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Morphological and biochemical characterization of the cutaneous poison glands in toads (Rhinella marina group) from different environments
Frontiers in Zoology volume 15, Article number: 46 (2018)
Amphibian defence against predators and microorganisms is directly related to cutaneous glands that produce a huge number of different toxins. These glands are distributed throughout the body but can form accumulations in specific regions. When grouped in low numbers, poison glands form structures similar to warts, quite common in the dorsal skin of bufonids (toads). When accumulated in large numbers, the glands constitute protuberant structures known as macroglands, among which the parotoids are the most common ones. This work aimed at the morphological and biochemical characterization of the poison glands composing different glandular accumulations in four species of toads belonging to group Rhinella marina (R. icterica, R. marina, R. schneideri and R. jimi). These species constitute a good model since they possess other glandular accumulations together with the dorsal warts and the parotoids and inhabit environments with different degrees of water availability.
We have observed that the toads skin has three types of poison glands that can be differentiated from each other through the morphology and the chemical content of their secretion product. The distribution of these different glands throughout the body is peculiar to each toad species, except for the parotoids and the other macroglands, which are composed of an exclusive gland type that is usually different from that composing the dorsal warts. Each type of poison gland presents histochemical and biochemical peculiarities, mainly regarding protein components.
The distribution, morphology and chemical composition of the different types of poison glands, indicate that they may have different defensive functions in each toad species.
One of the most striking features of amphibians is the presence of mucous and poison (or granular) glands in the skin, which play a key role in their lives, particularly in relation to chemical defence against predators and microorganisms [1, 2]. Regarding defence against predators, differently from venomous animals, in amphibians the arsenal of toxins stored in their skin cannot be inoculated in the aggressor due to the lack of an inoculatory apparatus. Poisoning only occurs when the aggressor attacks and bites the amphibian and comes into contact with the toxins via oral mucosa, which characterizes a passive mode of defence [3,4,5,6].
In venomous animals, the venom-producing glands usually have well-defined lumen, where the secretion accumulates after traversing the secretory epithelium cell membrane [7, 8]. In contrast, in anuran amphibians, the poison glands are formed by a single multinucleated cytoplasm mass, constituting a secretory syncytium . There is no lumen, and the gland is totally filled with the syncytial cytoplasm matrix. The secretion, in the form of granules, after being elaborated in the syncytial periphery, is stored throughout the cytoplasm .
In amphibians the poison glands can be distributed singly or in the form of clusters in specific regions of the body. When aggregated in low numbers, they form structures that are similar to warts, commonly found on the dorsal skin of toads (bufonids) . When grouped in large numbers, they can form conspicuous protrusions, known as macroglands [2, 10], among which the parotoids are clearly the most common: they are found in salamanders , phyllomedusin tree frogs , frogs  and toads .
Histologically, toad parotoids in genus Rhinella are identified as large accumulations of giant poison glands inserted into the dermis and arranged side by side, forming honeycomb-like structures [3, 6, 12]. Individual poison glands composing the parotoids show morphological characteristics that are similar to the other poison glands present in the rest of the skin. They are enveloped by a myoepithelial cell layer and are provided with a duct. However, differently from skin poison glands, the epithelium that internally lines the duct is very thick and obstructs the ductal canal, sometimes leaving just a narrow crevice in the centre [3,4,5,6, 12]. Moreover, differentiated mucous glands known as accessory glands surround each one of the ducts [3, 5, 12].
Due to the large size of the individual glands that compose the parotoids, these cutaneous organs can synthesize and store significant large amounts of poison used in chemical defence against predators [3, 5]. In toads in general, the secretion is composed of a mixture of steroids, biogenic amines and proteins, as well as mucus [3, 5, 10, 14, 15]. If ingested, toad skin secretion may cause death of several vertebrates, including humans [16,17,18,19,20].
Species of group Rhinella marina are typically large and terrestrial, with large parotoids . Because they have other macroglands besides parotoids, these species constitute excellent models for macrogland morphological and biochemical studies and for the better understanding of macrogland use in passive defence. In R. schneideri, for example, there are conspicuous tibial (paracnemic) macroglands on the hind limbs. In R. jimi, besides tibial macroglands, radial macroglands are observed on the anterior limbs. Another interesting fact is the large range of environments the species of R. marina group inhabit: they are found in forested areas such as the Atlantic Forest (R. icterica) and the Amazonia (R. marina), in open areas as the Cerrado (R. schneideri), and in regions exhibiting extreme xeric conditions, such as the Brazilian semiarid Caatinga (R. jimi).
In relation to literature referring to toad toxinology, most investment has been given to the parotoid macroglands, especially regarding poison biochemistry. The morphology and biochemistry, as well as the functional role of the other glandular accumulations, remain practically unknown.
This paper aims at the characterization of the poison glands in Rhinella marina, R. icterica, R. schneideri and R. jimi. We verified that all species studied have three different types of poison glands, which are characterized by the morphology and chemical composition, besides the topographic distribution.
Poison glands: Morphological characterization, histochemistry and distribution
In general, the dorsal skin surface of all studied species shows an irregular structure, with an abundance of warts (Fig. 1a). Parotoids and other macroglands are clearly distinguished from the rest of the body and from the dorsal warts due to their large volume and anatomical position (Fig. 1a–d).
Macroscopically, longitudinal sections across the dorsal warts reveal structures consisting of the accumulation of small poison glands (Fig. 2a). In contrast, the internal longitudinal view of the parotoids show the characteristic honeycomb structure formed by many secretory units, each one of them housing a large poison gland (Fig. 2b).
Histologically, the dorsal warts are composed of poison glands of various sizes inserted into the dermis and completely filled with secretion (Fig. 2c). Mucous glands consisting of a monolayer of secretory cells organized around a characteristic central lumen (Fig. 2c insert), are also observed just below the epidermis.
In the species here studied, the parotoids present a general morphology much similar to that described for all other species of Rhinella marina group [3, 5, 6, 22]: they are basically composed of very elongated poison glands that decrease in diameter from the macroglandular centre towards the periphery (Fig. 2d). Each of these giant poison glands is provided with a single duct obstructed by a plug composed of epithelial tissue (Fig. 2d inserted). Each duct is surrounded by a number of accessory glands, which are differentiated mucous glands (Fig. 2d inserted).
In the case of Rhinella jimi (Fig. 1a), it was clearly observed that, besides the parotoids (Fig. 1b), they show radial (Fig. 1c) and tibial macroglands (Fig. 1d), all of them with very similar morphology, although with variations in size and shape.
When the general topology, morphology and histochemistry of the granular glands are analysed together with the morphological appearance of the poison granules, it is possible to classify these glands into three basic types: skin common poison glands (COM), parotoid poison glands (PAR) and peripheral parotoid poison glands (PER).
Since COM poison glands are ordinary components of the dorsal skin, including the dorsal warts, and are also found throughout the ventral and pelvic skin, they are much more abundant when compared with the other two poison gland types. In COM glands the syncytial cytoplasm is light and have numerous evident peripheral nuclei and the poison granules are typically spherical, heterogeneously staining with toluidine blue (Fig. 3a–d). Although each species has its own typical characteristics, the general morphology of the secretion granules follows a similar pattern, always presenting internal subunits, either pale or dense (Fig. 3a–d). Cryofractures observed by SEM reveal that the surface of the granules is usually smooth (Fig. 3e) although it may show a rough appearance, depending on the species (Fig. 3f). The fractured granules exhibit subunits with a wide variety of shapes and different degrees of compaction (Fig. 3f insert). These subunits correspond to the unidimensional structures observed in the histological sections (Fig. 3a–d).
Analysis by TEM shows that the syncytium of COM glands is quite electron lucent and forms a halo around each one of the granules (Fig. 3g and h). The shape, size and electron density of the granules are variable, depending on the species (Fig. 3g–i). Organelles involved in poison synthesis such as rough endoplasmic reticulum and Golgi apparatus (Fig. 3h and i) are observed among the granules, throughout the syncytium, even in the most central portion of the gland.
Poison glands of PAR type are the major component of the parotoids in all studied species. Specifically, in Rhinella schneideri and R. jimi, the other macroglands besides the parotoids are also composed by PAR glands. Histologically, PAR glands consist on a dense syncytium with a lower number of nuclei when compared to COM glands (Fig. 4a). Moreover, the syncytium of PAR glands is characterized by a peripheral region composed of three clearly distinguishable layers (Fig. 4a). The first more external layer, subjacent to the glandular myoepithelium, is dense and about 2 μm thick and internally extends to the region where the syncytial nuclei are located (Fig. 4a). The second more internal layer, dense, wide and smooth, is characterized by scattered poison granules at different stages of formation and with a variety of sizes (Fig. 4a). The third central portion of the syncytium is full of light granules, most of them fusing to each other, immersed in a cytoplasm matrix that strongly stains with toluidine blue (Fig. 4a). Regardless the species analysed, the granules in PAR glands are always spherical or elliptical, very heterogeneous in size, and stain light and homogeneously with toluidine blue (Fig. 4a–d). Cryofractures observed by SEM reveal the wool-ball aspect of the granules (Fig. 4e) and clearly show that they are lodged within the cytoplasm matrix, which confers to the whole structure a spongy appearance (Fig. 4f).
Differently from COM glands, TEM observation of PAR glands reveals that the first external layer of the syncytium concentrates, besides the nuclei, all cytoplasm organelles (Fig. 4g–i), such as mitochondria, smooth and rough endoplasmic reticulum and Golgi apparatus (Fig. 4h). These organelles, in the second syncytial layer, give rise to the secretion granules (Fig. 4i), which gradually fuse to each other, increasing in size while they migrate towards the third central layer (Fig. 4j). The poison granules of PAR glands are quite homogeneous, and their electron lucent content do not outstand much from the syncytial matrix (Fig. 4j).
A third type of poison gland, here named PER, was found exclusively at the periphery (or margins) of the parotoids, as well as of other macroglands (Fig. 5a). PER glands are of an intermediate size between PAR and COM glands and, similarly to PAR glands, their syncytium is dense, and their ducts are always surrounded by accessory glands (Fig. 5b and c). At the same time, similarly to COM glands, PER glands histology and ultrastructure (TEM) reveal the conspicuous syncytial nuclei and the secretion granules that are spherical and with internal subunits (Fig. 5d–f). Moreover, organelles are dispersed amongst secretion granules throughout the syncytial cytoplasm is also very similar to what is observed in COM glands (Fig. 5g).
When the internal side of the skin preserved in formalin is observed with the naked eye, the glands of type PAR stand out due to their brownish colour. The use of this simple methodology made possible the observation that, exclusively in Rhinella schneideri and R. jimi, PAR glands, besides their occurrence in the macroglands, they are also present spread on other regions of the body in association with COM glands, especially in the dorsal skin, where they occur in large numbers, although with a smaller size when compared to those in the parotoids and other macroglands (Fig. 6). Subsequently, the identification of PAR glands was confirmed through histological and histochemical analysis (data not shown). In R. schneideri, PAR glands are found exclusively on the dorsal skin, occupying around 20% of the total area of the back (Fig. 6). In contrast, in R. jimi, these glands are even more widespread throughout the body, reaching 25% of the dorsal skin and occupying 6% of the ventral skin, where they form a non-protuberant occult glandular accumulation in the pectoral region (Fig. 6). The distribution pattern of PAR glands indicates that they are more abundant in the extremities and sides of the body (Fig. 6).
The glands of types COM and PER are histochemically different from PAR glands since their poison granules avidly stain with bromophenol blue, indicating high protein content (Fig. 7). On the other hand, the granules of PAR glands are rich in acid glycoconjugates, since they are strongly positive to alcian blue pH 2.5 (Fig. 7), but are immersed in a bromophenol blue positive matrix, rich in protein content. All three types of gland similarly react to the modified Masson-Fontana and Sudan black methods, indicating, respectively, the presence of biogenic amines and lipids in their contents (Fig. 7).
Table 1 summarizes the main morphological and histochemical results obtained for COM, PAR and PER glands.
Biochemical characterization of the poison in the dorsal warts and in the macroglands
SDS-PAGE of the poison extracted from the dorsal warts, structures that in Rhinella icterica and R. marina are typically composed of COM glands, presents a larger diversity of bands when compared to the poison extracted from the parotoids that are basically composed of PAR glands (Fig. 8a). In R. jimi, the poison from the dorsal warts, structures composed of PAR glands (differently from the other three toad species), presents a SDS-PAGE profile very similar to the profile observed for the poison extracted from parotoid, tibial and radial macroglands (Fig. 8b), structures composed of PAR glands in the four studied species.
In all four toad species, the poison from the parotoids was not able to cleave the tested substrates. In contrast, the poison extracted from the dorsal warts showed some bands with low proteolytic activity (Fig. 9). When gelatine was used as substrate in the gels, the poisons of Rhinella icterica, R. jimi and R. marina formed bands at approximately 5 kDa (Fig. 9a). In the gel containing fibrinogen, the poison of the dorsal warts of R. jimi and R. marina presented bands around 10 kDa (Fig. 9b). None of the tested samples showed caseinolytic or hyaluronidase activities (Fig. 9c and d).
The analysis of the poisons of the four species by RP-HPLC and mass spectrometry, revealed that, besides proteins, they are composed of low molecular mass molecules, such as biogenic amines, which are eluted at the beginning of the chromatography, and steroids, which are eluted in later times. Poisons of the dorsal warts and of the macroglands have very similar low molecular components, although with quantitative differences, in addition to some other exclusive molecules (Fig. 10a–d). In R. icterica, R. marina and R. schneideri, the poison of the dorsal warts shows different molecules from that of the parotoids (and, in the case R. schneideri, tibial macroglands also) (Fig. 10a–c). Exclusively in R. jimi, the poison of the dorsal warts is very similar to that of the parotoid, radial and tibial macroglands (Fig. 10d), which is compatible with the similarities observed through morphology, histochemistry and SDS-PAGE.
Although many papers have described the morphology of amphibian poison glands since the nineteenth century [23,24,25,26], none of them invested in an integrative approach, trying to gather morphological data with the amphibian biology and natural history . More recently, some studies have examined these glands in an interdisciplinary context, in order to increase the understanding of the morphology, biochemistry, and functioning of these structures [5, 6, 12, 13, 15, 22, 27,28,29,30].
Particularly within bufonids, the parotoid macroglands were always the preferred target of study, probably due to their more conspicuous structure. Very little attention has been given to other glandular accumulations such as the dorsal warts or the tibial and radial macroglands regarding the morphology and the biochemistry of their secretion. Our integrative approach, taking into consideration all types of glandular accumulation throughout the body, clearly revealed the existence of different types of poison glands (here named COM, PAR and PER glands) with peculiar distribution in each species.
In relation to glandular distribution, glands of type PAR showed a striking irregular pattern. While in Rhinella icterica and R. marina PAR glands are exclusively found composing the parotoids, in R. schneideri and R. jimi, besides composing the tibial and radial macroglands, PAR glands are also found in dorsal warts, as well as in other regions of the body. In R. jimi, for example, there is an evident accumulation of this gland type in the pectoral region, but, contrasting with the protuberant parotoids and warts on the back, they developed inward, not displaying any external volume. The development of macroglands, as well as their tendency to spread throughout the body, seems to provide to R. schneideri and R. jimi a greater protection against predators through the use of chemical defence when compared to the other toad species. Additionally, the macroglands may also provide physical protection to the regions where they are located, in a function similar to that of the parotoids, serving as bullet-proof vests and absorbing the bite impact, as described by Regis-Alves et al. .
Due to the unique morphological peculiarities presented by the three different glandular types, and to their pattern of distribution in each species, it seems unlikely that these glands could simply represent different stages of maturation of a single glandular type. Some studies have indicated that the macroglands are, in several anuran families, composed of glands with a different morphology from those found in the rest of the skin [12, 27, 31]. Nevertheless, none of the studies proceeded a comparative biochemistry of the poison of these two gland types. In this sense, Mailho-Fontana et al.  represented a breakthrough, showing that the poison of different types of macroglands in the frog Odontophrynus cultripes have different chemical compositions. The authors, however, did not discriminate the chemical composition of the poison from the dorsal warts.
The evolutionary origin of amphibian parotoids and other skin macroglands remains completely unknown. It is assumed that these glandular accumulations may have originated from the common skin poison glands as a response to selective pressure imposed by predation . Thus, body areas most likely to be attacked by predators, such as the extremities and flanks, must have developed differentiated glands in the skin. In this context, PER glands, which are specifically present at the periphery of the macroglands, seem to give an important clue about the process of formation of glandular accumulations. Our data indicate that PER glands may represent intermediate stages of glandular development, since they display hybrid morphology, with characteristics of both COM and PAR glands. Although the differentiation process is still totally unknown, facing our results, two possibilities are raised about PER glands: they may represent different evolutionary stages or, alternatively, they may represent intermediate ontogenetic stages of COM glands towards a gradual development into PAR glands throughout the toad’s life. At first glance, the latter hypothesis seems less plausible than the first one, since the present study was based exclusively on adult animals. Moreover, other studies show that the parotoid poison granules in newly metamorphosed toads already have morphology very similar to that of adults .
The simultaneous analysis of glandular morphology and chemical composition indicates a clear correlation between the form of the secretion granules and the class of molecules they contain. Granules mainly consisting of protein (as in COM glands) are always dense and have internal subunits. On the other hand, granules containing lower levels of proteins (as in PAR glands), do not show internal dense forms and, on the contrary, appear homogeneous. Our biochemical data confirm the difference between the poison of dorsal warts, with a higher diversity of proteins, and that of the parotoids. Literature analysis concerning the poison of bufonid parotoids, brings evidence that proteins, despite occurring in considerable amounts in the poison, have never received as much attention as the other compounds. Studies have shown that 25 to 35% of the dry weight of toad paratoid poison is represented by proteins [14, 15]. However, the identity and actual function of this category of molecules in bufonid poison is still quite controversial. Sciani et al.  questioned the role of parotoid proteins in chemical defence, since these authors did not find significant differences among several species of genus Rhinella.
In an attempt to clarify the functionality of poison proteins extracted from dorsal warts and parotoids of the four toad species, zymographic techniques were applied on SDS-PAGE gels to evaluate the existence of proteases. Proteolysis, albeit very mildly, was the only activity we could observe in the poison of dorsal warts emphasizing once more the differences among the gland types here described. This result agrees with that was observed by Sousa-Filho et al. , who showed that most proteins in the poison of Rhinella scheneideri parotoids are constitutive, and even those still unknown proteins do not show proteolytic activity.
Toads, similarly to other amphibians, have a typical passive mode of defence and, when bitten by a predator/aggressor, are unable to trigger a poisoning system . In contrast, venomous animals are able to actively inject their venom, usually rich in proteases, causing damage to the extracellular matrix and facilitating venom diffusion through the tissues [28, 34,35,36,37,38,39]. On the other hand, in toads, the steroids and biogenic amines present in the poison, due to their low molecular mass, must be able to cross the oral mucosa without the aid of proteases, rapidly reaching the bloodstream, and acting on the cardiovascular system where they increase blood pressure and/or raise heart contraction [40, 41].
The analysis of our data indicates the possibility that larger numbers of PAR poison glands on the body skin may favour toad adaptation to the terrestrial environment. This hypothesis is mainly based on the high hydrophilicity demonstrated by PAR glands, which are rich in acid glycoconjugates that may facilitate water absorption and retention during periods of drought, as discussed by Toledo & Jared  and later explored by Van Bocxlaer et al. . This idea seems even more plausible considering the the abundance of PAR glands both in Rhinella schneideri and R. jimi, species typical of xeric biomes. Taking into consideration that the skin is the interface between the animal and the environment, this hypothesis should be better investigated through the use of other approaches, opening new perspectives of study specially in the areas of physiology and ecology.
The present study clearly shows that, depending on the toad species, the poison produced by the dorsal warts is different from that produced by the macroglands. This observation opens a new perspective for future studies aiming to clarify the role of each one of these different skin gland types. Moreover, we concluded that the morphology of the poison granules is directly related to their biochemical composition. Regarding these aspects, we propose that the study of a larger number of toad species would help to elucidate the morphological and biochemical variation of bufonid skin glands, in an enlarged phylogenetic scenario. Finally, our results show that toads inhabiting xeric environments such as Rhinella jimi and, to a lesser extent, R. schneideri, have similar distribution of their skin gland types, although in different proportions. Summarizing, the data here presented indicate that the development of a more robust cutaneous defensive arsenal among toads, at least within the group R. marina, may have simultaneously contributed to a successful colonization of dry environments.
Specimens of Rhinella icterica and Rhinella schneideri were collected in different locations of São Paulo state, Brazil, in forested habitats (Atlantic Rainforest) or open savannah (Cerrado), respectively. Specimens of Rhinella marina were obtained in Amazonian Rainforest in Belterra, Pará. Specimens of Rhinella jimi were collected in Brazilian semiarid (Caatinga) in Angicos, Rio Grande do Norte state. Animals were obtained under collecting permit provided by Instituto Chico Mendes de Conservação da Biodiversidade (Sistema de Autorização e Informação em Biodiversidade #48080–2). All aspects of the study were carried out in accordance with protocols approved by the Ethics Committee on Animal Use of Instituto Butantan (protocol #1046/13).
Anatomy, histology and histochemistry
Eight adult specimens of Rhinella icterica, Rhinella marina, Rhinella schneideri and Rhinella jimi (n = 2, for each species) were euthanized with a lethal dose of thiopental and skin samples from dorsal, ventral and pelvic patch and the entire macroglands of all individuals were preserved in Bouin 4% or PBS buffered paraformaldehyde (pH 7.2). After dehydration in ethanol, the samples were embedded in transversal and longitudinal orientations using paraffin and glycol methacrylate (historesin Leica®). The blocks were sectioned in a Microm® HM 340 microtome (0.5 to 6 μm thick), using disposable steel blades (for paraffin) or glass knives (for historesin). The sections were stained with haematoxylin-eosin (for paraffin) or toluidine blue-fuchsine (for historesin). For basic characterization and distribution of the chemical composition of the glands the following histochemical methods were applied: bromophenol blue (for proteins), alcian blue pH 2.5 and periodic acid-Schiff (PAS) (for acid and basic mucopolysaccharides, respectively), modified Masson-Fontana (for biogenic amines), and Sudan black B (for lipids).
For transmission electron microscopy (TEM), fragments of dorsal warts and of the macroglands of two individuals per species were extracted and fixed according to Karnovsky (5% glutaraldehyde and 4% paraformaldehyde in 0.1 M cacodylate buffer, pH 7.2), post-fixed in 1% osmium tetroxide in 0.1 M cacodylate buffer and contrasted in 0.5% aqueous uranyl with 13.3% sucrose. After dehydration, the samples were embedded in epoxy resin (Polybed, Electron Microscopy Science). Ultrathin sections were contrasted with 2% uranyl and lead citrate and examined under the LEO 906E transmission electron microscope, operating at 80 kV.
For scanning electron microscopy (SEM), skin samples and macroglands were fixed following the same protocol described above, immersed in dimethyl sulfoxide (DMSO), frozen in liquid nitrogen and cryofractured with the aid of a frozen steel blade. After dehydration in ethanol, the samples were mounted on aluminium stubs, dried in a critical point apparatus, covered with gold in a sputtering device, and examined in a FEI Quanta 250 scanning electron microscope, operating at 10–12 kV.
Poison extraction and dilution
Poison samples from dorsal warts, as well as macroglands, were extracted from the animals by manual compression, collected in plastic tubes and kept in a freezer at − 20 °C. After thawing, part of each sample was diluted in a solution of ultrapure water containing 0.1% trifluoroacetic acid (TFA) and 5% acetonitrile (ACN), yielding a poison solution of approximately 5 mg/mL. For analysis by mass spectrometry, the samples were resuspended in ultrapure water containing 5% acetonitrile and 0.5% formic acid. The amount of proteins present in the poison was estimated using the bicinchoninic acid method.
Unidimensional electrophoresis (SDS-PAGE) e zymography
To analyse the protein profiles, poison samples (15 μg diluted in 30 μL) of the dorsal warts and macroglands were loaded onto a 12% polyacrylamide gel (PAGE) containing sodium dodecyl sulphate (SDS), under non-reducing conditions, according to Laemmli . After separation of the proteins by electrophoresis, the gels were stained with Coomassie brilliant blue or silver. In order to evaluate the presence of proteases in the poisons, zymography was applied [36, 37, 45], using casein, gelatine and fibrinogen as substrates in the SDS- PAGE 12%. After completion of electrophoresis, the gels were processed, stained with Coomassie brilliant blue and immersed in bleach solution. Clear areas in the gel indicated where enzymatic activity occurred.
RP-HPLC and mass spectrometry
A RP-HPLC reversed phase high performance liquid chromatography system (20A Prominence, Shimadzu Co., Japan) was used to obtain the chromatographic profile and purification of the secretions of the skin poison glands and parotoids with a C18 column (ACE C18, 5 μm, 100 Å, 250 mm × 4.6 mm). Chromatography was performed by injecting 10 μL of poison, eluted in a gradient from 0 to 100% of B in 30 min, solvent A being TFA/water (1:1000) and solvent B TFA/ACN/water (1:900:100), in a constant flow of 1 mL/min, at 38 °C. The eluted content was monitored by a Shimadzu SPD-M20A PDA detector, in the range of 200 to 500 nm.
Mass spectrometry (MS and MSn) were performed on-line in a nanoHPLC (UltiMate HPLC System, LC Packings, Dionex, USA) coupled to the mass spectrometer (LC-MS/MS). An ESI spectrometer (LCQDuoTM, ThermoFinnigan, USA) was used with a nanospray source. The samples were introduced into the spectrometer at a flow rate of 1 μL/min. The voltage used in the spray was 1.8 kV and the capillary voltage was 46 V, in a temperature of 180 °C. Spectra were obtained in the range of 50 to 2000 m/z. Data acquisition and processing was performed by Xcalibur.
Common poison gland
Liquid chromatography–mass spectrometry
- MSn :
Sequential Mass Spectrometry
Parotoid poison gland
Peripheral parotoid poison gland
Reversed-phase high-performance liquid chromatography
Sodium dodecyl sulphate polyacrylamide gel electrophoresis
Scanning electron microscopy
Transmission electron microscopy
Stebbins RC, Cohen NW. A Natural History of Amphibians. Princeton: University Press; 1995.
Duellman WE, Trueb L. The biology of amphibians. New York: MacGraw–Hill; 1994.
Jared C, Antoniazzi MM, Jordão AEC, Silva JRMC, Greven H, Rodrigues MT. Parotoid macroglands in toad (Rhinella jimi): their structure and functioning in passive defense. Toxicon. 2009;54:197–207. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2009.03.029.
Jared SGS, Jared C, Egami MI, Mailho-Fontana PL, Rodrigues MT, Antoniazzi MM. Functional assessment of toad parotoid macroglands: a study based on poison replacement after mechanical compression. Toxicon. 2014;87:92–103. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2014.05.020.
Mailho-Fontana PL, Antoniazzi MM, Toledo LF, Verdade VK, Sciani JM, Rodrigues MT, et al. Passive and active defence in toads: the parotoid macroglands in Rhinella marina and Rhaebo guttatus. J Exp Zool A. 2014;321:65–77. https://0-doi-org.brum.beds.ac.uk/10.1002/jez.1838.
Regis-Alves E, Jared S, Maurício B, Mailho-Fontana PL, Antoniazzi MM, Fleury-Curado MC, et al. Structural cutaneous adaptations for defense in toad (Rhinella icterica) parotoid macroglands. Toxicon. 2017;137:128–34. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2017.07.022.
Mackessey S, Baxter LM. Bioweapons synthesis and storage: the venom gland of front-fanged snakes. Zool Anz. 2006;245:147–59. https://0-doi-org.brum.beds.ac.uk/10.1016/j.jcz.2006.01.003.
Soliman BA, Shoukry NM, Mohallal ME, Fetaih HAW, Khaled HS. Fine structure of the stinger, histology and histochemistry of the venom gland in the scorpion Androctonus amoreuxi (Buthidae). J Basic Appl Zoo. 2013;66:41–6. https://0-doi-org.brum.beds.ac.uk/10.1016/j.jobaz.2013.03.001.
Delfino G, Nosi D, Giachi F. Secretory granule-cytoplasm relationships in serous glands of anurans: ultrastructural evidence and possible functional role. Toxicon. 2001;39:1161–71. https://0-doi-org.brum.beds.ac.uk/10.1016/S0041-0101(00)00253-1.
Toledo RC, Jared C. Cutaneous granular glands and amphibian venoms. Comp Biochem Phys A. 1995;111:1–29. https://0-doi-org.brum.beds.ac.uk/10.1016/0300-9629(95)98515-I.
Brodie ED Jr, Smatresk NL. The antipredator arsenal of fire salamanders: spraying of secretions from highly pressurized dorsal skin glands. Herpetologica. 1990;46:1–7.
Antoniazzi MM, Neves PR, Mailho-Fontana PL, Rodrigues MT, Jared C. Morphology of the parotoid macroglands in Phyllomedusa leaf frogs. J Zool. 2013;291:42–50. https://0-doi-org.brum.beds.ac.uk/10.1111/jzo.12044.
Mailho-Fontana PL, Antoniazzi MM, Rodrigues I, Sciani JM, Pimenta D, Brodie ED Jr, et al. Parotoid, radial, and tibial macroglands of the frog Odontophrynus cultripes: differences and convergence with toads. Toxicon. 2017;129:123–33. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2017.02.022.
Perry P. Proteins of parotoid gland secretions from toads of genus Bufo. Contemp Herpetol. 2000;2000:1–3.
Sousa-Filho LM, Freitas CD, Lobo MD, Monteiro-Moreira AC, Silva RO, Santana LA, et al. Biochemical profile, biological activities, and toxic effects of proteins in the Rhinella schneideri parotoid gland secretion. J Exp Zool A. 2016;325:511–23. https://0-doi-org.brum.beds.ac.uk/10.1002/jez.2035.
Sakate M, Lucas De Oliveira PC. Toad envenoming in dogs: effects and treatment. J Venom Anim Toxins. 2000;6:1–9. https://0-doi-org.brum.beds.ac.uk/10.1590/S0104-79302000000100003.
Doody JS, Green B, Sims R, Rhind D, West P, Steer D. Indirect impacts of invasive cane toads (Bufo marinus) on nest predation in pig-nosed turtles (Carettochelys insculpta). Wildl Res. 2006;33:349–54.
Griffiths AD, Mckay JL. Cane toads reduce the abundance and site occupancy of Merten’s water monitor (Varanus mertensi). Wildl Res. 2007;34:609–15.
Keomany S, Mayxay M, Souvannasing P, Vilayhong C, Stuart BL, Srour L, et al. Toad poisoning in Laos. Am J Trop Med Hyg. 2007;77:850–3.
Letnic M, Webb JK, Shine R. Invasive cane toads (Bufo marinus) cause mass mortality of freshwater crocodiles (Crocodylus johnstoni) in tropical Australia. Biol Conserv. 2008;141:1773–82. https://0-doi-org.brum.beds.ac.uk/10.1016/j.biocon.2008.04.031.
Pramuk JB. Phylogeny of south American toad Bufo (Anura: Bufonidae) inferred from combined analyses. Zool J Linnean Soc. 2006;146:407–52. https://0-doi-org.brum.beds.ac.uk/10.1111/j.1096-3642.2006.00212.x.
Regueira E, Dávila C, Hermida GN. Morphological changes in skin glands during development in Rhinella arenarum (Anura: Bufonidae). Anat Rec. 2016;299:141–56. https://0-doi-org.brum.beds.ac.uk/10.1002/ar.23284.
Wilber CG, Carroll PL. Studies on the histology of the glands in the skin of Anura. The parotoid gland of Bufo americanus holbrook. Trans Am Microsc Soc. 1940;59:123–8.
Lutz B. Venomous toads and frogs. In: Bücherl W, Buckey EE, editors. Venomous animals and their venoms. New York and London: Academic Press; 1971. p. 423–73.
Hostetler JR, Cannon MS. The anatomy of the parotoid gland in Bufonidae with some histochemical findings. I Bufo marinus. J Morphol. 1974;142:225–40. https://0-doi-org.brum.beds.ac.uk/10.1002/jmor.1051420208.
Licht LE, Sever DM. Structure and development of the paratoid gland in metamorphosed and neotenic Ambystoma gracile. Copeia. 1993;1:116–23.
Lenzi-Mattos R, Antoniazzi MM, Haddad CB, Tambourgi DV, Rodrigues MT, Jared C. The inguinal macroglands of the frog Physalaemus nattereri (Leptodactylidae): structure, toxic secretion and relationship with deimatic behaviour. J Zool. 2005;266:385–94. https://0-doi-org.brum.beds.ac.uk/10.1017/S095283690500703X.
Jared C, Mailho-Fontana PL, Antoniazzi MM, Mendes VA, Barbaro KC, Rodrigues MT, et al. Venomous frogs use heads as weapons. Curr Biol. 2015;25:2166–70. https://0-doi-org.brum.beds.ac.uk/10.1016/j.cub.2015.06.061.
Chen W, Hudson CM, DeVore JL, Shine R. Sex and weaponry: the distribution of toxin-storage glands on the bodies of male and female cane toads (Rhinella marina). Ecol Evol. 2017;7:8950–7. https://0-doi-org.brum.beds.ac.uk/10.1002/ece3.2914.
Jared C, Mailho-Fontana PL, Marques-Porto R, Sciani JM, Pimenta DC, Brodie ED, et al. Skin gland concentrations adapted to different evolutionary pressures in the head and posterior regions of the caecilian Siphonops annulatus. Sci Rep. 2018;8:3576.
Melzer S, Clerens S, Bishop P. Differential polymorphism in cutaneous glands of archaic Leiopelma species. J Morphol. 2011;272:1116–30. https://0-doi-org.brum.beds.ac.uk/10.1002/jmor.10960.
Chammas SM, Carneiro SM, Ferro RS, Antoiazzi MM, Jared C. Development of integument and cutaneous glands in larval, juvenile and adult toads (Rhinella granulosa): a morphological and morphometric study. Acta Zool. 2015;96:460–77. https://0-doi-org.brum.beds.ac.uk/10.1111/azo.12091.
Sciani JM, Angeli CB, Antoniazzi MM, Jared C, Pimenta DC. Differences and similarities among parotoid macrogland secretions in south american toads: a preliminary biochemical delineation. Sci World J. 2013;2013:1–9. https://0-doi-org.brum.beds.ac.uk/10.1155/2013/937407.
Tan NH, Ponnudurai G. Comparative study of the enzymatic, hemorrhagic, procoagulant and anticoagulant activities of some animal venoms. Comp Biochem Phys C. 1992;103:299–302.
Veiga SS, Da Silveira RB, Dreyfuss JL, Haoach J, Pereira AM, Mangili OC, et al. Identification of high molecular weight serine proteases in Loxosceles intermedia (brown spider) venom. Toxicon. 2000;38:825–39 10.1016/S0041-0101(99)00197-X.
Barbaro KC, Knysak I, Martins R, Hogan C, Winkel K. Enzymatic characterization antigenic cross-reactivity and neutralization of dermonecrotic activity of five Loxosceles spider venoms of medical importance in the Americas. Toxicon. 2005;45:489–99. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2004.12.009.
Barbaro KC, Lira MS, Soares SL, Malta MB, Garrone-Neto D, Cardoso JLC, et al. Comparative study on extracts from the tissue covering the spines of freshwater (Potamotrygon falkneri) and marine (Dasyatis guttata) stingrays. Toxicon. 2007;50:676–87. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2007.06.002.
Lira MS, Furtado MF, Martins LMP, Lopes-Ferreira M, Santoro ML, Barbaro KC. Enzymatic and immunochemical characterization of Bothrops insularis venom and its neutralization by polyspecific Bothrops antivenom. Toxicon. 2007;49:982–94. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2007.01.009.
Malta MB, Lira MS, Soares SL, Rocha GC, Knysak I, Martins R, et al. Toxic activities of Brazilian centipede venoms. Toxicon. 2008;52:255–63. https://0-doi-org.brum.beds.ac.uk/10.1016/j.toxicon.2008.05.012.
Daly JW, Spande TF, Garraffo HM. Alkaloids from amphibian skin: a tabulation of over eight-hundred compounds. J Nat Prod. 2005;68:1556–75. https://0-doi-org.brum.beds.ac.uk/10.1021/np0580560.
Ye M, Guo DA. Analysis of bufadienolides in the Chinese drug ChanSu by high-performance liquid chromatography with atmospheric pressure chemical ionization tandem mass spectrometry. Rapid Commun Mass Spectrom. 2005;19:1881–92. https://0-doi-org.brum.beds.ac.uk/10.1002/rcm.1989.
Toledo RC, Jared C. Cutaneous adaptations to water balance in amphibians. Comp Biochem Phys A. 1993;105:593–608. https://0-doi-org.brum.beds.ac.uk/10.1016/0300-9629(93)90259-7.
Van Bocxlaer I, Loader SP, Roelants K, Biju SD, Menegon M, Bossuyt F. Gradual adaptation toward a range-expansion phenotype initiated the global radiation of toads. Science. 2010;327:679.
Laemmli UK. Cleavage of structural proteins during assembly of the head of bacteriophage T4. Nature. 1970;227:680–5.
Heussen C, Dowdle EB. Electrophoretic analysis of plasminogen in polyacrylamide gels containing sodium dodecyl sulfate and copolymerized substrates. Anal Biochem. 1980;102:196–202. https://0-doi-org.brum.beds.ac.uk/10.1016/0003-2697(80)90338-3.
Mcclean S, Robinson RC, Shaw C, Smyth WF. Characterization and determination of indole alkaloids in frog-skin secretions by electrospray ionization ion trap mass spectrometry. Rapid Commun Mass Spectrom. 2002;16:346–54.
Maciel NM, Schwartz CA, Pires OR, Sebben A, Castro MS, Sousa MV, et al. Composition of indolealkylamines of Bufo rubescens cutaneous secretions compared to six other brazilian bufonids with phylogenetic implications. Comp Biochem Phys B. 2003;134:641–9. https://0-doi-org.brum.beds.ac.uk/10.1016/S1096-4959(03)00022-8.
Liu Y, Xiao Y, Xue X, Zhang X, Liang X. Systematic screening and characterization of novel bufadienolides from toad skin using ultra-performance liquid chromatography/electrospray ionization quadrupole time-of-flight mass spectrometry. Rapid Commun Mass Spectrom. 2010;24:667–78. https://0-doi-org.brum.beds.ac.uk/10.1002/rcm.4436.
We thank Beatriz Mauricio, Luciana Almeida Sato and Simone G.S. Jared for technical assistance. Grants were provided by CNPq and FAPESP.
CNPq to CJ, processes # 308178/2014–9 and 461457/2014–8.
CNPq to DCP, processes # 303792/2016–7.
CNPq to MMA, processes # 309589/2017–7.
FAPESP to PLMF, process # 2014/15334–4.
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All aspects of the study were carried out in accordance with protocols approved by the Ethics Committee on Animal Use of Instituto Butantan (protocol #1046/13).
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Mailho-Fontana, P.L., Antoniazzi, M.M., Sciani, J.M. et al. Morphological and biochemical characterization of the cutaneous poison glands in toads (Rhinella marina group) from different environments. Front Zool 15, 46 (2018) doi:10.1186/s12983-018-0294-5
- Granular glands