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For: Research in Veterinary Science, Special Issue: “Foodborne and Waterborne Zoonotic
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Parasites of Veterinary and Medical Importance”
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Title: Anisakiasis and Anisakis: an underdiagnosed emerging disease and its main etiological
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agents
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Authors: Francisco Javier Adroher-Auroux* and Rocío Benítez-Rodríguez#
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Address: Departamento de Parasitología, Facultad de Farmacia, Universidad de Granada,
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18071-Granada, Spain
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*Corresponding author: F.J. Adroher (fadroher@ugr.es). ORCID ID https://orcid.org/0000-
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0002-7969-6658
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Highlights
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1.- Anisakiasis is an emergent, cosmopolite, subdiagnosed seafood-borne parasitic zoonosis.
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2.- Awareness and training of health personnel is decisive for the diagnosis of anisakiasis.
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3.- Anisakiasis prevention and control measures are effective if implemented.
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4.- The development of less invasive and more specific diagnostic methods is required.
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5.- The relationship of anisakiasis with cancer and other diseases needs to be clarified.
1
This is the accepted preprint. Article published in Research in Veterinary Science 132: 535-545 (2020).
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Abstract
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Anisakiasis or anisakiosis is a human parasitic infection caused by the third-stage larvae (L3) of
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nematodes of the genus Anisakis, although the term is also used in medical literature for the
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much less frequent (<3% of cases) infection by L3 of other genera of anisakids, particularly
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Pseudoterranova. These parasites have a marine lifecycle. Humans are infected by the L3
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through ingesting of fish and squid, the intermediate/paratenic hosts. The live larvae generally
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penetrate the wall of the stomach or intestine causing, amongst other symptoms, intense pain
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or allergic symptoms. These are emerging, cosmopolite illnesses. Diagnosis and treatment is
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usually by endoscopy and extraction and identification of the larvae. Allergic forms are usually
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diagnosed by prick-test and/or allergen-specific IgE detection and treated with a suitable anti-
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allergy treatment. The patient is also warned against further consumption of marine fish or
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squid, as these may be infected with Anisakis. The most common method of prevention is
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thermal treatment of the entire fish or squid prior to consumption (>60 ºC, >1 min or -20 ºC,
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>24 h). Useful measures for the control of anisakiasis would be to establish a national register
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of cases, to initiate educational campaigns for the general public and consciousness-raising and
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training campaigns for health professionals. These would be complemented by control
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measures for the relevant sectors of the economy: fish operators, fish farming, fishermen,
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fishmongers, fish industry and catering facilities. Possible genetic predisposition for allergy to
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Anisakis and the possible relationship between anisakiasis and cancer would also require
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further investigation.
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Keywords: Anisakiasis; allergy; seafood-borne disease; Anisakis; diagnosis; control.
2
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Introduction.
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Anisakidosis or anisakiasis is an infradiagnosed, emerging, cosmopolite illness. It entails the
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accidental infection of humans by the third larval stage (L3) of parasitic nematodes of the
43
family Anisakidae (genera Anisakis, Pseudoterranova and, very rarely, Contracaecum), which,
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with an aquatic, mainly marine, lifecycle have marine mammals and fish-eating birds as
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definitive hosts and crustaceans, cephalopods and fish as intermediate/paratenic hosts. It has
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also been related to anisakiasis, although rarely, to raphidascarid Hysterothylacium aduncum
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(Yagi et al., 1996), which is very close to anisakids (Fig. 1). Cases of allergy to these parasites
48
are also considered as anisakiasis (Audícana and Kennedy, 2008).
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Infection by larvae of the genus Anisakis is specifically classified as anisakiosis, although the
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term anisakiasis is the term most commonly employed in medical literature, perhaps as a
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result of the etiological agent of 97% of cases of anisakiasis being L3 of the complex A. simplex
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sensu lato, specifically the species A. simplex sensu stricto and A. pegreffii.
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The presence of Anisakis in fish has been known at least since the 13th century (Myers, 1976).
54
In 1767, Linnaeus named it Gordius marinus, while, in 1809, Rudolphi described larvae in fish
55
and adults in porpoise, but without relating them (Rudolphi, 1809). Finally, in 1845, Dujardin
56
created the genus Anisakis, in which this parasite is included with the name Anisakis simplex
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(Rudolphi, 1809).
58
It was not known that it could affect humans. Hitchcock (1950) observed a larva, probably
59
Anisakis, in the faeces of an Inuit in Alaska. The first cases in which symptoms were associated
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with the presence of Anisakis larvae were diagnosed by Dr. Straub in the Netherlands in 1955-
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59 (van Thiel et al., 1960).
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The L3 of the genus Anisakis are very similar morphologically (Fig. 1), traditionally classified as
63
type I or type II larvae , with the species within each type being morphologically
3
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indistinguishable (Berland, 1961). They can however be differentiated molecularly and have
65
been grouped into 4 clades (Mattiucci and Nascetti, 2008) (Table 1).
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Transmission and epidemiology
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Humans are infected on ingesting viable L3 found in host fish and squid, especially by those in
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the muscle tissue since those in the visceral cavity are eliminated when the fish is gutted for
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culinary purposes. However, some small fish are consumed whole, in which case the worm
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larvae in the body cavity can also cause anisakiasis. Almost all species of teleost fish studied
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throughout the oceans can act as hosts for Anisakis larvae. Consequently, the consumption of
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fish or some species of squid is a source of infection in humans.
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Each year thousands of cases are reported globally, particularly in developed countries with a
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significant fishing industry, high per capita consumption of fish and where there is a culinary
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tradition of dishes featuring raw fish or squid. Japan is the country where most cases are
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diagnosed, over 500 annually (Suzuki and Murata, 2011), but estimated to be approximately
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7,000 (Sugiyama et al., 2013, cited in IARS, 2017). In other countries with high fish
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consumption, such as Spain, the number of reported cases is much lower, at around 150/year
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(Herrador et al., 2019). Although increased information and raising awareness in health
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professionals results in more effective diagnosis (Castán et al., 2002), some authors have
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expressed concern regarding the continued infradiagnosis. For example, in Spain, Bao et al.
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(2017) used a quantitative risk assessment model to predict around 8000 cases/year of
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anisakiasis due to consumption of anchovies, while Herrador et al. (2019), working with
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hospitalization data, calculated 10,000-20,000 cases. However, only around 500 cases are
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reported annually in the whole of Europe. The global frequency of infection is estimated at
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0.32 cases/100,000 inhabitants (Orphanet, 2020), with cases of anisakiasis diagnosed in more
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than 20 countries.
4
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The lifecycle of Anisakis (Fig. 2) can start in the stomach chambers of odontocete cetaceans,
89
definitive hosts, in which adult worms are free-living (Fig. 3). The female is fertilized by the
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male and lays eggs which are passed in the host’s faeces. The eggs develop in the sea up to L3
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which then hatch (Køie et al., 1995). The L3 (200-300 μm) is enclosed in a sheath, the L2
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cuticle, and can survive for up to 3-4 months (Højgaard, 1998) in seawater until predated by
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the first suitable intermediate host, a crustacean, generally euphausiids (Smith, 1983, 1971) or
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large calanoid copepods (Klimpel et al. 2004), although smaller plankton crustaceans could act
95
as paratenic hosts, prior to ingestion by the first intermediate host (Klimpel et al., 2004; Køie,
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2001; Shimazu, 1974). The L3, after losing its sheath, passes from the digestive system of the
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crustacean into the coelomic cavity. Here it undergoes a period of growth, which can reach up
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to 32.7 mm in these hosts (Smith, 1983). These larvae are now infective for the definitive host.
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However, in order to reach an odontocete cetacean, the cycle must continue through a second
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suitable intermediate host, in this case squid (rarely any other cephalopod) or teleost fish
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which predate on euphausiids. When the infected crustacean is ingested, the L3, in order to be
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infective for the host, must have attained a minimum size (L3 from 8.8 mm have been
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recorded in host fish; Smith, 1983). The L3 then passes from the host’s digestive system to the
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visceral cavity (Wootten and Smith, 1975). Occasionally, L3 pass from the visceral cavity to the
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fish musculature. This L3 will be infective for the definitive host, for which it must apparently
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have a suitable size (Asami and Inoshita, 1967; Iglesias et al., 1997; Kikuchi et al., 1967; vs
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Beverley-Burton and Pippy, 1977; Hays et al., 1998). Next, when the intermediate host is
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ingested by a cetacean the L3 occupy the stomach chambers, most often the first, and attach
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themselves to the gastric mucosa, normally in groups, where they cause an ulcer. The L3 moult
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to L4 which remain together in the ulcers until the final moult to adult when they generally
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free themselves and grow and mature in preparation for mating while roaming throughout the
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stomach chambers (Højgaard, 1999; Kikuchi et al., 1967; Smith, 1989, 1983; Young and Lowe,
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1969). The adult female (4.5-15.0 cm) is usually larger than the male (3.5-7.2 cm), with the
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cycle being completed when the male fertilizes the female (Grabda, 1976; Iglesias et al., 2001;
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van Banning, 1971).
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In nature this lifecycle is complicated by the undefined number of paratenic hosts which can
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potentially intervene (Fig.2). If an L3 can to infect the next host but its paratenic host is then
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ingested by a host from the same level the larva will again occupy the visceral cavity, either
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free or encapsulated, and will not progress. This host will thus be paratenic. As the
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intermediate and paratenic hosts are the same they are normally known as
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“intermediate/paratenic hosts” as they can perform both functions according to the larval
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development. This large number of potential hosts for the genus Anisakis, especially with
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regard to intermediate/paratenic hosts, allows the parasite to follow alternative lifecycles,
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depending on both biotic and abiotic factors, for its adaptation and survival at different marine
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latitudes (Klimpel et al., 2004; Kuhn et al., 2016). However, many aspects of the Anisakis
126
lifecycle remain unclear and must be studied to clarify them.
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Despite the large number of hosts that may be involved in the lifecycle of these parasites not
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all cetaceans are suitable definitive hosts for all species: Delphinidae are ideal for species of
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the complex A. simplex s.l. and for A. typica, Ziphiidae for A. ziphidarum and A. nascetti,
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Physeteridae for A. physeteris and Kogiidae for A. paggiae and A. brevispiculata (Klimpel et al.,
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2010; Mattiucci et al., 2018; Mattiucci and Nascetti, 2008). Other cetaceans, such as misticetes
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(Raga et al., 1986), can serve as occasional definitive hosts, but not other marine mammals,
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such as the pinnipeds, in which the parasites do not attain maturity (Skrzypczak et al., 2014).
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Clinics and pathogenesis
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Infection in wild and farmed fish.
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Fishermen have been aware of the presence of these parasites in fish for centuries, as
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commented. In some fish, such as herring, they were so abundant that that they were believed
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to be the main food source for these fish (see comment in van Beneden, 1870, p. 65).
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Templeman et al. (1957) drew attention to the commercial problem represented by the
140
presence of larvae of Porrocaecum (=Pseudoterranova) and Anisakis in fish, particularly cod,
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suggesting that a reduction in the number of seals (definitive hosts of Pseudoterranova) at the
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fishing grounds could reduce the parasite load of these fish. To date more than 200 species of
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fish, including many of commercial value, have been reported as hosts of Anisakis, with more
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added each year. Such valuable fish as cod, salmon, hake, saithe, redfish, blue whiting,
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pouting, horse mackerel, sardine, anchovy, mackerel, herring, etc. are habitual hosts, showing
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high prevalence and intensity, with these being affected by capture zone and the size/age of
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the fish (Adroher et al., 1996; Beck et al., 2008; Levsen and Lunestad, 2010; Molina-Fernández
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et al., 2018, 2015; Rello et al., 2009, 2008; Strømnes and Andersen, 1998; Valero et al., 2006).
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The presence of cetaceans in and around the fishing grounds may help to perpetuate the
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lifecycle of the parasite (Rello et al., 2009), while, since L3 of Anisakis can live within a fish for 3
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years or more (Smith, 1984), parasites tend to accumulate as the fish grows (Bussmann and
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Ehrich, 1979; Valero et al., 2000). Nonetheless, in some cases older fish may show a reduction
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in parasite intensity, possibly due to a better immune response from the host (Dezfuli et al.,
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2016; Serrat et al., 2019) or to the death of the hosts with the highest parasite load (Levsen
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and Berland, 2012; Strømnes and Andersen, 1998).
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The passage of Anisakis larvae through the stomach wall of the fish results in the formation of
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ulcers, although these do not seem to affect the normal performance of the organ (Jones,
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1994) and nor does the presence of the parasites in the visceral cavity (Fig. 4A) appear to
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significantly affect the host’s health, regardless of whether they are free or encapsulated on
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the liver (Wootten, 2012). The effects of Anisakis on fish have rarely been considered and are
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worthy of further study, particularly as Anisakis has recently been related to red-vent
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syndrome in Atlantic salmon (Beck et al., 2008). In any case, Fulton’s condition factor (CF)
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(Fulton, 1904) for fish is a general indicator of their health (Monstad, 1990). According to this,
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a parasitized fish should show a lower value of CF to one free from parasites. However, this is
7
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open to debate. Some authors have found CF in parasitized fish to be unaffected (Molina-
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Fernández et al., 2018, 2015; Mouritsen et al., 2010). On the other hand, other authors have
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suggested that CF is not only affected when the intensity of parasites is high but also by other
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factors such as season, age/length or maturity of the fish (Richards, 1977; see Rohde, 1984,
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and references therein). However, Serrat et al. (2019) suggest that the CF will only be affected
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if the parasite load affects the availability of energy for the fish. This controversial topic
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requires further study.
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In marine fish-farming, although the feed is processed to avoid infection, it is still possible for
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small prey animals (crustaceans, squid and small fish) infected with Anisakis to pass through
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the netting of the cages and to be ingested by the fish. However, although a few cases of
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caged fish being infected with Anisakis (reviewed by Lima dos Santos and Howgate, 2011; Mo
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et al., 2014) have been reported prevalence is generally very low or nil (Brooker et al., 2016;
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Cammilleri et al., 2018; Peñalver et al., 2010). Other practices such as the capture of wild fish
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such as cod and tuna for subsequent growing-on in cages present a greater risk as these may
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already be infected when captured and may cause anisakiasis when sold (Heuch et al., 2011;
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Smrzlić et al., 2012). Consequently, the possibility of farmed fish being parasitized should
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always be taken into consideration (Rückert et al., 2008).
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Infection in cetaceans.
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There are many species of cetaceans in which Anisakis has been detected in their stomach
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chambers (Fig. 4B). As described previously, these nematodes form clusters on the gastric
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mucosa forming an ulcer to which they remain attached until moulting to adults (Højgaard,
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1999; Young and Lowe, 1969), some 3-5 weeks later (Iglesias et al., 2001), by penetrating the
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mucosa with their anterior end, even reaching the submucosa (Kikuchi et al., 1967; Young and
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Lowe, 1969). These ulcers may be associated with oedemas, haemorrhages and alterations
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such as eosinophilic and granulomatous inflammation with giant cells, hemosiderosis, fibrosis
8
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and areas of necrosis associated with location of parasites within the gastric mucosa (Motta et
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al., 2008). Fernández-Maldonado (2016) suggested that the presence of Anisakis in cetaceans
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may be related to a state of immunosupression associated with microbial systemic infections
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in addition to significant digestive disorders. Dermal symptoms have also been described (van
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Beurden et al., 2015). Recent studies seem to show that Anisakis populations in cetaceans
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could be increasing over recent decades (Pons-Bordas et al., 2020). At least, captive marine
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mammals can be treated, with varying degrees of success, using thiabendazole or levimasole
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(Smith and Wootten, 1978).
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Infection in humans.
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Man is an accidental host of Anisakis in whom the live L3, ingested on consuming raw or
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under-cooked fish or squid, tend to attach to the gastric mucosa, and, on occasions, the
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intestinal mucosa (Fig. 4C). Their attempts to penetrate the mucosa are generally unsuccessful.
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A single larva can cause symptoms. This L3 very rarely moults to L4 in humans (van Thiel et al.,
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1960). The type of anisakiasis produced depends on the location of the larva and the
204
symptoms it is causing:
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Gastric anisakiasis: the attaching of the larva to the gastroduodenal mucosa gives rise to
206
intense epigastric pain which may be accompanied by other symptoms such as nausea,
207
vomiting, urticaria and diarrhoea (Furuya et al., 2018) which develop between 2 to 6 hours
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after ingestion of the larva. The symptoms last as long as the larva is alive. This is the most
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common form of anisakiasis, accounting for 72% of cases (Valls Sánchez et al., 2009).
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Intestinal anisakiasis: when the larva attaches to this part of the digestive system symptoms
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start to appear 2 to 3 days after ingestion, typically severe abdominal pain which may be
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accompanied by nausea, vomiting and/or diarrhoea. Occasionally, a chronic form develops,
213
resulting in the formation of granulomas or abscesses. These may resemble episodes of
9
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appendicitis or intestinal obstruction accompanied by an oedema with fibrinous exudate (Valls
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Sánchez et al., 2009).
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It is not clear why the larva attaches to the gastric or intestinal mucosa. However, in Japan the
217
intestinal form has been related to factors pertaining to the human host such as sex, habitual
218
consumption of alcohol or cardiac risk (Yamamoto et al., 2020). Geographical factors,
219
potentially related to culinary traditions, may also be involved. In both cases, in the zone of
220
attachment, the organism reacts by generating an eosinophilic granuloma which normally kills
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the larva in 1 to 2 weeks, at which point the symptoms disappear.
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Ectopic or extraintestinal anisakiasis: is rare, occurring when the larva passes through the
223
digestive wall giving rise to ‘visceral larva migrans syndrome’. There are no specific symptoms
224
and these depend on the organ affected.
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Allergic anisakiasis or ‘allergy to Anisakis’: occurs when the presence of larval allergens (due to
226
live or dead parasite larvae) triggers an allergic response in the host, with symptoms ranging
227
from urticaria (Kasuya et al., 1990) and/or angioedemas to anaphylaxis (Audícana et al., 1995;
228
see section 3.2.1 in EFSA-BIOHAZ, 2010). These usually appear within the first hour after
229
consuming the parasitized fish. Although it is not absolutely clear whether a dead larva
230
(following cooking or freezing of the fish) is capable of sensitizing the subject, there is evidence
231
to suggest that human sensitization can only be produced by contact with live larvae, although,
232
once sensitized, the subject will also exhibit an allergic response to dead larvae (Alonso-Gómez
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et al., 2004; Audícana et al., 2002; Daschner et al., 2012).
234
Gastroallergic anisakiasis: The requirement for contact with live larvae for sensitization to
235
occur has given rise to the name of this type of anisakiasis, in which digestive and allergic
236
symptoms are combined (Alonso et al., 1997; Daschner et al., 2000), being defined as a severe
237
case of IgE-mediated allergy, typically accompanied by gastric digestive symptoms (Valls
10
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Sánchez et al., 2009). This acute form may evolve, in some cases, into chronic urticaria
239
(Petithory, 2007).
240
Occupational anisakiasis: there is evidence for occupational allergy (dermatitis, asthma,
241
conjunctivitis) caused by A. simplex in fishermen, fishmongers or other fish industry workers
242
(Añíbarro and Seoane, 1998; Armentia et al., 1998; Carretero Añíbarro et al., 1997;
243
Nieuwenhuizen et al., 2006; Purello-D’Ambrosio et al., 2000).
244
Diagnosis
245
Diagnosis of anisakiasis is not easy due to the lack of specificity of the symptoms. An
246
anamnesis is necessary (Del Rey-Moreno et al., 2008) to establish the consumption, in the 72
247
hours previous to the appearance of symptoms, of sea fish, either raw, marinated, pickled in
248
vinegar, in brine or seared, that is, inadequately cooked such that it contains live larvae of
249
Anisakis, for patients with acute epigastric or abdominal pain. Following confirmation there
250
are several diagnostic tests to aid the doctor’s decision-making.
251
Diagnosis of infection by Anisakis.
252
From the first cases of anisakiasis to be identified up to the end of the 20th century diagnosis
253
was generally by identification of the larvae in the eosinophilic granulomas or in segments of
254
the digestive tract affected (Fig. 5), which were surgically resected. However, advances in
255
imaging techniques, especially in endoscopy, have made them more easily available and
256
financially viable for patients suspected of infection following the anamnesis. In this sense,
257
endoscopy is currently the technique of choice for diagnosing acute gastric or intestinal
258
anisakiasis (Bucci et al., 2013). In addition to being able to observe the larvae (Fig. 4C) or
259
fragments of these using gastroscopy or colonoscopy it is also possible to extract them for
260
posterior identification by their morphological features and thus avoid unnecessary surgery
261
(Fig. 6). Furthermore, it has been suggested that the computed tomography, performed before
262
endoscopy, is useful for the diagnosis (Ashida et al., 2017; Shibata et al., 2014).
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On occasions, in the absence of a precise diagnosis, particularly in the case of intestinal
264
anisakiasis, exploratory surgery is required. This enables observation and extraction of the
265
larvae from either the abscess or the eosinophilic phlegmon. The anatomopathological study
266
of these samples may reveal sections of the larvae: In the transverse sections we will observe a
267
fine cuticle without wings, a well-developed polymyarian subcuticular musculature, lateral
268
nerve cords in a “Y” shape and smaller dorsal and ventral cords. If the section is of the first
269
third of the larva the muscular esophagus with a tri-radiate lumen can be observed, as can the
270
excretory cell or the excretory tubule (Fig. 6). If the section is of the posterior two thirds the
271
intestine can be observed, as can its epithelium with columnar cells with the nucleus at the
272
base of each cell. Saggital or oblique sections are more difficult to identify. If the larva cannot
273
be identified due to its poor state, a molecular diagnosis can be carried out following DNA
274
extraction (D’Amelio et al., 2012; Paoletti et al., 2018).
275
Diagnosis of allergy to Anisakis.
276
When allergic symptoms are present a prick-test with Anisakis L3 antigen can be performed.
277
Other techniques may be used to determine specific IgE in the patient’s serum (Petithory,
278
2007) such as ImmunoCAP® with total antigen or with selected purified or recombinant
279
antigens from the parasite, the most widely utilized being Ani s 1, responsible for the majority
280
of cases of sensitization to Anisakis. Some authors have raised doubts concerning these
281
techniques due to possible cross reactions leading to false positive results (Mattiucci and
282
D’Amelio, 2014). Radioallergoabsorbence (RAST) permits differentiation between subclinical
283
allergy and anaphylaxis (Desowitz et al., 1985), but is an expensive technique.
284
Currently, the most highly-rated techniques are those based on microarrays (Armentia et al.,
285
2017) such as ImmunoCAP® ISAC (Immuno Solid-phase Allergen Chip) to detect, above all, the
286
thermostable allergens Ani s 1 and Ani s 3 as these permit differentiation between patients
287
who could experience anaphylaxis (sensitive to Anis s 1) and those only having a subclinical
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288
allergy (sensitive to Ani s 3). Furthermore, the former is detected in 88% of patients affected
289
by gastroallergic anisakiasis (Shimakura et al., 2004; Subiza, 2020).
290
Anadón et al. (2010) believed the recombinant allergens rAni s 1 and rAni s 7 to be the best
291
option for serological diagnosis of anisakiasis in terms of sensitivity and specificity (Trisakis-170
292
ELISA kit) since Ani s 3 (tropomyosin) is a panallergen and gives cross reactions with
293
tropomyosins from other invertebrates such as shrimps, cockroaches or mites (Daschner et
294
al., 2012; Guarneri et al., 2007).
295
Although these techniques are considered valid for the diagnosis of allergy to Anisakis, the fact
296
that part of the healthy population show positive responses to the allergens of Anisakis (Del
297
Rey Moreno et al., 2006) raises doubts regarding the choice of suitable techniques or allergens
298
(Table 2). In this sense, Mazzucco et al. (2018) emphasized that the estimates of
299
hypersensitivity varied greatly according to geographical zone, population characteristics,
300
diagnostic criteria and laboratory assays.
301
Treatment
302
The treatment for infection by Anisakis consists of extracting all the larvae found in the
303
digestive tract during the endoscopic examination (Fig. 7), either by gastroscopy or
304
colonoscopy, depending on the zone affected (Audícana Berasategui et al., 2007). There is no
305
completely efficacious drug available for the treatment of anisakiasis. However, since
306
endoscopy permits the immediate removal of the larvae, leading to an improvement in the
307
patient’s condition within a few hours, no pharmacological treatment is required in these
308
cases. The most widely-used drug is albendazole with other anthelmintics such as
309
thiabendazole, flubendazole or ivermectine also used, although none is completely efficacious
310
(Shimamura et al., 2016). Current studies are focusing on natural substances such as wood
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311
creosote (Sekimoto et al., 2011) and essential oils of plants and their components (reviewed by
312
Valero et al., 2015).
313
When the larva is located in zones of the intestine which are difficult to access, some authors
314
recommend a conservative treatment with fluid therapy and antibiotics, which usually improve
315
the patient’s condition (Audícana Berasategui et al., 2007; Shrestha et al., 2014). Occasionally,
316
however, laparotomy and resection of the affected fragment of the intestine is required.
317
‘Allergy to Anisakis’ should be treated immediately, with the recommendation that the patient
318
should avoid consuming marine fish (Petithory, 2007). In allergic patients suspected of
319
suffering anaphylactic shock, they must be provided with an injectable dose of adrenaline to
320
cope with the contingency and, if it occurs, immediate referral to hospital (Audícana
321
Berasategui et al., 2007).
322
Prevention and control
323
The prevention of anisakiasis is based on avoiding the ingestion of live larvae of Anisakis
324
through consumption of raw or under-cooked fish or squid. These should have undergone
325
some form of termal treatment since preparation with vinegar or lemon juice, smoking,
326
brining, pickling, marinating, etc. does not always inactivate all the larvae (EFSA-BIOHAZ,
327
2010). It is generally considered that fish and squid should be cooked at >60 ºC for >1 min or
328
frozen whole at -20 ºC for >24 h (or -35 ºC, >15 h) to ensure the death of the larvae (EU, 2011).
329
This eliminates the possibility of infection by Anisakis and sensitization to its allergens.
330
However, if the subject is already sensitized it is still possible for them to develop allergic
331
symptoms (Alonso-Gómez et al., 2004; Audícana et al., 2002; Daschner et al., 2012).
332
Anisakis is difficult to control due to its complex lifecycle and the large number of potential
333
hosts, particularly paratenic hosts. However, there is a variety of measures to reduce the
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334
incidence of human anisakiasis. The first is health education, which should principally consist
335
of raising awareness regarding prevention in consumers. This education should be broadened
336
and adapted to different economic sectors of the population, such as catering or fishing. Public
337
health agencies (FDA, 2019) and experts committees (EFSA-BIOHAZ, 2010) have recommended
338
a series of measures to become part of a countries’ legislation. In the European Union (EU,
339
2019, 2011, 2004) and other countries as Japan in 2012, most of these measures are now
340
included in current legislation. These measures require:
341
- establishments serving food or selling prepared food, to freeze fish and squid that are to be
342
consumed raw or under-cooked.
343
- high seas fish processors, to gut fish and squid to avoid migration from body cavity to muscle
344
tissues (Borderías and Sánchez-Alonso, 2011) and to destroy these viscera rather than to
345
dispose of them in the sea where they would disseminate parasites.
346
- boats, not to fish in zones where the parasites are known to be abundant, for example, those
347
close to areas with high numbers of cetaceans, definitive hosts of Anisakis, where prevalence
348
of the parasite in fish is usually higher than elsewhere (Rello et al., 2009).
349
- fish farms, to feed fish with products that are free of viable parasites capable of affecting
350
human health.
351
- food business operators, to guarantee that fish products are inspected visually to detect
352
visible parasites before going on sale and that fish with visible parasites are destroyed.
353
- food industry businesses selling fish products intended to be consumed raw, marinated,
354
salted or other treatments that are not sufficient to inactivate the parasites, to treat them, in
355
their entirety, at >60 °C for >1 min or, alternatively, to freeze them at -20 °C for >24 hours, or -
356
35 °C for >15 hours, to ensure inactivity of the larvae.
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357
Countries should incorporate these measures into their legislation. It may also be useful to
358
establish the prevalence of anisakiasis in each country with a view to implementing and
359
managing public health resources effectively. This would require that every country have a
360
mandatory national register of all diagnosed cases. Finally, the recommended thermal
361
treatment measures, applicable to many foods, prevent not only anisakiasis but many
362
foodborne pathogens.
363
Future studies and research needed.
364
While much progress has been made, our knowledge of Anisakis and anisakiasis is still limited.
365
Here, we will only address two important aspects: commercial and sanitary.
366
From a commercial viewpoint the presence of Anisakis in fish products is an aesthetic issue
367
since worms visible to the naked eye repel the consumer. Furthermore, the well-informed
368
consumer is also aware that this parasite can cause health problems. Consequently, the great
369
challenge for the fishing industry is to provide the consumer with a risk-free product, i.e. free
370
from Anisakis. The current parasite detection methods, based on visual inspection and
371
candling, are far from precise, despite being endorsed by European Union legislation, as some
372
worms may not be detected. The development of effective detection methods (Smaldone et
373
al., 2020), accompanied by clear and precise legislation, must be a priority and both are vital
374
for the industry (Fig. 8).
375
From a sanitary point of view, the cosmopolitan nature of Anisakis and the increased
376
awareness and knowledge of anisakiasis and its diagnosis by health professionals are
377
responsible for the increase in the number of cases reported in an increasing number of
378
countries, along with cultural and commercial globalization, since gastronomic products
379
prepared with raw or under-cooked fish or squid are consumed worldwide. So, dishes such as
380
sushi, sashimi, gravlax, groene haring, ceviche/cebiche, boquerones en vinagre, etc., can be
16
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381
sources of viable parasites and thus anisakiasis if not properly pre-frozen. However, it seems
382
clear that there is an infradiagnosis in many countries (Seal et al., 2020), related both to
383
awareness among health professionals and to diagnostic methods (Bao et al., 2017; Herrador
384
et al., 2019). Therefore, it is necessary to search for target molecules or infection markers that
385
can be identified with the development of new more sensitive, specific and cheaper diagnostic
386
techniques that are more reliable and accessible to laboratories that must unify diagnostic
387
criteria (Mazzucco et al., 2018).
388
A. simplex s.s. seems more pathogenic than A. pegreffii (Jeon and Kim, 2015; Quiazon et al.,
389
2011; Romero et al., 2013; Suzuki et al., 2010). However, this requires confirmation, while
390
possible differences between the two should be identified (Cavallero et al., 2020, 2018; Llorens
391
et al., 2018; Molina-Fernández et al., 2019; Torralbo-Ramírez et al., 2019), including allergens
392
(Arcos et al., 2014; Baird et al., 2016), as they may affect diagnostic methods. As it has also
393
been suggested that anisakiasis constitutes a risk factor for stomach and colon cancers
394
(Corcuera et al., 2018; García-Pérez et al., 2015), studies to determine its relationship with
395
these and other diseases are especially relevant. Furthermore, Sánchez-Velasco et al. (2000)
396
suggested a genetic predisposition to allergy to Anisakis, whose study could help prevent
397
hypersensitivity in at-risk subjects. Likewise, the study of immunogenic molecules for vaccine
398
development and the design allergen-specific immunotherapy are options for the future.
399
Finally, there are many potentially useful topics for research and development in the field of
400
anisakiasis and new omic tools will undoubtedly facilite the task (D’Amelio et al., 2020). Here,
401
we have only mentioned those that we consider most urgent regarding the prevention,
402
diagnosis and control of anisakiasis.
403
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404
Acknowledgements
405
Funding: This research did not receive any specific grant from funding agencies in the public,
406
commercial, or not-for-profit sectors. The authors are grateful to Drs Irene Adroher-Benítez,
407
Lola Molina-Fernández and Carolina Fernández-Maldonado for their help with the photos and
408
figures. Translation to English was by Robert Abrahams, BSc.
18
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902
39
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Table 1.- Molecular classification of known Anisakis species in clades (after Mattiucci et al.,
2018).
Clades
Clade 1
Clade 2
Clade 3
Clade 4
Anisakis species
A. simplex sensu stricto
A. pegreffii
A. berlandi
A. ziphidarum
A. nascetti
L3 typea
Type I
Type I
Type I
Type I
Type I
Anisakiasis
Humanb
Humanb
?c
?
?
Observations
A. physeteris
A. brevispiculata
A. paggiae
A. typica
Type II
Type II
Type II
Type I
Lab animalsb,d
?
Lab animalsb,d
?
Human anisakiasis by Anisakis larva
type II or A. physeteris (morphological
diagnosis) reportede.
Low frequency in fish muscle tissue
a
Low frequency in commercial fish
Low frequency in commercial fish
Low frequency in commercial fish
( ) Sensu Berland (1961), larvae of the same type (I or II) are morphologically indistinguishable.
(b) Confirmed by molecular diagnosis. (c) ?, Human and experimental infections have not been
proved. (d) Experimental infection by Romero et al. (2014). (e) See references in MolinaFernández et al. (2018a).
865
37
This is a preprint. Article published in Research in Veterinary Science 132: 535-545 (2020). © 2020 Elsevier Ltd. All rights reserved.
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Table 2.- Characteristics of the described allergens of third larval stage (L3) of Anisakis simplex s.l.
Allergena Origin
Protein features
Mw (kDa)a References
Ani s 1
ES
Kunitz-type serine-protease inhibitor; domain 21/24
Moneo et al., 2000
lustrine-type cystein-rich. Major allergen.
Shimakura et al., 2004
Thermostable.
Ani s 2
Somatic Paramyosin. Cross-reactivity with other helminth 97/100
Pérez-Pérez et al., 2000
and arthropod paramyosins.
Ani s 3
Somatic Tropomyosin. Cross-reactivity with arthropod
41
Asturias et al., 2000a, 2000b
tropomyosins.
Ani s 4
ES
Cysteine protease inhibitor. Thermostable.
9/12.7
Moneo et al., 2005
Resistant to pepsin digestion.
Rodríguez-Mahillo et al., 2007
Ani s 5
ES
SXP/RAL-2 family protein. Thermostable.
15
Kobayashi et al., 2007 Caballero
et al., 2008
Ani s 6
ES
Serine protease inhibitor. Resistant to pepsin
7
Kobayashi et al., 2007
digestion.
Ani s 7
ES
Glycoprotein with tandem repeat sequences.
139
Rodríguez et al., 2008 Anadón
Major allergen. Specific for Anisakis-infected
et al., 2009
patiens.
Ani s 8
ES
SXP/RAL-2 family protein. Thermostable.
15
Kobayashi et al., 2007b
Crossreactivity with Ani s 5.
Ani s 9
ES
SXP/RAL-2 family protein. Thermostable. Share
14
Rodríguez-Pérez et al., 2008
identity partial with Ani s 5 and Ani s 8.
Ani s 10
Somatic Unknown function. With repeat sequences.
21
Caballero et al., 2011
Thermostable.
Ani s 11
?
Unknown function. With repeat sequences. Ani s 27
Kobayashi et al., 2011
11-like 78% similarity (17 kDa)
Carballeda-Sangiao et al., 2016
Ani s 12
?
Unknown function. With repeat sequences.
31
Kobayashi et al., 2011
Ani s 13
?
Haemoglobin. No cross-reactivity to Ascaris suum 37
González-Fernández et al., 2015
haemoglobin.
Ani s 14
?
Unknown function. Share identity partial with Ani 24/27
Kobayashi et al., 2015
s 7 and Ani s 12.
a
Allergens nomenclature according to WHO/IUIS Allergen Nomenclature Sub-Committee (2020). ES, excretory-secretory. ?, no reported.
38
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903
Legends to Figures:
904
Figure 1.- Differential morphological features among third stage larvae (L3) of nematodes that
905
frequently occur in fish and that can potentially cause anisakidosis. Left: A freshly collected L3
906
from the body cavity of a blue whiting, host fish. Right: Drawings of the cephalic end,
907
ventricular area and caudal end of the larvae showing its external morphology and digestive
908
system. Note the differences between species, especially in the number of cecums in the
909
ventricular area. Also, note the position of the excretory pore to differentiate Contracaecum
910
and Hysterothylacium. Finally, note the differences between Anisakis type I (elongated
911
ventriculus with oblique join to the intestine, tail with mucron) and type II larvae (shorter,
912
thicker ventriculus with straight join to the intestine, conical tail). Abbreviations: a, anus; bt,
913
boring tooth; e, esophagus; ep, excretory pore; i, intestine; ic, intestinal caecum; m, mouth; nr,
914
nerve ring; p, papilla; r, rectum; rg; rectal gland; s, spine or mucron; v, ventriculus; va,
915
ventricular appendage. Drawing by Irene Adroher-Benítez.
916
917
Figure 2.- Lifecycle of Anisakis spp. L1, L2 and L3 are the first, second and third larval stages of
918
these parasitic nematodes into the eggs. L3 are also found in the body cavity of all
919
intermediate and paratenic hosts throughout the lifecycle of the worms. The fourth larval
920
stage (L4) and adults develop in the digestive tract of the final hosts. Note that L3 is the
921
infective stage for all hosts. Drawing by Lola Molina-Fernández.
922
923
Figure 3.- Anisakis simplex s.l., female adult obtained from in vitro culture described by Iglesias
924
et al. (2001). Scale in cm.
925
926
Figure 4.- Infection by Anisakis simplex s.l.: Worms (L3) in the body cavity of blue whiting,
927
Micromesistius poutassou (A), adults in the first gastric chamber of the bottlenose dolphin,
40
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928
Tursiops truncatus (B), and L3 in the human stomach (C). Credits: Image B courtesy of
929
Fernández-Maldonado (2016), and C from Shimamura et al. (2016).
930
931
Figure 5.- Anisakis simplex s.l. L3 section in human. A) L3 penetrating the digestive wall
932
surrounded by acute inflammatory cells (bar, 1 mm). B) Cross section of L3 surrounded by a
933
thick cuff of acute inflammatory cells with numerous eosinophils “showing transmural
934
infiltration of acute inflammatory cells with diffuse subserosal (ss) involvement” (bar, 500 µm).
935
From Takei and Powell (2007), courtesy from Elsevier ©.
936
937
Figure 6.- Cross section through the L3 of Anisakis simplex s.l. (M: polymyarian muscle layer;
938
LEC, lateral nervous cord; EG, excretory cell; DT, esophageal lumen). From Takei and Powell
939
(2007), courtesy from Elsevier ©.
940
941
Figure 7.- Extraction of a larva of Anisakis simplex s.l. from human digestive tract (after
942
Shimamura et al., 2016).
943
944
Figure 8. Observation of pressed and frozen fillets of blue whiting in UV-light allows the
945
detection of Anisakis larvae as bright fluorescent spots. The straight lines mark the boundary
946
between the epiaxial (dorsal) and hypoaxial (belly) muscles of each side of fish. Photo by A.
947
Levsen (EFSA-BIOHAZ, 2010).
41
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Figures protected by copyright.
Figure 1.
Figure 2.
41
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Figures protected by copyright.
Figure 3.
Figure 4.
Figure 5.
42
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© 2020 Elsevier Ltd. All rights reserved. Downloadable from:
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Figures protected by copyright.
Figure 6.
Figure 7.
43
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Figures protected by copyright.
Figure 8.
44