif Central of France. Folia Parasitol. 2006, 53: 37-43.
Hedrick RP, Groff JM, MacDowell TS, Willis M, Cox WT: Haematopoietic intranuclear microsporidian infections with features of leukemia in chinook salmon Oncorhynchus tshawytscha. Dis Aquat Org. 1990, 8: 189-197.
Morrison JK, MacConnell E, Chapman PF, Westgard RL: A microsporidium-induced lymphoblastosis in chinook salmon Oncorhynchus tshawytscha in freshwater. Dis Aquat Org. 1990, 8: 99-104.
Khattra JS, Gresoviac SJ, Kent ML, Myers MS, Hedrick RP, Devlin RH: Molecular detection and phylogenetic placement of a microsporidian from English sole (Pleuronectes vetulus) affected by X-cell pseudotumors. J Parasitol. 2000, 86: 867-871.
Lom J, Nilsen F: Fish microsporidia: fine structural diversity and phylogeny. Int J Parasitol. 2003, 33: 107-127. 10.1016/S0020-7519(02)00252-7.
Freeman MA, Sommerville C: Original observations of Desmozoon lepeophtherii, a microsporidian hyperparasite infecting the salmon louse Lepeophtheirus salmonis, and its subsequent detection by other researchers. Parasit Vectors. 2011, 4: 231-10.1186/1756-3305-4-231.
Nylund S, Nylund A, Watanbe K, Arnesen CE, Karlsbakk E: Paranucleospora theridion n. gn., n. sp. (Microsporidia, Enterocytozoonidae) with a life cycle in the salmon louse (Lepeophtheirus salmonis, Copepoda) and Atlantic salmon (Salmo salar). J Eukaryot Microbiol. 2010, 57: 95-114. 10.1111/j.1550-7408.2009.00451.x.
Heuch PA, Øines Ø, Knutsen JA, Schram TA: Infection of wild fishes by the parasitic copepod Caligus elongatus on the south east coast of Norway. Dis Aquat Org. 2007, 77: 149-158.
Dunn AM, Smith JE: Microsporidian life cycles and diversity: the relationship between virulence and transmission. Microbes Infect. 2001, 3: 381-388. 10.1016/S1286-4579(01)01394-6.
Terry RS, Smith JE, Bouchon D, Rigaud T, Duncanson P, Sharpe RG, Dunn AM: Ultrastructural characterization and molecular taxonomic identification of Nosema granulosis n. sp., a transovarially transmitted feminizing (TTF) microsporidium. J Eukaryot Microbiol. 1999, 46: 492-499. 10.1111/j.1550-7408.1999.tb06066.x.
Bruno DW, Munro ALS: Observations on Renibacterium salmoninarum and the salmonid egg. Dis Aquat Org. 1986, 1: 83-87.
Haugland GT, Jakobsen RA, Vestvik N, Ulven K, Stokka L: Phagocytosis and respiratory burst activity in lumpsucker (Cyclopterus lumpus L.) leucocytes analysed by flow cytometry. PLoS One. 2012, 7: 10-
The authors would like to thank the lumpfish fishermen who cooperated in helping us to sample fish from the fishery, the staff of the Marine Research Institute in Iceland for their support in collecting samples on the bottom trawl survey, Halldór G. Ólafsson at BioPol ehf in Skagastrond for his help during sampling and Dr. Sigurdur Helgason at the Institute for Experimental Pathology for his assistance with histopathological examination. The DNA analyses were supported by a University of Malaya HIR grant, No: UMC/625/1/HIR/027 and publication costs partly covered by University of Malaya RU funds.
The authors declare that they have no competing interests.
AK performed the histological examination and drafted the manuscript; JMK sampled the fish, provided prevalence data and helped write the manuscript; MAF made the initial diagnosis, did the molecular study, developed the nested PCR, performed the phylogenetic analyses and helped write the manuscript. All authors approved the final version of the manuscript.
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Freeman, M.A., Kasper, J.M. & Kristmundsson, Á. Nucleospora cyclopteri n. sp., an intranuclear microsporidian infecting wild lumpfish, Cyclopterus lumpus L., in Icelandic waters. Parasites Vectors 6, 49 (2013). https://doi.org/10.1186/1756-3305-6-49