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Fig. 5 in Worldwide sampling reveals low genetic variability in populations of the freshwater ciliate Paramecium biaurelia (P. aurelia species complex, Ciliophora, Protozoa)

Fig. 5 Haplotyp_ n_twork of Paramecium biaurelia construct_d using th_ 123 s_qu_nc_s of ribosomal ITS1- 5.8S-ITS2-5'LSU fragm_nts (a) and 139 of mitochondrial COI fragm_nts (b). Th_ n_twork pr_s_nts a comparison of haplotyp_s obtain_d in th_ Kraków ar_a vs. th_ oth_r localiti_s, wh_r_ mol_cular data for P. biaurelia is availabl_. Black dash_s on particular branch_s r_pr_s_nt nucl_otid_ substitutions b_tw__n particular haplotyp_s. Analys_s w_r_ conduct_d using th_ M_dian Joining m_thod in PopART softwar_ v. 1.7

Fig. 4 in Worldwide sampling reveals low genetic variability in populations of the freshwater ciliate Paramecium biaurelia (P. aurelia species complex, Ciliophora, Protozoa)

Fig. 4 Haplotyp_ n_twork of Paramecium biaurelia construct_d using th_ 123 s_qu_nc_s of ribosomal ITS1- 5.8S-ITS2-5'LSU fragm_nts (a) and 139 of mitochondrial COI fragm_nts (b). Th_ n_twork pr_s_nts r_ciprocal r_lationships b_tw__n, and th_ origin of P. biaurelia haplotyp_s id_ntifi_d in curr_nt study. Black dash_s on particular branch_s r_pr_s_nt nucl_otid_ substitutions b_tw__n particular haplotyp_s. Analys_s w_r_ conduct_d using th_ M_dian Joining m_thod in PopART softwar_ v. 1.7

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Figs. 1–28 in Study of Myxosporea (Myxozoa), infecting worldwide mullets with description of a new species

Figs. 1–28 Light microscope and ultrastructural data of some myxozoan parasitizing collected mullets. 1 Spores of M. muelleri. 2, 3 M. adeli sp. nov., spores (2) and spindle-shaped cysts of different maturity (3). 4, 7 M. episquamalis. Compact whitish masses on the distal parts of scales (4). Each cystic mass consists of numerous microcysts. Oval spores tapered at the anterior end (7). Polar capsules equal and pyriform. 5, 6 Spherical spores of M. ichkeulensis with oval polar capsules. No intercapsular appendix is visible (6). 8–13 M. parvus. Spores (8–11) and rounded-to-oval white cysts up to 2.0 mm in diameter (12, 13). Polar capsules contain four coils of longitudinally twisted polar filament (10). Two valvogenic cells form a good developed sutural ring (11). 14 Spores of M. nile with unequal polar capsules. 15 Spores of M. spinacurvatura. Polar capsules do not reach the midpoint of the spore length. 16–17 Alataspora sp. Spherical polar capsules located close to the anterior pole (16). Vegetative stages presented by rounded or oval-shaped bisporous plasmodia with transparent ectoplasm and small-grained endoplasm (17). 18 Kudoa trifolia. Four small subspherical polar capsules are located in the central part of the spore,

Fig. 5 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 5 Lectotype of modiomorphid bivalve Caspiconcha major (Gabb, 1869) MCZ 108539 from east of Knoxville, California, USA, Lower Cretaceous. The pairs A and B, C and D, and E and F are the same views, respectively with and without morphological interpretations. A, B. Left valve. C, D. Right valve. The shell of the specimen is missing forward of the anterior adductor muscle scar, leaving an internal mould. E, F. Dorsal view. G. Detail of ligament area of left valve. White arrowheads point to the anterior.

Fig. 4 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 4. Shell microstructure of modiomorphid bivalve Caspiconcha major (Gabb, 1869) CAS 72527−9 from Eagle Creek, California, USA, Upper Barremian (Lower Cretaceous). External shell surface upwards in all figures. A.Vertical cross section through shell in the pallial region; see Fig. 3B for location. B. Demarcation between middle (cross lamellar) and inner (complex cross lamellar) layers. C. Outer layer homogeneous structure. D. Lower part of inner layer, note diagenetic alteration at base.

Fig. 1. Locality map and outcrop photographs. A in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 1. Locality map and outcrop photographs. A. Locality map of the Utagoesawa Creek site, Hatonosu, Yubari City, Hokkaido, Japan. Also shown is the location of the Omagari seep site. Solid pattern is the outcrop area of the Cretaceous Yezo Group strata. B. Outcrop photograph of an Utagoesawa Creek carbonate body showing large Caspiconcha sp. and/or probable lucinid bivalve fossils. C. Locality map of hydrocarbon seeps in California. Subpanel shows locality map of the Eagle Creek site, Ono, California, USA. Solid circle with number indicates Caspiconcha bearing sites. 1, Eagle Creek; 2, Cold Fork of Cottonwood Creek; 3, Paskenta; 4, Bear Creek; 5, Wilbur Springs; 6, east of Knoxville (exact place is unknown); +

Fig. 12. Modiomorphid bivalve Myoconcha americana Stanton, 1895 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 12. Modiomorphid bivalve Myoconcha americana Stanton, 1895 (USNM 23042), right valve. A. External view. B. Dorsal view. C. Detail of the hinge area showing a possible tooth. D. Detail of shell surface ornamentation. Growth lines show rectoangular shape of shell. Black arrowheads point to faint radiaxial ribs mostly obscured by the glue in this image. White arrowheads point to the anterior.

Fig. 10 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 10. Modiomorphid bivalve Caspiconcha major (Gabb, 1869) from east of Berryessa (A and D), Cold Fork of Cottonwood Creek (B and E), and Wilbur Springs (C), all California, USA. A. Right valve of large specimen CAS 72535 with missing posterior area, right valve (A1), dorsal view (A2). B. Right valve of small specimen UCMP 10226. C. Internal mould of right valve of small specimen CAS 72537; see Fig. 9G for cast. D. Articulated specimen internal mould with missing posterior margin CAS 72536, left valve (D1), dorsal view (D2). See Fig. 9I for casts. E. Articulated small specimen internal mould UCMP 10225, right (E1) and left (E2) valves, dorsal view (E3). See Fig. 9A for cast. White arrowheads point to the anterior.

Fig. 3 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 3. Modiomorphid bivalve Caspiconcha major (Gabb, 1869) CAS 72527−9 from Eagle Creek, California, USA, Upper Barremian (Lower Cretaceous). Right valve. A. External view. B. Internal view. Details of pedal elevator muscle scar (C) and mantle muscle scars indicated by small arrowheads (D). Location of shell microstructure analysis (Fig. 4) is marked with a dotted white line. Black arrowheads point to the anterior.

Fig. 9 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 9. Silicone rubber casts of modiomorphid bivalve Caspiconcha major (Gabb, 1869) from Cold Fork of Cottonwood Creek (A), Wilbur Springs (B–G), + East Berryessa (H, I) and Bear Creek (J), all California, USA. A. Internal surface of articulated small specimen UCMP 10225, right valve (A1), left valve (A2). B. Internal surface of left valve of small specimen UCMP 152077. C. Internal surface of right valve of small specimen CAS 71880. D. Internal surface of left valve of small specimen with some shell remains along the ventral margin CAS 71882. E. Internal surface of left valve of small specimen CAS 71881. F. Internal surface of right valve of small specimen CAS 71883. G. Internal surface of right valve of small specimen with some shell remains in posterior area CAS 72537. H. Internal surface of left valve of small specimen CAS 72548. I. Internal surfaces of articulated specimen CAS 72536 with missing posterior margin, right valve (I1), left valve (I2). J. Internal surface of left valve of partial large specimen with internal shell details highlighted with dotted white lines CAS 72534. White arrowheads point to the anterior.

Fig. 15 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 15. Ranges and palaeoecological interpretations of major group of chemosynthetic bivalves and brachiopods from Late Jurassic to Recent hydrocarbon seeps. The epifauna and semi−infauna almost vanished at the end of Early Cretaceous and did flourish again from the Eocene with the appearance of vesicomyids and bathymodiolins. Caspiconcha was common until the end of the Early Cretaceous after which there was only one occurrence in the Late Cretaceous. In contrast, infaunal bivalves were present continuously from the late Mesozoic to the Recent.

Fig. 6 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 6. Paralectotypes of modiomorphid bivalve Caspiconcha major (Gabb, 1869). A. MCZ108540 from east of Knoxville, California, USA, Lower Cretaceous. Internal mould of left valve (A1), dorsal view (A2). B–D. Three specimens of Caspiconcha major (Gabb, 1869) from Wilbur Springs, California, USA, Hauterivian (Lower Cretaceous). B. Left valve of MCZ 108538A. C. Internal mould of right valve of MCZ 108538B. D. Right valve of MCZ 108538C. White arrowheads point to the anterior.

Fig. 14 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 14. Palaeobiogeographical distribution of Caspiconcha and Caspiconcha−like species in the late Mesozoic world's oceans. A. Palaeomap at 120 Ma from http://jan.ucc.nau.edu/~rcb7/index.html. B. Caspiconcha major (Gabb, 1869), Late Jurassic (Tithonian) to Early Cretaceous (Albian) from California, USA. The specimen is from the Eagle Creek site. C. Caspiconcha sp., Lower Cretaceous (Albian) of Basque, Spain (image from Agirrezabala et al. in press). D. Caspiconcha whithami Kelly, 2000, Lower Cretaceous (Barremian) of Greenland (SMUC K 8318, holotype). E. Possible Caspiconcha, described as Calyptogena sp. in Hikida et al. (2003) from the Upper Cretaceous (Campanian) Omagari site, Hokkaido, Japan. F. Caspiconcha sp., Lower Cretaceous (Albian), Utagoesawa Creek, Hokkaido, Japan. G. C. rubani Kiel et al. (2010), Lower Cretaceous (Hauterivian) of Ukraine (image from Kiel et al. 2010). H. Caspiconcha sp., Lower Cretaceous to Upper Cretaceous (Upper Albian to middle Cenomanian) of New Zealand (image from Kiel et al. in press).

Fig. 2 in Worldwide distribution of the modiomorphid bivalve genus Caspiconcha in late Mesozoic hydrocarbon seeps

Fig. 2. Schematic illustration of the right valve internal features of Caspiconcha major (Gabb, 1869).

Fig. 1 in Epidemiology of a major honey bee pathogen, deformed wing virus: potential worldwide replacement of genotype A by genotype B

Fig. 1. Relative proportion of DWV genotype A and B reads in publicly available NCBI transcriptome datasets of honey bees, V. destructor mites and bumble bees.

Fig. 2 in Epidemiology of a major honey bee pathogen, deformed wing virus: potential worldwide replacement of genotype A by genotype B

Fig. 2. First published records of DWV genotype B in Varroa destructor (closed box) or in Apis mellifera (red boxes: pre-2010; open boxes: 2010 onwards) from a country or geographic region; citations are in Table 3. (For interpretation of the references to colour in this figure legend, the reader is referred to the Web version of this article.)

Fig. 4 in Epidemiology of a major honey bee pathogen, deformed wing virus: potential worldwide replacement of genotype A by genotype B

Fig. 4. Temporal change in the proportion of DWV-A to DWV-B across our own datasets (a) (prevalence in Fig. 3); in published datasets (b) (UK data in Kevill et al. (2021); continental USA data in Ryabov et al. (2017); and Hawaii data in Grindrod et al. (2021)); and (c) in NCBI NGS honey bee datasets of Fig. 1 presented by geographic origin.

Fig. 3 in Epidemiology of a major honey bee pathogen, deformed wing virus: potential worldwide replacement of genotype A by genotype B

Fig. 3. Temporal change in the prevalence of DWV-A and DWV-B in honey bees in three original datasets separated by 5–6 years from the same sampling localities in the UK (individual honey bees collected at flowers), Germany (pooled honey bees from collapsing colonies) and Italy (NGS reads from pooled or individual honey bees); Germany 2019 samples were summed 2019–2020; Italy 2011 samples were summed 2009–2013 and Italy 2019 samples were summed 2018–2020.

Fig. 2 in Worldwide sampling reveals low genetic variability in populations of the freshwater ciliate Paramecium biaurelia (P. aurelia species complex, Ciliophora, Protozoa)

Fig. 2 Phylog_n_tic tr__ construct_d for Paramecium aurelia compl_x, P. jenningsi compl_x and P. schewiakoffi (two sp_ci_s: P. caudatum and P. multimicronucleatum w_r_ us_d as an outgroup). Th_ tr__ was construct_d on th_ basis of a comparison of s_qu_nc_s from th_ ribosomal ITS1-5.8S-ITS2-5'LSU fragm_nt using th_ maximum lik_lihood m_thod. Bootstrap valu_s for n_ighbor joining, maximum parsimony, maximum lik_lihood, and post_rior probabiliti_s for

Fig. 3 in Worldwide sampling reveals low genetic variability in populations of the freshwater ciliate Paramecium biaurelia (P. aurelia species complex, Ciliophora, Protozoa)

Fig. 3 Phylog_n_tic tr__ construct_d for Paramecium aurelia compl_x, P. jenningsi compl_x and P. schewiakoffi (two sp_ci_s: P. caudatum and P. multimicronucleatum w_r_ us_d as an outgroup). Th_ tr__ was construct_d on th_ basis of a comparison of s_qu_nc_s from th_ mitochondrial COI fragm_nt using th_ maximum lik_lihood m_thod. Bootstrap valu_s for n_ighbor joining, maximum parsimony, maximum lik_lihood, and post_rior probabiliti_s for Bay_sian inf_r_nc_ ar_