Formation and discharge of nematocysts is controlled by a proton gradient across the cyst membrane
© Springer-Verlag and AWI 2005
Received: 4 March 2005
Accepted: 24 October 2005
Published: 26 November 2005
Cnidaria catch and kill their prey by means of nematocysts. A nematocyst consists of a capsule containing a coiled tubule. On triggering, the cyst extrudes this tubule in an extremely rapid manner. The mechanisms and driving forces of discharge are still unknown. We found nematocysts of various cnidarians to be acidic inside and propose that the pH difference between cyst matrix and cytoplasm drives the discharge of cysts. For large cysts of Aiptasia we calculated that the internal concentration of protons and protonated carboxyl groups is about 5 M. Cysts contain polyacids in a high concentration. At a low pH several of the carboxyl groups of the polymer are uncharged. The carboxyl groups dissociate when, on triggering, the proton concentration becomes balanced across the cyst membrane. The speed of protons in water is extremely rapid. Thus, the equilibration of the proton concentration initially results in a negative net charge within the cyst and therefore in a sudden electrostatic repulsion between the dissociated carboxyl groups of the polymer. This causes an increase in the pressure of the matrix against the cyst wall. We suggest that this nonosmotic pressure increase causes the first and extremely rapid step of discharge. We propose that in a second step cations and water are taken up, generating an increase in osmotic pressure. A change in the pH value may also facilitate the invagination and evagination, respectively, of the tubule.
KeywordsCnidaria Nematocyte Polyglutamic acid pH gradient Lysosome
Stenoteles of Hydra are the best-studied nematocysts (for review, see Kass-Simon and Scappaticci 2002, Thurm et al. 2004). The whole process of tubule extrusion is completed within 3 ms. After an electric triggering the volume of the capsule instantaneously increases by more than 10%. Then a preformed opening, the operculum, opens and the stylet-bearing portion of the tubule is ejected. This phase is extremely short, taking less than 10 μs. Subsequently, after a short resting phase of about 150 ms, the tubule is completely extruded (Tardent and Holstein 1982; Holstein and Tardent 1984).
The mechanisms and driving forces of discharge have been studied by a large number of authors for more than 100 years (for review see Kühn 1916; Bouillon 1993; Kass-Simon and Scappaticci 2002). In general, a high internal osmotic pressure and mechanical energy stored in the walls of cysts and/or tubules have been suggested as causing the discharge when an external cue reaches the cnidocil. The cnidocil is a mechanoreceptor on the cell surface. The observation of Holstein and Tardent (1984) that a stenotele cyst swells immediately before discharge by about 10% is a particular challenge. The authors proposed that the initial volume increase is produced osmotically, whereas the subsequent discharge additionally involves the release of mechanical energy stored in the capsular wall. Weber (1989) argued that stenoteles in Hydra are under a constantly high internal osmotic pressure (15.3 MPa). The pressure is dominated by Donnan potential; all small, inorganic ions but not certain large polyanions (polyglutamic acid) are assumed to be able to move unhindered into and out of the capsule. The monomer concentration of the polyglutamic acid was calculated to reach 2 M. The pH was assumed to be almost identical with that of the surrounding cytoplasm (Weber 1989). With respect to various mastigophores of Anemonia viridis, Thomason (1991) proposed the discharge results from an increase of the intracapsular pressure ranging from 0.97 to 1.9 MPa.
However, most authors claim there is no convincing explanation of how the osmotic pressure can suddenly increase. Indeed, it is difficult to understand how a cyst that is in equilibrium with its surroundings can swell on triggering. Exocytosis (e.g., see Holstein and Tardent 1984; Golz 1994; Gitter and Thurm 1996), that is, the fusion of the cyst membrane with the cell membrane as the initial step of discharge, results in a net loss of the highly concentrated compounds. One would expect the osmotic pressure to decrease, rather than to increase initially. Furthermore, the idea that the discharge is driven by stored mechanical energy fits the volume decrease observed as a second step of the discharge of stenoteles (Tardent and Holstein 1982) but does not fit the initial volume increase. On discharge the volume of several types of cysts decreases only slightly, whereas in some cases it even increases (Lipin 1910, after Kühn 1916). However, if the energy is stored in the coiled tubule (Kass-Simon and Scappaticci 2002), one confronts the problem of explaining how such a tubule is taken up by the capsule and how a volume decrease of certain cysts (Kühn 1916) is obtained when such a cyst, including its invaginated tubule, takes its final step of development while already positioned in a tentacle. These obvious problems led Ewald (1915, after Kühn 1916) to propose that on triggering, compounds of the matrix change their state in such a way that they need a higher volume: “eine Substanz von labiler Zusammensetzung,” [die] “ihre Konstitution verändert und dadurch einen größeren Raum einnimmt” (p. 474). This change of state would result in a pressure against the cyst wall and could initiate the discharge. For a complete discharge, Ewald proposed, water is taken up, causing further swelling of the matrix. We suggest that precisely this takes place.
We suggest that the energy for the initial swelling and subsequent discharge is stored in a proton gradient across the cyst wall. Triggering may cause the release of protons, which results in an immediate dissociation of carboxyl groups of the stored polyacids in the cyst matrix. The resultant negative charge would cause an electrostatic repulsion among the carboxyl groups, followed by an increase in volume and the first step of discharge. Subsequently, water and cations may be taken up by the cyst, causing an increase of the osmotic pressure. The altered pH may affect components of the tubule wall in such a way that the evagination of the tubule is favored.
Materials and methods
Polyps of Aiptasia sp. (Anthozoa), Aurelia aurita (Scyphozoa), Clytia johnstoni (Hydrozoa), Thecocodium quadratum (Hydrozoa), Cladonema sp. (Hydrozoa), and Tripedalia cystophora (Cubozoa) were cultured at 20°C in artificial seawater of 1050 mosmol (Tagis Tropic Marine, Dreieich, Germany). In experiments with medusae, only freshly released specimens were used. Hydra vulgaris (strain Zürich) was cultured in buffered artificial fresh water at 20°C (Zeretzke et al. 2002).
Acontia of Aiptasia sp. were isolated mechanically and placed on the top of a FET pH-meter (Shindengen, Electric MFG Co, Tokyo, Japan). Then seawater was removed down to a volume of about 15 μl. Finally, 40 μl of distilled water was added. This treatment resulted in a discharge of cysts. Polyps of A. aurita were induced to produce medusae (strobilation), according to Kroiher et al. (2000). Only medusae (ephyrae) that dropped off were put on the FET, the amount of seawater was reduced down to a volume of about 15 μl, and distilled water was added. Spontaneously produced medusae of C. johnstoni, Cladonema sp., and T. quadratum were treated in the same way. Polyps of H. vulgaris (strain Zürich) were taken from a mass culture and placed on the FET. After removing culture medium to about 15 μl, saturated NaCl (in culture medium, 10–20 μl) was added to cause nematocyst discharge (Will 1914, after Kühn 1916).
Fixed and also living animals were stained with Acridin orange and DAPI (4′,6-diamidino-2-phenylindole), respectively, according to Szczepanek et al. (2002). Animals were fixed in 4% formaldehyde. Further, living animals were treated with LysoSensor (TM) Blue DND-167 (Molecular Probes) dissolved in dimethylsulfoxide (DMSO) as described in the distributor’s instructions. Poly-DL-aspartic acid, sodium salt 40 wt% solution in water (Sigma), was mixed 1:1 with concentrated HCl. The precipitate was washed two times with concentrated HCl and then transferred to diluted HCl. CM-Sephadex C-25 (Pharmacia) was equilibrated with 0.5 M sodium phosphate buffer at pH 3.0 and pH 4.0, respectively. Microscopic observations and photographs were made using an Axiocam camera and an Axioskop fluorescence microscope (Zeiss) equipped with a UV-filterset (Ex 365 nm, Em 445/50 nm) and an FITC/GFP filterset (Ex 470/40 nm, Em 525/50 nm).
Maximal observed decrease of pH in surrounding water after discharge of nematocysts
Class, species/developmental state or organ
pH in seawater (15 μl)
pH after adding distilled water (40 μl)
Anthozoa, Aiptasia sp./isolated acontia of polyp
Scyphozoa, Aurelia aurita/ephyra (young medusa)
Cubozoa, Tripedalia cystophora/polyp
Cubozoa, Tripedalia cystophora/medusa
Hydrozoa, Clytia johnstoni/medusa
Hydrozoa, Thecocodium quadratum/medusa
Hydrozoa, Cladonema sp./medusa
Hydrozoa, Hydra vulgaris/polyp
When the experiment was performed with acontia isolated about 4 h before treatment or with acontia isolated from animals fed some hours before treatment, we found a discharge of nematocysts as well, but the pH only dropped to values just below or still above pH 7. We suggest that only a fraction of the nematocyst population responds very sensitively to external changes such as mechanical handling and contact with prey animals.
About 15 young medusae (ephyrae) of the scyphozoon A. aurita were placed on the top of a FET. Then the amount of seawater was reduced to 15 μl, and 40 μl of distilled water was added. The pH dropped to minimally pH 6.3, a value well below that of the cytoplasm (Table 1). We treated in a similar way polyps and medusae of the cubozoan T. cystophora (about 30 polyps and 8 medusae, respectively, per experiment), medusae of C. johnstoni (Hydrozoa) (about 20 animals per experiment), medusae of T. quadratum (Hydrozoa) (about 30 animals per experiment), and medusae of Cladonema sp. (about 12 animals per experiment). In all cases a drop of the pH was observed (Table 1). Nematocysts of Hydra do not discharge when not treated with distilled water, but when transferred to saturated NaCl solution. About ten H. vulgaris were placed on the top of a FET in about 15 μl culture medium. Following the application of 10–20 μl saturated NaCl solution, the pH dropped to minimally 6.0 (Table 1).
The minimal pH reached after discharge was not the same in repetitive experiments with the same species. In the repetitions we used different numbers of animals, and the amount of culture medium per volume of seawater present in the final test volume was certainly not identical. Both seawater and the Hydra culture medium have a buffering capacity. When seawater (15 μl) was mixed with distilled water (40 μl) and Hydra culture medium (15 μl) with saturated NaCl solution (40 μl), we did not observe a fall of the pH.
In a second set of experiments we used various fluorescent probes to study the matrix of nematocysts. We followed the protocol of Szczepanek et al. (2002) and stained nematocysts of Hydra with Acridin orange (AO) and DAPI (4′,6-diamidino-2-phenylindole), respectively. Animals were fixed with formaldehyde in a buffer (pH 7.6) containing EDTA to prevent Ca2+-ions to enter the cyst matrix (Ca2+-ions were found to hinder the staining of the cyst matrix). As observed by Szczepanek et al. (2002), the procedure results in a brilliant staining of both the nuclei and the cyst matrix. The color of the nuclei differs from that of the cyst; as in the latter, a metachromic shift in the emission spectrum is caused by binding to poly-γ-glutamic acid. In another experiment we added the dyes Acridin orange and DAPI, respectively, directly to the culture medium to get a vital staining, and found the nuclei stained immediately but hardly stained the cyst matrix even when the dye had been applied for days. The staining of nuclei indicates that the dyes are able to penetrate unit membranes such as the plasma membrane, whereas the cyst matrix does not appear to be in a condition that allows an enrichment of the dyes. Szczepanek et al. (2002) showed that Ca2+-ions hinder a staining of the cyst matrix, but they also showed that in living animals Ca2+-ions are lacking in the matrix. Thus the results obtained by vital staining call for a different explanation. We suggest that for living animals the pH of the matrix of nematocysts from the onset of polyacid synthesis onward (see later) is much lower than after fixation at pH 7.6.
Specimen of Hydra polyps, Aurelia ephyrae, and acontia of Aiptasia were treated with LysoSensor (TM) Blue DND-167. Because of its low pK a value (pK a =5.1) the probe was almost nonfluorescent at neutral pH and displayed a blue fluorescence in acidic compartments. Our treatment lasted from a few minutes up to 6 days. With increasing time, we found that background staining increased in intensity. A few nematocysts were found to generate a light blue fluorescence (less than 1%), whereas the majority appeared black despite having been treated for 6 days; that is, most did not even display the overall background staining (Fig. 2c, d). It appears that the majority of nematocysts do not accumulate the dye. In another experiment we simulated compartments containing polyacids in undissociated form by suspending poly-DL-aspartic acid in diluted HCl. After application of the LysoSensor, the solution delivered a strong fluorescence and the precipitated crystals of poly-DL-aspartic acid appeared dark (Fig. 2e, f). This shows that undissociated carboxyl groups do not accumulate the dye. We further treated CM-Sephadex beads equilibrated with 0.5 M sodium phosphate buffer at pH 3.0 and pH 4.0, respectively, with the LysoSensor and found that the beads enriched the probe at pH 4 but not at pH 3.0 (Fig. 2g, h). Thus, we propose that in the matrix of nematocysts the carboxyl groups are largely undissociated.
Arguments that nematocysts are acidic inside and display a low osmotic pressure
The current view is that a cyst displays a high internal osmotic pressure and a neutral pH. Nematocysts of various cnidarians contain large amounts of polypeptides rich in glutamic and aspartic acids (Blanquet 1970; Mariscal 1974) including poly-γ-glutamic acid (pG) (Weber 1990). In stenoteles of Hydra, Weber (1989) found a glutamic acid monomer concentration of about 2 M (chain length of the polymer about 20 units). He argued that the stenoteles are under a constantly high internal osmotic pressure (15.3 MPa) that is dominated by Donnan potential: All small inorganic ions, but not large polyanions, can move unhindered into and out of the capsule. The interior of the capsule was said to display an almost neutral pH, although the pH value had not been measured. A calculation based on these data and textbooks of physical chemistry leads to an osmotic pressure difference between cyst and cytoplasm in the range of only 0.2–0.5 MPa. This calculation is based on a pG concentration of 0.1 M (2 M glutamic acid monomer, a mean of 20 units per polymer) 2 M K+ (Gerke et al. 1991) and a neutral pH. For reasons of physics the concentration of polymers cannot be much higher. Thus, the contribution of possibly overlooked polymers to the pressure can be ignored. The probability that overlooked low-molecular-weight compounds add to the pressure is low, because they only can exert the pressure to the unit membrane at the outer surface of the capsule but not to the rigid capsule itself. The unit membrane cannot withstand a high pressure. As the cytoplasm contains both small ions and polymers and that pG is not a strong electrolyte, the osmotic pressure difference at about pH 7 may be closer to 0.2 than to 0.5 MPa.
Isolated cysts contain large amounts of Ca2+ (Blanquet 1970, 1988, Weber et al. 1987). Once bound to the matrix, Ca2+ is extremely difficult to remove (Weber et al. 1987). Only in the presence of Ca2+-chelators during fixation it is possible to stain fixed cysts with cationic dyes such as Acridin orange (Szczepanek et al. 2002). It appears that cysts in their natural state do not contain Ca2+. Either the unit membrane prevents the uptake efficiently, or the matrix is in a state unable to enrich Ca2+. We suggest that the latter is more important. Poly-γ-glutamic acid is argued to be largely protonated and therefore unable to bind Ca2+.
The usual argument for an isolated cyst being still in natural state is its ability to discharge on stimulation. Weber (1989) induced a discharge of isolated cysts that have lost their outer (unit) membrane to discharge by treatment with subtilisin (a protease) or dithioerythritol. This treatment destabilizes the capsule wall. The observed explosion indicates an osmotic pressure difference across the wall and/or mechanical energy stored in the capsule wall and the tubule. However, there is an initial volume increase under natural conditions (Holstein and Tardent 1984). This indicates that the discharge is not primarily driven by an existing high internal osmotic pressure or by existing stored mechanical energy, but that on triggering forces are generated that cause an increase in pressure and volume.
What are the arguments for the cyst matrix being acidic? (1) When the discharge is triggered, the surroundings become acidified. For cysts of acontia of Aiptasia, we estimated the internal concentration of protonated carboxyl groups to be about 5 M. A contribution of lysosomes to the observed acidification of the surroundings cannot be excluded, but may be ignored because the largest part of the acontia consists of cysts, whereas lysosomes are almost missing. (2) Treatments with AO and DAPI indicate that in the matrix conditions naturally exist that prevent Ca2+-ions to bind to the pG. It seems difficult to find conditions other than a low pH to explain this finding appropriately. (3) Treatments with AO, DAPI, and LysoSensor did not stain the matrix of cysts in natural state (in vivo). Controls showed that the probes can penetrate membranes and that cysts contain pG, which at neutral condition can accumulate the probes. In this case, too, it appears difficult to find conditions other than a low pH that could explain these results. We thus propose that cysts contain polyacids that are largely protonated. This fits our findings that CM-Sephadex enriches the LysoSensor at pH 4.0 but not at pH 3.0. (4) On the basis of a low matrix pH, it is possible to explain that on discharge the volume increases initially. At a low pH a large number of the carboxyl groups of the polyacids are protonated and therefore uncharged. Two uncharged carboxyl groups of compounds such as pG can combine each by forming rather stable hydrogen bonds, which causes the formation of aggregates. Apolar interactions between uncharged parts of the molecules further reduce the number of freely diffusible molecules in the cyst, and only such molecules or aggregates contribute to the osmotic pressure. Taking these observations together, we argue that at a low pH the contribution of the pG to the matrix osmotic pressure can be ignored. The osmotic pressure in a cyst is almost identical with that of the surrounding cytoplasm.
We speculate that anionic polymers are also present in partly dissociated form in lysosomes and in related vesicles, and serve there as a proton store or buffer. This may explain why a vital staining of cells of various animals with Acridin orange causes lysosomes to appear orange, whereas nuclei appear green (Stockinger 1964). It appears possible that nematocysts have evolved from such vesicles.
Most of these findings are difficult to explain on the basis of the current view that the internal pressure exceeds 100 bar. With the first pG to be synthesized in the matrix, at neutral pH the pressure exceeds that of the surrounding cytoplasm. This increased pressure should prevent indentations in the wall, a bending during migration and a reduction of volume as a final step of development. Furthermore, one has to explain why an accidental explosion does not occur. In our view cnidarians apply an improved mechanism: the acidification of a subcellular compartment.
In a ready-to-discharge cyst the pH of the cyst matrix is well below the pH of the cytoplasm of the host cell (Fig. 3). Thus a large number of the carboxyl groups of the polyacids are protonated and therefore uncharged. The osmotic pressure may reach that of the surrounding cytoplasm. Discharge is suggested to start when the membrane can no longer maintain the high internal proton concentration. The leakage of some protons causes (1) an acidification of the surroundings, (2) a change of the membrane potential, and (3) an increased number of dissociated carboxyl groups in the interior of the cyst. Both—an increased proton concentration at the outer surface and an altered membrane potential—may somehow facilitate a further leakage of protons. However, there are several observations that isolated cysts did not discharge when a current was applied or when treated with diluted acids or a concentrated NaCl solution (Will 1914, after Kühn 1916). It seems these treatments normally act by causing depolarization of the cell membrane, which initiates the loss of protons at the top of the cyst, which in turn results in the opening of the operculum. If the loss starts too slow or at a different site, the operculum may not open properly or even not at all.
At pH 3, the internal proton concentration would be 10,000 times higher than that of the surroundings. This difference is the driving force of discharge. The movement of protons across the membrane is a rapid process. Protons from the interior of the cyst compensate extremely fast for the loss close to the inner surface of the membrane. In fact, the speed of protons in water is much faster than that of any other cations. This is because in water protons do not simply spread by diffusion but mainly through a shift of charge in chains of water molecules. At acidic conditions polyglutamic acid molecules combine via hydrogen of their protonated carboxyl groups. These groups are therewith close to each other. Because of the loss of protons, the groups dissociate and both aquire a negative charge. This results in an electrostatic repulsion of the pG molecules, which in turn causes an increase of pressure on the capsular wall and an increase in the capsule volume (Fig. 3). The loss of protons in the cyst’s interior and its compensation by dissociation of carboxyl groups is so fast that initially this loss of positive charge is not compensated for by an equivalent uptake of potassium or other cations. We suggest this extremely fast (about 50 μsec, Holstein and Tardent 1984) volume increase to have features of a so-called Coulomb explosion. We therefore suggest the initial volume increase is not caused by ion and water uptake (this process is much too slow) and thus not by an increased osmotic pressure. In fact, an increased pressure from electrostatic repulsion would cause water to leave the cyst. Thus, in several types of cysts only a sudden pressure increase may be able to cause discharge. If the proton concentration equilibrates only slowly, the loss of water may be quick enough to obviate an increase in cyst volume (see next).
The second step of discharge is caused by the uptake of inorganic cations and water, resulting in an increase of the osmotic pressure and/or cyst volume. The uptake of these two components is much slower than the loss of protons. In cysts that do not discharge very fast, the loss of protons may take too long a time to cause a volume increase. In this case discharge is not caused by electrostatic repulsion but rather by an increasing osmotic pressure. Both the first and the second step together cause a volume increase that is well known to people working with ion exchangers based on carboxyl groups, such as CM-Sephadex C-50: The bead volume almost doubles when the pH is changed from 3 to 6 at constant ionic strength.
We consider the evagination of the tubule not only to be the result of an increased internal pressure but also to include a conformational change of wall components, driven by the altered pH. Such a change was reported to take place at the outer surface (the former interior) of tubules of discharged cysts: strings in form of spirals (“Quellspiralen”) were found to swell on discharge (Will 1914, after Kühn 1916). In addition, several tubules are decorated with rows of barbed spines that are packed tightly before discharge and extend in the surroundings after discharge. Their unfolding may be facilitated by the pH increase. In Anthozoa some nematocysts were found to have a thin wall and a matrix that could not be stained (Pax 1914). For these nematocysts we hypothesize that the concentration of polyanions is low and that the evagination of the tubule is largely driven by conformational changes of wall components. Thus the speed of discharge should be low. In fact, these nematocysts do not kill a prey but, rather, glue the anthozoan specimen to a substrate.
In summary we suggest that three driving forces are involved in the discharge of nematocysts, all resulting from a loss of protons: electrostatic repulsion, generation of osmotic pressure, and conformational change at the inner tubule’s surface. The contribution of these different forces, however, may vary depending on the type of cyst.
Our view of nematocyst formation and discharge may help to explain the occurrence of the so-called kleptocnides, that is, nematocysts produced by cnidarians but exposed closely to the surface of noncnidarians that feed on cnidarians. In certain ciliates, ctenophores, plathelminthes, and mollusks these cysts have been described as functional (for review see Kühn 1916; Bouillon 1993). We suggest that cysts that are fully developed but not yet ready to discharge are incorporated. A supply of ATP may be sufficient to cause the final acidification of the cysts that renders them functional.
We thank W. Weinhold and G. Firmenich for growing the various species used in the experiments.
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