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All issues Volume 23 (2016) Parasite, 23 (2016) 47 Full HTML
Open Access
Issue
Parasite
Volume 23, 2016
Article Number 47
Number of page(s) 10
DOI https://doi.org/10.1051/parasite/2016057
Published online 15 November 2016

© S. Greani et al., published by EDP Sciences, 2016

Licence Creative CommonsThis is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Introduction

The absence of fossils is a feature in Platyhelminthes, especially parasites. Therefore, to understand the relationships between species and their phylogeny, it is possible to research extant taxa, and include morphological and ultrastructural data, and more recently molecular analysis findings. Although the number of ultrastructural studies of vitellogenesis in digeneans has increased, several species (or families) have not been significantly examined to date. In fact, among the 18,000 digenean species [3, 10] that have been described, fewer than 20 were studied for their vitellogenesis [7, 8, 12–15, 21–24, 30, 32, 37, 42, 45, 46]. Crepidostomum metoecus (Braun, 1900) is already listed in several studies as a parasite of brown trout in European countries [39]. According to Quilichini et al. (2007), the wide geographical distribution has led to diversity of intermediate hosts [39]. The vitelline cells provide the material necessary for the formation of the eggshell and the essential nutrient material for the development of the future embryo. The oogenesis of trematodes has been the subject of several studies by light and electron microscope [2, 4, 6, 16, 18, 20, 25, 29, 31, 33, 40, 43, 44, 48, 49, 50–53]. The female reproductive system of Platyhelminthes shows great morphological variability with significant differences in anatomical organization and cell structure between taxa. Platyhelminthes have been subdivided into two levels of organization, according to the female reproductive system. The Archoophora possess homocellular female gonads consisting of only germaria with oocytes which produce both yolk and eggshell forming precursors. The Neoophora are characterized by heterocellular female gonads composed of an ovary and vitelline glands. The neoophoran digenean Crepidostomum metoecus belongs to the Allocreadiidae family (Looss, 1902). The Allocreadiidae are relatively small digeneans that are parasites of the digestive system of teleosts, and occasionally snakes, salamanders, and frogs. The present study shows, for the first time, the ultrastructure of the female gonads of an Allocreadiidae. The aim of this study was to describe the ultrastructural characteristics of oocytes and vitellocytes during their differentiation.

Materials and methods

Adult specimens of Crepidostomum metoecus were collected live from the intestine of naturally infected Salmo trutta (Linnaeus, 1758) collected in Corsica. Worms were removed from their hosts, fixed in cold (4 °C) 2.5% glutaraldehyde in 0.1 M sodium cacodylate buffer at pH 7.2, rinsed in 0.1 M sodium cacodylate buffer at pH 7.2, postfixed in cold (4 °C) 1% osmium tetroxide in the same buffer for 1 h, dehydrated in ethanol and propylene oxide, embedded in Spurr, and polymerized at 60 °C for 24 h. Ultrathin sections (60–90 nm) of the worms, at the level of the ovary or vitelline follicles, were cut on an ultramicrotome (PowerTome PC, RMC Boeckeler). Sections were placed on 300- and 200-mesh copper and gold grids. Sections on copper grids were stained with uranyl acetate and lead citrate [41]. Sections on gold grids were stained with periodic acid, thiocarbohydrazide, and silver proteinate [47]. This technique was used to detect glycogen. Sections were examined on a Hitachi H-7650 transmission electron microscope, operating at an accelerating voltage of 80 kV, in the “Service d’Étude et de Recherche en Microscopie Électronique” of the University of Corsica (Corte, France).

Results

Vitellogenesis

The vitelline glands of C. metoecus contain vitellocytes at various stages of development, with younger cells localized in the periphery of the vitelline lobes. One cell type is observed and there are no cytoplasmic extensions between vitellocytes. Follicular vitellarium is surrounded by a basal lamina (Figs. 1, 3). Vitellocyte maturation is divided into four main stages. At the first stage, vitellocytes are undifferentiated cells showing a high nucleo-cytoplasmic ratio (Figs. 1, 15) and measure about 6 μm in diameter. The cytoplasm is mainly filled with free ribosomes, some mitochondria, and scarce endoplasmic reticulum sacculi (Fig. 2). Some heterochromatin is present in the nucleoplasm. At the second stage, the nucleo-cytoplasmic ratio decreases (Figs. 3, 15), and Golgi complexes are evident in the cytoplasm (Fig. 4). At this stage, single shell inclusions coalesce to form clusters of electron-dense globules delimited by a membrane and measure about 10 μm in diameter. The nucleus often contains a large nucleolus (Fig. 3). At the third stage, single shell globules coalesce into clusters (Figs. 5, 15) and vitellocytes measure about 14 μm in diameter. There are less mitochondria and reticulum endoplasmic sacculi (Fig. 6). Some small lipid droplets were seen in the cytoplasm, and glycogen particles were detected according to the Thiéry method (Fig. 7). At the last stage, there are many shell globule clusters in the cytoplasm (>30 per cross-section), measuring about 19 μm in diameter. The cytoplasm also contains some mitochondria, and scarce endoplasmic reticulum sacculi at the periphery of the cell (Fig. 8). Mature vitellocytes of Crepidostomum metoecus possess a high amount of saturated lipid content (>10 lipid droplets per cell cross-section) (Figs. 8, 9) and many glycogen particles (Figs. 10, 15).

thumbnail Figures 1–4.

Stages 1 and 2 of vitellogenesis in C. metoecus. (1) An immature vitellocyte (Stage 1) at the periphery of the follicle. The nucleus is filled with heterochromatin and the cell possesses a high nucleo-cytoplasmic ratio. Scale bar = 1 μm. (2) Immature vitellocyte at first stage of maturation filled with ribosomes, mitochondria, and few endoplasmic reticulum saccules. Scale bar = 1 μm. (3) Electron micrograph of second stage of vitelline cells’ maturation (arrowheads: basal lamina). Scale bar = 1 μm. (4) Part of the cytoplasm of a cell at second stage of maturation showing Golgi complexes and granular endoplasmic reticulum. Scale bar = 1 μm. GC: golgi complex; GER: granular endoplasmic reticulum; Hch: heterochromatin; M: mitochondrion; N: nucleus; Nl: nucleolus; SG: shell globule.

thumbnail Figures 5–8.

Stages 3 and 4 of vitellogenesis in C. metoecus. (5) General observation of a vitelline cell at the third stage of maturation. Scale bar = 1 μm. (6) The third stage of vitellocyte maturation showing the coalescence of single shell globules into a cluster surrounded by a membrane. Scale bar = 1 μm. (7) Cytoplasm of a vitelline cell at the third stage of maturation containing shell globule cluster and saturated lipid droplets, surrounded by glycogen granules. Stained according to the Thiéry method. Scale bar = 1 μm. (8) Electron micrograph of a vitelline cell at the fourth stage of maturation filled with shell globule clusters and lipid droplets. Scale bar = 1 μm. G: glycogen particle; GER: granular endoplasmic reticulum; L: lipid droplet; M: mitochondrion; N: nucleus; Nl: nucleolus; SG: shell globule; SGC: shell globule cluster.

thumbnail Figure 9–12.

Stage 4 of vitellogenesis and primary oocyte stage of oogenesis in C. metoecus. (9) A group of saturated lipid droplets, surrounded by glycogen granules, and a few shell globule clusters. Scale bar = 1 μm. (10) A part of the cytoplasm of a vitelline cell at the fourth stage of maturation. Note the abundance of glycogen granules around lipid droplets. Stained according to the Thiéry method. Scale bar = 1 μm. (11) Electron micrograph cross-section of ovary (arrowheads: basal lamina). Germ cells of the four stages of maturation are observed (I–IV). Scale bar = 2 μm. (12) Primary oocyte showing a small amount of cytoplasm, filled with free ribosomes, mitochondria, few granular endoplasmic reticula, and a chromatoid body. Scale bar = 1.5 μm. CB: chromatoid body; G: glycogen particle; GER: granular endoplasmic reticulum; L: lipid droplet; M: mitochondrion; N: nucleus; Nl: nucleolus; P: parenchyma; SGC: shell globule cluster.

thumbnail Figure 13 and 14.

Developing and mature oocytes in C. metoecus. (13) General observation of a developing oocyte. Note the presence of synaptonemal complexes indicating the zygotene-pachytene stage of the first meiotic division. Inset: detail of a synaptonemal complex. Scale bar = 2 μm. (14) General observation of a fully mature germ cell, with a low nucleo-cytoplasmic ratio. Cortical granules are at the periphery of the cell, and a chromatoid body is surrounded by clusters of mitochondria in the cytoplasm. Nuclear vacuoles are observed in the nucleolus. Scale bar = 2 μm. CB: chromatoid body; CG: cortical granule; GER: granular endoplasmic reticulum; M: mitochondrion; Nl: nucleolus; Nv: nuclear vacuole; SC: synaptonemal complex.

Oogenesis

The ovary is surrounded by a basal lamina (Fig. 11). It contains germ cells at various development stages that are closely packed, with younger cells generally localized in the periphery of the ovarian lobes (Fig. 11). Few organelles are observed between cells in the ovary. Four stages are observed during oogenesis in C. metoecus: oogonia, primary oocytes, developing oocytes, and mature oocytes. Oogonia are typically undifferentiated cells, showing a high nucleo-cytoplasmic ratio, measure about 5 μm in diameter and have a roundish shape. The scant cytoplasm is filled with free ribosomes and contains few mitochondria (Figs. 11, 16); no nucleoli are present in the nucleus, only heterochromatin. Primary oocytes possess a higher nucleo-cytoplasmic ratio (Figs. 11, 12, 16) and measure about 8 μm in diameter. The cytoplasm contains chromatoid bodies in the perinuclear region and is filled with free ribosomes, mitochondria, and few granular endoplasmic reticula. The nucleus often shows a nucleolus at this stage. Developing oocytes (Figs. 11, 13, 16) enter in the zygotene-pachytene stage of the first meiotic division, as evidenced by the appearance of synaptonemal complexes in the nucleus (Fig. 13 inset) and measure about 11 μm in diameter. There may be up to eight synaptonemal complexes in a nucleus (by transversal section). The cytoplasm contains less mitochondrion but more granular endoplasmic reticulum. The mature oocytes are located in the central region of the ovary (Figs. 11, 14, 16) and possess elongated cytoplasmic extensions. These cells often show a triangular shape and measure about 18 μm in diameter. In all mature oocytes, a chromatoid body (2 μm of diameter) is present in the cytoplasm, near the granular endoplasmic reticulum and surrounded by mitochondria. Cortical granules are in a monolayer close to the periphery of the cell (approximately 50 per cell). The granular endoplasmic reticulum often takes a parallel shape, and mitochondria are clustered at a pole of the cell.

thumbnail Figure 15.

Diagram showing the four stages (I–IV) of vitellogenesis in Crepidostomum metoecus. G; glycogen particle; GER: granular endoplasmic reticulum; L: lipid droplet; M: mitochondrion; N: nucleus; Nl: nucleolus; SG: shell globule; SGC: shell globule cluster.

thumbnail Figure 16.

Diagram showing the four stages (I–IV) of the oogenesis of Crepidostomum metoecus. CB: chromatoid body; CG: cortical granule; GER: granular endoplasmic reticulum; Hch: heterochromatin; M: mitochondrion; Nl: nucleolus; Nv: nuclear vacuole; SC: synaptonemal complex.

Discussion

Vitellogenesis

Although vitellogenesis has a similar evolution in all neodermatan trematodes, some ultrastructural variations occur during maturation. Some vitelline follicles of Digenea possess interstitial cells (or nurse cells) with cytoplasmic extensions between vitellocytes that are believed to be involved in the selection and transport of materials from the parenchyma to the developing vitelline cells [1, 13, 14, 28]. In Crepidostomum metoecus, as in Plagiorchis elegans, or Maritrema feliui, nurse cells were not found [15, 46]. Vitelline cells provide nutrition for the eggs, and also provide the eggshell substance, in addition to the Mehlis’ gland [13, 28]. The abundance of endoplasmic reticulum, Golgi complexes, and free ribosomes, produces this high synthetic activity [24]. This synthesis gives rise to shell globules that coalesce to form clusters of dense globules surrounded by a limiting membrane (polygranular content). The shape and amount of shell globules in the cluster, the number of clusters per cell, and the size of shell globules and clusters, differ by species (Table 1). Data listed in this table were either taken from the text of corresponding publications or obtained by measuring the structures from figures in these publications [15]. Vitelline cells accumulate nutritive reserves (lipid droplets and glycogen particles) for the developing embryo [30]. The nutritive amount varies among digenean lineages (Table 1). Thus two groups of trematodes are observed: those whose vitelline cells produce a large amount of nutritive reserves as is the case in C. metoecus [7, 8, 15], and those whose vitellocytes contain a small amount of nutritive substances [22, 23]. Poddubnaya et al. (2013) investigated the vitellogenesis of Brandesia turgida and showed that the cytoarchitecture of vitellocytes reveals a specific life cycle. According to their analysis, the development of C. metoecus larva seems to occur after egg-laying, due to the high quantity of nutritive reserves in vitellocytes, unlike Brandesia turgida, which possess few nutritive substances [38]. The presence of such substances in eggs is necessary for the developing embryo that is less able or not able to receive nutrients from the parent worm. In vitelline cells of C. metoecus, only β-glycogen particles have been observed, as in other species [24, 30, 37, 42]. In some trematodes, α-glycogen rosettes and β-glycogen particles have been found [15]. The lack of densely coiled endoplasmic reticulum in fully mature vitellocytes of C. metoecus contributes to the conclusion that maturation ended at the fourth stage. In some other digenean species, a fifth stage presented secretion of densely coiled endoplasmic reticulum [12, 15, 30] and glycogen particles that are condensed in the whole cytoplasm. Moreover, vitelline cells providing shell globules participate in eggshell formation to protect the developed embryo. In the present study, we observed a great amount of shell globule clusters (about 30 per cell cross-section) composed of many shell globules (>30 globules/cluster). Nevertheless, the cluster size is one of the lowest in the vitelline gland of digenean species (Table 1). The variation of eggshell supply can be explained by the difference of life cycle between trematodes [1]. This feature can represent a phylogenetic point of comparison between families of trematodes, like many other characteristics.

Table 1.

Ultrastructural characteristics of mature vitellocytes of Crepidostomum metoecus compared with those of other studied trematodes.

Oogenesis

On the basis of the female gonad structure, Platyhelminthes are subdivided into two levels of organization. In Neoophoran Platyhelminthes, the production of yolk and shell-forming precursors occurs in vitellaria, unlike in Archoophorans where it takes place in germaria [9]. The presence of organelles between growing oocytes supposes the presence of interstitial cells that may transport organelles. The initial phase of oocyte maturation takes place during the prophase of the first meiotic division in the ovary. As for Metadena depressa [14], no nucleus has been observed in the thin interstitial cytoplasmic layer between growing oocytes and the basal lamina, unlike in other Platyhelminthes where syncytial structures may occur in the ovary [34]. Oogonia are present along the wall of the ovary as for Cryptocotyle lingua [5], but do not contain a nucleolus-like Zygocotyle lunata [49]. Developing oocytes enter the zygotene-pachytene stage of the first meiotic division recognizable by the presence of synaptonemal complexes in the nucleoplasm, except in some digenean species where it takes place in the uterus [18]. During maturation, oocytes migrate to the center of the ovary. The metaphase takes place in the proximal part of the uterus where fertilization occurs [17]. A granular mass transfer from nucleus to cytoplasm occurs before the last stages of maturation. This material, named either “chromatoid body”, “nuclear extrusion”, or “nucleolus-like cytoplasmic body” [4, 18, 27, 35], probably contains RNA [4, 25]. This structure is often surrounded by mitochondria and granular endoplasmic reticulum [14], as in the present study. Movements of mitochondria during oogenesis were described by Yosufzai (1952), who studied this in Fasciola hepatica, where mitochondria are at one pole of oogonia, then form a ring around the nucleus in growing oocytes, and are finally evenly distributed in the cytoplasm of mature oocytes [52]. Such movement has not been observed in C. metoecus. In the fully mature oocytes, inclusions are obvious near the cytoplasmic membrane. These small vesicles initially randomly distributed in the cytoplasm, migrate to the cortical cytoplasm where they form a monolayer just beneath the oolemma. This can be observed in several fully mature digenean oocytes [2, 4, 6, 11, 18, 19, 27, 31, 34, 36, 49, 51]. The function of these granules could be the same as that of oocytes of other animals, which act in the blocking of polyspermy during fertilization [31]. The Thiéry method [47] allows us to exclude protein composition of these particles. The low protein composition of mature oocytes differs from that of other studied trematodes, such as Paramphistomum cervi [20], Gastrothylax crumenifer, and Ceylonocotyle dawesi [26]. This pattern, associated with the large nutrient content of vitellocytes of C. metoecus, enables us to consider that oocytes do not take part in the nutrition of the future embryo of the miracidium. Although some minimal differences occur between oogenesis of C. metoecus and some other digeneans, the general pattern of oogenesis corresponds to other neodermatan worms, and more generally to Platyhelminthes.

References

  1. Adiyodi KG, Adiyodi RG. 1988. Accessory Sex Glands, Adiyodi RG, Editor. John Wiley & Sons, New York. p. 1–50. [Google Scholar]
  2. Björkman N, Thorsell W. 1964. On the ultrastructure of the ovary of the liver fluke (Fasciola hepatica L.). Zeitschrift Für Zellforschung und Mikroskopische Anatomie, 63, 538–549. [CrossRef] [Google Scholar]
  3. Bray RA, Gibson DI, Jones A. 2002. Keys to the Trematoda, Bray RA, Gibson DI, Jones A, Editors. CAB International and Natural History Museum: Wallingford, London, UK. p. 824. [Google Scholar]
  4. Burton PR. 1963. A histochemical study of vitelline cells, egg capsules, and Mehlis’ gland in the frog lung-fluke, Haematoloechus medioplexus. Journal of Experimental Zoology, 154, 247–257. [CrossRef] [Google Scholar]
  5. Cable RM. 1931. Studies on the germ-cell cycle of Cryptocotyle lingua Creplin – 1. Gametogenesis in the adult. Quarterly Journal of Microscopical Science, 74, 563–590. [Google Scholar]
  6. Cifrian B, Martinez-Alos S, Gremigni V. 1993. Ultrastructural and cytochemical studies on the germarium of Dicrocoelium dendriticum (Plathelminthes, Digenea). Zoomorphology, 113, 165–171. [CrossRef] [Google Scholar]
  7. Erasmus DA. 1973. Comparative study of reproductive system of mature, immature and unisexual female Schistosoma mansoni. Parasitology, 67, 165–183. [CrossRef] [PubMed] [Google Scholar]
  8. Erasmus DA, Popiel I, Shaw JR. 1982. A comparative study of the vitelline cell in Schistosoma mansoni, S. haematobium, S. japonicum and S. mattheei. Parasitology, 84, 283–287. [CrossRef] [PubMed] [Google Scholar]
  9. Falleni A, Ghezzani C, Lucchesi P. 2010. The use of transmission electron microscopy to solve problems in the study of the female gonad in platyhelminths, Mendez-Vilas A., Diaz J., Editors. Microscopy: Science, Technology, Applications and Education, Formatex: Badajoz. p. 162–169. [Google Scholar]
  10. Gibson DI, Jones A, Bray RA. 2002. Keys to the Trematoda, Gibson DI, Jones A, Bray RA, Editors. CAB International and Natural History Museum: Wallingford, London, UK. p. 521. [Google Scholar]
  11. Govaert J. 1953. Deoxyribonucleic acid content of the germinal vesicle of the ovocyte in Fasciola hepatica. Nature, 172, 302–303. [CrossRef] [PubMed] [Google Scholar]
  12. Grant WC, Harkema R, Muse KE. 1977. Ultrastructure of Pharyngostomoides procyonis Harkema 1942 (Diplostomatidae). 2. Female reproductive-system. Journal of Parasitology, 63, 1019–1030. [CrossRef] [Google Scholar]
  13. Greani S, Quilichini Y, Foata J, Marchand B. 2012. Ultrastructural study of vitellogenesis of Aphallus tubarium (Rudolphi, 1819) Poche, 1926 (Digenea: Cryptogonimidae), an intestinal parasite of Dentex Dentex (Pisces: Teleostei). Journal of Parasitology, 98, 938–943. [CrossRef] [Google Scholar]
  14. Greani S, Quilichini Y, Foata J, Swiderski Z, Marchand B. 2012. Ultrastructural study of vitellogenesis and oogenesis of Metadena depressa (Stossich, 1883) Linton, 1910 (Digenea, Cryptogonimidae), intestinal parasite of Dentex dentex (Pisces, Teleostei). Comptes Rendus Biologies, 335, 657–667. [CrossRef] [PubMed] [Google Scholar]
  15. Greani S, Quilichini Y, Foata J, Greiman SE, Ndiaye PI, Tkach VV, Marchand B. 2014. Vitellogenesis of the digenean Plagiorchis elegans (Rudolphi, 1802) (Plagiorchioidea, Plagiorchiidae). Parasitology International, 63, 537–543. [CrossRef] [PubMed] [Google Scholar]
  16. Gresson RAR. 1958. The gametogenesis of the digenetic trematode Sphaerostoma bramae (Muller) Luhe. Parasitology, 48, 293–302. [CrossRef] [PubMed] [Google Scholar]
  17. Gresson RAR. 1964. Electron microscopy of the ovary of Fasciola hepatica. Quarterly Journal of Microscopical Science, 105, 213–218. [Google Scholar]
  18. Gresson RAR. 1964. Oogenesis in the hermaphroditic Digenea (Trematoda). Parasitology, 54, 409–421. [CrossRef] [Google Scholar]
  19. Gupta BC, Parshad VR, Guraya SS. 1983. Morphological and histochemical observations on the oocapt and oviducal transport of oocytes in Paramphistomum cervi (Zeder, 1790) (Digenea: Trematoda). Journal of Helminthology, 57, 149–153. [CrossRef] [PubMed] [Google Scholar]
  20. Gupta BC, Parshad VR, Guraya SS. 1984. Morphological and histochemical studies on the ovarian development and oogenesis in Paramphistomum cervi (Digenea, Paramphistomatidae). Folia Parasitologica, 31, 147–156. [PubMed] [Google Scholar]
  21. Hendow HT, James BL. 1989. Ultrastructure of vitellarium, vitellogenesis and associated ducts in Maritrema linguilla (Digenea, Microphallidae). International Journal for Parasitology, 19, 489–497. [CrossRef] [Google Scholar]
  22. Holy JM, Wittrock DD. 1986. Ultrastructure of the female reproductive organs (ovary, vitellaria, and Mehlis gland) of Halipegus eccentricus (Trematoda, Derogenidae). Canadian Journal of Zoology, 64, 2203–2212. [CrossRef] [Google Scholar]
  23. Irwin SWB, Maguire JG. 1979. Ultrastructure of the vitelline follicles of Gorgoderina vitelliloba (Trematoda – Gorgoderidae). International Journal for Parasitology, 9, 47–53. [CrossRef] [PubMed] [Google Scholar]
  24. Irwin SWB, Threadgold LT. 1970. Electron microscope studies on Fasciola hepatica. 8. Development of vitelline cells. Experimental Parasitology, 28, 399–411. [CrossRef] [PubMed] [Google Scholar]
  25. Justine JL, Mattei X. 1984. Ultrastructural observations on the spermatozoon, oocyte and fertilization process in Gonapodasmius, a gonochoristic trematode (Trematoda, Digenea, Didymozoidae). Acta Zoologica, 65, 171–177. [CrossRef] [Google Scholar]
  26. Kanwar U, Agarwal M, Nath V. 1980. Cytochemical analysis of the non-enzymatic components of the digenetic trematodes Gastrothylax crumenifer and Ceylonocotyle dawesi. Zoologica Poloniae, 28, 189–198. [Google Scholar]
  27. Koulish S. 1965. Ultrastructure of differentiating oocytes in trematode Gorgoderina attenuata. I. The nucleolus-like cytoplasmic body and some lamellar membrane systems. Developmental Biology, 12, 248–268. [CrossRef] [PubMed] [Google Scholar]
  28. Levron C, Poddubnaya L, Oros M, Scholz T. 2010. Vitellogenesis of basal trematode Aspidogaster limacoides (Aspidogastrea Aspidogastridae). Parasitology International, 59, 532–538. [CrossRef] [PubMed] [Google Scholar]
  29. Markell EK. 1943. Gametogenesis and egg-formation in Probolitrema californiense Stunkard, 1935 (Trematoda: Gorgoderidae). Transactions of the American Microscopical Society, 62, 27–56. [CrossRef] [Google Scholar]
  30. Martinez-Alos S, Cifrian B, Gremigni V. 1993. Ultrastructural Investigations on the vitellaria of the digenean Dicrocoelium dendriticum. Journal of Submicroscopic Cytology and Pathology, 25, 583–590. [PubMed] [Google Scholar]
  31. Meepool A, Sobhon P. 2009. Ooogenesis of the liver fluke Fasciola gigantica. Journal of Microscopy Society of Thailand, 23, 15–19. [Google Scholar]
  32. Neves RH, De Lamare Biolchini C, Machado-Silva JR, Carvalho JJ, Branquinho TB, Lenzi HL, Hulstijn M, Gomes D. 2005. A new description of the reproductive system of Schistosoma mansoni (Trematoda: Schistosomatidae) analyzed by confocal laser scanning microscopy. Parasitology Research, 95, 43–49. [CrossRef] [PubMed] [Google Scholar]
  33. Nez MM, Short RB. 1957. Gametogenesis in Schistosomatium douthitti (Cort) (Schistosomatidae: Trematoda). Journal of Parasitology, 43, 167–182. [CrossRef] [Google Scholar]
  34. Orido Y. 1987. Development of the ovary and the female reproductive cells of the lung fluke, Paragonimus ohirai (Trematoda, Troglotrematidae). Journal of Parasitology, 73, 161–171. [CrossRef] [Google Scholar]
  35. Pennypacker MI. 1940. The chromosomes and extranuclear material in the maturing germ cells of a frog lung fluke, Pneumonoeces similiplexus Stafford. Journal of Morphology, 66, 481–495. [CrossRef] [Google Scholar]
  36. Poddubnaya LG, Gibson DI, Olson PD. 2007. Ultrastructure of the ovary, ovicapt and oviduct of the spathebothriidean tapeworm Didymobothrium rudolphii (Monticelli, 1890). Acta Parasitologica, 52, 127–134. [Google Scholar]
  37. Poddubnaya LG, Brunanska M, Swiderski Z, Gibson DI. 2012. Ultrastructure of the vitellarium in the digeneans Phyllodistomum angulatum (Plagiorchiida, Gorgoderidae) and Azygia lucii (Strigeida, Azygiidae). Acta Parasitologica, 57, 235–246. [CrossRef] [PubMed] [Google Scholar]
  38. Poddubnaya LG, Brunanska M, Brazova T, Zhokhov AE, Gibson DI. 2013. Ultrastructural characteristics of the vitellarium of Brandesia turgida (Brandes, 1888) (Digenea: Pleurogenidae) and an examination of the potential usefulness of such vitelline traits in digenean systematics. Helminthologia, 50, 119–126. [CrossRef] [Google Scholar]
  39. Quilichini Y, Foata J, Orsini A, Mattei J, Marchand B. 2007. Parasitofauna study of the brown trout, Salmo trutta (Pisces, Teleostei) from Corsica (Mediterranean island) rivers. Parasite, 14, 257–260. [CrossRef] [EDP Sciences] [PubMed] [Google Scholar]
  40. Rees G. 1940. Studies on the germ cell cycle of the digenetic trematode Parorchis acanthus Nicoll. Parasitology, 32, 372–391. [CrossRef] [Google Scholar]
  41. Reynolds ES. 1963. Use of lead citrate at high pH as an electron-opaque stain in electron microscopy. Journal of Cell Biology, 17, 208–212. [CrossRef] [Google Scholar]
  42. Sampour M. 2008. The study of vitelline gland of Haploporus lateralis (Digenea: Trematoda). Pakistan Journal of Biological Sciences, 11, 113–117. [CrossRef] [Google Scholar]
  43. Sanderson AR. 1959. Maturation and fertilization in two digenetic trematodes, Haplometra cylindracea (Zeder 1800) and Fasciola hepatica (L.). Proceedings of the Royal Society of Edinburgh, 67, 83–99. [Google Scholar]
  44. Saxena RM. 1979. Cytological studies on the oogenesis and fertilization of Halipegus mehransis (Trematoda: Halipegidae). Helminthologia, 16, 45–50. [Google Scholar]
  45. Spence IM, Silk MH. 1971. Ultrastructural studies of the blood fluke Schistosoma mansoni. V. The female reproductive system – a preliminary report. South African Journal of Medical Sciences, 36, 41–50. [Google Scholar]
  46. Swiderski Z, Bakhoum AJS, Montoliu I, Feliu C, Gibson DI, Miquel J. 2011. Ultrastructural study of vitellogenesis in Maritrema feliui (Digenea, Microphallidae). Parasitology Research, 109, 1707–1714. [CrossRef] [PubMed] [Google Scholar]
  47. Thiéry JP. 1967. Mise en évidence des polysaccharides sur coupes fines en microscopie électronique. Journal de Microscopie, 6, 987–1018. [Google Scholar]
  48. Van der Woude A. 1954. Germ cell cycle of Megalodiscus temporatus (Stafford, 1905) Harwood, 1932 (Paramphistomidae: Trematoda). American Midland Naturalist, 51, 172–202. [CrossRef] [Google Scholar]
  49. Willey C, Godman GC. 1951. Gametogenesis, fertilization and cleavage in the trematode, Zygocotyle lunata (Paramphistomidae). Journal of Parasitology, 37, 283–296. [CrossRef] [Google Scholar]
  50. Willey C, Koulish S. 1947. Gametogenesis in Gorgoderina attenuata. Anatomical Record, 99, 640–641. [Google Scholar]
  51. Willey CH, Koulish S. 1950. Development of germ cells in the adult stage of the digenetic trematode, Gorgoderina attenuata Stafford, 1902. Journal of Parasitology, 36, 67–79. [CrossRef] [Google Scholar]
  52. Yosufzai HK. 1952. Female reproductive system and egg-shell formation in Fasciola hepatica L. Nature, 169, 549–549. [CrossRef] [PubMed] [Google Scholar]
  53. Yosufzai HK. 1953. Shell gland and egg-shell formation in Fasciola hepatica L. Parasitology, 43, 88–93. [CrossRef] [PubMed] [Google Scholar]

Cite this article as: Greani S, Quilichini Y & Marchand B: Ultrastructural study of vitellogenesis and oogenesis of Crepidostomum metoecus (Digenea, Allocreadiidae), intestinal parasite of Salmo trutta (Pisces, Teleostei). Parasite, 2016, 23, 47.

All Tables

Table 1.

Ultrastructural characteristics of mature vitellocytes of Crepidostomum metoecus compared with those of other studied trematodes.

In the text

All Figures

thumbnail Figures 1–4.

Stages 1 and 2 of vitellogenesis in C. metoecus. (1) An immature vitellocyte (Stage 1) at the periphery of the follicle. The nucleus is filled with heterochromatin and the cell possesses a high nucleo-cytoplasmic ratio. Scale bar = 1 μm. (2) Immature vitellocyte at first stage of maturation filled with ribosomes, mitochondria, and few endoplasmic reticulum saccules. Scale bar = 1 μm. (3) Electron micrograph of second stage of vitelline cells’ maturation (arrowheads: basal lamina). Scale bar = 1 μm. (4) Part of the cytoplasm of a cell at second stage of maturation showing Golgi complexes and granular endoplasmic reticulum. Scale bar = 1 μm. GC: golgi complex; GER: granular endoplasmic reticulum; Hch: heterochromatin; M: mitochondrion; N: nucleus; Nl: nucleolus; SG: shell globule.
In the text
thumbnail Figures 5–8.

Stages 3 and 4 of vitellogenesis in C. metoecus. (5) General observation of a vitelline cell at the third stage of maturation. Scale bar = 1 μm. (6) The third stage of vitellocyte maturation showing the coalescence of single shell globules into a cluster surrounded by a membrane. Scale bar = 1 μm. (7) Cytoplasm of a vitelline cell at the third stage of maturation containing shell globule cluster and saturated lipid droplets, surrounded by glycogen granules. Stained according to the Thiéry method. Scale bar = 1 μm. (8) Electron micrograph of a vitelline cell at the fourth stage of maturation filled with shell globule clusters and lipid droplets. Scale bar = 1 μm. G: glycogen particle; GER: granular endoplasmic reticulum; L: lipid droplet; M: mitochondrion; N: nucleus; Nl: nucleolus; SG: shell globule; SGC: shell globule cluster.
In the text
thumbnail Figure 9–12.

Stage 4 of vitellogenesis and primary oocyte stage of oogenesis in C. metoecus. (9) A group of saturated lipid droplets, surrounded by glycogen granules, and a few shell globule clusters. Scale bar = 1 μm. (10) A part of the cytoplasm of a vitelline cell at the fourth stage of maturation. Note the abundance of glycogen granules around lipid droplets. Stained according to the Thiéry method. Scale bar = 1 μm. (11) Electron micrograph cross-section of ovary (arrowheads: basal lamina). Germ cells of the four stages of maturation are observed (I–IV). Scale bar = 2 μm. (12) Primary oocyte showing a small amount of cytoplasm, filled with free ribosomes, mitochondria, few granular endoplasmic reticula, and a chromatoid body. Scale bar = 1.5 μm. CB: chromatoid body; G: glycogen particle; GER: granular endoplasmic reticulum; L: lipid droplet; M: mitochondrion; N: nucleus; Nl: nucleolus; P: parenchyma; SGC: shell globule cluster.
In the text
thumbnail Figure 13 and 14.

Developing and mature oocytes in C. metoecus. (13) General observation of a developing oocyte. Note the presence of synaptonemal complexes indicating the zygotene-pachytene stage of the first meiotic division. Inset: detail of a synaptonemal complex. Scale bar = 2 μm. (14) General observation of a fully mature germ cell, with a low nucleo-cytoplasmic ratio. Cortical granules are at the periphery of the cell, and a chromatoid body is surrounded by clusters of mitochondria in the cytoplasm. Nuclear vacuoles are observed in the nucleolus. Scale bar = 2 μm. CB: chromatoid body; CG: cortical granule; GER: granular endoplasmic reticulum; M: mitochondrion; Nl: nucleolus; Nv: nuclear vacuole; SC: synaptonemal complex.
In the text
thumbnail Figure 15.

Diagram showing the four stages (I–IV) of vitellogenesis in Crepidostomum metoecus. G; glycogen particle; GER: granular endoplasmic reticulum; L: lipid droplet; M: mitochondrion; N: nucleus; Nl: nucleolus; SG: shell globule; SGC: shell globule cluster.
In the text
thumbnail Figure 16.

Diagram showing the four stages (I–IV) of the oogenesis of Crepidostomum metoecus. CB: chromatoid body; CG: cortical granule; GER: granular endoplasmic reticulum; Hch: heterochromatin; M: mitochondrion; Nl: nucleolus; Nv: nuclear vacuole; SC: synaptonemal complex.
In the text

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