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Рис. 3. Battaristis chagresi M. Omelko et N. Omelko sp. nov.: A, B — внешний виΑ бабочки; C, D — генитаΛии самца (D — винкуΛум, юкста и эΑеагус) Fig. 3. Battaristis chagresi M. Omelko et N. Omelko sp. nov.: A, B — general appearance of moth; C, D — male genitals (D — vinculum, juxta and aedeagus) in New species of gelechiid moths of the genera Photodotis Meyrick 1911 and Battaristis Meyrick 1914 (Lepidoptera, Gelechiidae) from Panama

Рис. 3. Battaristis chagresi M. Omelko et N. Omelko sp. nov.: A, B — внешний виΑ бабочки; C, D — генитаΛии самца (D — винкуΛум, юкста и эΑеагус) Fig. 3. Battaristis chagresi M. Omelko et N. Omelko sp. nov.: A, B — general appearance of moth; C, D — male genitals (D — vinculum, juxta and aedeagus)

Рис. 2. Battaristis conifera M. Omelko et N. Omelko sp. nov.: A–C — внешний виΑ бабочки (C — гоΛова и нижнегубной щупик); D, E — генитаΛии самца Fig. 2. Battaristis conifera M. Omelko et N. Omelko sp. nov.: A–C — general appearance of moth (C — head and labial palpus); D, E — male genitals in New species of gelechiid moths of the genera Photodotis Meyrick 1911 and Battaristis Meyrick 1914 (Lepidoptera, Gelechiidae) from Panama

Рис. 2. Battaristis conifera M. Omelko et N. Omelko sp. nov.: A–C — внешний виΑ бабочки (C — гоΛова и нижнегубной щупик); D, E — генитаΛии самца Fig. 2. Battaristis conifera M. Omelko et N. Omelko sp. nov.: A–C — general appearance of moth (C — head and labial palpus); D, E — male genitals

Рис. 3. Namlika orbiculatovalva M. Omelko et N. Omelko, sp. nov., генитаΛии (A–C — самец: A — общий виΑ, B — эΑеагус, C — стернит и тергит 8-го сегмента брюшка с пучками анΑрокониаΛьных чешуек; D, E — самка) Fig. 3. Namlika orbiculatovalva M. Omelko et N. Omelko, sp. nov., genitalia, (A–C — male: A — general side view, B — aedeagus, C — sternite, tergite and bundles of androconial scales on the 8th abdominal segment; D, E — female) in Two new species of gelechiid moths from the genus Namlika M. Omelko et N. Omelko (Lepidoptera: Gelechiidae, Gelechiinae) from Borneo

Рис. 3. Namlika orbiculatovalva M. Omelko et N. Omelko, sp. nov., генитаΛии (A–C — самец: A — общий виΑ, B — эΑеагус, C — стернит и тергит 8-го сегмента брюшка с пучками анΑрокониаΛьных чешуек; D, E — самка) Fig. 3. Namlika orbiculatovalva M. Omelko et N. Omelko, sp. nov., genitalia, (A–C — male: A — general side view, B — aedeagus, C — sternite, tergite and bundles of androconial scales on the 8th abdominal segment; D, E — female)

Рис. 2. Namlika aculeatovalva M. Omelko et N. Omelko, sp. nov., генитаΛии (A, B — самец: A — общий виΑ со стернитом, тергитом и пучком анΑрокониаΛьных чешуек, B — эΑеагус; C — самка) Fig. 2. Namlika aculeatovalva M. Omelko et N. Omelko, sp. nov., genitalia (A, B – male: A — general side view with sternite, tergite and bundle of androconial scales; B — aedeagus; C — female) in Two new species of gelechiid moths from the genus Namlika M. Omelko et N. Omelko (Lepidoptera: Gelechiidae, Gelechiinae) from Borneo

Рис. 2. Namlika aculeatovalva M. Omelko et N. Omelko, sp. nov., генитаΛии (A, B — самец: A — общий виΑ со стернитом, тергитом и пучком анΑрокониаΛьных чешуек, B — эΑеагус; C — самка) Fig. 2. Namlika aculeatovalva M. Omelko et N. Omelko, sp. nov., genitalia (A, B – male: A — general side view with sternite, tergite and bundle of androconial scales; B — aedeagus; C — female)

Рис. 1. Внешний виΑ бабочек: A, B, C, D — Anicilla bicornuta M. Omelko et N. Omelko nom. nov., sp. nov. (A — гоΛова и нижнегубной щупик; B, C — самцы; D — самка), E — Semipsoricoptera longiaurita gen. nov., sp. nov., самец Fig. 1. General appearance of moths: A, B, C, D — Anicilla bicornuta M. Omelko et N. Omelko nom. nov., sp. nov. (A — head and labial palpus; B, C — males; D — female); E — Semipsoricoptera longiaurita gen. nov., sp. nov., male in A new genus and two new species of gelechiid moths from the subfamily Gelechiinae (Lepidoptera, Gelechiidae) from Borneo

Рис. 1. Внешний виΑ бабочек: A, B, C, D — Anicilla bicornuta M. Omelko et N. Omelko nom. nov., sp. nov. (A — гоΛова и нижнегубной щупик; B, C — самцы; D — самка), E — Semipsoricoptera longiaurita gen. nov., sp. nov., самец Fig. 1. General appearance of moths: A, B, C, D — Anicilla bicornuta M. Omelko et N. Omelko nom. nov., sp. nov. (A — head and labial palpus; B, C — males; D — female); E — Semipsoricoptera longiaurita gen. nov., sp. nov., male

Рис. 2. Anicilla bicornuta M. Omelko et N. Omelko, nom. nov., sp. nov., генитаΛии (A, B — самец: A — общий виΑ сбоку; B — стернит, тергит и пучки анΑрокониаΛьных чешуек на 8-м сегменте брюшка; C — самка) Fig. 2. Anicilla bicornuta M. Omelko et N. Omelko nom. nov., sp. nov., genitalia (A, B — male: A — lateral view; B — sternite, tergite and bundles of androconial scales on the 8th abdominal segment; C — female) in A new genus and two new species of gelechiid moths from the subfamily Gelechiinae (Lepidoptera, Gelechiidae) from Borneo

Рис. 2. Anicilla bicornuta M. Omelko et N. Omelko, nom. nov., sp. nov., генитаΛии (A, B — самец: A — общий виΑ сбоку; B — стернит, тергит и пучки анΑрокониаΛьных чешуек на 8-м сегменте брюшка; C — самка) Fig. 2. Anicilla bicornuta M. Omelko et N. Omelko nom. nov., sp. nov., genitalia (A, B — male: A — lateral view; B — sternite, tergite and bundles of androconial scales on the 8th abdominal segment; C — female)

Fig. 4 in Intestinal coccidiosis of anadromous and landlocked alewives, Alosa pseudoharengus, caused by Goussia ameliae n. sp. and G. alosii n. sp. (Apicomplexa: Eimeriidae)

Fig. 4. Goussia alosii from the intestine of landlocked alewives, bar = 10 μm. Wet mount of (A) highly elongated unsporulated oocysts and (B) sporulated oocysts with a thicker oocyst wall making up a very regular oval shape containing four highly elongated sporocysts. (C–E) Histology of coccidial stages in the intestine; (C) various stages of coccidia with an epicellular position within the intestinal epithelium; elongated unsporulated oocysts (arrows) found within the (D) intestinal epithelium and (E) within mucoid casts in the intestinal lumen.

Fig. 3 in Intestinal coccidiosis of anadromous and landlocked alewives, Alosa pseudoharengus, caused by Goussia ameliae n. sp. and G. alosii n. sp. (Apicomplexa: Eimeriidae)

Fig. 3. Goussia ameliae from landlocked alewives, bar = 10 μm. (A–C) Wet mounts of fresh coccidia preparations with (A) unsporulated oocysts and (B,C) sporulated oocysts containing four elongated sporocysts. (D–H) Histology documenting the development of the coccidian in the pyloric cecum, stained with H&E. (D) Meronts containing merozoites within the brush border on the surface of the intestinal epithelium; (E) early developmental stages (arrowheads) embedded within the brush border; (F) macrogamonts with an epicellular position on the intestinal epithelium; (G) microgametocytes (arrowhead) and unsporulated oocysts (arrow) which have sloughed from the epithelial surface; (H) severe coccidiosis with various developmental stages occupying most of the surface of the intestinal epithelium.

Fig. 2 in Intestinal coccidiosis of anadromous and landlocked alewives, Alosa pseudoharengus, caused by Goussia ameliae n. sp. and G. alosii n. sp. (Apicomplexa: Eimeriidae)

Fig. 2. Histology of coccidia infection in the intestine of anadromous alewives, stained with H&E, bar = 10 μm. (A,B) Spherical early developmental stages (arrowheads) within the brush border of the intestinal epithelium; (C) macrogamonts (arrowhead) (notice the notches nearly midway through the parasite, embedded within the surface of the intestinal epithelium); (D) macrogamonts with notches (arrowhead) and unsporulated elongated oocysts (arrows) within the intestinal epithelium.

Fig. 1 in Intestinal coccidiosis of anadromous and landlocked alewives, Alosa pseudoharengus, caused by Goussia ameliae n. sp. and G. alosii n. sp. (Apicomplexa: Eimeriidae)

Fig. 1. Goussia ameliae from anadromous alewives, bar = 10 μm. (A–C) Wet mounts of fresh coccidia preparations with (A) unsporulated oocysts, (B) oocysts in the process of sporulation, and (C) sporulated oocysts containing four sporocysts. (D–H) Histology documenting various stages of coccidia infection in the pyloric cecum, stained with H&E. (D) Intestinal epithelium with a severe infection of coccidia stages including gamonts and unsporulated oocysts covering the intestinal epithelium; (E) meront containing merozoites (arrow) attached to the microvillar surface of intestinal epithelial cells; (F) gamogony with macrogamonts (arrow) and microgametocytes (arrowhead) with an epicellular position; (G) unsporulated oocysts with an epicellular position (notice below, the focal necrosis to the intestinal epithelium); (H) a focal erosion in the intestinal epithelium with unsporulated and sporulated (arrow) oocysts released into the lumen.

Fig. 5 in Intestinal coccidiosis of anadromous and landlocked alewives, Alosa pseudoharengus, caused by Goussia ameliae n. sp. and G. alosii n. sp. (Apicomplexa: Eimeriidae)

Fig. 5. Line drawings of sporulated oocysts of Goussia ameliae from (A) anadromous and (B) landlocked alewives and (C) G. alosii sampled from landlocked alewives, bar = 5 μm.

Fig. 6 in Intestinal coccidiosis of anadromous and landlocked alewives, Alosa pseudoharengus, caused by Goussia ameliae n. sp. and G. alosii n. sp. (Apicomplexa: Eimeriidae)

Fig. 6. Phylogenetic tree based on maximum likelihood analysis (-ln = 5197.3909) based on 16 sequences obtained from Genbank and one sequence from this study (G. ameliae denoted with a bold circle). Goussia ameliae fit into a fish Goussia clade, which is distinct from other fish coccidians (*). Theilleria parva was used as an outgroup to root the tree.

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Figure 3 in Severe glomerular disease in juvenile grey snapper Lutjanus griseus L. in the Gulf of Mexico caused by the myxozoan Sphaerospora motemarini n. sp.

Figure 3. SSU rDNA-based maximum likelihood (GTR + Γ model) tree of 26 myxosporean sequences showing the phylogenetic position of Sphaerospora motemarini n. sp. amongst all other polysporoplasmid Sphaerospora spp. sequenced to date (red) and within the Sphaerospora sensu stricto clade (yellow). Members of marine (blue) and freshwater (green) myxosporean lineages were used as outgroups. Maximum likelihood bootstraps/maximum parsimony bootstraps/Bayesian posterior probabilities shown at nodes. Dashes indicate bootstrap values <50 or not present in the maximum parsimony or Bayesian tree.

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Figure 2 in Severe glomerular disease in juvenile grey snapper Lutjanus griseus L. in the Gulf of Mexico caused by the myxozoan Sphaerospora motemarini n. sp.

Figure 2. Line drawing of spore of Sphaerospora motemarini n. sp. summarizing all morphological details in two dimensions; spore with bilateral symmetry, labels given only on one side: SV = spore valve, VN = nucleus of valve cell, OP = ornamental surface pits on posterior part of spore valve, PC = polar capsule containing coiled polar filament (PF), PN = nucleus of polar capsule, SP = uninucleated sporoplasms (6); bar = 5 µm.

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Figure 1 in Severe glomerular disease in juvenile grey snapper Lutjanus griseus L. in the Gulf of Mexico caused by the myxozoan Sphaerospora motemarini n. sp.

Figure 1. Morphology and histopathology of Sphaerospora motemarini n. sp. in grey snapper, Lutjanus griseus. (A) Mature spore in fresh kidney smear showing thickened suture at apical part (transparent arrowhead), two prominent bulges at posterior part (black arrowheads) and valve surface ornamentation (detailed in D) at the posteriolateral part of the spore; bar = 10 µm. (B) DAPI nuclear staining showing polysporoplasmic nature of spore (4 out of 6 sporoplasms visible in plane of image); bar = 10 µm. (C) Pseudoplasmodium containing two croissant-shaped sporoplasms (only visible around left spore) and two spores; bar = 10 µm. (D) SEM showing spore surface ornamentation in the shape of pits providing an opening to a multilayered canal system; bar = 5 µm. (E) Fresh smear of kidney showing early plasmodial stages (arrowheads) in a glomerulus; bar = 20 µm. (F–H) Histological sections stained with H&E; bar = 50 µm (F). Histopathological changes showing massive enlargement of renal corpuscles, with arrows in small insert (bottom left) indicating uninfected corpuscles of normal size in an uninfected kidney; bar = 50 µm. (G) Thickening of Bowman's capsule (arrows) and proliferation of mesangial cells; bar = 50 µm. (H) Engulfment of a spore by a melanin-rich macrophage (brown color); bar = 10 µm.

Fig. 6 in Negative effects of Kudoa islandica n. sp. (Myxosporea: Kudoidae) on aquaculture and wild fisheries in Iceland

Fig. 6. SSU rDNA maximum likelihood phylogenetic tree of 16 Kudoa spp. Kudoa islandica is robustly and consistently placed with other Kudoa taxa in all analyses, but is not well supported in the clade it is placed in. Numbers at the nodes represent bootstrap support from 1000 samplings, nodes with a support of <50 are considered not supported (ns).

Fig. 4 in Negative effects of Kudoa islandica n. sp. (Myxosporea: Kudoidae) on aquaculture and wild fisheries in Iceland

Fig. 4. Line drawings of Kudoa islandica n. sp. in apical view (A) and lateral view (B). Scanning electron microscope images of K. islandica n. sp. (C–E). Mature spore in lateral view showing extruded polar filaments (arrow) (C). Single spore in apical view (D) showing the sutures of the four valves (broad arrows), the four apical projections (thin arrow) and cytoplasmic projections (arrowhead). Single spore in posterior view (E) showing the suture of the four valves (broad arrows), Scale bars: (A) and (B) = 2 µm; (C), (D) and (E) = 1 µm.

Fig. 3 in Negative effects of Kudoa islandica n. sp. (Myxosporea: Kudoidae) on aquaculture and wild fisheries in Iceland

Fig. 3. Fresh mature spores of Kudoa islandica n. sp. as seen in fresh squash preparations from muscular tissue of Atlantic wolffish, Anarhichas lupus. Note the protruding polar filament of one of the spores (arrow). Nomarski differential interference contrast. Scale bar = 10 µm.

Fig. 5 in Negative effects of Kudoa islandica n. sp. (Myxosporea: Kudoidae) on aquaculture and wild fisheries in Iceland

Fig. 5. (A) and (B) Muscle section from lumpfish, Cyclopterus lumpus, fixed 24 h post mortem. (A) Ruptured Kudoa plasmodia with subsequent liberation of mature spores causing focal necrosis of the muscle fibre enveloping the plasmodium. (B) Higher magnification showing liberated spores (arrows) and a focal necrosis in the vicinity of the spores (asterisk). (C) Muscle section of an uninfected fish at approx. 48 h p.m. (D) Section of muscle of a heavily infected fish at approximately 48 h p.m. showing extensive myoliquefaction (asterisk). (E) A close up of the affected area showing numerous Kudoa spores (arrowhead) and the associated liquefactive necrosis. Scale bars: (A) = 50 µm, (B) = 10 µm, (C) and (D) = 200 µm, (E) = 10 µm. Abbreviations: MF = Muscle fibres, AC = Adipocytes.

Fig. 2 in Negative effects of Kudoa islandica n. sp. (Myxosporea: Kudoidae) on aquaculture and wild fisheries in Iceland

Fig. 2. (A) Stained histological section of a lumpfish muscle showing a considerable portion of the muscle fibres substituted with Kudoa islandica n. sp. plasmodia. (B) A single infection. (C) A double infection. (D) Multiple infection; numerous plasmodia developing inside a single muscle fibre, separated from each other and the muscle tissue with a thin membrane (arrows). (E) Plasmodial membranes separating two plasmodia (arrows). Inside each plasmodium are numerous mature Kudoa spores. Scale bars: (A) = 300 µm (B) and (C) = 25 µm; (D) = 150 µm; (E) = 5 µm.