Protocolo de tincion para el estudio histologico de anemonas (Anthozoa: Actiniaria), con recomendaciones para la anestesia y fijacion de especimenes.
Permanent histological preparations play a fundamental role in taxonomic studies of sea anemones. Many of the characteristics used in the identification of species must go through a dying process to be analyzed. Basilar musculature, for instance, has been traditionally employed on taxonomic keys (Stephenson, 1935; Carlgren, 1949) to distinguish large groups within Actiniaria. Certain muscles such as the sphincter not only vary in shape and degree of development, but also in the tissue derivation (endodermal or mesogleal), which, until today, has been particularly useful to define families. Even at genus level, there are specific biological characteristics (e.g., type of reproduction) that can only be verified through histology. In all of these cases, descriptions depend on tested protocols in this group of organisms that can acquire a clear differentiation between the mesoglea and epithelial and muscle areas.
Since there is no standardized method for analyzing these structures, there are now as many histological techniques as sea anemone studies. Given the problems this creates to the taxonomic work, some authors have compared the different methods of anesthesia (see Moore, 1989), fixation (see Dunn, 1975) and staining (see Stotz, 1981), to establish which techniques are the most appropriate for these organisms. Parts of these procedures, however, depend largely on the specimens characteristics (e.g., body size), information that usually is not considered in the methodologies. In fact, many of the protocols used are often unpublished modifications of the classical histological techniques. In Chile, only Stotz (1981) has compared different methods of anesthesia and staining, studying its effects on Anthothoe chilensis (Lesson, 1830), Antholoba achates (Drayton, 1846) and Phymactis papillosa (Lesson, 1830). This short communication introduces new observations for the narcotization and preservation of intertidal species Anthopleura hermaphroditica (Carlgren, 1899) and Bunodactis hermafroditica (Calgren, 1959), including some modifications to the Masson's trichrome method according to the results obtained by Spano et al. (in press). Therefore, this paper aims to promote the histological study of sea anemones, providing practical recommendations and a staining protocol suitable even in other marine invertebrates, such as flatworms, polychaetes and nematodes.
Methods of anesthesia
Before preservation, specimens of many taxa (especially invertebrates) must be relaxed to prevent contraction of the body and mucus secretion (Haussermann & Forsterra, 2009). Menthol crystals, magnesium salts, chloral hydrate, tricaine methanesulfonate (MS-222), alcohol or formalin (drip) and even relaxation by freezing are documented narcotization methods for sea anemones. Of these, few have yet proven to be suitable for histological studies (Moore, 1989). Today, the most accepted anesthetics for anemones are menthol crystals and magnesium salts (Mg[Cl.sub.2] and MgS[O.sub.4] at 3.5-7.5%); nevertheless, they can equally macerate the tissue depending on the time of exposure (Haussermann, 2004). In fact, although menthol crystals are especially effective in small organisms (column diameter 0.5-2 cm) (Stotz, 1981), very large amounts or very long exposure times always had deleterious effects on the internal anatomy of Anthopleura hermaphroditica and Bunodactis hermafroditica, species with a pedal disc near to a centimeter of diameter. Particularly in B. hermafroditica, 23 of the 25 specimens used for this study (>90% of the sample) wholly or partially contracted when anesthetized for over an hour. Because the amount of anesthetic depends both on the specimens as well as the volume of water used, the crystal size and the exposure time (Stephenson, 1928), a standardized protocol cannot be formulated since parameters are always species-specific. For A. hermaphroditica, for example, it was found that exposing the specimens to more than 10 g of menthol crystals in 50 mL of water for more than three hours, irreversibly damaged smaller individuals (<2 mm diameter pedal disc) and caused most of the large specimens to evert the actinopharynx. On the other hand, even when the animals do not respond to tactile stimuli, very short relaxation times can cause a delayed contraction of the organisms when immersed in the fixative. For A. hermaphroditica, the best results in terms of expansion were obtained by anesthetizing the specimens in less than 100 mL of water with 50 g of menthol crystals for no more than one hour. In both species, very good results were observed by additionally administering small doses (1 to 2 mL) of 6% Mg[Cl.sub.2] directly into the gastrovascular cavity of the animal, right before being immerse in the fixative. If they are kept in optimal conditions (e.g., low light, water temperature below zero degrees), a 50 mL jar can satisfactorily relax up to 10 small specimens (<6 mm pedal disc diameter). While simple measures can be taken to control some of these variables (Stotz, 1981), in order to effectively elaborate a narcotization method, the anesthesia parameters must first be related to the ontogenetic characteristics of each species to be studied.
Methods of fixation
The selection of the fixative is particularly important for samples that are intended for histological processing. Although the most frequently used fixatives for sea anemones are seawater formalin and picric acid solutions such as aqueous Bouin, good results have also been achieved with heavy-metal based fixing fluids such as Heidenhain (Susa), Zenker and Helly. Each one influences the quality of the preparations differently according to the tissue characteristics of the species and the dyes used. The trichrome techniques, for example, it is recommended for organisms that were fixed in formalin to mordant for at least two days in picric acid before staining. For species with a thin mesoglea layer (<100 [mu] column), such as A. hermaphroditica and B. hermafroditica, Bouin's fixative penetrated tissue in less than 48 h, but, due to the high concentration of formalin (Bouin weak: 15% and strong: >20%), the specimens hardened and deteriorated at cellular level. A maceration of muscle fibers caused by the section on poorly preserved and, presumably, badly anesthetized specimens were observed several times in preparations. To favor a good fixation of the internal structures, especially in large organisms, it is sometimes desirable to inject small doses of the fixative solution through the mouth (Stephenson, 1928). Furthermore, specimens can dilute a lot of the preservative medium due to the water retained inside the tissues. In this regard, it is recommended to cover 20 times the volume of the body in the fixative (Lopez et al., 1982) or at least replace it after a couple of days of use (Haussermann & Forsterra, 2009). At tissue level, the best results were observed in preparations fixed for long periods in 8% seawater formalin. When requiring trichrome techniques, it is suggested to fix the specimens first in seawater formalin for a period exceeding two months and then mordant them in Bouin's solution (very weak, ideally 8%) for one or two weeks. Formalin concentration (5 to 15%) as well as the fixation time (two to six months) will depend primarily on the size of the specimens to be preserved (Haussermann, 2004).
Methods of staining
Several staining methods have been applied in sea anemones for taxonomic work. Among the protocols reported in the literature for this group, highlights the trichromics of Mallory (Pantin, 1948), Azocarmine (Humason, 1967), Heidenhain Azan (Presnell & Schreibman, 1997) and the Nuclear Red Picroindigocarmine (Romeis, 1948); the latter being recommended by Stotz (1981). For general purposes, bicomponent staining of eosin with Weigert's iron, Harris's or Ehrlich's hematoxylin have also reported good results in anemones. Even in toto staining (prior sectioning), such as borax carmine (Carter, 1965), has proven to be a useful way to gain primary insights into these animals' anatomy. Masson's trichrome (Sumner & Sumner, 1969) was suggested by Manuel (1981) as a general stain for Anthozoa, allowing for a good contrast between the mesoglea and the cellular regions. The original method of Masson (1928) was initially thought for carcinoids analysis, integrating four dyes (Regaud's hematoxylin, acid fuchsin with Ponceau de xylidine and aniline blue) which have been repeatedly combined on later modifications. Among the many changes made to this method, it is worth mentioning the modifications yielded by Humason (1962) and Luna (1968) (fide Lopez et al., 1982) by facilitating the control of the acid dyes. From the last protocol, some modifications were made according to the results obtained from histological preparations of Anthopleura hermaphroditica and Bunodactis hermafroditica (Table 1).
The entire procedure (from deparaffinize to mount) takes no more than two hours, utilizes relatively few reagents and offers the possibility of controlling the times during each stage of differentiation. Following this protocol, the mesoglea turns to a deep blue color while the cytoplasmic elements and epithelia differentiate to pink-reddish tones, clearly highlighting loaded nematocysts structures (e.g., mesenterial filaments, acontia, acrorhagi). To prevent discoloration of the tissue, dehydration prior to mounting must be direct (to 100% ethanol) and preferably fast (at two steps of 5 min each). Likewise, it is very important to renew the dyes after several months of use, as this also influences the quality of the preparations. Although good results were obtained with A. hermaphroditica and B. hermafroditica (Fig. 1), it is always advisable to proceed initially with a full protocol test to verify the results on each step of the method according to the species of study and the laboratory equipment. If the sections are stretched on a hotplate, for example, it is very important to control the times of adhesion because fine tissues, such as mesenteries, are very sensitive to temperature. Also note that for samples fixed in aqueous Bouin, the wash must be in 70% ethanol. If working with a strong Bouin solution, it is also desirable to keep the specimens in the final ethanol wash for a longer period of time (overnight) and then clear the samples with butanol according to Gabe (1968). Given the small size of these species, many of these details finally determined the specimen's resistance to the histological process. Taking into account these recommendations, this staining method has demonstrated very good results for the histological study of sea anemones.
The authors thank the Department of Ecology at the Pontificia Universidad Catolica de Chile for all their support, especially to Professor Nicolas Rozbaczylo for his backing and help through all this study. Many thanks to the two anonymous reviewers, for their constructive comments on the manuscript, and to Katie McConnell and Daniel Genter, for their assistance with the translation of this paper. This publication is drawn from the graduate thesis of the corresponding author and represents publication number 93 of Huinay Scientific Field Station.
Carlgren, O. 1949. A survey of the Ptychodactiaria, Corallimorpharia and Actiniaria. K. Svenska Vetenskapsakad. Handl., 1(1): 1-121.
Carter, D. 1965. Actinias de Montemar, Valparaiso. Rev. Biol. Mar., 12: 129-160.
Dunn, D.F. 1975. Reproduction of the externally brooding sea anemone Epiactis prolifera Verrill, 1869. Biol. Bull., 148: 199-218.
Gabe, M. 1968. Techniques histologiques. Masson et Cie Editeurs, Paris, 1113 pp.
Haussermann, V. 2004. Identification and taxonomy of soft-bodied hexacorals exemplified by Chilean sea anemones, including guidelines for sampling, preservation and examination. J. Mar. Biol. Assoc. UK., 84: 931-936.
Haussermann, V. & G. Forsterra. 2009. Fauna marina bentonica de la Patagonia Chilena. Nature in Focus, Santiago, 1000 pp.
Humason, G.L. 1962. Animal tissue techniques. W.H. Freeman & Company, San Francisco, 468 pp.
Humason, G.L. 1967. Animal tissue techniques. W.H. Freeman & Company, San Francisco, 494 pp.
Lopez, M.A., C. Leyton & M.E. Graf. 1982. Tecnicas de histologia y citologia. Universidad de Chile, Santiago, 242 pp.
Luna, L.G. 1968. Manual of histologic staining methods of the Armed Forces Institute of Pathology. McGrawHill, New York, 258 pp.
Manuel, R.L. 1981. British Anthozoa, keys and notes for the identification of species. Academic Press, London, 241 pp.
Masson, P. 1928. Carcinoids (argentaffin-cell tumors) and nerve hyperplasia of the appendicular mucosa. Am. J. Pathol., 4: 181-211.
Moore, S.J. 1989. Narcotising sea anemones. J. Mar. Biol. Assoc. UK., 69: 803-811.
Pantin, C.F.A. 1948. Notes on microscopical technique for zoologists. Cambrigde University Press, Cambrigde, 79 pp.
Presnell, J.K. & M.P. Schreibman. 1997. Humason's animal tissue techniques. Johns Hopkins University Press, Baltimore, 572 pp.
Romeis, B. 1948. Mikroskopische technik. LeibnizVerlag, Munchen, 695 pp.
Spano, C., N. Rozbaczylo, V. Haussermann & R. Bravo. 2013. Redescription of the sea anemones Anthopleura hermaphroditica and Bunodactis hermafroditica (Cnidaria: Anthozoa: Actiniaria) from Chile. Rev. Biol. Mar. Oceanogr. (in press).
Stephenson, T.A. 1928. The British sea anemones, volume I. Dulau & Co., London, 176 pp.
Stephenson, T.A. 1935. The British sea anemones, volume II. Dulau & Co., London, 464 pp.
Stotz, W.B. 1981. Metodos de anestesia y tincion para el trabajo taxonomico de actinias (Anthozoa, Actiniaria). Invest. Mar., Valparaiso, 9(1-2): 61-70.
Sumner, A.T. & B.E.H. Sumner. 1969. A laboratory manual of microtechnique and histochemistry. Blackwell Scientific Publications, Oxford, 93 pp.
Received: 13 June 2013; Accepted: 7 October 2013
Carlos Spano (1,2) * & Veronica Flores (2)
(1) Facultad de Ciencias del Mar y de Recursos Naturales, Universidad de Valparaiso P.O. Box 5080, Renaca, Vina del Mar, Chile
(2) Departamento de Ecologia, Facultad de Ciencias Biologicas, Pontificia Universidad Catolica de Chile P.O. Box 114-D, Santiago, Chile
Corresponding author: Carlos Spano (firstname.lastname@example.org)
Table 1. Detail of Masson's trichrome method (1928) with its respective modifications. * Check results under microscope. Masson Trichrome Stain Humason's modification (1928) (1962) Deparaffinize and hydrate Deparaffinize and hydrate to water. to water. Mordant with iron alum Mordant with iron alum 5%: 5 min (45[degrees]- 4%: 1/2 h. 50[degrees]C). Wash in water Wash in running water: 5 min. Stain in Regaud's Stain in Delafield's hematoxylin: 5 min hematoxylin: 1/2 h. (45[degrees]- 50[degrees]C). Rinse in 95% alcohol. Wash in running water: 5 minutes. Differentiate in picric Differentiate in alcohol. saturated aqueous picric acid. Wash in running water. Wash in running water: >10 min. Stain in solution acid fuchsin 0.3%--Ponceau de xylidine Stain in acid fuchsin 1%: 5 min. 0.3%: 5 min. Rinse in distilled water until excess stain is removed.* Rinse in distilled water. Differentiate in Stain in Ponceau de phosphomolybdic acid 1%: xylidine 1%: 1-5 min. 5 min. Stain in acetic aniline Rinse in tap water. * blue 2%: 5 min. Rinse in distilled water. Differentiate in phosphomolybdic acid 1%: 5 min. Back to phosphomolybdic Stain in acetic fast acid 1%: 5 min. green 2%: 2 min. Differentiate in acetic Differentiate in acetic acid 1%: acid 1% rinse: 1-2 min. 5 min. Dehydrate, clear and Dehydrate, clear and mount. mount. Luna's modification Spano & Flores's (1968) modification (this study) Deparaffinize and hydrate Deparaffinize and hydrate to distilled water. to distilled water. Stain in Weigert's iron Stain in Harri's hematoxylin: 10 min. hematoxylin: 3-5 min. Wash in tap water: 10 Rinse (several times) in min. tap water. Wash in distilled water. Differentiate in hydrochloric alcohol 1%: 30 seconds *. Stain in solution Rinse (several times) in Biebrich Scarlett 1% - tap water. acid fuchsin 1%: 2 min Wash in distilled water. Wash in distilled water: 5 min. Stain in solution acid fuchsin Differentiate with 0.1%--Ponceau de xylidine solution of 0.2%: 6-10 min. phosphomolybdic acid 2.5% -phosphotungstic acid 2.5%: 10-15 min. Rinse in distilled water Rinse in distilled water (quick step). (two times). Stain in acetic aniline Differentiate with blue 2%: 5 min. phosphotungstic acid 5%: 4-8 min *. Wash in distilled water. Rinse in distilled water (two times). Differentiate in acetic Stain in acetic aniline acid 1% rinse: 3-4 min. blue 2%: 5-10 min. Dehydrate, clear and Differentiate in acetic mount. acid 1% rinse until excess stain is removed. * Dehydrate (quickly), clear and mount.
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|Title Annotation:||articulo en ingles|
|Author:||Spano, Carlos; Flores, Veronica|
|Publication:||Latin American Journal of Aquatic Research|
|Date:||Nov 1, 2013|
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