Abstract and Keywords
Two dichotomies exist within the swim systems of jellyfish—one centered on the mechanics of locomotion and the other on phylogenetic differences in nervous system organization. For example, medusae with prolate body forms use a jet propulsion mechanism, whereas medusae with oblate body forms use a drag-based marginal rowing mechanism. Independent of this dichotomy, the nervous systems of hydromedusae are very different from those of scyphomedusae and cubomedusae. In hydromedusae, marginal nerve rings contain parallel networks of neurons that include the pacemaker network for the control of swim contractions. Sensory structures are similarly distributed around the margin. In scyphomedusae and cubomedusae, the swim pacemakers are restricted to marginal integration centers called rhopalia. These ganglionlike structures house specialized sensory organs. The swim system adaptations of these three classes (Hydrozoa, Scyphozoa, and Cubozoa), which are constrained by phylogenetics, still adhere to the biomechanical efficiencies of the prolate/oblate dichotomy. This speaks to the adaptational abilities of the cnidarian nervous system as specialized in the medusoid forms.
Biomechanics of Swimming in Medusae
The mechanics of jellyfish swimming have been investigated in representative species from all three classes with medusoid members. From these studies, a significant dichotomy emerged that was based on medusoid bell structure, but was independent of phylogenetic grouping. In general, prolate medusae are characterized by swimming bells that are taller than they are wide (Figures 1A, D), while oblate forms have bells that are wider then they are tall (Figures 1B, C).
Kinematic and vortex analyses show that swimming performance is related to bell streamlining and velar aperture development (Colin & Costello, 2002). Prolate medusae with well-developed velums use a jet propulsion–type swimming mechanism that forms well-developed vortices with each swim contraction (Colin & Costello, 2002; Dabiri, Colin, & Costello, 2006). The primary vortices are fast moving, and secondary vortices of opposite signs remain trapped in the subumbrella (Lipinski & Mohseni, 2009).
Oblate medusa, which do not have well-developed velums, do not produce well-defined jets. Rather, they produce vortices at the bell margin in a form of swimming referred to as drag-based rowing (Colin & Costello, 2002; Lipinski & Mohseni, 2009; Sahin, Mohseni, & Colin, 2009). As a comparison, the vortices of oblate forms remain in the region of marginal tentacles 10 times longer than those of prolate medusae (Lipinski & Mohseni, 2009). Jet propulsion is well suited for rapid swimming, but it is more energetically costly than rowing locomotion (Sahin et al., 2009). For this reason, jet propulsion is size limiting: prolate medusae are comparatively small, while oblate medusa can achieve a large size because rowing locomotion remains efficient even at large bell diameters (Costello, Colin, & Dabiri, 2008). With this predictive relationship, cubomedusae represent a confounding situation. Cubomedusae generally are described as prolate medusae that use jet propulsion, and yet some can reach a large size that defies predictions based on the efficiency of jet propulsion (Colin, Costello, Katija, Seymour, & Kiefer, 2013). Investigation of swim mechanics in two species of cubomedusae revealed that they use jet propulsion when they are small but switch to a rowing-jetting hybrid when larger (Colin et al., 2013).
The marginal rowing mechanism observed in oblate forms highlights a close link between swimming and feeding as the slow-moving toroid vortices occur in the region of marginal and oral tentacles (Costello & Colin, 1994, 1995; Dabiri, Colin, & Costello, 2005). This has led to a similar correlation between swim mechanics and predation style, as the slower-swimming oblate forms appear as cruising predators, while fast-swimming prolate forms are ambush predators (Costello et al., 2008). Equally interesting is the observation that the foraging style of oblate forms is not restricted by phylogenetic grouping because representatives of both hydromedusae and scyphomedusae show this close association between swimming and feeding.
This raises interesting questions about selective pressures that affected swimming mechanics, foraging behavior, and nervous system organization, particularly in light of the significant differences in the nervous system organization described in this article for hydromedusae, scyphomedusae, and cubomedusae.
The Fundamental Experiments of G. J. Romanes
Independent of the biomechanical dichotomy associated with the medusan bell shape, an additional dichotomy was found regarding the neuronal organization of the swim systems, in what the biologist George J. Romanes called the naked-eyed medusae (hydromedusae) and the covered-eyed medusae (scyphomedusae).
Romanes (1885) used cutting experiments to localize the neuronal tissue responsible for initiating contractions in the subumbrellar musculature. In the covered-eyed medusae (scyphomedusae), discrete sensory structures were evenly spaced around the margin of the bell. Most medusae had eight, but some species had more (the number was usually a multiple of four). We now refer to these structures as rhopalia. Removal of rhopalia without damaging any marginal tissue around them left the medusa motionless. Leaving a single rhopalium was sufficient for subumbrellar contractions to continue, but they lacked the regularity of a fully intact medusa.
Romanes also examined the nature of the subumbrellar conducting system responsible for activating the swim musculature in scyphomedusae. By using a series of interdigitating cuts, he provided evidence for a diffuse, nerve net–like character of the peripheral nervous system (Figure 2). Finally, he provided evidence for two independent diffuse nerve nets: one that is conducted around the bell without significant muscular contraction, but with marginal tentacle withdrawal; and one with contraction of the subumbrellar swim musculature. The two interact at the rhopalia, with the former capable of initiating a contraction in the latter.
In the naked-eyed medusae (hydromedusae), distinct rhopalia are lacking. Romanes found that the entire margin had to be removed to paralyze the medusae. Only a small portion of the margin had to be left intact to allow subumbrellar contractions. From this, he concluded that the structures necessary for initiation swim contractions are distributed throughout the margin rather than being localized in discrete neuronal-sensory structures. Cutting experiments in the subumbrellar had less clear results, and evidence for two distinct subumbrellar nerve nets was lacking.
Romanes used a variety of naked-eyed medusae (hydromedusae) in his experiments, including both prolate and oblate forms. The naked-eyed medusae (scyphomedusae) that he used were oblate. The class Hydrozoa includes medusae with varied bell shapes, ranging from extremely prolate to extremely oblate, while the class Scyphozoa includes primarily oblate forms. The class Cubozoa, which fit into Romanes’s covered-eyed medusae classification and was initially considered a group within the Scyphozoa (Hyman, 1940), has bells in which the height and width are approximately equal, thus fitting best into the prolate category.
Neurobiology and the Romanes Dichotomy
Following decades of research on medusoid neurobiology, Romanes’s work still provides a fundamental distinction between the hydromedusae and the scyphozoan/cubozoan assemblage. Comparative work on numerous species of the three groups allows us to describe basic components of the nervous systems of each of the three groups (classes), and then to highlight species-specific differences that are superimposed onto these basic systems. Each of the three groups will be discussed in this article in general terms and in some cases, also with descriptions of key species that have been used to describe the neuronal organization of their swim systems.
Swimming and Associated Behaviors
Hydromedusae have representatives of both prolate and oblate forms. In both types, swimming involves coordinated contraction of sheets of circular, striated muscle that lines the inside of the bell (subumbrella). The efficiency of swimming is aided by a velum—a ring of contractile tissue that projects at a near-right angle to the subumbrellar walls and narrows the opening of the bell for more efficient propulsion (Figure 3). As noted in the biomechanical studies, the velum is very effective in aiding water jet formation in prolate forms, but relatively ineffective in doing so in oblate forms. The velum has circular, striated muscle on the subumbrellar side, which contracts with the rest of the swim musculature, and radial muscle on the exumbrellar side, which can deform the velum for directional jet formation and turning.
Two other behavioral reactions affect swimming, and while they are similar for all hydromedusae, they show species-specific differences in the details of their neuronal control. Feeding typically involves the transfer of prey from tentacles to the manubrium. Because all species vary in tentacular anatomy, the responses will be different, but all involve regional rather than global reactions of the tentacles and bell. On the other extreme, a protective reaction, called crumpling, involves a global contraction of tentacles and an inward curling of the margin of the bell (Mackie & Singla, 1975; Spencer, 1975, 1978; Singla, 1978b; Mackie, 2004b; Satterlie, 2002, 2008, 2011). Crumpling typically is triggered by injurious stimuli to any parts of the animal. The impact of feeding reactions on the swim system (inhibition or excitation) is species-specific, whereas crumpling always inhibits swimming.
Responses to different types of sensory input vary between species and depend on the unique sensory armament of each species. For example, a variety of statocystlike structures have been described from hydrozoan species (Singla, 1975), and similarly, variations in the presence or absence of eyelike structures have been found (Singla, 1974).
Common Elements of the Swim Systems
In 1977, intracellular recordings were made from oversized neurons in the inner nerve ring of Polyorchis penicillatus, a prolate hydromedusa (Anderson & Mackie, 1977). Subsequent recordings demonstrated that these neurons comprise an electrically coupled network in the inner nerve ring that activates the swim musculature (Anderson & Mackie, 1977; Singla, 1978b; Spencer & Satterlie, 1980; Spencer, 1981; Satterlie & Spencer, 1983; Satterlie, 1985a, 1985b; Meech & Mackie, 1995; Lin, Gallin, & Spencer, 2001; Figure 4). In addition, the network functions as a pacemaker network for swim contractions (recalling Romanes’s conclusions about the distribution of pacemakers in hydromedusae). Intracellular injections of Lucifer Yellow through a recording electrode revealed that the neurons were not only electrically coupled, but also dye-coupled (Spencer & Satterlie, 1980; Figure 4A). This network performs two functions: that of pacemaker cells and of motor neurons for swim contractions.
Later, recordings were made from a similar network in Aequorea victoria, an oblate hydromedusa; this network also functioned as the swim pacemaker and as motor neurons to the swim musculature (Satterlie, 1985b; Figure 5). A subsequent comparative study of 14 hydromedusan species from several different orders suggested that this network of oversized, electrically coupled, and dye-coupled neurons in the inner nerve ring is a common feature of hydromedusan swim systems, and that the presence of this network is independent of bell shape, present in both prolate and oblate species (Satterlie & Spencer, 1983).
An additional common feature emerged from these comparative investigations. There is widespread electrical and dye coupling throughout circular muscle sheets of the subumbrella and the velum (Mackie & Singla, 1975; Keough & Summers, 1976; Singla, 1978a, 1978b; Spencer, 1979; Anderson, 1980; Satterlie, 1985a, 1985b, 2008; Satterlie & Spencer, 1983; Kerfoot, Mackie, Meech, Roberts, & Singla, 1985; Figure 6). This includes nonmuscular epithelial cells overlying the inner nerve ring, so there is electrical continuity from the velum to the subumbrella. Electrical recordings demonstrated that the epithelial cells were postsynaptic to the identified neuronal network in the inner nerve ring, such that synaptic potentials triggering long duration action potentials were recorded from the epithelial cells (Spencer, 1982; Satterlie, 1985a). Ultrastructural and electrophysiological work showed that these connections are via chemical synaptic transmission. Once initiated, the action potentials spread throughout the subumbrella and velum via the gap junctions, aided in some species by subumbrellar nerve nets. The long-duration action potentials in the epithelial and muscle cells are reflected in long-duration contractions in the swim musculature (Spencer, 1979; Satterlie, 1985a). The action potentials resemble those of another fluid pump, the vertebrate heart. This led to the conclusion that if a fluid pump is attached, it will move the fluid. If the fluid pump is not attached, it will move through the fluid.
One additional common property is related to the feeding and crumpling behaviors of hydromedusae (Mackie & Singla, 1975; Spencer, 1975, 1978; Singla, 1978b; King & Spencer, 1981; Mackie, 2004b; Satterlie, 2002, 2008, 2011). Both responses utilize the activation of subumbrellar radial muscle, although the organization of that radial muscle is species-specific, or at least specific for the two forms of bell structure. This will be addressed later in this article, when discussing individual species.
The common features of hydromedusae include an electrically coupled and dye-coupled network of oversized neurons in the inner nerve ring that function as the pacemakers and motor neurons for the swim system; widespread electrical coupling within the subumbrella tissue, including the circular muscle of the subumbrella and velum and the nonmuscular epithelial cells overlying the nerve ring; and use of the radial muscle to produce feeding and crumpling reactions of the bell. All these features are found in both prolate and oblate species.
Prolate Specializations: The Polyorchis Story
As with other hydromedusae, swim contractions are initiated by a network of electrically coupled neurons in the inner nerve ring (Anderson & Mackie, 1977; Anderson, 1979; Spencer & Satterlie, 1980; Satterlie & Spencer, 1983; Satterlie, 1985b; also see Figure 4). In Polyorchis, this motor network extends up each of the four radii and across the top of each muscle quadrant to surround the muscle sheets (Lin et al., 2001). Each contraction is preceded by a single action potential in this swim network. As noted previously, an action potential in the neurons of the inner nerve ring synaptically activates an action potential in the overlying epithelial cells, which then spreads throughout the subumbrellar muscle sheets and velum (Spencer, 1981, 1982). Presumably, similar synaptic activation occurs through the periphery of each muscle quadrant. The sheet of striated muscle cells in each quadrant is aneural, so spread of an action potential takes place via gap junctions (Spencer, 1978; also see Figure 6). This myoid conduction is relatively slow, so both radial and circular coordination of the four muscle quadrants depend on the faster conduction velocity of the neural network.
Circular coordination of the swim contraction has been well studied in Polyorchis, with a particular focus on conduction in the motor network of the inner nerve ring. Spencer (1981) noted that the action potential duration decreased as it was conducted around the bell from the site of initiation. This is translated as differences in synaptic transmission, and particularly synaptic delays in production of the muscle action potentials (Spencer, 1982). Because synaptic activation at any point depends on multiple inputs from the motor network, synchrony of activation of the neurons in the region influences the neuronal action potential. In the areas distant from the site of action potential initiation, the firing of neurons is more synchronous than in the initiation region, thus producing an action potential of shorter duration than in the former region (Spencer, 1981). This greater synchrony produces larger synaptic potentials and shorter latencies for both the synaptic potentials and for muscle action potential production. The shorter latencies that occur with larger distances from the initiation site promote great synchrony of contraction throughout the bell that partially compensates for conduction time through the motor network (Spencer, 1982).
Crumpling behavior in Polyorchis is accomplished by the contraction of four smooth muscle strips that run from the margin to the manubrium in each of the radii (Spencer, 1978). Their contraction pulls the bell margin upward and inward, and it is associated with inhibition of the motor network, as recorded in the inner nerve ring. This means that at least two separate, parallel conducting systems are localized to the radii of Polyorchis. This organization, compressed nerve nets to form nervelike pathways, represents a simple form of centralization in cnidarian nervous systems. Similarly, multiple, parallel conducting systems in these nervelike pathways add to the concept of cnidarian nervous centralization.
The swim network of Polylorchis is modulated by photic inputs that originate in two separate networks in the outer nerve ring (Spencer & Arkett, 1984; Arkett, 1985; Arkett & Spencer, 1986a, 1986b). The B system is comprised of electrically coupled neurons that are connected to ocelli found at the tentacle bases. During light conditions, the B system produces regular action potential activity. At light-off, a burst of action potentials produces contraction of the tentacles and of the subumbrellar swim muscle. The O system is directly photosensitive and nonspiking, exhibiting membrane potential oscillations when illuminated. At light-off, the system hyperpolarizes and the oscillations cease.
The inner and outer nerve rings contain multiple, parallel conducting systems, with the former including the motor networks for swimming and crumpling and the latter including sensory networks (Spencer & Arkett, 1984). Each hydromedusan species has unique sensory capabilities, highlighted by the variety of photoreceptors (Singla, 1974) and the variety of statocystlike structures (Singla, 1975) found in different medusae. The compression of multiple, parallel conducting system into the two nerve rings, as well as their interconnections, represent the height of neuronal concentration in hydromedusae and the centralized nervous system of the group.
Oblate Specializations: The Aequorea Story
The swim network of Aequorea is unique in that it involves firing a burst of action potentials for each individual swim contraction (Satterlie, 1985b; also see Figure 5). This burst produces a burst of summing synaptic potentials in the overlying epithelial cells (Satterlie, 1985a). As with Polyorchis, the epithelial cells are electrically coupled and dye-coupled with circular muscle cells of the subumbrella and the velum (Figure 6). Several differences are noted in the subumbrellar organization of Aequorea.
The subumbrella is divided into numerous wedge-shaped muscle sheets by radii that include a radial canal and gonad. In addition, each wedge contains more than circular muscle. The subumbrellar epithelium includes a sheet of radially oriented epitheliomuscular cells that lie immediately over the sheet of circular muscle cells (Satterlie, 1985a, 2008). The radial muscle of each wedge contracts during a crumple response. All circular muscle cells are electrically coupled, as in Polyorchis, while the radial muscle cells form a separate, electrically coupled muscle sheet (Figure 6).
Rather than being aneural, the subumbrella of Aequorea has two distinct nerve nets—one associated with the circular swim muscle and the other with the radial muscle sheet (Satterlie, 2008; also see Figure 7). A conducted contraction in the subumbrella thus requires synaptic input from the swim network in the inner nerve ring, input from the subumbrellar nerve net, and electrical coupling between muscle cells. Similarly, the radial muscle contraction requires initiation from the nerve rings, input from its nerve net, and electrical coupling within the muscle sheet.
The oblate bell shape of Aequorea, the arrangement of muscle sheets in many segments, and the organization of radial muscle allow localized radial contractions for feeding purposes, as well as the widespread contractions that occur during a crumple response (Satterlie, 2008). Feeding responses are accompanied by an equally localized inhibition of burst activity in the motor network via hyperpolarizing input that decreases or delays the action potentials in a burst. A more significant hyperpolarization, as well as total inhibition, occur during crumpling.
Aequorea do not have ocelli, and a photic response has not been demonstrated. They do have multiple statocysts distributed around the bell margin, however, suggesting an effective righting response.
It is tempting to speculate on the prolate-oblate dichotomy in the case of the mechanism of activation of swim musculature, with aneural muscle sheets in prolate forms and oblate forms that have subumbrellar nerve nets. Three additional oblate species, Phialidium hemisphericum, Eutonina indicans, and Mitrocomella polydiademata, all have subumbrellar nerve nets (Satterlie & Spencer, 1983). However, all these species are in the order Leptomedusae, and further study of oblate species of the other orders (Anthomedusae, Limnomeduase, Narcomedusae, and Trachymedusae) is needed, as is an analysis of representative prolate species. Also, at least one prolate species has neuronal processes in the subumbrella (see Aglantha, discussed next), but this is a special arrangement, as the processes are neurons that are electrically coupled to giant neurons that run in the radii, so they do not represent a synaptic nerve net (Mackie, 2004a).
A Special Case: Escape Swimming and Giant Neurons in Aglantha
Aglantha digitale is a small, prolate medusa with a unique response to sudden, strong mechanical stimulation. They produce a ballistic swim contraction of the subumbrellar muscle that rapidly propels the medusa away from the stimulus (Donaldson, Mackie, & Roberts, 1980; Roberts & Mackie, 1980). Aglantha thus have two forms of swimming that use the same subumbrellar muscle.
Slow (normal) swimming contractions comply with the generalized structures of hydromedusan swim systems (Mackie, 2004a). An electrically coupled network of neurons in the inner nerve ring acts as the pacemaker and motor neuron for swim contractions. In addition, however, giant neurons with a radial orientation are found in each of the eight radii (called radial giants; Mackie, 2004b; Figure 8). These neurons also conduct motor impulses to the swim muscle during normal swimming in a unique way, described later in this article. In addition to the large-diameter radial process, numerous fine processes extend from neurons that are electrically coupled to the radial giants and run across the muscle sheets in a circular direction. Transmission from radial giants and the coupled neurons to muscle cells takes place via chemical synapses. This is critical because the electrical coupling between muscle cells of the subumbrellar sheets is not strong enough to allow myoid spread of the muscle activation. Also, there is no motor nerve net (MNN) in these subumbrellar regions. The radial giants and their electrically coupled neurons are thus essential for the spreading of the contraction during slow swimming (Singla, 1978a; Weber, Singla, & Kerfoot, 1982; Mackie, 2004b).
Appropriate stimulation of mechanoreceptive bristle pads (tactile combs) at the bases of the tentacles (Arkett & Mackie, 1988) activates another giant neuron that runs around the margin of the animal in the outer nerve ring (called the ring giant; Mackie, 2004b). This cell is electrically coupled to a giant neuron in each of the tentacles. The ring giant also synaptically activates the eight radial giants in the subumbrella, which then produce a forceful contraction of the subumbrellar muscle and a ballistic escape response (Meech & Mackie, 1995). The connection from the ring giant to the radial giants is polysynaptic, suggesting the intervention of an additional system, called the carrier system. This system also mediates the connection from the ring giant to the giant neurons of the tentacles (Mackie, 2004b).
An important question centers on how the radial giants can be involved in both normal and escape swim contractions. The answer is unique and surprising. The radial giants can produce two types of propagated action potentials: a low-threshold calcium spike and a high-threshold sodium spike (Mackie & Meech, 1985). During slow swimming, the calcium spikes are involved in activating the swim musculature and produce relatively weak subumbrellar contractions. The calcium spikes have slower rise times and lower peak voltages than the sodium spikes (Meech & Mackie, 1993a, 1993b). This system uses the swim network of the inner nerve ring, which also synaptically activates muscle sheets of the subumbrella and velum.
Each escape swim contraction can propel the animal five times as far as a single contraction of normal swimming, and the greater contractions are initiated by propagated sodium spikes in the radial giants. The sodium spikes provide greater excitation to the swim musculature, and with a shorter latency, to produce the stronger contractions.
Mechanical stimulation from within the bell does not activate the ring giant, but it still can produce an escape swim. In this case, coordination of the radial giants occurs via a system of rootlet interneurons, which are electrically coupled with the radial giants (Mackie, 2004a). Rootlet interneurons activate each other via chemical synapses, and their location around the bell margin allows activation of the entire system or radial giants to produce the escape swim. The normal pacemaker network for slow swimming produces subthreshold synaptic potentials in rootlet interneurons; however, action potentials in the rootlet interneurons produce 1:1 action potentials in the pacemaker network. In this way, the pacemaker network is also activated during escape swimming.
Overall, 13 conducting systems have been described in the nerve rings and tentacles of Aglantha. This complexity further argues for the concept of a centralized nervous system in hydromedusae and speaks for the integrative capabilities of this nervous organization.
Scyphomedusae: Common Features of Swim Control in Oblate Medusae
As noted by Romanes (1885), the location of pacemakers and the method of muscle activation are very different in scyphomedusae than in hydromedusae. Perhaps the most distinct feature of the scyphozoan swim system is the rhopalium (Figure 9A). These sensory/neural structures house the pacemakers for swim contractions, but they also represent integration centers for rhopalial and extrarhopalial sensory structures/systems (Passano, 1965; Satterlie, 1979; Satterlie & Spencer, 1979). In this way, they can be considered the cnidarian version of ganglia. As noted by Romanes, removal of the rhopalia stops swim contractions.
Each rhopalium includes one or more pigmented ocelli, a statolith, and ciliated sensory cells (Hyman, 1940; Horridge, 1956a; Yamasu & Yoshida, 1973; Hundgen & Biela, 1982; Nakanishi, Hartenstein, & Jacobs, 2009; Satterlie & Eichinger, 2014). Outgoing fibers join with a subumbrellar nerve net that activates the swim musculature (the MNN, formerly called the giant fiber nerve net), while incoming fibers from a second nerve net, the diffuse nerve net (DNN), are capable of modulating pacemaker activity and muscle contractility (Figures 9B, C).
The two primary properties of scyphozoan nerve nets help explain the conducting properties originally described by Romanes. The networks allow diffuse conduction that can survive a variety of interdigitating cuts. The morphological organization of neurons in the nerve net demonstrated the diffuse nature of this neuronal organization (Shafer, 1878; Horridge, 1954a, 1954b). In addition, conduction is nonpolarized—the initiation site for an excitation wave can be variable, and the resultant action potential will pass through the nerve net in any direction.
Horridge (1954b) first demonstrated a critical property of individual neurons with regard to the nonpolarized nature of the nerve nets. By dissecting a smaller and smaller bridge within the subumbrella of Aurelia, he was able to produce a bridge that contained a single neuron (visible with substage illumination). He found that the neuron could conduct a contraction wave from one side of the cut to the other, in either direction. That meant that communication between this neuron and other neurons in the intact tissue pieces had to be bidirectional. Subsequently, neurons of the MNN were found to produce individual action potentials that, in turn, activate other neurons, as well as contractions of the circular swim muscle, via chemical synapses (Patton & Passano, 1972; Passano, 1973; Schwab & Anderson, 1980, 1981; Anderson & Schwab, 1981, 1982, 1983, 1984; Anderson & Greenberg, 2001).
Neuroneuronal synapses in this network are symmetrical and are able to transmit synaptic excitation in either direction (Horridge & Mackay, 1962; Horridge, Chapman, & MacKay, 1962; Westfall, 1973, 1996; Anderson & Schwab, 1981; Anderson, 1985; Anderson & Grunert, 1988; Anderson & Trapido-Rosenthal, 2009; also see Figure 10). In this way, neurons communicating by symmetrical chemical synapses can achieve the same diffuse conduction as electrically coupled neurons or muscle cells. Individual neurons of the MNN are not electrically coupled or dye-coupled to one another (Anderson & Schwab, 1981). Similarly, electrical connections have not been found between muscle cells of scyphozoans. To date, gap junctions and gap junction proteins have not been found in any scyphozoans—a clear and basic distinction between scyphozoans and hydrozoans (Mackie, Anderson, & Singla, 1984).
The second subumbrellar nerve net, the DNN, is similarly diffuse and nonpolarized (Figure 9C). It conveys sensory information from the periphery to the rhopaliba, but it also can, in some species, modulate swim muscle contractions (Horridge, 1956a; Passano, 1965, 1982, 2004; Satterlie & Eichinger, 2014). This separation of MNN and DNN is supported by different immunohistochemical properties, as the MNN is labeled by antitubulin antibodies and the DNN is labeled with anti-RFamide antibodies (Satterlie & Eichinger, 2014; also see Figures 9B, C). Immunoreactive networks of both types innervate the tentacles and manubrium as well. In the tentacles, the tubulin-immunoreactive fibers are associated with the tentacular musculature, while the RFamide-immunoreactive network includes epithelial sensory cells.
The number of rhopalia in each species differs, with a minimum of eight. In species with larger numbers, the total number is typically in multiples of four (reflecting the body symmetry). A swim contraction can be initiated in any one of the rhopalia, and the activated wave of excitation is believed to reset the other pacemakers (Horridge, 1959; Lerner, Mellen, Waldron, & Factor, 1971). In this way, the rhopalium with the fastest rhythm drives swimming until its rate drops and another rhopalium takes over. Horridge and others examined this apparent pacemaker redundancy and found that each rhopalium had an inherent rhythm that was irregular. In both cutting and modeling experiments, additional pacemakers each contributed to the overall output of the swim systems in two important ways. They produced greater regularity in the overall swim system activity, and the overall rhythm was faster (Horridge, 1959; Lerner et al., 1971).
These two contributions are critical in terms of the properties of the neuromuscular system in scyphomedusae. Neuromuscular transmission occurs via chemical synapses (Westfall, 1973). Furthermore, the contractile activity of the muscles is based on frequency-dependent facilitation (Bullock, 1943; Pantin & Vianna Dias, 1952; Horridge, 1953, 1954b). In this system, the amplitude of muscle contractions depends on the interpulse intervals of the previous contractions. The efficiency of swim contractions thus depends on the number of rhopalia in the network. Reduction of the rhopalial number, either through damage or experimental excision, also reduces the overall rate and regularity of swimming, and therefore its facilitation-based efficiency. Because swimming and feeding are interrelated in scyphomedusae, changes in swimming efficiency can affect feeding efficiency as well.
Species-specific differences in scyphomedusae include the arrangement of the swim musculature and in the organization of marginal and oral tentacles. In Aurelia aurita, the subumbrellar muscle forms an uninterrupted circular sheet, while in Cynea capillata, circular muscle is interrupted by bands of radial muscle (both cocontract during swimming). In both cases, the MNN and DNN are similar in organization. The presence of marginal tentacles and the arrangement of oral tentacles are extremely variable and likely affect swim and feeding mechanics is species-specific ways.
Cubomedusae: Strong Swimmers Built on the Scyphomedusan Plan
Cubozoans were originally classified as an order within the Scyphozoa, but unique features of their development, their body plan, and their neuromuscular organization warranted the establishment of a new class—Cubozoa (Werner, Cutress, & Studebaker, 1971; Werner, Chapman, & Cutress, 1976). This development has been supported by subsequent phylogenetic analyses (Collins, 2002, 2009; Marques & Collins, 2004; Bentlage et al., 2009). Yet in terms of the Romanes dichotomy, they are clearly within the covered-eyed medusae category.
Cubomedusae are strong swimmers, so they can escape dominance by water movements like currents, tides, and waves (Hamner, Jones, & Hamner, 1995; Shorten et al., 2005). While they are members of the pelagic community, they are not planktonic. They can steer accurately, turn 90 degrees in one or two swim contractions, and avoid obstacles (Garm et al., 2007a; Garm, O’Connor, Parkefelt, & Nilsson, 2007b; Petie, Garm, & Nilsson, 2011). The structure and optics of their lensed eyes are unparalleled in the phylum (Berger, 1898; Martin, 2004; Garm et al., 2007a; O’Connor, Garm, & Nilsson, 2009).
The swim mechanics of Cubomedusae are more like those of prolate medusae than oblate medusae, but they are able to achieve a significant size through a hybrid mechanism of propulsion (Colin et al., 2013; see also Gladfelter, 1973; Shorten et al., 2005). Feeding responses include longitudinal contraction of the stimulated tentacle; inward bending of the pedalium, which attaches the tentacle to the bell; and a directional movement of the manubrium toward the prey-bearing tentacle (Larson, 1976). A protective crumple response involves similar contraction and inward bending of all four tentacles, as well as inhibition of swimming.
The cubomedusan nervous system is built on the same plan as scyphomedusae, with some modifications and some advances. Swim pacemakers are located in four rhopalia, each positioned near the margin in a perradial, exumbrellar position (Berger, 1898; Satterlie, 1979; also see Figure 11). Removal of the rhopalia stops swim contractions, as in scyphomedusae. The rhopalia are sensory-neural structures with a significantly greater complexity than their scyphozoan counterparts. Each rhopalium has two lensed, image-forming eyes on the oral midline, two lateral spot ocelli, and two lateral slit ocelli (Figure 11). A secreted statolith is located at the end of the rhopalium. Neuronal tracts have been described that interconnect the eyes and ocelli and the pacemaker region (Skogh, Garm, Nilsson, & Ekstrom, 2006; Garm & Ekstrom, 2010). These tracts are directional, suggesting the presence of discrete neuronal pathways that are unlike the traditional nerve nets.
The eyes and ocelli influence the swim pacemakers in different ways and contribute to a versatile, visually guided locomotory system (Garm & Bielecki, 2008; Garm & Mori, 2009; Garm, Hedal, Majken, & Gurska, 2013). The lensed eyes are of the camera type, opsin based, but with fairly poor resolution (Martin, 2004; Nilsson, Coates, Gislen, Skogh, & Garm, 2005; Coates, Garm, Theobald, Thompson, & Nilsson, 2006; Garm et al., 2007a; O’Connor et al., 2009; Gray, Martin, & Satterlie, 2009). Based on electroretinograms, the lensed eyes have relatively slow response times (Garm et al., 2007a; O’Connor, Nilsson, & Garm, 2010).
The cubomedusan rhopalium is constructed like a typical invertebrate ganglion, with an outer layer or nerve cell bodies and a central neuropil (Satterlie, 2002; Parkefelt, Skogh, Nilsson, & Ekstrom, 2005; Skogh et al., 2006). Neural pathways extend from the retinal layer of the eye and ocelli and form discrete neuronal tracts that show a bilateral symmetry (Martin, 2002, 2004; Satterlie, 2002; Parkefelt et al., 2005; Skogh et al., 2006; Parkefelt & Ekstrom, 2009). In addition, compressed nerve nets are present, as exemplified by a ringlike network of RFamide-immunoreactive neurons that are found in the pacemaker region of the rhopalium (Martin, 2002, 2004; Satterlie, 2002; Plickert & Schneider, 2004; Skogh et al., 2006; Parkefelt & Ekstrom, 2009; Eichinger & Satterlie, 2014). This organization of discrete, directed neuropillar tracts intermixed with compressed networks represents the height of cnidarian centralization.
The rhopalia are connected to the subumbrellar conducting system via a rhopalial stalk, and paired neuronal tracts exit the stalk and join a subumbrellar nerve ring (Satterlie, 1979; Garm et al., 2006; Garm, Poussart, Parkefelt, Edstrom, & Nilsson, 2007c; Eichinger & Satterlie, 2014; Satterlie, 2014). The nerve ring connects the four rhopalia and the four tentacle bases (located at the interradial margin; see Figure 11). The nerve ring represents an advance over scyphomedusae and allows rapid communication between rhopalia. At least four conducting systems are found in the nerve ring, including elements of the swim system, a system conducting photic responses between rhopalia, a crumpling system that coordinates all four tentacles, and a local system for feeding reactions (Satterlie, 2014).
Neurons diverge from the nerve ring and form subumbrellar nerve nets that innervate the circular swim muscle (striated cells) (Satterlie, 1979; Laska & Hundgen, 1984; Eichinger & Satterlie, 2014; also see Figure 12). As in scyphomedusae, the neurons of the subumbrellar nerve net interact via symmetrical chemical synapses and use polarized synapses to activate the muscle cells (Satterlie, 1979). Electrical and dye coupling have not been found in the nerve net or between muscle cells of cubomedusae (Satterlie, 2011, 2015b). The subumbrellar nerve net is the equivalent of the MNN of scyphomedusae. Action potentials in MNN neurons are similar to those of scyphozoan neurons, and they trigger long-duration muscle action potentials in a 1:1 relationship (Satterlie & Spencer, 1979; Satterlie, 1979). Frequency-dependent facilitation produces muscle plasticity through variations in pacemaker frequency and regularity (Satterlie, 1979).
A velarium extends inward from the margin and functions like the velum of hydromedusae—it narrows the bell opening to enhance the forceful ejection of water from the subumbrella, but it also aids in turning via asymmetrical contraction and directional nozzle formation (Gladfelter, 1973; Shorten et al., 2005; Garm et al., 2007b; Petie et al., 2011). The velarium is considered analogous to, rather than homologous with, the hydromedusan velum. As with the velum, the velarium has circular, striated muscle that contracts with the subumbrellar muscle, but the latter lacks the exumbrellar radial muscle and must rely on a different mechanism for producing the asymmetrical contractions during turning (Satterlie, Thomas, & Gray, 2005). Neurons diverge from the nerve ring to innervate the velarium, as with the subumbrella (Eichinger & Satterlie, 2014; also see Figure 12).
Pacemaker redundancy was tested using rhopalial ablation, as well as network modeling (Satterlie & Nolen, 2001). As with scyphomedusae, each rhopalium in isolation had an irregular pacemaker output, and with the addition of pacemakers, the overall output of the swim system became more regular and the mean contraction frequency increased. The modeling experiments were unique, however. One tested model (the resetting model) included pacemakers that were linked with resetting connections, so that the active pacemaker reset all the others. Another model (the independent model) did not include any connections between the pacemakers. Evaluation of data from real animals and both models suggested that the animal data fell between the two (i.e., semi-independent) (Satterlie & Nolen, 2001). Since the rhopalial pacemakers receive several types of sensory inputs, some excitatory and some inhibitory, the semi-independent model suggests that while pacemaker interactions are resetting, some inputs can take a rhopalium out of the network temporarily or cause it to fire prior to receiving input from another active pacemaker.
A second subumbrellar conducting system, similar to the DNN of scyphomedusae, is missing in cubomedusae. Instead, a compressed network is found in the nerve ring, rhopalia, and tentacle bases that shows the same RFamide immunoreactivity as the scyphozoan DNN (Eichinger & Satterlie, 2014). In the rhopalia, immunoreactive neurons form a tight network in the pacemaker region that includes epithelial sensory cells that are similar to the touch pad of scyphomedusae (Satterlie, 2011; Eichinger & Satterlie, 2014). The cluster of immunoreactive neurons in the nerve ring area of the tentacle bases may be of similar origin as rhopalia, which develop from polyp tentacles.
Perradial strips of radial muscle (smooth type) run from just above the rhopalial-nerve ring junction to the manubrium (Satterlie et al., 2005; also see Figure 12). Two compressed networks of neurons are found in association with the radial muscle (Satterlie & Eichinger, 2014). These muscle strips contract to help pull the margin of the bell inward during either a single-tentacle feeding response or a coordinated crumple response. Cuts through the nerve ring destroy this tentacle coordination, suggesting that a crumple pathway runs in the nerve ring (Satterlie, 2014). Crumpling inhibits swimming as occurs in hydromedusae.
Cubomedusan advances (over scyphomedusae) include the elaborate rhopalia with lensed eyes and increased neural complexity. The rhopalia are the cnidarian version of ganglia. The DNN of scyphomedusae appears to be represented by a compressed network in the nerve ring that connects to well-developed networks of neurons in the rhopalia and tentacle bases.
Centralization in the Nervous Systems of Cnidarian Medusae and the Evolution of Multicellular Nervous Systems
Cnidarians are frequently referred to as nerve net animals; however, the classical nerve net does not represent the centralized portions of their nervous systems (Garm, Ekstrom, Boudes, & Nilsson, 2006; Satterlie, 2011). The primary characteristic of the cnidarian centralized nervous system is a coaggregation of sensory and neuronal elements around the margins of the bells. Condensation of neuronal conducting systems allows rapid integration of sensory information with the output distributed via nerve nets or nervelike compressed networks. In hydromedusae, the inner and outer nerve rings together make up the centralized nervous system. Multiple, compressed conducting systems form a circumferentially distributed ring that functions like a ganglion or ring of ganglia.
In scyphomedusae, the rhopalia represent a very different form of centralization, with a concentration of nervous tissue in association with several types of sensory cells. This system of discrete bodies has multiple repeats spaced around the bell margin. Because radial symmetry does not provide a body arrangement with a region that predominately leads during locomotion, or a region that receives a majority of sensory input, the multiple rhopalia are distributed in a way that is responsive to sensory fields throughout 360 degrees and activates muscle sheets that are also distributed through 360 degrees (Satterlie, 2011).
The scyphozoan plan is elaborated in cubomedusae to include fast pathways between rhopalia and tentacles via the nerve ring. Rhopalial elaboration follows the extreme development of sensory structures, including the lensed eyes. These developments are associated with directed, agile, and rapid locomotory responsiveness, as well as a significant dependence on vision for locomotory adjustments.
Each of the three groups (hydromedusae, scyphomedusae, and cubomedusae) shows some degree of centralization in neuronal systems, including compressed nerve nets to form nervelike pathways, multiple conducting systems compressed into nerve rings, and ganglionlike rhopalia with their associated sensory structures (Satterlie, 2002, 2011). Nerve nets make up the most noticeable but least integrative parts of medusan nervous systems. However, they are wonderfully suited for the specific task of conducting excitation throughout flat, two-dimensional muscle sheets in which excitation can come from a number of sites and in which conduction of information is nonpolarized. The nerve net organization may be more a result of the demands of coordinating widespread muscle sheets in a radially symmetrical animal than a simple primitive neuronal condition (Satterlie, 2015a).
Two types of suspected evolutionary convergence are present in cnidarian medusae. One is centered on body form and swim mechanics and is not limited by the second, phylogenetic differences in the organization of swim control systems. The interesting tie between foraging method and limitations in body form, based on swim mechanics, presents an interesting adaptational view of the link between nervous control systems for swimming and feeding (Costello et al., 2008). The fact that this relationship is not limited by the second dichotomy, which includes very different ways that medusae control swim musculature (Romanes’s naked-eyed/covered-eyed medusa dichotomy), speaks of a relative sophistication in the ways that the drastically different nervous systems of the two forms converged to incorporate nervous control that was able to conform to body structure, body size, and swim/feeding strategy-limitations. This sophistication goes well beyond nerve nets and argues for highly efficient and remarkably responsive centralized nervous control of the radially symmetrical organization of effectors and sensory structures in the phylum. It is particularly impressive that these supposedly primitive nervous systems were able to adapt within the limitations of swim mechanics in two very different lineages of nervous system organization in order to reflect the prolate/oblate dichotomy consistently.
Anderson, P. A. V. (1979). Ionic basis of the action potentials and bursting activity in the hydromedusan jellyfish Polyorchis pennicilatus. Journal of Experimental Biology, 78, 299–302.Find this resource:
Anderson, P. A. V. (1980). Epithelial conduction: Its properties and functions. Progress in Neurobiology, 15, 161–203.Find this resource:
Anderson, P. A. V. (1985). Physiology of a bidirectional, excitatory, chemical synapse. Journal of Neurophysiology, 53, 821–835.Find this resource:
Anderson, P. A. V., & Greenberg, R. M. (2001). Phylogeny of ion channels: Clues to structure and function. Comparative Biochemistry and Physiology Part B, 129, 17–28.Find this resource:
Anderson, P. A. V., & Grunert, U. (1988). Three-dimensional structure of bidirectional, excitatory chemical synapses in the jellyfish Cyanea capillata. Synapse, 2, 606–613.Find this resource:
Anderson, P. A. V., & Mackie, G. O. (1977). Electrically coupled, photosensitive neurons control swimming in a jellyfish. Science, 197, 186–188.Find this resource:
Anderson, P. A. V., & Schwab, W. E. (1981). The organization and structure of nerve and muscle in the jellyfish Cyanea capillata. Journal of Morphology, 170, 383–399.Find this resource:
Anderson, P. A. V., & Schwab, W. E. (1982). The action potential in the motor neuron nerve net of a jellyfish. Federation Proceedings, 41, 1114.Find this resource:
Anderson, P. A. V., & Schwab, W. E. (1983). The action potential in neurons of the motor nerve net of Cyanea (Coelenterata). Journal of Neurophysiology, 50, 671–683.Find this resource:
Anderson, P. A. V., & Schwab, W. E. (1984). An epithelial cell-free preparation of the motor nerve net of Cyanea (Coelenterata; Scyphozoa). Biological Bulletin, 166, 396–408.Find this resource:
Anderson, P. A. V., & Trapido-Rosenthal, H. G. (2009). Physiological and chemical analysis of neurotransmitter candidates at the fast excitatory synapse in jellyfish Cyanea capillata (Cnidaria, Scyphozoa). Invertebrate Neuroscience, 9, 167–173.Find this resource:
Arkett, S. A. (1985). The shadow response of a hydromedusan (Polyorchis penicillatus): Behavioral mechanisms controlling diel and ontogenic vertical migration. Biological Bulletin, 169, 297–312.Find this resource:
Arkett, S. A., & Mackie, G. O. (1988). Hair cell mechanoreception in the jellyfish Aglantha digitale. Journal of Experimental Biology, 135, 329–342.Find this resource:
Arkett, S. A., & Spencer, A. N. (1986a). Neuronal mechanisms of a hydromedusan shadow reflex. I. Identified reflex components and sequence of events. Journal of Comparative Physiology A, 159, 201–213.Find this resource:
Arkett, S. A., & Spencer, A. N. (1986b). Neuronal mechanisms of a hydromedusan shadow reflex. II. Graded response of reflex components, possible mechanisms of photic integration, and functional significance. Journal of Comparative Physiology A, 159, 215–225.Find this resource:
Bentlage, B., Cartwright, P., Yanagihara, A. A., Lewis, C., Richards, G. S., & Collins, A. G. (2009). Evolution of box jellyfish (Cnidaria: Cubozoa), a group of highly toxic invertebrates. Proceedings of the Royal Society of London B, 277, 493–501.Find this resource:
Berger, E. W. (1898). The histological structure of the eyes of cubomedusae. Journal of Comparative Neurology, 8, 223–230.Find this resource:
Bullock, T. H. (1943). Neuromuscular facilitation in scyphomedusae. Journal of Cellular and Comparative Physiology, 22, 251–272.Find this resource:
Coates, M. M., Garm, A., Theobald, J. C., Thompson, S. H., & Nilsson, D.-E. (2006). The spectral sensitivity in the lens eyes of a box jellyfish, Tripedalia cystophora. Journal of Experimental Biology, 209, 3758–3765.Find this resource:
Colin, S. P., & Costello, J. H. (2002). Morphology, swimming performance, and propulsive mode of six co-occurring hydromedusae. Journal of Experimental Biology, 205, 427–437.Find this resource:
Colin, S. P., Costello, J. H., Katija, K., Seymour, J., & Kiefer, K. (2013). Propulsion in cubomedusae: mechanisms and utility. PlosONE, 8, e56393,Find this resource:
Collins, A. G. (2002). Phylogeny of medusozoan and the evolution of cnidarian life cycles. Journal of Evolutionary Biology, 15, 418–432.Find this resource:
Collins, A. G. (2009). Recent insights into cnidarian phylogeny. Smithsonian Contributions to the Marine Sciences, 38, 139–149.Find this resource:
Costello, J. H., & Colin, S. P. (1994). Morphology, fluid motion, and predation by the scyphomedusae Aurelia aurita. Marine Biology, 121,327–334.Find this resource:
Costello, J. H., & Colin, S. P. (1995). Flow and feeding by swimming scyphomedusae. Marine Biology, 124, 399–406.Find this resource:
Costello, J. H., Colin, S. P., & Dabiri, J. O. (2008). Medusan morphospace: Phylogenetic constraints, biomechanical solutions, and ecological consequences. Invertebrate Biology, 127, 265–290.Find this resource:
Dabiri, J. O., Colin, S. P., & Costello, J. H. (2005). Flow patterns generated by oblate medusan jellyfish: Field measurements and laboratory analyses. Journal of Experimental Biology, 208, 1257–1265.Find this resource:
Dabiri, J. O., Colin, S. P., & Costello, J. H. (2006). Fast-swimming hydromedusae exploit velar kinematics to form an optimal vortex wake. Journal of Experimental Biology, 209, 2025–2033.Find this resource:
Donaldson, S., Mackie, G. O., & Roberts, A. (1980). Preliminary observations on escape swimming and giant neurons in Aglantha digitale (Hydromedusae: Trachylina). Canadian Journal of Zoology, 58, 549–552.Find this resource:
Eichinger, J. M., & Satterlie, R. A. (2014). Organization of the ectodermal nervous structures in medusae: Cubomedusae. Biological Bulletin, 226, 41–55.Find this resource:
Garm, A., & Bielecki, H. (2008). The swim pacemakers of box jellyfish are modified by visual input. Journal of Comparative Physiology A, 194, 641–651.Find this resource:
Garm, A., Coates, M. M., Gad, R., Seymour, R., & Nilsson, D.-E. (2007a). The lens eyes of the box jellyfish Tripedalia cystophora and Chiropsalmus sp. are slow and color-blind. Journal of Comparative Physiology A, 193, 547–557.Find this resource:
Garm, A., & Ekstrom, P. (2010). Evidence for multiple photosystems in jellyfish. International Review of Cell and Molecular Biology, 280, 41–78.Find this resource:
Garm, A., Ekstrom, P., Boudes, M., & Nilsson, D.-E. (2006). Rhopalia are integrated parts of the central nervous system of box jellyfish. Cell and Tissue Research, 325, 333–343.Find this resource:
Garm, A., Hedal, I., Majken, I., & Gurska, D. (2013). Pattern- and contrast-dependent visual response in the box jellyfish Tripedalia cystophora. Journal of Experimental Biology, 216, 4520–4529.Find this resource:
Garm, A., & Mori, S. (2009). Multiple photoreceptor systems control the swim pacemaker activity in box jellyfish. Journal of Experimental Biology, 212, 3951–3960.Find this resource:
Garm, A., O’Connor, M., Parkefelt, L., & Nilsson, D.-E. (2007b). Visually guided obstacle avoidance in the box jellyfish Tripedalia cystophora and Chiropsella bronzie. Journal of Experimental Biology, 210, 3616–3623.Find this resource:
Garm, A., Poussart, Y., Parkefelt, L., Edstrom, P., & Nilsson, D.-E. (2007c). The ring nerve of the box jellyfish Tripedalia cystophora. Cell and Tissue Research, 329, 147–157.Find this resource:
Gladfelter, W. G. (1973). A comparative analysis of the locomotory systems of medusoid cnidaria. Helgolaender Wissenschaftliche Meeresuntersuchungen, 25, 228–272.Find this resource:
Gray, G. C., Martin, V. J., & Satterlie, R. A. (2009). Ultrastructure of the retinal synapses in cubozoans. Biological Bulletin, 217, 35–49.Find this resource:
Hamner, W. M., Jones, M. S., & Hamner, P. P. (1995). Swimming, feeding, circulation, and vision in the Australian box jellyfish, Chironex fleckeri (Cnidaria, Cubozoa). Marine & Freshwater Research, 46, 985–990.Find this resource:
Horridge, G. A. (1953). An action potential from the motor nerves of the jellyfish Aurellia aurita Lamarck. Nature, 171, 400.Find this resource:
Horridge, G. A. (1954a). The nerves and muscles of medusae. I. Conduction in the nervous system of Aurellia aurita Lamarck. Journal of Experimental Biology, 31, 594–600.Find this resource:
Horridge, G. A. (1954b). Observations on the nerve fibres of Aurellia aurita. Quarterly Journal of Microscopical Science, 95, 85–92.Find this resource:
Horridge, G. A. (1956a). The nerves and muscles of medusae. V. Double innervation in scyphozoa. Journal of Experimental Biology, 33, 366–383.Find this resource:
Horridge, G. A. (1956b). The nervous system of the ephyra larva of Aurellia aurita. Quarterly Journal of Microscopical Science, 97, 59–74.Find this resource:
Horridge, G. A. (1959). The nerves and muscles of medusae. VI. The rhythm. Journal of Experimental Biology, 36, 72–91.Find this resource:
Horridge, G. A., Chapman, D. M., & MacKay, B. (1962). Naked axons and symmetrical synapses in an elementary nervous system. Nature, 193, 899–900.Find this resource:
Horridge, G. A., & MacKay, B. (1962). Naked axons and symmetrical synapses in coelenterates. Quarterly Journal of Microscopical Science, 103, 531–541.Find this resource:
Hundgen, L. H., & Biela, C. (1982). Fine structure of touch-plates in the scyphomedusan Aurelia aurita. Journal of Ultrastructure Research, 80, 178–184.Find this resource:
Hyman, L. H. (1940). The invertebrates: Protozoa through Ctenophora. New York: McGraw-Hill.Find this resource:
Kerfoot, P. A. H., Mackie, G. O., Meech, R. W., Roberts, A., & Singla, C. L. (1985). Neuromuscular transmission in the jellyfish Aglantha digitale. Journal of Experimental Biology, 116, 1–25.Find this resource:
King, M. G., & Spencer, A. N. (1981). The involvement of nerves in the epithelial control of crumpling behaviour in a hydrozoan jellyfish. Journal of Experimental Biology, 94, 203–218.Find this resource:
Keough, E. M., & Summers, R. G. (1976). An ultrastructural investigation of the striated subumbrellar musculature of the anthomedusan, Pennaria tiarella. Journal of Morphology, 149, 507–526.Find this resource:
Larson, R. J. (1976). Cubomedusae: Feeding, functional morphology, behaviour, and phylogenetic position. In G. O. Mackie (Ed.), Coelenterate ecology and behaviour (pp. 237–245). New York: Plenum Press.Find this resource:
Laska, G., & Hundgen, M. (1984). Die Ultrastruktur des neuromuscularen Systems der Medusen von Tripedalia cystophora und Carybdea marsupialis (Coelenterata, Cubozoa). Zoomorphology, 104, 163–170.Find this resource:
Lawn, I. D. (1976). Swimming in the sea anemone Stomphia coccinea triggered by a slow conduction system. Nature, 262, 708–709.Find this resource:
Lerner, J., Mellen, S. A., Waldron, I., & Factor, R. M. (1971). Neural redundancy of swimming beats in scyphozoan medusae. Journal of Experimental Biology, 55, 177–184.Find this resource:
Lin, Y.-C., Gallin, W. J., & Spencer, A. N. (2001). The anatomy of the nervous system of the hydrozoan jellyfish Polyorchis penicillatus, as revealed by a monoclonal antibody. Invertebrate Neuroscience, 4, 65–75.Find this resource:
Lipinski, D., & Mohseni, K. (2009). Flow structures and fluid transport for the hydromedusae Sarsia tubulosa and Aequorea Victoria. Journal of Experimental Biology, 212, 2436–2447.Find this resource:
Mackie, G. L., & Singla, C. L. (1975). Neurobiology of Stomotoca. I. Action systems. Journal of Neurobiology, 6, 339–356.Find this resource:
Mackie, G. O. (2004a). Central neural circuitry in the jellyfish Aglantha. Neurosignals, 13, 5–19.Find this resource:
Mackie, G. O. (2004b). Epithelial conduction: Recent findings, old questions, and where do we go from here? Hydrobiologia, 530/531, 73–80.Find this resource:
Mackie, G. O., Anderson, P. A. V., & Singla, C. L. (1984). Apparent absence of gap junctions in two classes of cnidaria. Biological Bulletin, 167, 120–123.Find this resource:
Mackie, G. O., & Meech, R. W. (1985). Separate sodium and calcium spikes in the same axon. Nature, 313, 791–793.Find this resource:
Marques, A. C., & Collins, A. G. (2004). Cladistic analysis of medusozoan and cnidarian evolution. Inverterbrate Biology, 123, 23–42.Find this resource:
Martin, V. J. (2002). Photoreceptors in Cnidarians. Canadian Journal of Zoology, 80, 1703–1722.Find this resource:
Martin, V. J. (2004). Photoreceptors of cubozoan jellyfish. Hydrobiologia, 530/531, 135–144.Find this resource:
Meech, R. W., & Mackie, G. O. (1993a). Ionic currents in giant motor axons of the jellyfish, Aglantha digitale. Journal of Neurophysiology, 69, 884–893.Find this resource:
Meech, R. W., & Mackie, G. O. (1993b). Potassium channel family in giant motor axons of Aglantha digitale. Journal of Neurophysiology, 69, 894–901.Find this resource:
Meech, R. W., & Mackie, G. O. (1995). Synaptic potentials underlying spike production in motor giant axons of Aglantha digitale. Journal of Neurophysiology, 74, 1662–1670.Find this resource:
Nakanishi, N., Hartenstein, B., & Jacobs, D. K. (2009). Development of the rhopalial nervous system in Aurelia sp.1 (Cnidaria, Scyphozoa). Development Genes and Evolution, 219, 301–317.Find this resource:
Nilsson, D.-E., Coates, M. M., Gislen, I., Skogh, C., & Garm, A. (2005). Advanced optics in a jellyfish eye. Nature, 435, 201–205.Find this resource:
O’Connor, M., Garm, A., & Nilsson, D.-E. (2009). Structure and optics of the eyes of the box jellyfish Chiropsella bronzie. Journal of Comparative Physiology A, 195, 557–569.Find this resource:
O’Connor, M., Nilsson, D.-E., & Garm, A. (2010). Temporal properties of the lens eyes of the box jellyfish Tripedalia cystophora. Journal of Comparative Physiology A, 196, 213–220.Find this resource:
Pantin, C. F. A., & Vianna Dias, M. (1952). Rhythm and afterdischarge in medusae. Anais da Academia Brasileira de Ciências, 24, 351–364.Find this resource:
Parkefelt, L., & Ekstrom, P. (2009). Prominent system of RFamide immunoreactive neurons in the rhopalia of box jellyfish (Cnidaria: Cubozoa). Journal of Comparative Neurology, 516, 157–165.Find this resource:
Parkefelt, L., Skogh, C., Nilsson, D.-E., & Ekstrom, P. (2005). Bilateral symmetric organization of neuronal elements in the visual system of a coelenterate, Tripedalia cystophora. Journal of Comparative Neurology, 492, 251–262.Find this resource:
Passano, L. M. (1965). Pacemakers and activity patterns in medusae: Homage to Romanes. American Zoologist, 5, 465–489.Find this resource:
Passano, L. M. (1973). Behavioral control systems in medusae: A comparison between hydro- and scyphomedusae. Publications of the Seto Marine Biological Laboratory, 20, 615–645.Find this resource:
Passano, L. M. (1982). Scyphozoa and cubozoa. In G. A. B. Shelton (Ed.), Electrical conduction and behaviour in “simple” invertebrates (pp. 149–202). Oxford: Clarendon Press.Find this resource:
Passano, L. M. (2004). Spasm behavior and the diffuse nerve-net in Cassiopea xamachana (Scyphozoa: Coelenterata). Hydrobiologia, 530/531, 91–96.Find this resource:
Patton, M. L., & Passano, L. M. (1972). Intracellular recordings from the giant fiber nerve net of a scyphozoan jellyfish. American Zoologist, 12, 35.Find this resource:
Petie, R., Garm, A., & Nilsson, D.-E. (2011). Visual control of steering in the box jellyfish Tripedalia cystophora. Journal of Experimental Biology, 214, 2809–2815.Find this resource:
Plickert, G., & Schneider, B. (2004). Neuropeptides and photic behavior in Cnidaria. Hydrobiologia, 530/531, 49–57.Find this resource:
Roberts, A., & Mackie, G. O. (1980). The giant axon escape system of a hydrozoan medusa, Aglantha digitale. Journal of Experimental Biology, 84, 303–318.Find this resource:
Robson, E. A. (1961). Some observations on the swimming behavior of the anemone Stomphia coccinea. Journal of Experimental Biology, 38, 343–363.Find this resource:
Robson, E. A. (1963). The nerve-net of a swimming anemone Stomphia coccinea. Quarterly Journal of Microscopical Science, 104, 535–549.Find this resource:
Romanes, G. J. (1885). Jellyfish, starfish, and sea urchins. London: Kegan Paul, Trench, and Co.Find this resource:
Sahin, M., Mohseni, K., & Colin, S. P. (2009). The numerical comparison of flow patterns and propulsive performances for the hydromedusae Sarsia tubulosa and Aequorea victoria. Journal of Experimental Biology, 212, 2656–2667.Find this resource:
Satterlie, R. A. (1979). Central control of swimming in the cubomedusan jellyfish Carybdea rastonii. Journal of Comparative Physiology A, 133, 357–367.Find this resource:
Satterlie, R. A. (1985a). Central generation of swimming activity in the hydrozoan jellyfish Aequorea aequorea. Journal of Neurobiology, 16, 41–55.Find this resource:
Satterlie, R. A. (1985b). Control of swimming in the hydrozoan jellyfish Aequorea aequorea: Direct activation of the subumbrella. Journal of Neurobiology, 16, 211–226.Find this resource:
Satterlie, R. A. (2002). Neural control of swimming in jellyfish: A comparative story. Canadian Journal of Zoology, 80, 1654–1669.Find this resource:
Satterlie, R. A. (2008). Control of swimming in the hydrozoan jellyfish Aequorea victoria: Subumbrellar organization and local inhibition. Journal of Experimental Biology, 211, 3467–3477.Find this resource:
Satterlie, R. A. (2011). Commentary: Do jellyfish have central nervous systems? Journal of Experimental Biology, 214, 1215–1223.Find this resource:
Satterlie, R. A. (2014). Multiple conducting systems in the cubomedusa Carybdea marsupialis. Biological Bulletin, 227, 274–284.Find this resource:
Satterlie, R. A. (2015a). Cnidarian nerve nets and neuromuscular efficiency. Integrative and Comparative Biology, 55, 1050–1057.Find this resource:
Satterlie, R. A. (2015b). The search for ancestral nervous systems: An integrative and comparative approach. Journal of Experimental Biology, 218, 612–617.Find this resource:
Satterlie, R. A., & Eichinger, J. M. (2014). Organization of the ectodermal nervous structures in jellyfish: Scyphomedusae. Biological Bulletin, 226, 29–40.Find this resource:
Satterlie, R. A., & Nolen, T. G. (2001). Why do cubomedusae have only four swim pacemakers? Journal of Experimental Biology, 204, 1413–1419.Find this resource:
Satterlie, R. A., & Spencer, A. N. (1979). Swimming control in a cubomedusan jellyfish. Nature, 281, 141–142.Find this resource:
Satterlie, R. A., & Spencer, A. N. (1983). Neural control of locomotion in hydrozoan medusae: A comparative story. Journal of Comparative Physiology, 150, 195–206.Find this resource:
Satterlie, R. A., Thomas, K. S., & Gray, G. C. (2005). Muscle organization of the cubozoan jellyfish Tripedalia cystophora (Conant 1897). Biological Bulletin, 209, 154–163.Find this resource:
Schwab, W. E., & Anderson, P. A. V. (1980). Intracellular recordings of spontaneous and evoked electrical events in the motor neurons of Cyanea capillata. American Zoologist, 20, 941.Find this resource:
Schwab, W. E., & Anderson, P. A. V. (1981). Symmetrical chemical synapses. American Zoologist, 21, 942.Find this resource:
Shafer, E. A. (1878). Observations on the nervous system of Aurelia aurita. Philosophical. Transactions of the Royal Society of London, 169, 563–575.Find this resource:
Shorten, M. O., Davenport, J., Seymour, J. E., Cross, M. C., Carrette, T. J., Woodward, G., & Cross, T. F. (2005). Kinematic analysis of swimming in Australian box jellyfish, Chiropsalmus sp., and Chironex fleckeri (Cubozoa, Cnidaria, Chirodropidae). Journal of Zoology (London), 267, 371–380.Find this resource:
Singla, C. L. (1974). Ocelli of hydromedusae. Cell and Tissue Research, 149, 413–429.Find this resource:
Singla, C. L. (1975). Statocysts of hydromedusae. Cell and Tissue Research, 158, 391–407.Find this resource:
Singla, C. L. (1978a). Fine structure of the neuromuscular system of Polyorchis penicillatus (Hydromedusae, Cnidaria). Cell and Tissue Research, 193, 163–174.Find this resource:
Singla, C. L. (1978b). Locomotion and neuromuscular system of Aglantha digitale. Cell and Tissue Research, 188, 317–327.Find this resource:
Skogh, C., Garm, A., Nilsson, D.-E., & Ekstrom, P. (2006). Bilaterally symmetrical rhopalial nervous system of the box jellyfish Tripedalia cystophora. Journal of Morphology, 267, 1391–1405.Find this resource:
Spencer, A. N. (1975). Behavior and electrical activity in the hydrozoan Proboscidactyla flavicirrata (Brandt). II. The medusa. Biological Bulletin, 149, 236–250.Find this resource:
Spencer, A. N. (1978). Neurobiology of Polyorchis. I. Function of effector systems. Journal of Neurobiology, 9, 143–157.Find this resource:
Spencer, A. N. (1979). Neurobiology of Polyorchis. II. Structure of effector systems. Journal of Neurobiology, 10, 95–117.Find this resource:
Spencer, A. N. (1981). The parameters and properties of a group of electrically coupled neurons in the central nervous system of a hydrozoan jellyfish. Journal of Experimental Biology, 93, 33–50.Find this resource:
Spencer, A. N. (1982). The physiology of a coelenterate neuromuscular synapse. Journal of Comparative Physiology, 148, 353–363.Find this resource:
Spencer, A. N., & Arkett, S. A. (1984). Radial symmetry and the organization of central neurons in a hydrozoan jellyfish. Journal of Experimental Biology, 110, 69–90.Find this resource:
Spencer, A. N., & Satterlie, R. A. (1980). Electrical and dye-coupling in an identified group of neurons in a coelenterate. Journal of Neurobiology, 11, 13–19.Find this resource:
Weber, C., Singla, C. L., & Kerfoot, P. A. H. (1982). Microanatomy of the subumbrellar motor innervation in Aglantha digitale (Hydromedusae: Trachylina). Cell and Tissue Research, 223(2), 305–312.Find this resource:
Werner, B., Chapman, D. M., & Cutress, C. E. (1976). Muscular and nervous systems of the cubopolyp (Cnidaria). Experientia, 32, 1047–1049.Find this resource:
Werner, B., Cutress, C. E., & Studebaker, J. P. (1971). Life cycle of Tripedalia cystophora Conant (Cubomedusae). Nature, 232, 582–583.Find this resource:
Westfall, J. A. (1973). Ultrastructural evidence for neuromuscular systems in coelenterates. American Zoologist, 13, 237–246.Find this resource:
Westfall, J. A. (1996). Ultrastructure of synapses in the first-evolved nervous systems. Journal of Neurocytology, 25, 735–746.Find this resource:
Yamasu, T., & Yoshida, M. (1973). Electron microscopy on the photoreceptors of an anthomedusa and a scyphomedusa. Publications of the Seto Marine Biological Laboratory, 20, 757–778.Find this resource: