Skip to main content

Diphyllobothrium sprakeri n. sp. (Cestoda: Diphyllobothriidae): a hidden broad tapeworm from sea lions off North and South America

Abstract

Background

The systematic of several marine diphyllobothriid tapeworms of pinnipeds has been revised in recent years. However, 20 species of Diphyllobothrium from phocids and otariids are still recognized as incertae sedis. We describe a new species of Diphyllobothrium from the intestine of California sea lions Zalophus californianus (Lesson) (type-host) and South American sea lions Otaria flavescens (Shaw).

Methods

Zalophus californianus from the Pacific coast of the USA and O. flavescens from Peru and Argentina were screened for parasites. Partial fragments of the large ribosomal subunit gene (lsrDNA) and the cytochrome c oxidase subunit 1 (cox1) mitochondrial gene were amplified for 22 isolates. Properly fixed material from California sea lions was examined using light and scanning electron microscopy.

Results

A total of four lsrDNA and 21 cox1 sequences were generated and aligned with published sequences of other diphyllobothriid taxa. Based on cox1 sequences, four diphyllobothriid tapeworms from O. flavescens in Peru were found to be conspecific with Adenocephalus pacificus Nybelin, 1931. The other newly generated sequences fall into a well-supported clade with sequences of a putative new species previously identified as Diphyllobothrium sp. 1. from Z. californianus and O. flavescens. A new species, Diphyllobothrium sprakeri n. sp., is proposed for tapeworms of this clade.

Conclusions

Diphyllobothrium sprakeri n. sp. is the first diphyllobothriid species described from Z. californianus from the Pacific coast of North America, but O. flavescens from Argentina, Chile and Peru was confirmed as an additional host. The present study molecularly confirmed the first coinfection of two diphyllobothriid species in sea lions from the Southern Hemisphere.

Background

The systematic of the tapeworms (Cestoda) has been under detailed revision since the last decade including adding new molecular data [1]. However, current knowledge and systematics of the tapeworms of marine mammals are still superficial [2,3,4,5,6,7]. The pinnipeds are well-known hosts of several groups of tapeworms composed of two orders, Tetrabothriidea with only seven members of the genus Anophryocephalus Baylis, 1922, and Diphyllobothriidea with around 30 species of several genera [7, 8]. Waeschenbach et al. [4] revised the systematic of diphyllobothriids based on morphological as well as molecular data and proposed systematic changes mainly in the polyphyletic genus Diphyllobothrium Cobbold, 1858, which now includes only seven species parasitizing cetaceans. Non-monophyletic Diphyllobothrium (designated as ‘Diphyllobothrium’ by Waeschenbach et al. [4])  provisionally comprises 20 species mainly from pinnipeds (eight of which have been characterized molecularly) that do not form a monophyletic assemblage and are considered incertae sedis [4].

The California sea lion Zalophus californianus (Lesson) (CSL) is a well-known otariid species of North America whose range in the Pacific is from Baja California, Mexico, to British Columbia, Canada. Nowadays, its population is increasing and includes around 340,000 individuals [9, 10]. The first diphyllobothriid tapeworm from CSL was reported by Stunkard [11] who studied a scolex of 'Diphyllobothrium' sp. (see fig. 2 in Stunkard [11]). Later, several authors reported diphyllobothriids from CSL as Adenocephalus pacificus Nybelin, 1931 (under the names D. glaciale [Cholodkovsky, 1915] or D. pacificum [Nybelin, 1931]) [12,13,14,15,16,17]. The recent revision of metazoan parasites of CSL considered 24 valid species, including two undescribed tapeworm species [18].

The South American sea lion Otaria flavescens (Shaw) (SASL) is distributed exclusively in South America from the Pacific coast of Peru to the Atlantic coast of southern Brazil [19]. Nowadays, its population has been estimated as at least 445,000 individuals [20]. The first diphyllobothriid tapeworm from SASL was reported by Baylis [21] from Falkland Island (Islas Malvinas) as Diphyllobothrium scoticum (Rennie & Reid, 1912). This material was later studied by Markowski [22] who confirmed Baylis’ specimens as D. scoticum. However, the evaluation Baylis’ [21] material by Baer et al. [23] and Hernández-Orts et al. [2] suggested that these specimens belong to A. pacificus. Hermosilla et al. [24] reported a ‘Diphyllobothrium scoticum-like cestode’ from SASLs from the Pacific coast of Chile to be molecularly conspecific with samples from CSLs. The recent revision of metazoan parasites of SASL by Ebmer et al. [25] reported 44 metazoan taxa (only 25 were identified to the species level), including A. pacificus with its synonyms, Clistobothrium delphini (Bosc, 1802) [as Phyllobothrium delphini (Bosc, 1802)] and unidentified species of Anophryocephalus Baylis, 1922 and 'Diphyllobothrium'.

A detailed study of newly obtained material, examination of museum specimens, as well as molecular phylogenetic analysis and extensive literature revision confirmed the presence of an undescribed species of the genus Diphyllobothrium which parasitizes CSLs. The main goal of this article is the description of a new species previously reported as ‘Diphyllobothrium’ sp. 1 by Waeschenbach et al. [4], Hermosilla et al. [24] and Kuzmina et al. [18] on the basis of detailed morphological and molecular data.

Methods

Sample collection

A total of 39 CSLs, 9–10 months to 16 years old, were collected stranded on the Pacific coast of central California (36°57′–38°32′N, 121°95–123°00′W), USA, between 2012 and 2018 (see [18] for details). CSLs died in the Marine Mammal Center (Sausalito, California, USA) from different causes and were necropsied using a standard procedure [26]. Two recently dead SASLs were collected from two localities in South America: (i) a subadult male from Bellavista beach (12°04′S, 77°07′W), Callao City, Callao, Peru, in October 2017; (ii) a subadult female from Playa Unión (43°19′S, 65°03′W), Chubut, Argentina, in October 2013. The intestines of fresh SASLs were excised from the carcasses, opened and washed with tap water through a series of sieves. Intestinal contents were placed in Petri dishes with saline and examined under a dissecting microscope. Tapeworms were washed in saline and killed with hot (90 °C) tap water and fixed in 70% ethanol. A few posterior proglottids of selected specimens were cut off and fixed in molecular-grade ethanol (99%) for DNA sequencing before killing the worm.

Molecular data and phylogenetic analyses

Three diphyllobothriid specimens from CSLs and 18 from SASLs (17 from Peru and one from Argentina) were selected for molecular studies. Pieces of strobila were used for DNA isolation and sequencing. The remaining parts of the worms were stained and mounted in Canada balsam and were kept as molecular vouchers (i.e. hologenophores sensu Pleijel et al. [27]). Total genomic DNA was extracted using DNeasy Blood and Tissue Kit (Qiagen, Hilden, Germany) according to the manufacturer’s protocol. Phylogenetic relationships of the studied diphyllobothriids were evaluated based on two molecular markers: the large subunit nuclear ribosomal RNA gene (lsrDNA) and the cytochrome c oxidase subunit 1 (cox1) mitochondrial gene.

Partial lsrDNA (D1–D3 domains, ca. 1400 bp) sequences were generated using the primers LSU5 (5′-TAG GTC GAC CCG CTG AAY TTA AGC A-3′; [28]) and 1500R (5′-GCT ATC CTG AGG GAA ACT TCG-3′; [29]). Partial (ca. 420 bp) and almost complete (ca. 1500 bp) cox1 sequences were amplified using the primers JB3 (5′-TTT TTT GGG CAT CCT GAC GTT TAT-3′; [30]) and JB 4,5 (5′-TAA AGA AAG AAC ATA ATG AAA ATG-3′ [30]) or the primers Cox1Forward (5′-TAT CAA ATT AAG TTA AGT AGA CTA-3′; [31]) and Cox1Reverse (5′-CCA AAT AGC ATG ATG CAA AAG-3′; [31]), respectively. PCR amplification reactions were performed following the procedures described by Brabec et al. [32] for the lsrDNA gene and Wicht et al. [31] or Gomez-Puerta et al. [33] for the cox1 gene. All products were purified through an enzymatic treatment with Exonuclease I and FastAP alkaline phosphatase (Thermo Fisher Scientific, Waltham, MA, USA) or using a Microcon® Centrifugal Filters (Millipore, Bedford, MA, USA). Purified products were Sanger sequenced at GATC Biotech (Konstanz, Germany) or using BigDye™ Terminator Cycle Sequencing Ready Reaction Kit (Applied Biosystems, Foster City, CA, USA) and an ABI 3100 automated sequencer (Applied Biosystems).

Sequences were assembled and inspected for errors using Geneious v.11 and deposited in the GenBank database (accession numbers MW600336–MW600339 for the lsrDNA sequences and MW596661–MW596682 for the cox1 sequences). Newly generated sequences were aligned in two independent datasets following the alignments from Hernández-Orts et al. [2] and Waeschenbach et al. [4]. Sequences from other diphyllobothriids were retrieved from GenBank and aligned with our novel sequences using default settings of MUSCLE [34] implemented in Geneious (Additional file 1: Table S1). The extremes were trimmed resulting in an alignment with 1574 bp for the lsrDNA (Additional file 2: lsrDNA_alignment) and 1571 bp for the cox1 (Additional file 3: cox1_alignment). A combined lsrDNA + cox1 alignment (3145 bp; Additional file 4: lsrDNA_cox1_alignment) was also constructed using only taxa with sequences for both markers available from GenBank (Additional file 1: Table S1).

Bayesian inference (BI) and maximum likelihood (ML) analyses were performed for each dataset. jModelTest 2.1.10 software [35] was used to select the best nucleotide substitution model under the Akaike information criterion. The TIM2 + I + G model was chosen for the lsrDNA and cox1 datasets and the TIM2 + I + G & TIM1 + I + G for the combined dataset. Bayesian inference analyses were constructed using MrBayes 3.2.6 [36]. The BI analyses were estimated via two independent Markov Chain Monte Carlo runs of four chains with standard settings for 10,000,000 generations with a sampling frequency of 1000th generations. Burn-in periods were set to 25% of generations. The ML analyses were run with raxmlGUI v.2.0 [37]. Bootstrap nodal support values were computed by running 1000 bootstrap resamples. The resulting trees for BL and ML were visualized in FigTree 1.4.4 [38]. Genetic distances (uncorrected p-distance) were calculated with MEGA 10.1.8 [39] from the total number of nucleotide differences from the lsrDNA alignment and from the full cox1 alignment excluding partially characterized sequences (i.e. < 1400 bp).

Morphological examination

For morphological evaluation, selected tapeworms were stained with Mayer’s hydrochloric carmine, dehydrated through an ethanol series, cleared with eugenol and mounted in permanent slides in Canada balsam. Selected pieces of the strobila were embedded in paraffin wax, cross-sectioned (thickness 15 µm), stained with hematoxylin–eosin, and mounted in Canada balsam. Mounted specimens were examined with an Olympus BX51 microscope (Olympus Corp., Tokyo, Japan). Measurements were taken from digital images with the QuickPHOTO CAMERA 3.2 image analysis software (Promicra Ltd., Prague, Czech Republic). Measurements are expressed in micrometers unless otherwise stated and presented as the range (minimum–maximum), with the mean followed by the standard deviation (SD) and the number of measured specimens or structures in parentheses. Detailed line drawings were made using a drawing tube attached to an Olympus BX51 microscope.

Selected scoleces and proglottids were prepared for scanning electron microscopy (SEM). Specimens were dehydrated through an ethanol series, transferred to hexamethyldisilazane (Ted Pella, Inc., Redding, CA, USA) and allowed to air dry. Samples were mounted on aluminium stubs on double-sided adhesive carbon tape, gold sputter-coated and examined with a JEOL JSM 7401-F scanning electron microscope (JEOL Ltd., Tokyo, Japan) at 4 kV at the Laboratory of Electron Microscopy, Institute of Parasitology, Biology Centre, Czech Academy of Sciences. Terminology of microtriches follows Chervy [40].

Tapeworms collected in the present study were compared with voucher material of the following immature diphyllobothriid species collected from Z. californianus identified as 'Diphyllobothrium latum (L.)' and deposited at the Natural History Museum (NHML), London, UK: two vouchers from San Diego County (NHML 1980.6.3.196–8), one from Los Angeles (NHML 1980.6.3.200), one from an unknown locality in California, USA (NHML 1994.7.21.12–13), and one from Mexican waters (NHML 1980.6.3.189).

Specimens of the type series and voucher specimens from the present study are deposited in the Helminthological Collection of the Institute of Parasitology (IPCAS), Biology Centre, Czech Academy of Sciences, České Budějovice, Czech Republic; the National Museum of Natural History of the Smithsonian Institution (NMNH-USNM), Washington, DC, USA; the Parasite Collection of the Museum of Natural History (PCMNH), National University of San Marcos, Lima, Peru; and the Collection of the Laboratory of Epidemiology and Veterinary Economics (LEVE), School of Veterinary Medicine, National University of San Marcos, Lima, Peru.

Results

More than 150 tapeworm specimens (including immature and gravid specimens) were collected in the intestine of CSLs. In the SASLs from Argentina and Peru, 13 and 18 immature tapeworms were collected, respectively.

Phylogenetic relationships and genetic divergence

A total of four partial lsrDNA sequences (1450–1481 bp long; three isolates from CSLs, USA, and an isolate from SASL, Argentina) were generated. Additionally, one almost complete (1565 bp long; isolate from SASL, Argentina) and 21 partial cox1 sequences (415–420 bp long; four isolates from CSLs, USA, and 17 isolates from SASL, Peru) were generated (see Additional file 1: Table S1).

The resulting phylograms inferred with BI and ML analyses for the lsrDNA dataset (34 taxa) showed generally similar topologies (Fig. 1) and congruent results with those of Waeschenbach et al. [4]. Our four newly generated sequences formed a well-supported clade with sequences of a putative new species ‘Diphyllobothrium’ sp. 1 from CSL of California (KY552829) [4] and ‘Diphyllobothrium’ sp. 1 from SASL of Chile (KY945917) [19] (Fig. 1). The clade composed by our novel sequences and 'Diphyllobothrium' sp. 1 appeared to be sister to a sequence generated from a diphyllobothriid plerocercoid (reported as Diphyllobothriidae gen. sp.) from Trematomus bernacchii Boulenger of Antarctica (KY552830) [4] (Fig. 1). 'Diphyllobothrium' sp. 1 and Diphyllobothriidae gen. sp. form the sister group of a clade which includes ‘Diphyllobothrium’ scoticum from Mirounga leonina (L.) and A. pacificus isolates, but these two lineages with low support (Fig. 1).

Fig. 1
figure1

Bayesian analysis for the partial lsrDNA dataset for selected representatives of the family Diphyllobothriidae. Numbers represent posterior probabilities from BI analysis (> 0.95 shown only) followed by nodal supports from ML analysis (bootstrap values > 70% shown only). The newly generated sequences are indicated in red. GenBank accession numbers are shown before the species names. The scale bar indicates the expected number of substitutions per site

Intraspecific sequence variability of 0.14% was only detected between the four isolates from CSLs and the two from SASLs for the lsrDNA gene. The lsrDNA sequences of isolates from CSLs and SASL diverged 0.64–0.78% from the sequences of Diphyllobothriidae gen. sp. from T. bernacchii from Antarctica. Genetic divergence values between our lineage and ‘Diphyllobothrium’ scoticum were 2.48–2.55% and between A. pacificus ranged from 1.99–2.06%. Intergeneric distance between 'Diphyllobothrium' scoticum and A. pacificus was 1.13%. The interspecific distances in the lsrDNA region of 'Diphyllobothrium' spp. of pinnipeds range between 0.36% (‘Diphyllobothrium’ cordatum (Leuckart, 1863) vs ‘Diphyllobothrium’ lanceolatum (Krabbe, 1865)) to 3.70% (‘Diphyllobothrium’ tetrapterum (von Siebold, 1848) vs ‘Diphyllobothrium’ cf. cameroni Rausch, 1969).

Both ML and BI analyses of the cox1 dataset (59 taxa) resulted in generally similar topologies (Fig. 2), but slightly differed from the recent phylogenetic study of Waeschenbach et al. [4]. Four newly generated sequences from isolates from CSLs and 14 novel sequences from SASLs (13 from Peru and 1 from Argentina) formed a strongly supported clade with three sequences identified as 'Diphyllobothrium' sp. 1., including one sequence from an isolate from CSL (KY552890) and two from SASLs (MF893274 and KY945922) (Fig. 2). The genetic divergence between isolates from CSLs and SASLs in the cox1 gene was 2.87–3.07%. In the phylogenetic tree, the clade formed by our novel sequences + 'Diphyllobothrium' sp. 1. appeared also as sister to the sequence of Diphyllobothriidae gen. sp. from T. bernacchii (KY552888). Genetic divergence between our newly generated sequences + ‘Diphyllobothrium’ sp. 1 and the isolate reported as Diphyllobothriidae gen. sp. ranged from 14.56–14.94%.

Fig. 2
figure2

Bayesian analysis of the cox1 dataset for representatives of the family Diphyllobothriidae. Numbers represent posterior probabilities from BI analysis (> 0.95 shown only) followed by nodal supports from ML analysis (bootstrap values > 70% shown only). The newly generated sequences are indicated in red. GenBank accession numbers are shown before the species names. The scale bar indicates the expected number of substitutions per site

In contrast to the phylograms inferred for the lsrDNA dataset, our novel sequences + 'Diphyllobothrium' sp. 1 + Diphyllobothriidae gen. sp. formed the sister group, although with low support, to an unresolved clade of diphyllobothriids (Fig. 2). The interspecific distances in the cox1 region of 'Diphyllobothrium' spp. of pinnipeds ranged between 1.88% ('Diphyllobothrium' tetrapterum vs 'Diphyllobothrium' schistochilus) to 14.30% ('Diphyllobothrium' tetrapterum vs 'Diphyllobothrium' cf. hians (Diesing, 1850)). Finally, four newly generated partial sequences from isolates from SASL from Peru formed a strongly supported monophyletic lineage with the previously published sequences of A. pacificus (Fig. 2).

The phylogenetic trees inferred with the combined (lsrDNA + cox1) dataset (33 taxa) were similar to the topologies inferred for the lsrDNA and cox1 datasets (Additional file 5: Fig. S1). Our newly generated sequences formed a well-supported clade with sequences of 'Diphyllobothrium' sp. 1 from CSL of California [4] and 'Diphyllobothrium' sp. 1 from SASL of Chile [19].

In summary, both ML and BI analyses for the lsrDNA, cox1 and the combined datasets revealed that most of our newly generated sequences from isolates from CSLs and SASLs belong to an as yet undescribed species reported as 'Diphyllobothrium' sp. 1 [4]. Genetic variation was detected between sequences from isolates of the putative new species from CSLs and SASLs. However, these values were somewhat lower, especially for cox1, than the interspecific variation between other ‘Diphyllobothrium’ species of pinnipeds included in our phylogenetic analyses. Therefore, we consider isolates of the putative new species of 'Diphyllobothrium' from CSLs and SASLs from North and South America, respectively, to be conspecific. This new tapeworm species is described below.

Family Diphyllobothriidae Lühe, 1910

Genus Diphyllobothrium Cobbold, 1858

Diphyllobothrium sprakeri Hernández-Orts, Kuzmina, Gomez-Puerta & Kuchta n. sp.

Synonyms: Diphyllobothrium sp. 1 of Waeschenbach et al. [4], Hermosilla et al. [24] and Kuzmina et al. [18]

Type-host: Zalophus californianus (Lesson) (Carnivora: Otariidae), California sea lion.

Type-locality: Off central California (36°57'–38°32'N, 121°95–123°00'W), USA.

Other host: Otaria flavescens Shaw (Carnivora: Otariidae), South American sea lion.

Other localities: Los Angeles and San Diego, California, USA; Mexican waters (see below); Playa Unión (43°19′S, 65°03′W), Chubut, Argentina; beach of Bellavista (12°04′S, 77°07′W), Callao City, Callao, Peru.

Site in host: Small intestine.

Prevalence in type-host: 38% (15 out of 39 examined sea lions).

Intensity in type-host: 1–30 (average = 9.5) tapeworms per sea lion; most of the tapeworm specimens collected (> 70%) were in immature stage.

Intensity in South American sea lions: 1–17 immature tapeworms per host.

Representative DNA sequences: GenBank accession numbers: MW600337–MW600339 (lsrDNA) and MW596662–MW596665 (cox1) from Z. californianus: MW600336 (lsrDNA) and MW596661, MW596666–MW596673, MW596675–MW596678, MW596680 (cox1) from O. flavescens.

Deposition of specimens: Holotype (IPCAS C-765/1), seven slides of whole mounts and five slides of histological sections; one paratype (NMNH-USNM 1642475), 14 slides of whole mounts; one voucher (NMNH-USNM 1642476), eight slides of whole mounts; 10 vouchers (LEVE 986–990, 992–995, 997), two vouchers (PCMNH 4711, 4712) and one voucher (IPCAS C-765/2) immature worms from O. flavescens of Peru; three vouchers (IPCAS C-765/3), immature worms from O. flavescens of Argentina.

ZooBank registration: The Life Science Identifier (LSID) of the article is urn:lsid:zoobank.org:pub: 68C9D942-6D3A-4CF9-8732-4766EBA494DB. The LSID for the new name Diphyllobothrium sprakeri n. sp. is urn:lsid:zoobank.org:act: B95F5960-A589-4B34-BBE2-21E1D2EF368A.

Etymology: The species is named after Prof. Terry R. Spraker from the Colorado State University, Colorado, USA, for his valuable contribution to the collection of this species and studies of various groups of parasites of marine mammals.

Description

[Based on 20 specimens from CSLs. All tapeworms collected from SASL were immature specimens and were not included in the description]. Diphyllobothriidea, Diphyllobothriidae. Specimens anapolytic, long worms up to 2 m (holotype 56 cm; Fig. 3a) in length; maximum width ca. 8 mm. Immature worms may reach 1 m in length. Scolex surface covered with capilliform filitriches and coniform spinitriches (Fig. 4a, b). Microtriches on strobila surface not observed.

Fig. 3
figure3

Line drawings of ‘Diphyllobothrium’ sprakeri n. sp. from Zalophus californianus, California, USA. a Selected anterior, middle and posterior proglottids of holotype, ventral view. b Scoleces, dorsoventral view. Scolex of holotype marked with an asterisk. c Genitalia of mature proglottids of holotype, ventral view, vitelline follicles omitted on left side and testes on the right side of proglottid. d Schematic drawing of gravid proglottids of holotype showing the position of the sac-like structure of the uterus. Abbreviations: cs, cirrus sac; esv, external seminal vesicle; ga, genital atrium; mg, Mehlis' gland; ov, ovary; te, testes; up, uterine pore; uss, uterine sac-like structure; ut, uterus; vf, vitelline follicle; vg, vagina

Fig. 4
figure4

Scanning electron micrographs of ‘Diphyllobothrium’ sprakeri n. sp. from Zalophus californianus, California, USA. a Capilliform filitriches on the lateral scolex surface. b Coniform spinitriches on the dorsoventral scolex surface. c–e Scoleces, dorsoventral view. f Scolex in apical view. g Ventral surface of gravid proglottids showing numerous papillae surrounding the genital atrium. h–i Eggs and surface of egg shell. j Detail of egg surface with pits

Excretory system consists of cortical and medullary longitudinal canals extending throughout strobila; canals in cortex numerous, interspersed in layer of vitelline follicles or displaced towards tegument; 2 pairs of main excretory canals in medulla alongside median axis. Longitudinal musculature formed by muscle bundles, in layer surrounding transverse musculature (Fig. 5a,c,d); longitudinal muscle layer 51–100 (71.2 ± 18, n = 10) wide.

Fig. 5
figure5

Photomicrographs of histological sections of holotype of ‘Diphyllobothrium’ sprakeri n. sp. from Zalophus californianus, California, USA. a Gravid proglottid, cross section. b Gravid proglottids, sagittal section. c Detail of cirrus sac and genital atrium in gravid proglottid, cross section. d Detail of longitudinal musculature. Abbreviations: cs, cirrus sac; esv, external seminal vesicle; lm, longitudinal musculature; te, testes; uss, uterine sac-like structure; vf, vitelline follicle

Scolex lanceolate, roundish or slightly elongated to triangular in dorsoventral view (Figs. 3b, 4c–e); 999–1484 (1207 ± 120, n = 15) long by 807–1275 (935 ± 132, n = 15) wide. Bothria with wide margins in lateral view, fan-like (Figs. 3b, 4c–e); bothrial margins fused anteriorly, leaving opening of varying degrees in middle and posterior parts (Figs. 3b, 4 c–f). Neck absent.

Proglottids craspedote, much wider than long, first eggs appear around 10 cm posterior to scolex; first proglottids posterior to scolex short, much wider than long, 51–188 (105.9 ± 37, n = 30) long by 821–1553 (1141 ± 214, n = 30) wide; proglottid width/length ratio 1:0.04–0.22 (0.1, n = 30). Mature proglottids, i.e. with spermatozoa in vas deferens, few, 1–3 in number (Fig. 3c), 281–401 (340 ± 42, n = 7) long by 3115–6202 (4451 ± 1177, n = 7) wide; proglottid width/length ratio 1:0.05–0.12 (0.08, n = 7). Gravid proglottids numerous, larger and wider, not enlarging, 287–736 (519 ± 130, n = 7) long by 2681–7890 (4712 ± 1921, n = 7) wide; proglottid width/length ratio 1:0.05–0.22 (0.14, n = 7).

Testes medullary, subspherical to oval, 44–70 (56 ± 6, n = 16) in diameter, 220–384 (325 ± 61, n = 7) in number, arranged in a single dorsoventral layer (Figs. 3c, 5a), form 2 lateral fields confluent at anterior and posterior margins of proglottid, not overlapping anterior uterine loops, absent in central area of cirrus sac, uterus and ovary (Fig. 3c). Vas deferens coiled, runs dorsally to uterus in midline to posterior border of external seminal vesicle (Fig. 3c). External seminal vesicle muscular, wall up to 27 thick, posterodorsal to cirrus sac, oval to almost elliptical in sagittal section (Figs. 3c, 5b), 58–122 (103 ± 19, n = 9) long by 38–120 (82 ± 21, n = 9) wide in dorsoventral view; length/width ratio 1:0.7–1 (0.8, n = 9). Cirrus sac thin-walled, wall up to 23 thick, larger than external seminal vesicle, oval in sagittal section (Fig. 5b), 142–286 (206 ± 40, n = 9) long by 92–159 (127 ± 18, n = 9) wide; length/width ratio 1:0.5–0.7 (0.6, n = 9). Cirrus sac opening in anterior region of genital atrium (Fig. 5b). Internal sperm duct thin-walled, strongly coiled; cirrus unarmed. Genital atrium ventral, median, pre-equatorial, situated 79–242 (201 ± 32, n = 7) from anterior margin of proglottid, representing 29–60% (40%) of proglottid length; surface area surrounding genital atrium covered with numerous papillae (Fig. 4g).

Ovary bilobed, situated dorsally near posteriormost margin of proglottid, 1029–1550 (1302 ± 167, n = 10) wide; ovarian lobes 135–233 (181 ± 30, n = 10) long, posteriorly enclosing Mehlis' gland (Fig. 3c). Vagina runs ventrally, 19–22 wide in cross sections (Fig. 5b). Female genital pore posterior to male genital opening in genital atrium (Fig. 5b). Vitelline follicles cortical, subspherical, numerous, 18–38 (29 ± 5, n = 18) in maximum diameter in dorsoventral view (Fig. 3c); area surrounding genital atrium devoid of vitelline follicles (Figs. 3c, 5c). Uterus tightly coiled, containing fully developed, but unembryonated eggs, forms bilateral uterine loops; uterine loops 3–4 (3, n = 5) in number on each side of mid-line (Fig. 3c). Terminal part of uterus enlarged, forming a thick-walled sac-like structure (Fig. 3c, d). Uterine pore situated 16–152 (75 ± 44, n = 7) from anterior margin of proglottid, representing 5–31% (21%) of proglottid length. Eggs oval, thick-walled, operculated (Fig. 4h, i), 59–75 (65 ± 3; n = 152) long by 40–47 (43 ± 2; n = 152) wide. Egg shell slightly pitted, with around 39–57 (n = 2) pits/10 µm2 (Fig. 4j).

Remarks

The new species is placed in the genus Diphyllobothrium because of its typical shape of the scolex, composition of genital organs, absence of transverse papilla-like tegumental protuberances on the ventral surface of the proglottids and using pinnipeds as its definitive host (see [4]).

Kuchta and Scholz [3] reported 20 species of ‘Diphyllobothrium’ (incertae sedis) from the intestine of pinnipeds. Of these, D. sprakeri n. sp. can be distinguished from D. archeri (Leiper & Atkinson, 1914), D. cameroni Rausch, 1969, D. cordatum (Leuckart, 1863), D. elegans (Krabbe, 1865), D. fayi Rausch, 2005, D. hians (Diesing, 1850), D. lanceolatum (Krabbe, 1865), D. lashleyi (Leiper & Atkinson, 1914), D. minutus Andersen, 1987, D. mobile (Rennie & Reid, 1912), D. phocarum Delyamure, Kurochkin & Skryabin, 1964, D. pseudowilsoni Wojciechowska & Zdzitowiecki, 1995, D. quadratum (von Linstow, 1892), D. rauschi Andersen, 1987, D. roemeri (Zschokke, 1903), D. schistochilos (Germanos, 1895), D. tetrapterum (von Siebold, 1848) and D. wilsoni (Shipley, 1907) by having an enlarged thick-walled sac-like structure in the terminal part of the uterus in mature and gravid proglottids [41].

Recently, Hermosilla et al. [24] collected two headless tapeworms from fecal samples of SASLs in Chile and considered them a ‘Diphyllobothrium scoticum-like cestode.’ The morphological description of these tapeworms by Hermosilla et al. [24] is incomplete; however, they are similar to D. sprakeri n. sp. in having a thick-walled sac-like structure in the terminal part of the uterus, longitudinal muscle layer wide (51–100 vs 100) and egg size (54–61 × 38–44 vs 59–75 × 40–47). The new species slightly differs from the the ‘Diphyllobothrium scoticum-like cestode’ by having smaller gravid proglottids (287–736 × 2681–7890 vs 825–1385 × 7077–7418) and number of uterine loops (3–4 vs 5–6). However, the size of diphyllobothriids and the number of uterine loops have a limited taxonomic value in distinguishing species (see [2, 5] and references therein). Our phylogenetic analyses confirmed that specimens of D. sprakeri n. sp. recovered from CSLs are conspecific with those from SASLs from Chile (Figs. 1, 2).

Two species of ‘Diphyllobothrium’ described from Antarctic phocids, i.e. D. scoticum and D. lobodoni Yurakhno & Maltsev, 1994, are similar to D. sprakeri n. sp. in having a thick-walled sac-like structure in the terminal part of the uterus [22, 42,43,44,45,46]. The new species can be distinguished from D. scoticum and D. lobodoni by its smaller scolex (< 1484 vs > 1800 and > 1900, respectively), absence of a neck, lower number of uterine loops (3–6 vs 5–17 and 7–22, respectively) and somewhat smaller eggs (59–75 × 39–47 vs 60–100 × 42–53 and 71–74 × 51–53, respectively) (minimum and maximum range for biometrical data for D. scoticum estimated from all available descriptions; see Table 1 for details). ‘Diphyllobothriumsprakeri n. sp. can be further differentiated from D. scoticum and D. lobodoni in the natural definitive hosts and the disparate geographical distribution (otariids from temperate waters of North and South America vs Antarctic phocids) (see below).

Table 1 Comparison of selected biometrical data among ‘Diphyllobothrium’ sprakeri n. sp., ‘Diphyllobothrium’ scoticum and ‘Diphyllobothrium’ lobodoni. The incomplete description of D. scoticum from leopard seals from Macquarie Island, Antarctica, by Johnston [44] is not included. Measurements in micrometers, unless otherwise stated

Our molecular analyses reported immature specimens of A. pacificus and D. sprakeri n. sp. in the intestine of a SASL from Peru. Immature specimens of both species are morphologically indistinguishable. Adult specimens of A. pacificus can be distinguished from the new species by the presence of the papilla-like protuberances anterior to the male gonopore [2] and the absence of a thick-walled sac-like structure in the terminal part of the uterus. To our knowledge, this is the first confirmed report of coinfection of two species of diphyllobothriid tapeworms in a single otariid from the Southern Hemisphere. Voucher specimens of A. pacificus collected in this study are deposited in the Laboratory of Epidemiology and Veterinary Economics (LEVE 910, 913, 917, 923, 925), Lima, Peru.

The voucher material identified as ‘Diphyllobothrium latum’ from CSLs off Mexico and the USA deposited in London (NHML) was substantially decomposed. These specimens were immature without developed genital organs crucial for identification. However, D. sprakeri n. sp. is similar to these specimens in the shape of the scolex and the absence of a neck. ‘Diphyllobothriumsprakeri n. sp. has been the only species of ‘Diphyllobothrium’ reported from the intestine of CSLs ([18], present study). Based on this evidence, the voucher material deposited in London is tentatively conspecific with the new species. One voucher specimen deposited in London (NHML 1980.6.3.189) was collected from a CSL stranded on the Mexican coast. In Mexico, CSLs are distributed along the east and west coasts of the Baja California Peninsula [47]. Therefore, this peninsula may represent an additional locality for D. sprakeri n. sp.

Discussion

The taxonomy of diphyllobothriids is insufficiently resolved. Identification of individual species is complicated because of their uniform strobilar morphology, the high amount of intraspecific and intraindividual variation for most morphological characters and incomplete original descriptions [3, 8].

Diphyllobothriids of pinnipeds have been revised by the present authors for more than 10 years based on detailed morphological examination of well-fixed material combined with molecular data (see [2, 4,5,6, 8, 40]). Our previous studies suggested that otariids are only definitive hosts of three diphyllobothriid species: A. pacificus, widely distributed in both hemispheres, and D. tetrapterum and Pyramicocephalus phocarum (Fabricius, 1780), limited to the Northern Hemisphere [2, 5, 8]. However, a revision of the metazoan parasites of CSLs recognized a new undescribed diphyllobothriid tapeworm which is different from these three species [4, 5, 18]. This species showed a uterine sac-like structure in mature and gravid proglottids, which is an uncommon character in diphyllobothriids. ‘Diphyllobothriumsprakeri n. sp. is the first diphyllobothriid species described from CSLs and, with A. pacificus, the second valid species of otariids from the Southern Hemisphere.

A uterine sac-like structure was described in D. scoticum from leopard seals Hydrurga leptonyx (Blainville) from several localities in Antarctica [22, 42,43,44,45,46]. This tapeworm species has also been reported in Weddell seals Leptonychotes weddellii (Lesson) in Antarctica and recently confirmed using molecular markers from southern elephant seals Mirounga leonina (L.) from Macquarie Island (Southwestern Pacific Ocean) [8, 46, 48].

Yurahkno and Maltsev [45] described D. lobodoni from the intestine of crabeater seals Lobodon carcinophagus (Hombron & Jacquinot) from Antarctica. This diphyllobothriid species differs from D. scoticum by the size of the strobila, scolex, neck and uterine sac-like structure, the shape of proglottids, thickness of the tegument and muscle layer, number of testes and the position of the cirrus sac and external seminal vesicle. However, the size of the strobila and scolex and number of testes and other structures may depend on the fixation methods, host species, its size, physiological state or intensity of infection (see [5], and references therein) and are not suitable characters in species delimitation [2, 3]. Moreover, most of the used discriminant characteristics of D. lobodoni overlap with those of D. scoticum reported from leopard seals (type-host) by other authors (Table 1). Further studies of the type material and molecular data from the type-host of D. lobodoni are necessary to confirm the validity and systematic position of this species.

Our study suggests that D. sprakeri n. sp. has a wide geographical distribution in both hemispheres, including the Pacific and Atlantic Oceans, and infects at least two otariid species. The distribution of D. sprakeri n. sp. in the Northern Hemisphere is limited to the Pacific coast of California, USA, and Baja California, Mexico. Interestingly, our new species has not been recorded in the North Pacific coast, where the diversity of diphyllobothriid tapeworms from otariids has been comprehensively evaluated in recent years [2, 5, 49, 50]. In the Southern Hemisphere, D. sprakeri n. sp. is more widely distributed, occurring in temperate waters of the Pacific coast of South America (Peru and Chile) and the Southwest Atlantic along the Patagonian coast of Argentina.

The life cycle of D. sprakeri n. sp. probably includes marine fishes as the second intermediate hosts. Recently, Mondragón Martínez [51] reported plerocercoids of A. pacificus and an unidentified species of Diphyllobothrium in marine fishes from Peru based on partial cox1 sequences. According to the phylogenetic analysis of Mondragón Martínez [51], unidentified diphyllobothriid plerocercoids, collected from anchoveta Engraulis ringens Jenyns and Pacific jack mackerel Trachurus symmetricus (Ayres), formed a clade sister to A. pacificus and Diphyllobothrium spp. Unfortunately, partial cox1 sequences of these diphyllobothriid plerocercoids are not available in the GenBank dataset. These plerocercoids probably belong to D. sprakeri n. sp.; however, sequences generated from these plerocercoids need to be analyzed in a more robust phylogenetic context for reliable species identification.

The Pacific broad tapeworm Adenocephalus pacificus is considered the most important causative agent of diphyllobothriosis among humans in South America [52]. Diphyllobothriosis caused by this species has been reported predominantly in Peru, where human infections are associated with the habits of consuming raw or undercooked marine fishes [23, 52]. Our new species may be also causative agent of human fish-borne disease in the Pacific coast of South America, but not yet recognized and certainly misidentified as A. pacificus. Molecular-based diagnoses represent the most reliable tool to identify clinical samples of diphyllobothriid tapeworms [53], especially because clinical samples or immature specimens of A. pacificus and D. sprakeri n. sp. could be morphologically indistinguishable.

Availability of data and materials

The type- and voucher material is deposited in the Helminthological Collection of the Institute of Parasitology, Česke Budějovice, Czech Republic, the National Museum of Natural History of the Smithsonian Institution, Washington DC, USA, the Parasite Collection of the Museum of Natural History, National University of San Marcos, Lima, Peru, and the Parasite Collection of the Laboratory of Epidemiology and Veterinary Economics, National University of San Marcos, Lima, Peru (see Results for accession numbers). DNA sequences generated in this study were deposited in the GenBank database (see Additional file 1: Table S1 for details). Alignments used in this study are included as additional files.

Abbreviations

BI:

Bayesian inference

cox1:

Cytochrome c oxidase subunit 1 gene

cs:

Cirrus sac

CSL:

California sea lion

esv:

External seminal vesicle

ga:

Genital atrium

IPCAS:

Helminthological Collection of the Institute of Parasitology

LEVE:

Parasite Collection of the Laboratory of Epidemiology and Veterinary Economics

lsrDNA:

Large ribosomal subunit nuclear ribosomal RNA gene

mg:

Mehlis' gland

ML:

Maximum likelihood

NMNH-USNM:

National Museum of Natural History of the Smithsonian Institution

ov:

Ovary

PCMNH:

Parasite Collection of the Museum of Natural History

SASL:

South American sea lion

te:

Testes

up:

Uterine pore

uss:

Uterine sac-like structure

ut:

Uterus

vf:

Vitelline follicle

vg:

Vagina

References

  1. 1.

    Caira JN, Jensen K. Planetary biodiversity inventory (2008–2017): Tapeworms from Vertebrate Bowels of the Earth. Lawrence: University of Kansas, Natural History Museum, Special Publication No. 25; 2017.

  2. 2.

    Hernández-Orts JS, Scholz T, Brabec J, Kuzmina T, Kuchta R. High morphological plasticity and global geographical distribution of the Pacific broad tapeworm Adenocephalus pacificus (syn. Diphyllobothrium pacificum): molecular and morphological survey. Acta Trop. 2015;149:168–78.

    Article  Google Scholar 

  3. 3.

    Kuchta R, Scholz T. Diphyllobothriidea. In: Caira JN, Jensen K, editors. Planetary Biodiversity Inventory (2008–2017): Tapeworms from Vertebrate Bowels of the Earth. Lawrence: University of Kansas, Natural History Museum, Special Publication No. 25; 2017. p. 167–89.

  4. 4.

    Waeschenbach A, Brabec J, Scholz T, Littlewood DTJ, Kuchta R. The catholic taste of broad tapeworms—multiple routes to human infection. Int J Parasitol. 2017;47:831–43.

    CAS  Article  Google Scholar 

  5. 5.

    Hernández-Orts JS, Scholz T, Brabec J, Kuzmina T, Kuchta R. Does the number of genital organs matter? Case of the seal tapeworm Diphyllobothrium (syn. Diplogonoporus) tetrapterum (Cestoda: Diphyllobothriidea). Can J Zool. 2018;96:193–204.

    Article  Google Scholar 

  6. 6.

    Schaeffner BC, Ditrich O, Kuchta R. A century of taxonomic uncertainty: re-description of two species of tapeworms (Diphyllobothriidea) from Arctic seals. Polar Biol. 2018;41:2543–59.

    Article  Google Scholar 

  7. 7.

    Mariaux J, Kuchta R, Hoberg EP. 2017. Tetrabothriidea Baer, 1954. In: Caira JN, Jensen K, editors. Planetary Biodiversity Inventory (2008–2017): Tapeworms from Vertebrate Bowels of the Earth. Lawrence: University of Kansas, Natural History Museum, Special Publication No. 25;2017: p. 357–70.

  8. 8.

    Scholz T, Kuchta R, Brabec J. Broad tapeworms (Diphyllobothriidae), parasites of wildlife and humans: recent progress and future challenges. Int J Parasitol Parasites Wildl. 2019;9:359–69.

    Article  Google Scholar 

  9. 9.

    Carretta JV, Forney KA, Lowry MS, Barlow J, Baker J, Hanson B, Muto MM. U.S. Pacific Marine Mammal Stock Assessments: 2007. Washington: US Department of Commerce NOAA Technical Memorandum, NMFS–SWFSC–414; 2007.

  10. 10.

    McClatchie S, Field J, Thompson AR, Gerrodette T, Lowry M, Fiedler PC, et al. Food limitation of sea lion pups and the decline of forage off central and southern California. R Soc Open Sci. 2016;3:150628.

    Article  Google Scholar 

  11. 11.

    Stunkard HW. Variation and criteria for generic and specific determination of diphyllobothriid cestodes. J Helminthol. 1965;39:281–96.

    CAS  Article  Google Scholar 

  12. 12.

    Dailey MD, Hill BL. A survey of metazoan parasites infesting the California (Zalophus californianus) and Steller (Eumetopias jubatus) sea lion. Bull South Calif Acad Sci. 1970;69:126–32.

    Google Scholar 

  13. 13.

    Dailey MD, Brownell RL Jr. A checklist of marine mammal parasites. In: Ridgway SH, editor. Mammals of the sea, biology and medicine. Springfield: Charles C. Thomas; 1972. p. 528–89.

    Google Scholar 

  14. 14.

    Margolis L, Dailey MD. Revised annotated list of parasites from sea mammals caught of the west coast of North America. NOAA technical report NMFS, SSRF-647. Seattle: National Oceanic and Atmospheric Administration; 1972.

  15. 15.

    Dailey MD. The distribution and intraspecific variation of helminth parasites in pinnipeds. Rapp P-V Réun Cons Int Explor Mer. 1975;169:338–52.

    Google Scholar 

  16. 16.

    Dailey MD. Baseline data on parasites from marine mammals in the Southern California Bight area. Marine mammal and seabird survey of the Southern California Bight area. Vol. III. Principal investigator's reports. Book 1. Pinnipedia, Cetacea and Parasitology. Santa Cruz: California University; 1978. p. 442–72.

  17. 17.

    Felix JR. Reported incidences of parasitic infections in marine mammals from 1892 to 1978. Lincoln: Zea E-Books; 2013.

    Google Scholar 

  18. 18.

    Kuzmina TA, Spraker TR, Kudlai O, Lisitsyna O, Zabludovskaja SO, Karbowiak G, et al. Metazoan parasites of California sea lions (Zalophus californianus): a new data and review. Int J Parasitol Parasites Wildl. 2018;7:326–34.

    Article  Google Scholar 

  19. 19.

    Crespo EA, Oliva D, Dans S, Sepúlveda M. Current status of the South American sea lion along the distribution range. Valparaíso: Editorial Universidad de Valparaíso; 2012.

    Google Scholar 

  20. 20.

    Cárdenas-Alayza S, Crespo EA, Oliveira LR. Otaria byronia. The IUCN Red List of Threatened Species; 2016. https://doi.org/10.2305/IUCN.UK.2016-1.RLTS.T41665A61948292.en

  21. 21.

    Baylis HA, in (sic) Hamilton JE. The Southern sea lion, Otaria byronia (De Blainville). Discovery Rep. 1934;8:306.

  22. 22.

    Markowski S. The cestodes of seals from the Antarctic. Brit Bull Nat Hist. 1952;1:125–50.

    Google Scholar 

  23. 23.

    Baer JG, Miranda H, Fernandez W, Medina TJ. Human diphyllobothriasis in Peru. Z Parasitenkd. 1967;28:227–89.

    Article  Google Scholar 

  24. 24.

    Hermosilla C, Hirzmann J, Silva LMR, Scheufen S, Prenger-Berninghoff E, Ewers C, et al. Gastrointestinal parasites and bacteria in free-living South American sea lions (Otaria flavescens) in Chilean Comau Fjord and new host record of a Diphyllobothrium scoticum-like cestode. Front Mar Sci. 2018;5:459.

    Article  Google Scholar 

  25. 25.

    Ebmer D, Navarrete MJ, Muñoz P, Flores LM, Gärtner U, Brabec J, et al. Anthropozoonotic parasites circulating in synanthropic and Pacific colonies of South American sea lions (Otaria flavescens): Non-invasive techniques data and a review of the literature. Front Mar Sci. 2020;7:543829.

    Article  Google Scholar 

  26. 26.

    Spraker TR. Basic Necropsy Procedures. In: McCurnin DM, editor. Clinical textbook for the animal health technician. London: W.B. Saunders Company; 1985. p. 4702–816.

    Google Scholar 

  27. 27.

    Pleijel F, Jondelius U, Norlinder E, Nygren A, Oxelman B, Schander C, et al. Phylogenies without roots? A plea for the use of vouchers in molecular phylogenetic studies. Mol Phylogenet Evol. 2008;48:369–71.

    CAS  Article  Google Scholar 

  28. 28.

    Littlewood DTJ, Curini-Galletti M, Herniou EA. The interrelationships of Proseriata (Platyhelminthes: Seriata) flatworms tested with molecules and morphology. Mol Phylogenet Evol. 2000;16:449–66.

    CAS  Article  Google Scholar 

  29. 29.

    Olson PD, Cribb TH, Tkach VV, Bray RA, Littlewood DTJ. Phylogeny and classification of the Digenea (Platyhelminthes: Trematoda). Int J Parasitol. 2003;33:733–55.

    CAS  Article  Google Scholar 

  30. 30.

    Bowles J, McManus DP. Genetic characterization of the Asian Taenia, a newly described taeniid cestode of humans. Am J Trop Med Hyg. 1994;50:33–44.

    CAS  Article  Google Scholar 

  31. 31.

    Wicht B, Yanagida T, Scholz T, Ito A, Jiménez JA, Brabec J. Multiplex PCR for differential identification of broad tapeworms (Cestoda: Diphyllobothrium) infecting humans. J Clin Microbiol. 2010;48:3111–6.

    CAS  Article  Google Scholar 

  32. 32.

    Brabec J, Scholz T, Králová-Hromadová I, Bazsalovicsová E, Olson PD. Substitution saturation and nuclear paralogs of commonly employed phylogenetic markers in the Caryophyllidea, an unusual group of non-segmented tapeworms (Platyhelminthes). Int J Parasitol. 2012;42:259–67.

    Article  Google Scholar 

  33. 33.

    Gomez-Puerta LA, Alarcon V, Pacheco J, Franco F, Lopez-Urbina MT, Gonzalez AE. Molecular and morphological evidence of Taenia omissa in pumas (Puma concolor) in the Peruvian Highlands. Rev Bras Parasitol Vet. 2016;25:368–73.

    CAS  Article  Google Scholar 

  34. 34.

    Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32:1792–2179.

    CAS  Article  Google Scholar 

  35. 35.

    Darriba D, Taboada GL, Doallo R, Posada D. jModelTest 2: more models, new heuristics and parallel computing. Nat Methods. 2012;9:772.

    CAS  Article  Google Scholar 

  36. 36.

    Huelsenbeck JP, Ronquist F. MRBAYES: Bayesian inference of phylogenetic trees. Bioinformatics. 2001;17:754–5.

    CAS  Article  Google Scholar 

  37. 37.

    Edler D, Klein J, Antonelli A, Silvestro D. raxmlGUI 2.0; 2019. https://antonellilab.github.io/raxmlGUI/

  38. 38.

    Rambaut A. FigTree v. 2.0; 2018. http://tree.bio.ed.ac.uk/software/

  39. 39.

    Kumar S, Stecher G, Li M, Knyaz C, Tamura K. MEGA X: molecular evolutionary genetics analysis across computing platforms. Mol Biol Evol. 2018;35:1547–9.

    CAS  Article  Google Scholar 

  40. 40.

    Chervy L. Unified terminology for cestode microtriches: a proposal from the International Workshops on Cestode Systematics in 2002–2008. Folia Parasitol. 2009;56:199–230.

    Article  Google Scholar 

  41. 41.

    Delyamure SL, Skryabin AS, Serdiukov AM. Diphyllobothriata—Flatworm parasites of man, mammals and birds. In: Sudarikov VE, editor. Principles of Cestodology. Vol. 11. Moscow: Izdatel’stvo Nauka: 1985, p. 200. (in Russian)

  42. 42.

    Rennie J, Reid A. The Cestoda of the Scottish Antarctic Expedition (Scotia). Trans R Soc Edinburgh. 1912;48:441–53.

    Article  Google Scholar 

  43. 43.

    Fuhrmann O. Die Cestoden der Deutschen Südpolar-Expedition 1901–1903. Deutsche Südpol-Exped. 1920;1901–1903(16):469–524.

    Google Scholar 

  44. 44.

    Johnston TH. The Cestoda of the Australasian Antarctic Expedition. Sci Rep Aust Antarctic Exped. 1937;10:1–74.

    Google Scholar 

  45. 45.

    Yurakhno MV, Maltsev VN. Diphyllobothrium lobodoni sp. n. (Cestoda: Diphyllobothriidae)—The parasite of the crabeater seal. Parazitologiya. 1994;28:270–5. (in Russian)

  46. 46.

    Wojciechowska A, Zdzitowiecki K. Cestodes of Antarctic seals. Acta Parasitol. 1995;40:125–31.

    Google Scholar 

  47. 47.

    Szteren D, Aurioles D, Gerber LR. Population status and trends of the California sea lion (Zalophus californianus californianus) in the Gulf of California, Mexico. In: Trites AW, Atkinson SK, DeMaster DP, Fritz LW, Gelatt TS, Rea LD, Wynne KM, editors. Sea Lions of the World. Fairbanks: Alaska Sea Grant College Program; 2006. p. 369–84.

    Google Scholar 

  48. 48.

    Yurakhno MV, Maltsev VN. An infection of seals from Antarctica with cestodes. Parazitologiya. 1997;31:81–9 (in Russian).

    Google Scholar 

  49. 49.

    Kuzmina TA, Hernández-Orts JS, Lyons ET, Spraker TR, Kornyushyn VV, Kuchta R. The cestode community in northern fur seals (Callorhinus ursinus) on St. Paul Island, Alaska. Int J Parasitol Parasites Wildl. 2015;4:256–63.

    Article  Google Scholar 

  50. 50.

    Kuzmina TA, Kuzmin YI, Dzeverin I, Lisitsyna OI, Spraker TR, Korol EM, Kuchta R. Review of metazoan parasites of the northern fur seal (Callorhinus ursinus) and the analysis of the gastrointestinal helminth community of the population on St. Paul Island, Alaska. Parasitol Res. 2021;120:117–32.

    Article  Google Scholar 

  51. 51.

    Mondragón Martínez AM. Identificación molecular de los estadios de plerocercoide y adulto de Diphyllobothrium sp. obtenidos de humanos, lobos marinos y peces. Bachelor Thesis. Lima: Universidad Ricardo Palma; 2017. p. 82. http://repositorio.urp.edu.pe/handle/urp/1007.

  52. 52.

    Kuchta R, Serrano-Martínez ME, Scholz T. Pacific broad tapeworm Adenocephalus pacificus as a causative agent of globally reemerging diphyllobothriosis. Emerg Infect Dis. 2015;21:1697–703.

    Article  Google Scholar 

  53. 53.

    Scholz T, Garcia HH, Kuchta R, Wicht B. Update on the human broad tapeworm (genus Diphyllobothrium), including clinical relevance. Clin Microbiol Rev. 2009;22:146–60.

    CAS  Article  Google Scholar 

Download references

Acknowledgements

The authors thank Frances Gulland, Christine Fontaine, Barbie Halaska, Padraig Duignan and other colleagues from the Marine Mammal Center, Sausalito, California, USA, for their help performing the parasitological examination of dead CSL and providing some specimens of cestodes. We also thank the staff of the Laboratorio de Mamíferos Marinos, Centro para el Estudio de Sistemas Marinos (CESIMAR – CCT CONICET – CENPAT), Puerto Madryn, Argentina, for their assistance with the examination of stranded SASL. The SASL from Peru was kindly donated by the National Forest Service and Wildlife (SERFOR) of Peru. We also thank Jan Brabec (Institute of Parasitology, Czech Republic) for providing some new sequences for this study.

Funding

This study was partially supported by the joint research project "Helminth parasites in aquatic ecosystems: their diversity and life-cycles in the changing world" between the National Academy of Science of Ukraine and the Czech Academy of Sciences (2013–2016). JSH-O benefited from a postdoctoral fellowship of the National Council of Science and Technology (CONACYT) of Mexico (Postdoctoral Number. 177603).

Author information

Affiliations

Authors

Contributions

JSH-O, TK and LG-P obtained the samples. LG-P contributed to the major part of the sequencing. JSH-O and LG-P undertook phylogenetic analyses. JSH-O, TK and RK performed the identification and morphological characterisation of the tapeworms. All authors discussed the results, helped draft the MS, read and approved the final manuscript.

Corresponding author

Correspondence to Jesús S. Hernández-Orts.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary Information

Additional file 1: Table S1.

List of taxa used in the phylogenetic analyses.

Additional file 2:

lsrDNA_alignment. Trimmed lsrDNA alignment (34 taxa; 1574 bp).

Additional file 3: cox1_alignment.

Trimmed cox1 alignment (59 taxa; 1571 bp).

Additional file 4:

lsrDNA_cox1_alignment. Combined lsrDNA + cox1 alignment (33 taxa; 3145 bp).

Additional file 5: Figure S1.

Bayesian analysis for the combined (lsrDNA + cox1) alignment. Numbers represent posterior probabilities from BI analysis (> 0.95 shown only) followed by nodal supports from ML analysis (bootstrap values > 70% shown only). The newly generated sequences are indicated in red. The scale bar indicates the expected number of substitutions per site.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Hernández-Orts, J.S., Kuzmina, T.A., Gomez-Puerta, L.A. et al. Diphyllobothrium sprakeri n. sp. (Cestoda: Diphyllobothriidae): a hidden broad tapeworm from sea lions off North and South America. Parasites Vectors 14, 219 (2021). https://doi.org/10.1186/s13071-021-04661-1

Download citation

Keywords

  • Parasites
  • Helminths
  • cox1
  • lsrDNA
  • Pinnipedia
  • Otariidae
  • Zalophus californianus
  • Otaria flavescens
\