| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
1Institute of Neurobiology and Department of Anatomy, University of Puerto Rico Medical Sciences Campus, San Juan, Puerto Rico 00901; and 2Department of Physiology and Biophysics, Mount Sinai School of Medicine, New York, New York 10029
Submitted 27 May 2004; accepted in final form 29 June 2004
 |
ABSTRACT |
|---|
|
|
|
INTRODUCTION |
|---|
|
; Kupfermann 1979; Pearson 1993). Compelling evidence has come from studies of many model systems (e.g., Hultborn and Kiehn 1992; Sillar et al. 2002; Weiss et al. 1992) including, notably, the decapod crustaceans. In crustacean motor systems, modulation occurs at every level from sensory-motor integration (Edwards et al. 2002; Glanzman and Krasne 1983) through central pattern generation (Harris-Warrick and Marder 1991; Harris-Warrick et al. 1988; Miller and Sullivan 1981) to neuromuscular transmission (Breen and Atwood 1983; Florey and Rathmayer 1978; Kravitz et al. 1980).
In neuromodulatory architectures, two broad themes have been distinguished: in the terminology of Cropper (1987) and Katz and Frost (1996), "intrinsic" and "extrinsic" modulation. Intrinsic modulation is locally integrated into the structure of the "mediating" network. It is automatically set in motion when the network is active to provide local adjustments, although these adjustments may have global consequences in a well-connected, dynamically sensitive network such as a central pattern generator (CPG). The functional roles of intrinsic modulation have been relatively well studied (see, e.g., Brezina and Weiss 1997; Katz 1999; Katz and Frost 1996; Marder and Thirumalai 2002).
Extrinsic modulation, by contrast, arrives from an external source such as a modulatory neuron that is not itself part of the mediating circuitry. Such extrinsic modulatory systems of crustaceans have been described as overall "gain setters" (Kravitz 1988; Ma et al. 1992). Because extrinsic modulation is not obligatorily coupled to the activity of any particular part of the mediating system, it is free to exert widespread actions. In crustaceans, dopamine is of particular interest in this regard because it appears to regulate multiple motor systems (Barthe et al. 1989; Berlind 1977; Harris-Warrick et al. 1998; Meyrand and Moulins 1986; Miller et al. 1984, 1985; Rajashekhar and Wilkens 1992; Wood 1995). In those species in which it has been localized, dopamine has been found to be present in a relatively small number of neurons with extensive projections (Cournil et al. 1994, 1995; Tierney et al. 2003; Wood and Derby 1996). Based on observations of this kind, it has been conjectured that the role of extrinsic modulation in motor systems is to modulate multiple parts of motor circuits, and multiple motor circuits, so as to integrate their activities into a global, coordinated whole. Whether external modulation really plays this role, and what functional consequences might flow from such actions, has, however, not been rigorously established. In part this has been because of the lack of a suitable simple experimental preparation. Our first aim in this paper is to identify and characterize such a preparation.
The cardiac system of decapod crustaceans is an exceptionally simple system that is known to receive substantial modulatory regulation. The heartbeat in marine species is driven by a simple (usually 9 neurons) central pattern generating circuit, the cardiac ganglion (CG), positioned within the dorsal wall of the heart (Cooke 1988, 2002). The CG is directly controlled by a small number of modulatory fibers that originate in the CNS (Delgado et al. 2000; Field and Larimer 1975; Maynard 1960; Yazawa and Kuwasawa 1994). The heartbeat is also regulated by modulators that originate from the pericardial organs (POs), neurohaemal structures that flank the heart and release bioactive products into the general circulation (Alexandrowicz and Carlisle 1953; Cooke and Sullivan 1982). Recognition of the crustacean CG as "an autonomously active, rhythmic, pattern-forming, neural system integrating its own spontaneity with sensory and neurohumoral influences" (Cooke 1988) led early investigators to emphasize its utility as a very simple model for more complex nervous systems (Alexandrowicz 1932; Hagiwara 1961; Welsh and Maynard 1951).
Perhaps the most important aspect of global coordination is that between center and periphery. Experimental studies suggest that motor systems are, as theoretical studies suggest they must be, coordinately modulated both in the center and in the periphery to ensure efficient, adaptive behavior (Brezina et al. 2000b; Calabrese 1989; Chiel and Beer 1997; Meyrand and Marder 1991). The present study was intended to establish the crustacean cardiac system, seen as a simple model of a CPG complete with its effector system, as a suitable preparation in which to study the coordination of central and peripheral modulation. Anatomical and physiological methods were used to show that a single central dopaminergic neuron is likely to exert actions both on the periphery (neurohormonal modulation of contractions of the heart muscle) and on the central pattern generator (direct innervation of the CG) of the cardiac system of the blue crab Callinectes sapidus. These inferences were examined with experiments in which dopamine was applied to intact hearts, isolated cardiac ganglia, and a novel semi-intact working heart preparation in which central and peripheral effects could be compared directly.
|
|
METHODS |
|---|
|
Histology
Tyrosine hydroxylase (th) immunohistochemistry.
Specimens were covered in ice (30 min) to achieve immobilization. Tissues were dissected, secured to Sylgard-lined petri dishes with minuten pins, and fixed for 1 h in freshly prepared 4% paraformaldehyde. Standard whole mount immunohistochemical protocols were followed (see Miller et al. 1991 for detailed buffer composition, incubation, and wash procedures). Ganglia were washed (5x, room temperature with agitation) in PTA (0.1 M phosphate buffer containing 2% Triton X-100 and 0.1% sodium azide). After preincubation with normal goat serum (0.8%), tissues were immersed (48 h, room temperature) in a 1:200 dilution of the primary TH antibody (mouse monoclonal; Immunostar, Stillwater, MN). After repeated PTA washes (5x, 
30 min each, room temperature), ganglia were incubated in secondary antibodies conjugated to a fluorescent marker [Alexa 488 goat anti-mouse IgG (H+L) conjugate; Molecular Probes, Eugene, OR: A-11029]. The secondary antibody dilutions ranged from 1:1,000 to 1:3,000. The Alexa 488 was viewed with the G-2A filter block of the Nikon Optiphot or using the preconfigured FITC channel of a Zeiss Pascal LSM5 laser-scanning confocal microscope. Standard images were captured using the ACT1 (Nikon) software package. Confocal images were reconstructed (AIM Software) from sequential images captured in the z-axis plane of the tissue. Images were transported as TIFF files to Adobe Photoshop (Version 6) for adjusting overall contrast and brightness. Finally, they were imported to Corel Draw 9 for addition of labels, cropping, and organization of panels.
Nerve backfills.
The biotin–avidin protocol followed the methods of Xin et al. (1999) with modifications based on Díaz-Ríos et al. (1999). The tissue of interest was pinned out near a small Vaseline well that was formed on the Sylgard surface. The nerve being examined was cut and drawn into the well. Care was taken to avoid contact between the end of the nerve and the Vaseline. The tip of the nerve was cut one more time and then the crab saline inside the well was withdrawn and replaced with a saturated aqueous solution (1.6 mg/30 µl) of biocytin (Sigma Chemical, St. Louis, MO). The walls of the well were then built up with successive layers of Vaseline, forming an "igloo" that effectively isolated the biocytin pool from the saline surrounding the ganglion. The preparation was covered and incubated overnight at 14°C. The well was then removed, and ganglia were washed 3–5 times, repinned, and fixed in paraformaldehyde as described above. The fixed ganglia were transferred to microcentrifuge tubes, washed 5 times (30 min each) with PTA solution and incubated overnight (room temperature, with shaking) in Rhodamine600 Avidin D (Vector Laboratories, Burlingame, CA) diluted 1:3,000 in PTA (24–48 h, room temperature). Tissues were then washed 5 times with PTA and the quality of the backfill was assessed before further immunohistochemical processing. In the double-labeling experiments, THli was visualized using the Alexa 488 goat anti-mouse secondary antibody (see above). A barrier filter (546 nm green interference) was used to eliminate "bleed through " of rhodamine when examining and photographing THli fluorescence.
Neurobiotin injection.
Methods for intracellular staining were modified from the methods of Delgado et al. (2000). Microelectrode tips were filled with 4% Neurobiotin (Vector Laboratories) dissolved in 0.5 M KCl and 50 mM Tris (pH 7.6). The electrode shafts were filled with 2 M KCl, resulting in resistances ranging from 10 to 30 M
. Depolarizing current pulses (1–2 nA; 0.5 s; 1 Hz; 10–60 min) were used to eject the Neurobiotin. This procedure did not appear to affect the resting potential or spontaneous electrical activity of the injected neuron. The preparations were usually left at room temperature for 2–3 h to allow material to diffuse from the injection site (cell body) to distant processes and dye-coupled cells. They were then repinned if necessary, and fixed in paraformaldehyde as described above. The fixed ganglia were transferred to microcentrifuge tubes, washed 5 times (30 min each) with PTA solution, and incubated in Rhodamine600 Avidin D diluted (1:3,000 to 1:5,000) in PTA (24–48 h, room temperature). Tissues were then washed 5 times with PTA, examined, and processed for THli as described above.
Physiology
Working heart (fig. 1a).
Hearts were removed intact and the sternal artery was cannulated with a modified syringe needle and mounted in a 20-ml organ bath. The heart was suspended using a fine monofilament nylon thread attached to the force plates of a Grass FT03 isometric force transducer and placed under a resting load (
0.5 g). Perfusion with saline was maintained at a constant rate (2 ml/min) and pressure. The crab saline composition was based on Pantin's saline for Cancer pagarus: 487 mM NaCl, 13.6 mM KCl, 13.4 mM CaCl2, 13.6 mM MgCl2, 1.4 mM sodium sulfate, 3 mM HEPES (N-[2-hydroxyethyl] piperazine-N'-[2-ethanesulfonic acid]), adjusted to pH 7.4 with sodium hydroxide. Perfusion rate and pressure were maintained when dopamine trials were performed.
|
Hearts were dissected and pinned in Sylgard-lined petri dishes, in an arrangement as similar as possible to that in the intact crab. A small incision was made in the ventral wall of the heart to expose part of the nerve ring containing the motor neuron axons. The ring was cut and the severed end proximal to the ganglion was drawn into an extracellular suction electrode. The heart was then connected to the force plates of a Grass FT03 isometric force transducer with a hook and nylon thread and placed under a resting load (0.5 g). The preparation was continually internally perfused with saline at a constant rate (2 ml/min) and pressure. Perfusion rate and pressure were maintained when dopamine trials were performed.
Isolated cardiac ganglion (fig. 1c).
Hearts were pinned ventral side up in Sylgard-lined petri dishes. A cut was made in the ventral musculature exposing the cardiac ganglion. Dissection was achieved principally by teasing away the adhering muscles. Previous investigators (Tazaki and Cooke 1979a) noted that the region within the confluence of the motor roots at each end of the ganglion contains the dendritic endings of the ganglionic neurons (see also Fig. 2B). A small noncontracting remnant was therefore retained at either end of the ganglion. Extracellular suction electrode recordings were obtained from at least one of the 4 cut ganglionic roots. Membrane potentials were recorded from anterior and/or posterior motor neurons using 2 M KCl-filled or Neurobiotin-tipped microelectrodes (10–30 M). Preparations were continuously superfused with saline (2 ml/min).
|
20 min) between the application of different dopamine concentrations. |
|
RESULTS |
|---|
|
We first sought to characterize features of the Callinectes cardiac system relevant to its suitability for examining the coordination of central and peripheral modulation. Injection of Neurobiotin into any of the large neurons within the cardiac ganglion revealed, through dye coupling, its full complement of 5 motor neurons. The cell bodies of 3 of the motor neurons were located at the anterior end of the ganglion (Fig. 2A, asterisks). These cells projected large-caliber axons into the ganglionic trunk in the posterior direction. Two large posterior motor neurons (Fig. 2B, asterisks) projected axons in the anterior direction. The 5 axons came into close apposition within the anterior half of the trunk. The axons originating from the anterior cells bifurcated on reaching the posterior end of the ganglion and projected branches into each of the posterior connectives (Fig. 2B). Similarly, the axons of the posterior cells bifurcated at the anterior end of the ganglion and projected branches into each of the anterior connectives. A single dendritic process emerged from the distal end of each motor neuron (Fig. 2B). These processes branched within or close to the ganglion and terminated as fine projections in the cardiac muscle adjacent to the ganglion within the confluence of the major connectives (see also Tazaki and Cooke 1979a, 1983a, b). When large quantities of the tracer were injected, small neurons could be discerned in the most posterior region of the ganglionic trunk (Fig. 2B, dashed box). Although the dye coupling between the large cells and the small cells was relatively weak, 4 small cells were observed in the best instances.
Intracellular recording from the large motor neurons combined with extracellular recording from the major connectives was used to examine the electrical properties and functional organization of the cardiac ganglion (Fig. 2, C and D). In the isolated CG, all motor neurons produced simultaneous spontaneous rhythmic burst activity (Fig. 2C). In other decapods, electrical coupling among CG motor neurons and common synaptic input is thought to underlie such coordinated bursting and thus simultaneous contraction of the entire myocardium (Hagiwara 1961; Mirolli et al. 1987; Tazaki and Cooke 1979a). Indeed, as in other decapods (Friesen 1975a, b; Hartline 1979; Tazaki and Cooke 1979a, 1983a), each of the large motor neurons in Callinectes received synchronous excitatory postsynaptic potentials (EPSPs) in the initial and late phases of each burst (Fig. 2D, arrows). Impulses corresponding to these EPSPs were not detected in the motor trunks, indicating that they originate from the small interneurons, the projections of which are confined to the CG (Mirolli et al. 1987; Tazaki and Cooke 1979a, 1983a, b).
In the crab cardiac ganglia that have been investigated to date, the spatiotemporal properties of the electrical coupling and synaptic signaling result in precise synchrony of the motor neuron firing (Berlind 1982; Mirolli et al. 1987; Tazaki 1972; Tazaki and Cooke 1979a, b, 1983a, b). Simultaneous recording from an anterior motor neuron, a posterior motor neuron, a branch of the anterior connective, and a branch of the posterior connective revealed that such synchrony of firing is also a property of the Callinectes CG (Fig. 2, C and D). Intracellular recordings from any of the anterior motor neurons (Fig. 2, C and D, Ant. MN) revealed, in each burst, 5 to 10 nonovershooting impulses (10–15 mV) superimposed on a slow potential (500–900 ms in duration). The motor neuron slow potential has been shown to reflect the combined actions of an endogenous regenerative driver potential and the chemically mediated EPSPs originating from the small interneurons (Tazaki and Cooke 1979a, 1983a). In somatic recordings of posterior motor neurons (Fig. 2, C and D, Post. MN), the amplitudes of the impulses (3–5 mV) and the EPSPs (0.5–2 mV) were considerably smaller than those in the anterior motor neurons (10–15 and 2–4 mV), probably reflecting their origin in the anterior half of the ganglion (see Tazaki and Cooke 1983a). Examination of a single burst with an expanded time axis revealed that the impulses of the posterior neurons occurred in precise synchrony with those of the anterior motor neurons (Fig. 2D, 2 top records). Moreover, recordings from each of the major connectives (Fig. 2D, 2 bottom records) exhibited identical impulse trains that corresponded to the synchronous firing of the 2 sets of motor neurons.
The semi-intact working heart preparation
The observed synchrony of motor neuron firing suggested that recording from any of the 4 connectives would reflect the motor output of the ganglion and thus the patterned input to the entire cardiac musculature. This reasoning prompted us to develop a preparation, termed the semi-intact working heart (S-IWH; see METHODS), in which we could record the motor output of the ganglion in a minimally dissected contracting heart (Fig. 1B). Because this preparation required some removal of cardiac muscle and severing one connective, we performed an initial comparison of the parameters of heartbeat activity in the S-IWH with those in the fully intact working heart (WH) preparation (Fig. 1A). Contraction amplitudes were substantially reduced in the S-IWH (compare Fig. 1, A2 and B2), attributed presumably to the reduced mass of heart muscle and the reduced motor drive resulting from cutting the connective. However, the heartbeat frequency of the S-IWH (15.8 ± 1.8 beats/min, mean ± SE, n = 12) did not differ significantly from that of the intact WH (16.5 ± 1.2 beats/min, n = 20; 2-tailed Student's t-test, P = 0.74; Fig. 3A1). Moreover, the time to peak contraction (WH: 336.6 ± 29.7 ms, S-IWH: 364.9 ± 30.5 ms; P = 0.53) and the contraction duration (WH: 594.0 ± 104.7 ms, S-IWH: 612.0 ± 112.6 ms; P = 0.91) did not differ between the 2 preparations (Fig. 3, A2 and A3).
|
Together, these observations demonstrated that the semi-intact working heart preparation retained the essential properties of the intact heart. However, there were significant differences between the motor patterns produced by the S-IWH and the isolated CG, underscoring the importance of examiningcardiac modulation in the context of the entire, integrated CPG–effector system.
Dopaminergic regulation of the cardiac system: anatomical substrates
In a series of immunohistochemical experiments, we used a monoclonal antibody generated against tyrosine hydroxylase (TH) to identify possible sources and modes of dopaminergic modulation of the Callinectes cardiac system. In a previous mapping of the catecholaminergic system of Callinectes by Wood and Derby (1996), the staining pattern of TH-like immunoreactivity (THli) was found to be virtually identical to that observed with an antibody against dopamine (see also Cournil et al. 1994). In view of this, and the reported inability to detect norepinephrine and epinephrine in crustacean nervous tissue using chromatographic techniques (Barker et al. 1979; Sullivan et al. 1977), THli is commonly equated with the localization of dopamine in these species.
We observed THli in a limited number of neurons in the brain and ventral nerve cord (Figs. 4 and 5). In agreement with the previous description (Wood and Derby 1996) the largest central THli neuron was observed in the commissural ganglion (Fig. 4A, arrow). This cell corresponds to a dopaminergic neuron, termed the "L-cell" (Selverston et al. 1976), that has been described in a number of crustacean species, including the crab Carcinus maenas (Cooke and Goldstone 1970), the lobsters Panulirus interruptus (Kushner and Maynard 1977), Homarus gammarus (Cournil et al. 1984, 1994), Homarus americanus (Pulver et al. 2003; Siwicki et al. 1987), and the crayfish Oronectes rusticus (Tierney et al. 2003). The L-cell axon gave rise to multiple neurites within the commissural ganglion before its entry into the circumesophageal connective (C conn.). Four additional smaller THli neurons were observed in the commissural ganglion (Fig. 4A, arrowheads). A slender fiber projected into the superior esophageal nerve (son; Fig. 4A). This fiber did not appear to be a collateral of the L-cell axon, but it was also not possible to associate it definitively with any of the small neurons. Branches of the small neurons appeared to contribute to the central neuropil network, but their individual projections could not be distinguished from each other or from that of the L-cell.
|
|
). Near the point at which the L-cell axon reversed its direction at the junction of the C conn. and the brain, it gave rise to a small branch that contributed to the THli innervation of the tritocerebrum (Fig. 4, C and D; see also Tierney et al. 2003). On reaching the subesophageal ganglion, the L-cell axon coursed slightly past the origin of the first segmental nerve (SN1; nomenclature of Maynard 1961a, b) and then turned back to enter the nerve at a characteristic acute angle (Fig. 5, A and B).
Because projections from the CNS to the heart and pericardial organs are typically associated with the subesophageal segmental nerves (see Cooke and Sullivan 1982; Maynard 1961b), the projection of the L-cell axon into SN1 provided a possible anatomical substrate for dopaminergic regulation of the heart. We performed double-labeling experiments to confirm that the L-cell axon indeed projected into SN1. Biocytin backfills of the nerve revealed a bundle of fibers that curved in the anterior direction on entering the subesophageal ganglion. The position and trajectory of this fiber bundle suggested that it originated from the C-cell cluster in the anterior thoracic ganglia (Maynard 1961b; Wood et al. 1996). Toward the posterior edge of the nerve, a single large-diameter fiber (Fig. 5B1, arrow) could be followed into the ganglion, where it turned sharply to enter the C Conn. Only this fiber was observed to label for THli (Fig. 5B2, arrow), indicating that the sole dopaminergic fiber in SN1 originates from the L-cell. Occasionally, a smaller THli fiber also entered SN1, but it always terminated close to the ganglion and was never backfilled.
The large L-cell axon in SN1 could be followed to the pericardial organ in the lateral region of the thorax. On reaching the PO, it ramified repeatedly, projecting branches into each of the major bars and longitudinal trunks of the PO (Fig. 6; terminology of Alexandrowicz 1953). Within the central core of each bar and trunk, multiple smooth THli fibers ran in parallel fashion (Fig. 6, C and D). These fibers gave rise to finer, more irregular branches that reached the superficial cortex or secretory layer of the PO (Fig. 6E; see Maynard and Maynard 1962). No immunoreactive cell bodies were observed in the PO. These observations are consistent with previous descriptions of the anatomical features of catecholaminergic projections to the pericardial organs of 6 other brachyuran species (Cooke and Goldstone 1970) and the embryonic lobster Homarus americanus (Pulver and Marder 2002).
|
|
Cardioactive actions of dopamine
We tested the effects of exogenous dopamine on each of the 3 preparations: the fully intact working heart, the semi-intact working heart, and the isolated cardiac ganglion. In the intact WH, DA produced increases in contraction frequency and amplitude (Fig. 8). For both parameters, the DA dose–response relation revealed threshold responses in the nanomolar range, with gradual increases in the magnitude of the response up to the micromolar range (Fig. 8, A, C, and D). Despite increases in contraction amplitude of 80–100% above control values in the presence of high DA concentrations, no obvious changes in the shape of the contractions (i.e., in their temporal characteristics such as rise time and decay time) were noted in the presence of DA (Fig. 8B, inset). Phase plots in which the rate of change of the force was plotted against the force of contraction (Fig. 8B) had similar shapes in the presence of DA as under control conditions, indicating that the rates of rise and decay both changed in direct proportion to the increase in the force of contraction.
|
|
3 x 10–7 M) and EC50 of 6.8 x 10–7 M (Fig. 9D). The number of impulses per burst was not significantly changed by DA at any of the concentrations tested (Fig. 9E). In the ICG, application of DA increased burst frequency, burst duration, and the number of impulses per burst. It had a relatively small effect on the burst frequency (maximal increase about 20%), but with a low EC50, 1.4 x 10–8 M (Fig. 10, A and B). On the other hand, the effects of DA on the burst duration and the number of impulses were much larger (increases of 200 and 60%, respectively), but had much higher EC50 values, 1.2 x 10–6 M and 2.0 x 10–6 M, respectively (Fig. 10, C and D).
|
|
|
|
DISCUSSION |
|---|
|
An important aim of the present work was to establish the Callinectes cardiac system as a suitable experimental preparation for the study of extrinsic modulation and its functional consequences. For this, it was necessary at the outset to confirm the basic functional topography of the Callinectes cardiac system, even though this could be expected to be in many ways similar to that studied in other crab species. Indeed, the general morphological and physiological features of the Callinectes CG that we have described here (see also Hawkins and House 1978) are in agreement with descriptions in other crabs, including Eriocher japonicus (Tazaki 1972), Podophthalmus vigil (Berlind 1982), and Carcinus maenas (Saver et al. 1999). In particular, our characterization enables us to conclude that the number (5), position (3 anterior and 2 posterior), and physiological properties of the motor neurons in the Callinectes system correspond to the previous detailed description of crab cardiac functional anatomy in Portunus sanguinolentus (Tazaki and Cooke 1979a, b, 1983a).
Of particular importance for our subsequent investigation, the 5 motor neurons were found to fire in precise synchrony. In other crab species, the synchrony is thought to reflect highly effective electrical coupling close to the region of synaptic integration and impulse initiation of all 5 motor neurons. This critical integrative area is located within the anterior portion of the CG (Mirolli et al. 1987; Tazaki and Cooke 1979a, 1983a). The synchrony appears to be unique to crab cardiac systems. In lobsters, the motor neurons of the CG also fire in coordinated bursts but—because the individual neurons have unique, often multiple sites of impulse initiation—not in a precisely synchronized fashion (Friesen 1975a; Hartline 1967). The synchrony of motor neuron firing in the crab CG is experimentally advantageous because it permits monitoring of the motor output from any of the connectives projecting from the CG to the heart musculature. Recordings from muscle fibers demonstrate that excitatory junctional potentials corresponding to this motor pattern occur throughout the myocardium (Benson 1981; our observations). No evidence for synaptic drive to the muscle from any other source is observed.
Catecholaminergic innervation of the cardiac system
In this work we have used THli as a marker of catecholaminergic localization. For the reasons already presented in RESULTS, the catecholamine that the THli reflects in Callinectes, and probably other crustaceans, is very likely to be dopamine.
The distribution of THli in Callinectes (see also Wood and Derby 1996) indicates that the catecholaminergic innervation of the cardiac system originates from a single CNS neuron, the L-cell. The convoluted course of the L-cell axon that we have observed in the CNS is very characteristic. Maynard (1961b) reported that the largest fiber in the crab segmental nerve 1, which he designated the "a" fiber, followed a unique course on entering the subesophageal ganglion, turning "sharply" toward the circumesophageal connective. Using histofluorescent methods in Carcinus maenas, Cooke and Goldstone (1970) then determined that the "a" fiber originated from a large catecholaminergic cell in the commissural ganglion. They were able to trace the large axon of this cell to the brain, back to the subesophageal ganglion, and into a segmental nerve projecting to the pericardial organ. In Callinectes itself, Wood and Derby previously identified the L-cell and followed its axon to the brain and back past the commissural ganglion. These investigators likewise postulated that the Callinectes L-cell projected to the PO. Here we have confirmed this projection. In addition, we have made the novel finding, critical for understanding the regulation of the cardiac system, that a branch of the L-cell axon then continues beyond the PO, to the heart. Within the heart, the innervation of the cardiac ganglion by this fiber is consistent with previous descriptions of cardioaccelerator fibers in several crustacean species (Field and Larimer 1975; Maynard 1960; Sakurai and Yamagishi 1998; Yazawa and Kuwasawa 1994).
In studies of the stomatogastric system of lobsters, the L-cell was found to receive depolarizing input corresponding to the esophageal motor rhythm of the foregut (Selverston et al. 1976). Subsequently, the firing pattern of the L-cell of Homarus was shown to be influenced by 4 distinct foregut rhythms (Robertson and Moulins 1981). Given the previously demonstrated excitatory effects of dopamine on the pyloric central pattern generator in the stomatogastric ganglion (Anderson and Barker 1981), the L-cell was postulated to regulate the activity of the gut through a positive feedback loop by release of dopamine from its terminals in the PO (Robertson and Moulins 1981). The projections of the L-cell that we have documented here suggest that the L-cell may play an even broader integrative role that includes cardiac responses to increased metabolic or behavioral demands (see Guirguis and Wilkens 1995). The demonstration of long-lasting (16–18 h) increases in heart rate associated with food detection and consumption in Callinectes (McGaw and Reiber 2000) is consistent with such a broader role.
Neurons that correspond to the L-cell in a range of decapods all appear to exhibit a catecholaminergic phenotype: Carcinus maenas (Cooke and Goldstone 1970); Panulirus interruptus (Barker et al. 1979; Kushner and Barker 1983), Homarus gammarus (Cournil et al. 1984, 1994); Homarus americanus (Siwicki et al. 1987); Cancer irroratus and borealis (Marder 1987); Callinectes sapidus (Wood and Derby 1996; this study); and Macrobrachim rosenbergii (Sosa et al. 2002). However, there appears to be substantial variability in the cotransmitter content of L-cells. In Homarus gammarus (Cournil et al. 1984) and Macrobrachium rosenbergii (Sosa et al. 2002), the L-cell contains serotonin immunoreactivity. Proctolin-like immunoreactivity is present in the L-cell of Homarus americanus (Siwicki et al. 1987), Cancer irroratus and C. borealis (Marder et al. 1986), but not in Procambarus clarkii (Siwicki and Bishop 1986), Panulirus interruptus (Siwicki and Bishop 1986), or Callinectes, the subject of the present study (Wood and Derby 1996; Wood et al. 1996). In view of such cotransmitter diversity, it will be interesting to examine the generality of the L-cell projection to the CG that we have identified. It is possible that the cotransmitter diversity reflects somewhat different modes of use of the L-cell in different species. Some species may use the L-cell mostly for hormonal release through the PO, others for direct modulation of the CG, and still others in the dual mode of modulation that, we propose, occurs in Callinectes.
The limited distribution of THli within the CG appears to arise exclusively from the single pair of L-cell fibers that enter the heart by the dorsal nerves (Fig. 7; see also Yazawa and Kuwasawa 1994). The presence of dopamine within these fibers may account for earlier biochemical measurements of catecholamines in the lobster cardiac ganglion (Ocorr and Berlind 1983). The localization of THli does not support a role for dopamine as the neurotransmitter of the motor neurons, a function for which L-glutamate is currently a leading candidate (Benson 1981; Cooke 1966; Delgado et al. 2000; Yazawa et al. 1998). The absence of THli innervation in the region of the cell bodies of the posterior motor neurons (Fig. 7B) suggests that the innervation of the 5 motor neurons may not be uniform. Direct modulation of the posterior motor neurons cannot be excluded, however, because their synaptic input and impulse initiation occur in the anterior portion of the ganglion, in a region that receives substantial THli innervation (Fig. 7A; see Cooke 2002; Mirolli et al. 1987; Tazaki and Cooke 1983a). It is also notable that the THli projections are confined to the ganglion itself. In this regard, they differ from the "System II" cardioregulatory fibers described by Alexandrowicz (1932) and the catecholaminergic innervation of the hermit crab, where the regulatory axons innervate myocardial cells (Yazawa and Kuwasawa 1994). Finally, the localization of THli terminals to the neuropil and somatic regions of the ganglion indicates that the distal dendritic processes projecting into adjacent muscle fibers (Fig. 2B) are also not targets of this regulation. This contrasts to GABAergic inhibitory regulation for which extensive dendritic innervation has been observed ("System I" fiber of Alexandrowicz 1932; Delgado et al. 2000).
In sum, we propose that the pattern of L-cell innervation that we have found indicates a dual mode of action of the L-cell neurotransmitter, dopamine, on the cardiac system of Callinectes. Dopamine released from the L-cell terminals in the pericardial organs is likely to act in a neurohormonal fashion on the entire cardiac system, including its periphery, the cardiac musculature. At the same time, dopamine released from the terminals in the cardiac ganglion acts as a local modulator of the central motor pattern generated by the ganglion. We propose that this dual innervation provides an anatomical substrate for the physiological actions of dopamine that we have found, as discussed next.
Cardioactive actions of dopamine
The cardioactive effects observed here are in many ways similar to those reported in other arthropods where dopamine typically produces increases in contraction frequency and amplitude (Augustine et al. 1982; Berlind et al. 1970; Cooke and Sullivan 1982; Florey and Rathmayer 1978). Because dopamine also produces increases in burst frequency, burst duration, and the number of impulses per burst in isolated cardiac ganglia (Berlind 1998; Miller et al. 1984), it is easy to assume that all of the effects observed in the cardiac system are a simple consequence of its central actions. However, when the actions of dopamine are quantitatively compared on the CG with and without the peripheral cardiac musculature, as we have done here, it becomes clear that matters are likely to be considerably more complex.
The similarity between the basal contraction parameters of the S-IWH and the fully intact WH (Fig. 3, A1–A3), coupled with the comparable dose dependency of the effect of dopamine on contraction amplitude (Fig. 11A), support the conclusion that (except for the absolute magnitude of the contraction) the properties of the S-IWH faithfully reflect those of the intact system. In the S-IWH, and so presumably in the WH, there is essentially no effect of dopamine on the burst parameters of the underlying motor pattern, such as burst duration (Fig. 11C) or the number of impulses per burst (Fig. 11D). Yet there is a large increase in contraction amplitude (Fig. 11A). This increase could be a secondary consequence of the dopamine-induced increase in burst and contraction frequency (Fig. 11B; see Mahadevan et al. 2004). Alternatively or in addition, however, it could also be produced by a direct action of dopamine on the peripheral cardiac musculature. Peripheral effects of modulators, including dopamine, acting both presynaptically at neuromuscular junctions and postsynaptically on the myocytes themselves, are common in other muscles of decapods (e.g., Breen and Atwood 1983; Djokaj et al. 2001; Fischer and Florey 1983; Florey and Rathmayer 1978; Jorge-Rivera et al. 1998; Kravitz et al. 1980; Lingle 1981), other arthropods, and invertebrates generally (Calabrese 1989; Evans and Myers 1986; Worden 1998). A peripheral dopaminergic action would presumably be attributable to dopamine released neurohormonally from the pericardial organs (dashed arrows in the summary diagram presented in Fig. 12A and in more detail in Fig. 12B), given that the cardiac musculature is not directly innervated by the dopaminergic L-cell.
|
; see also Berlind 1998, 2001a). We propose therefore that the effect on frequency is achieved primarily by dopamine release from the projections of the L-cell that terminate in the area of the small interneurons (thin solid arrows in Fig. 12, A and B), which act as pacemakers of the crab cardiac system (Tazaki and Cooke 1979a, 1983a, b).
There is yet a third effect of dopamine, which is seen in the ICG and is thus presumably a direct central effect: the large increase in burst duration and the number of impulses per burst (Fig. 11, C and D). This effect is clearly different from that on frequency, given that it occurs at much higher dopamine concentrations. Interestingly, dopaminergic actions on the large neurons of the crabs Portunus and Podophthalmus, manifested in a somewhat comparable manner as a lowered threshold for eliciting repetitive driver potentials, occurred only with high dopamine concentrations (10 to 100 times higher than the actions on the small interneurons; Miller et al. 1984). We propose therefore that the third effect of dopamine may be achieved by release of dopamine from the L-cell terminals in the anterior motor neuron region of the CG (thick solid arrows in Fig. 12, A and B). The "high" DA concentrations required to produce these effects are still only of the order of 10–6 M, and thus quite possibly reached with endogenous release of dopamine. However, the physiological significance of these observations remains to be established.
The most intriguing feature of this third effect of dopamine is that it is seen in the isolated CG but not when the CG remains embedded within the cardiac musculature. Furthermore, as with frequency, even the basal values of these parameters, the burst duration and the number of impulses per burst, are different in the ICG and S-IWH (Fig. 3, B2 and B3). We conclude that, in the intact system, feedback from the cardiac musculature regulates the parameters of the motor pattern produced by the CG as well as the modulation of these parameters. Several feedback mechanisms that could help explain our data are already known to exist in crustacean cardiac systems. First, the CG burst duration is typically found to be reciprocally related to the burst frequency. This relation is attributable, at least in part, to the properties of the motor neuron driver potentials, which are smaller at higher frequencies (Tazaki and Cooke 1990). Because dopamine increases burst frequency by acting on the small pacemaker interneurons, this relation, opposing the simultaneous increases in burst duration and the number of impulses per burst produced by the action of dopamine directly on the motor neurons, could serve to maintain these parameters approximately constant (Fig. 12B), as we have observed is the case in the intact system. However, at least in its simplest form, this mechanism would provide purely central feedback, operating within the CG itself. More interestingly, Sakurai and Wilkens (2003) recently reported that increasing tension of the cardiac musculature [i.e., contraction amplitude (Fig. 12B)] exerts negative feedback effects on parameters of the motor pattern produced by the CG. Mechanistically, this kind of negative feedback from the periphery to the center could be implemented by direct mechanosensitive hyperpolarization of the motor neuron dendrites that extend into the muscle surrounding the CG (Fig. 2B; Sakurai and Wilkens 2003; see Cooke 2002) or by a retrograde diffusible messenger (e.g., NO: see Mahadevan et al. 2004).
Central-peripheral integration through extrinsic modulation
The relation between the CG motor pattern and contractions of the myocardium is not well understood and is likely to be complex. Development of tension in crustacean muscle fibers is thought to be directly related to the degree to which the muscle membrane is depolarized (Orkand 1962). For example, Anderson and Cooke (1971) showed that each burst of impulses from a lobster CG produced a complex synaptic depolarization that preceded and accompanied the early phase of cardiac contraction (see also Benson 1981). Contraction was graded and could be elicited with depolarizations as small as 5 mV. Regenerative membrane responses were not detected in the lobster myocardium, but they have been observed in other crustacean hearts (compiled in Anderson and Cooke 1971). Precisely to bridge such complexities of contraction–excitation coupling, a general analytical approach, termed the neuromuscular transform, was recently developed (Brezina et al. 2000a, b, 2003a, b). This approach simply considers the input–output relation between the motor neuron firing pattern and the muscle contraction. In the S-IWH preparation that we have developed here, we can record and, preliminary work (Fort et al. 2004) shows, also experimentally manipulate simultaneously, both the motor neuron firing pattern and the contractions. This ability promises to make the Callinectes cardiac system highly suitable to the neuromuscular-transform approach. Indeed, the work presented here has already produced a body of data that can begin to be analyzed in this way.
Work with the neuromuscular transform in Aplysia (Brezina et al. 2000b), as well as more general computational and neuroethological considerations (Chiel and Beer 1997), suggest that central motor commands and the properties of the peripheral musculature must be matched and coordinated if functional behavior is to be produced. This coordination must be maintained throughout all plastic changes in the behavior. Such coordination can ideally be implemented by extrinsic modulation, originating from a single source but ramifying to both the center and the periphery. In this work, we have documented the likely existence of such a mechanism in the Callinectes cardiac system. The anatomy of the L-cell suggests that it releases dopamine both as a neurohormone onto the entire heart and as a local neurotransmitter within the CG, and we have found multiple physiological effects of dopamine that probably correspond. Furthermore, by comparing the 3 preparations in which the cardiac musculature was removed from the CG to different degrees, we have found evidence for feedback coupling from the periphery to the center. Such feedback—in more complex systems, implemented by dedicated sensory neurons—is common in neuromuscular systems, and its presence immediately raises important dynamical issues, of stability for example, that the mechanisms of central-peripheral coordination and modulation must deal with. These issues were not addressed in the original work with the neuromuscular transform in Aplysia, largely because of a lack of suitable experimental preparation. In its exceptional simplicity and experimental tractability, yet already with multiple sites of modulation and feedback, we believe that the Callinectes cardiac system will prove to be a suitable preparation for the study of these questions.
|
|
GRANTS |
|---|
|
|
|
FOOTNOTES |
|---|
Address for reprint requests and other correspondence: M. W. Miller, Institute of Neurobiology, University of Puerto Rico, 201 Blvd del Valle, San Juan, Puerto Rico 00901 (E-mail: mmiller{at}rcm.upr.edu).
|
|
REFERENCES |
|---|
|
Alexandrowicz JS. Nervous organs in the pericardial cavity of the decapod Crustacea. J Mar Biol Assoc UK 31: 563–580, 1953.
Alexandrowicz JS and Carlisle DB. Some experiments on the function of the pericardial organs in Crustacea. J Mar Biol Assoc UK 32: 175–192, 1953.
Anderson M and Cooke IM. Neural activation of the heart of the lobster, Homarus americanus. J Exp Biol 55: 449–468, 1971.
Anderson WW and Barker DL. Synaptic mechanisms that generate network oscillations in the absence of discrete postsynaptic potentials. J Exp Zool 216: 187–191, 1981.[CrossRef][Web of Science][Medline]
Atwood HL. Crustacean neuromuscular mechanisms. Am Zool 7: 527–551, 1967.
Augustine GJ, Fetterer R, and Watson WH III. Amine modulation of the neurogenic Limulus heart. J Neurobiol 13: 61–74, 1982.[CrossRef][Web of Science][Medline]
Barker DL, Kushner PD, and Hooper NK. Synthesis of dopamine and octopamine in the crustacean stomatogastric nervous system. Brain Res 161: 99–113, 1979.[CrossRef][Web of Science][Medline]
Barthe JY, Mons N, Cattaert D, Geffard M, and Clarac F. Dopamine and motor activity in the lobster, Homarus gammarus. Brain Res 497: 368–373, 1989.[CrossRef][Web of Science][Medline]
Beltz BS. Distribution and functional anatomy of amine-containing neurons in decapod crustaceans. Microsc Res Tech 44: 105–120, 1999.[CrossRef][Web of Science][Medline]
Beltz BS and Kravitz EA. Mapping of serotonin-like immunoreactivity in the lobster nervous system. J Neurosci 3: 585–602, 1983.[Abstract]
Benson JA. Burst reset and frequency control of the neuronal oscillators in the cardiac ganglion of the crab, Portunus sanguinolentus. J Exp Biol 87: 285–313, 1980.
Benson JA. Synaptic and regenerative responses of cardiac muscle fibres in the crab, Portunus sanguinolentus. J Comp Physiol 143: 349–356, 1981.[CrossRef]
Berlind A. Neurohumoral and reflex control of scaphognathite beating in the crab Carcinus maenas. J Comp Physiol 116: 77–90, 1977.[CrossRef]
Berlind A. Spontaneous and repetitive driver potentials in crab cardiac ganglion neurons. J Comp Physiol 149: 263–276, 1982.[CrossRef]
Berlind A. Dopamine and 5-hydroxytryptamine actions on the cardiac ganglion of the lobster Homarus americanus. J Comp Physiol 182A: 363–376, 1998.[CrossRef]
Berlind A. Effects of haloperidol and phentolamine on the crustacean cardiac ganglion. Comp Biochem Physiol C Toxicol Pharmacol 130: 85–95, 2001a.[CrossRef][Web of Science][Medline]
Berlind A. Monoamine pharmacology of the lobster cardiac ganglion. Comp Biochem Physiol C Toxicol Pharmacol 128: 377–390, 2001b.[CrossRef][Web of Science][Medline]
Berlind A, Cooke IM, and Goldstone MW. Do the monoamines in crab pericardial organs play a role in peptide neurosecretion? J Exp Biol 53: 669–677, 1970.
Breen CA and Atwood HL. Octopamine—a neurohormone with presynaptic activity-dependent effects at crayfish neuromuscular junctions. Nature 303: 716–718, 1983.[CrossRef][Medline]
Brezina V, Orekhova IV, and Weiss KR. The neuromuscular transform: the dynamic, nonlinear link between motor neuron firing patterns and muscle contraction in rhythmic behaviors. J Neurophysiol 83: 207–231, 2000a.
Brezina V, Orekhova IV, and Weiss KR. Optimization of rhythmic behaviors by modulation of the neuromuscular transform. J Neurophysiol 83: 260–279, 2000b.
Brezina V, Orekhova IV, and Weiss KR. Neuromuscular modulation in Aplysia. I. Dynamic model. J Neurophysiol 90: 2592–2612, 2003a.
Brezina V, Orekhova IV, and Weiss KR. Neuromuscular modulation in Aplysia. II. Modulation of the neuromuscular transform in behavior. J Neurophysiol 90: 2613–2628, 2003b.
Brezina V and Weiss KR. Analyzing the functional consequences of transmitter complexity. Trends Neurosci 20: 538–543, 1997.[CrossRef][Web of Science][Medline]
Calabrese RL. Modulation of muscle and neuromuscular junctions in invertebrates. Semin Neurosci 1: 25–34, 1989.
Chiel HJ and Beer RD. The brain has a body: adaptive behavior emerges from interactions of nervous system, body and environment. Trends Neurosci 20: 553–557, 1997.[CrossRef][Web of Science][Medline]
Cooke IM. The sites of action of pericardial organ extract and 5-hydroxytryptamine in the decapod crustacean heart. Am Zool 6: 107–121, 1966.[Web of Science][Medline]
Cooke IM. Studies on the crustacean cardiac ganglion. Comp Biochem Physiol C Toxicol Pharmacol 91: 205–218, 1988.
Cooke IM. Reliable, responsive pacemaking and pattern generation with minimal cell numbers: the crustacean cardiac ganglion. Biol Bull 202: 108–136, 2002.
Cooke IM and Goldstone MW. Fluorescence localization of monoamines in crab neurosecretory structures. J Exp Biol 53: 651–668, 1970.
Cooke IM and Hartline DK. Neurohormonal alteration of integrative properties of the cardiac ganglion of the lobster Homarus americanus. J Exp Biol 63: 33–52, 1975.
Cooke IM and Sullivan RE. Hormones and neurosecretion. In: The Biology of Crustacea, vol. 3, Neurobiology: Structure and Function, edited by Atwood HL and Sandeman DC. New York: Academic Press, 1982, p. 205–290.
Cournil I, Casasnovas B, Helluy SM, and Beltz BS. Dopamine in the lobster Homarus gammarus. II. Dopamine-immunoreactive neurons and development of the nervous system. J Comp Neurol 362: 1–16, 1995.[CrossRef][Web of Science][Medline]
Cournil I, Geffard M, Moulins M, and Le Moal M. Coexistence of dopamine and serotonin in an identified neuron of the lobster nervous system. Brain Res 310: 397–400, 1984.[CrossRef][Web of Science][Medline]
Cournil I, Helluy SM, and Beltz BS. Dopamine in the lobster Homarus gammarus. I. Comparative analysis of dopamine and tyrosine hydroxylase immunoreactivities in the nervous system of the juvenile. J Comp Neurol 344: 455–469, 1994.[CrossRef][Web of Science][Medline]
Cropper EC, Lloyd PE, Reed W, Tenenbaum R, Kupfermann I, and Weiss KR. Multiple neuropeptides in cholinergic motor neurons of Aplysia: evidence for modulation intrinsic to the motor circuit. Proc Natl Acad Sci USA 84: 3486–3490, 1987.
Delgado J, Oyala E, and Miller MW. Localization of GABA- and glutamate-like immunoreactivity in the cardiac ganglion of the lobster Panulirus argus. J Neurocytol 29: 605–619, 2000.[CrossRef][Web of Science][Medline]
Díaz-Ríos M, Suess E, and Miller MW. Localization of GABA-like immunoreactivity in the central nervous system of Aplysia californica. J Comp Neurol 413: 255–270, 1999.[CrossRef][Web of Science][Medline]
Djokaj S, Cooper RL, and Rathmayer W. Presynaptic effects of octopamine, serotonin, and cocktails of the two modulators on neuromuscular transmission in crustaceans. J Comp Physiol A Sens Neural Behav Physiol 187: 145–154, 2001.
Edwards DH, Yeh SR, Musolf BE, Antonsen BL, and Krasne FB. Metamodulation of the crayfish escape circuit. Brain Behav Evol 60: 360–369, 2002.[CrossRef][Web of Science][Medline]
Evans PD and Myers CM. Peptidergic and aminergic modulation of insect skeletal muscle. J Exp Biol 124: 143–176, 1986.
Field LH and Larimer JL. The cardioregulatory system of crayfish: neuroanatomy and physiology. J Exp Biol 62: 519–530, 1975.
Fischer L and Florey E. Modulation of synaptic transmission and excitation–contraction coupling in the opener muscle of the crayfish, Astacus leptodactylus, by 5-hydroxytryptamine and octopamine. J Exp Biol 102: 187–198, 1983.
Florey E and Rathmayer W. The effects of octopamine and other amines on the heart and neuromuscular transmission in decapod crustaceans: further evidence for a role as neurohormone. Comp Biochem Physiol C Toxicol Pharmacol 61: 229–237, 1978.
Fort TJ, Brezina V, and Miller MW. Modulation of the crab cardiac system: assessment with controlled stimulus trains. Soc Neurosci Abstr 314.16, 2004.
Friesen WO. Physiological anatomy and burst pattern in the cardiac ganglion of the spiny lobster Panulirus interruptus. J Comp Physiol 101: 173–189, 1975a.[CrossRef]
Friesen WO. Synaptic interactions in the cardiac ganglion of the spiny lobster Panulirus interruptus. J Comp Physiol 101: 191–205, 1975b.[CrossRef]
Glanzman DL and Krasne FB. Serotonin and octopamine have opposite modulatory effects on the crayfish's lateral giant escape reaction. J Neurosci 3: 2263–2269, 1983.[Abstract]
Goldstone MW and Cooke IM. Histochemical localization of monoamines in the crab central nervous system. Z Zellforsch Mikrosk Anat 116: 7–19, 1971.[CrossRef][Web of Science][Medline]
Guirguis MS and Wilkens JL. The role of the cardioregulatory nerves mediating heart rate responses to locomotion, reduced stroke volume, and neurohormones in Homarus americanus. Biol Bull 188: 179–185, 1995.[Abstract]
Hagiwara S. Nervous activities of the heart of Crustacea. Ergeb Biol 24: 287–311, 1961.[Medline]
Harris-Warrick RM, Flamm RE, Johnson BR, and Katz PS. Modulation of neural networks in Crustacea. Am Zool 29: 1305–1320, 1988.
Harris-Warrick RM, Johnson BR, Peck JH, Kloppenburg P, Ayali A, and Sharbinski J. Distributed effects of dopamine modulation in the crustacean pyloric network. In: Neuronal Mechanisms for Generating Locomotor Activity, edited by Kiehn O, Harris-Warrick RM, Jordan LM, Hultborn H, and Kudo N. New York: The New York Academy of Sciences, 1998, vol. 860, p. 155–167.
Harris-Warrick RM and Marder E. Modulation of neural networks for behavior. Annu Rev Neurosci 14: 39–57, 1991.[CrossRef][Web of Science][Medline]
Hartline DK. Impulse identification and axon mapping of the nine neurons in the cardiac ganglion of the lobster. J Exp Biol 47: 327–340, 1967.
Hartline DK. Integrative neurophysiology of the lobster cardiac ganglion. Am Zool 19: 53–65, 1979.[Web of Science]
Hawkins WD and House HD. A light and electron microscopic study of the cardiac ganglion of the blue crab Callinectes sapidus Rathbun. Trans Am Microsc Soc 97: 363–380, 1978.
Hultborn H and Kiehn O. Neuromodulation of vertebrate motor neuron membrane properties. Curr Opin Neurobiol 2: 770–775, 1992.[CrossRef][Medline]
Jorge-Rivera JC, Sen K, Birmingham JT, Abbott LF, and Marder E. Temporal dynamics of convergent modulation at a crustacean neuromuscular junction. J Neurophysiol 80: 2559–2570, 1998.
Katz PS. editor. Beyond Neurotransmission: Neuromodulation and Its Importance for Information Processing. New York: Oxford Univ. Press, 1999.
Katz PS and Frost WN. Intrinsic neuromodulation: altering neuronal circuits from within. Trends Neurosci 19: 54–61, 1996.[CrossRef][Web of Science][Medline]
Kravitz EA. Hormonal control of behavior: amines and the biasing of behavioral output in lobsters. Science 241: 1775–1781, 1988.
Kravitz EA, Glusman S, Harris-Warrick RM, Livingstone MS, Schwarz T, and Goy MF. Amines and a peptide as neurohormones in lobsters: actions on neuromuscular preparations and preliminary behavioural studies. J Exp Biol 89: 159–175, 1980.
Kupfermann I. Modulatory actions of neurotransmitters. Annu Rev Neurosci 2: 447–465, 1979.[CrossRef][Web of Science][Medline]
Kushner PD and Barker DL. A neurochemical description of the dopaminergic innervation of the stomatogastric ganglion of the spiny lobster. J Neurobiol 14: 17–28, 1983.[CrossRef][Web of Science][Medline]
Kushner PD and Maynard EA. Localization of monoamine fluorescence in the stomatogastric nervous system of lobsters. Brain Res 129: 13–28, 1977.[CrossRef][Web of Science][Medline]
Lingle C. The modulatory action of dopamine on crustacean foregut neuromuscular preparations. J Exp Biol 94: 285–299, 1981.
Ma PM, Beltz BS, and Kravitz EA. Serotonin-containing neurons in lobsters: their role as gain-setters in postural control mechanisms. J Neurophysiol 68: 36–54, 1992.
Mahadevan A, Lappé J, Rhyne RT, Cruz-Bermúdez ND, Marder E, and Goy MF. Nitric oxide inhibits the rate and strength of cardiac contractions in the lobster Homarus americanus by acting on the cardiac ganglion. J Neurosci 24: 2813–2824, 2004.
Marder E. Neurotransmitters and neuromodulators. In: The Crustacean Stomatogastric System: A Model for the Study of Central Nervous System, edited by Selverston AI and Moulins M. Heidelberg, Germany: Springer-Verlag, 1987, p. 263–300.
Marder E, Hooper SL, and Siwicki KK. Modulatory action and distribution of the neuropeptide proctolin in the crustacean stomatogastric nervous system. J Comp Neurol 243: 454–467, 1986.[CrossRef][Web of Science][Medline]
Marder E and Thirumalai V. Cellular, synaptic, and network effects of neuromodulation. Neural Networks 15: 479–493, 2002.[CrossRef][Web of Science][Medline]
Maynard DM. Circulation and heart function. In: The Physiology of Crustaceans, vol. 1, edited by Waterman TH. New York: Academic Press, 1960, p. 161–226.
Maynard DM. Thoracic neurosecretory structures in Brachyura. I. Gross anatomy. Biol Bull Mar Biol Lab Woods Hole 121: 316–329, 1961a.
Maynard DM. Thoracic neurosecretory structures in Brachyura. II. Secretory neurons. Gen Comp Endocrinol 1: 237–263, 1961b.[CrossRef][Web of Science][Medline]
Maynard DM. Integration in crustacean ganglia. Symp Soc Exp Biol 20: 111–149, 1965.
Maynard DM and Maynard EA. Thoracic neurosecretory structures in Brachyura. III. Microanatomy of peripheral structures. Gen Comp Endocrinol 2: 12–28, 1962.[CrossRef][Web of Science][Medline]
Maynard DM and Welsh JM. Neurohormones of the pericardial organs of brachyuran crustaceans. J Physiol 149: 215–227, 1959.
McGaw IJ and Reiber CL. Integrated physiological responses to feeding in the blue crab Callinectes sapidus. J Exp Biol 203: 359–368, 2000.[Abstract]
Mercier AJ, Orchard I, and Schmoeckel A. Catecholaminergic neurons supplying the hindgut of the crayfish Procambarus clarkii. Can J Zool 69: 2778–2785, 1991.
Meyrand P and Marder E. Matching neural and muscle oscillators: control by FMRFamide-like peptides. J Neurosci 11: 1150–1161, 1991.[Abstract]
Meyrand P and Moulins M. Myogenic oscillatory activity in the pyloric rhythmic motor system of Crustacea. J Comp Physiol A Sens Neural Behav Physiol 158: 489–503, 1986.
Miller MW, Alevizos A, Cropper EC, Vilim FS, Karagogeos D, Kupfermannn I, and Weiss KR. Localization of myomodulin-like immunoreactivity in the central nervous system and peripheral tissues of Aplysia californica. J Comp Neurol 314: 627–644, 1991.[CrossRef][Web of Science][Medline]
Miller MW, Benson JA, and Berlind A. Excitatory effects of dopamine on the cardiac ganglia of the crabs Portunus sanguinolentus and Podophthalmus vigil. J Exp Biol 108: 97–118, 1984.
Miller MW, Parnas H, and Parnas I. Dopaminergic modulation of neuromuscular transmission in the prawn. J Physiol 363: 363–375, 1985.
Miller MW and Sullivan RE. Some effects of proctolin on the cardiac ganglion of the Maine lobster, Homarus americanus (Milne Edwards). J Neurobiol 12: 629–639, 1981.[CrossRef][Web of Science][Medline]
Mirolli M, Cooke IM, Talbott SR, and Miller MW. Structure and localization of synaptic complexes in the cardiac ganglion of a portunid crab. J Neurocytol 16: 115–130, 1987.[CrossRef][Web of Science][Medline]
Mulloney B, Acevedo LD, and Bradbury AG. Modulation of the crayfish swimmeret rhythm by octopamine and the neuropeptide proctolin. J Neurophysiol 58: 584–597, 1987.
Ocorr KA and Berlind A. The identification and localization of a catecholamine in the motor neurons of the lobster cardiac ganglion. J Neurobiol 14: 51–59, 1983.[CrossRef][Web of Science][Medline]
Orkand RK. The relation between membrane potential and contraction in single crayfish muscle fibers. J Physiol 161: 143–159, 1962.
Pasztor VM and Bush BM. Peripheral modulation of mechano-sensitivity in primary afferent neurons. Nature 326: 793–795, 1987.[CrossRef][Medline]
Pearson KG. Common principles of motor control in vertebrates and invertebrates. Annu Rev Neurosci 16: 265–297, 1993.[Web of Science][Medline]
Pulver SR and Marder E. Neuromodulatory complement of the pericardial organs in the embyonic lobster Homarus americanus. J Comp Neurol 451: 79–90, 2002.[CrossRef][Web of Science][Medline]
Pulver SR, Thirumalai V, Richards KS, and Marder E. Dopamine and histamine in the developing stomatogastric system of the lobster Homarus americanus. J Comp Neurol 462: 400–414, 2003.[CrossRef][Web of Science][Medline]
Rajashekhar KP and Wilkens JL. Dopamine and nicotine, but not serotonin, modulate the crustacean ventilatory pattern generator. J Neurobiol 23: 680–691, 1992.[CrossRef][Web of Science][Medline]
Robertson RM and Moulins M. A corollary discharge of total foregut motor activity is monitored by a single interneurone in the lobster Homarus gammarus. J Physiol (Paris) 77: 823–827, 1981.
Sakurai A and Wilkens JL. Tension sensitivity of the heart pacemaker neurons in the isopod crustacean Ligia pallasii. J Exp Biol 206: 105–115, 2003.
Sakurai A and Yamagishi H. Identification of two cardioacceleratory neurons in the isopod crustacean, Ligia exotica and their effects on cardiac ganglion cells. J Comp Physiol A Sens Neural Behav Physiol 182: 145–152, 1998.[CrossRef]
Sandeman D, Sandeman R, Derby C, and Schmidt M. Morphology of the brain of crayfish, crabs, and spiny lobsters: a common nomenclature for homologous structures. Biol Bull 183: 304–326, 1992.[Abstract]
Saver MA, Wilkens JL, and Syed NI. In situ and in vitro identification and characterization of cardiac ganglion neurons in the crab, Carcinus maenas. J Neurophysiol 81: 2964–2976, 1999.
Schneider H, Trimmer BA, Rapus J, Eckert M, Valentine DE, and Kravitz EA. Mapping of octopamine-immunoreactive neurons in the central nervous system of the lobster. J Comp Neurol 329: 129–142, 1993.[CrossRef][Web of Science][Medline]
Selverston AI, Russell DF, Miller JP, and King DG. The stomatogastric nervous system: structure and function of a small neural network. Prog Neurobiol 7: 215–290, 1976.[CrossRef][Medline]
Shimahara T. The inhibitory post-synaptic potential in the cardiac ganglion cell of the lobster, Panulirus japonicus. Sci Rep Tokyo Kyoiku Daigaku B 14: 9–26, 1969.
Sillar KT, McLean DL, Fischer H, and Merrywest SD. Fast inhibitory synapses: targets for neuromodulation and development of vertebrate motor behaviour. Brain Res Rev 40: 130–140, 2002.[CrossRef][Medline]
Siwicki KK, Beltz BS, and Kravitz EA. Proctolin in identified serotonergic, dopaminergic, and cholinergic neurons in the lobster, Homarus americanus. J Neurosci 7: 522–532, 1987.
Siwicki KK and Bishop CA. Mapping of proctolinlike immunoreactivity in the nervous systems of lobster and crayfish. J Comp Neurol 243: 435–453, 1986.[CrossRef][Web of Science][Medline]
Sosa MA, Hernández CM, Rivera N, and Rolon S. Tyrosine hydroxylase and FMRFamide immunohistochemistry in the CNS of the freshwater prawn Macrobrachium rosenbergii. Program No. 59.2. 2002 Abstract Viewer/Itinerary Planner. Washington, DC: Society for Neuroscience, online, 2002.
Sullivan RE, Friend BJ, and Barker DL. Structure and function of spiny lobster ligamental nerve plexuses: evidence for synthesis, storage and secretion of biogenic amines. J Neurobiol 8: 581–605, 1977.[CrossRef][Web of Science][Medline]
Sullivan RE and Miller MW. Dual effects of proctolin on the rhythmic burst activity of the cardiac ganglion. J Neurobiol 15: 173–196, 1984.[CrossRef][Web of Science][Medline]
Tazaki K. The burst activity of different cell regions and intercellular co-ordination in the cardiac ganglion of the crab, Eriocheir japonicus. J Exp Biol 57: 713–726, 1972.
Tazaki K and Cooke IM. Spontaneous electrical activity and interaction of large and small cells in the cardiac ganglion of the crab, Portunus sanguinolentus. J Neurophysiol 42: 975–999, 1979a.
Tazaki K and Cooke IM. Isolation and characterization of slow, depolarizing responses of cardiac ganglion neurons in the crab, Portunus sanguinolentus. J Neurophysiol 42: 1000–1021, 1979b.
Tazaki K and Cooke IM. Topographical localization of function in the cardiac ganglion of the crab, Portunus sanguinolentus. J Comp Physiol 151: 311–328, 1983a.[CrossRef]
Tazaki K and Cooke IM. Neural mechanisms underlying rhythmic bursts in crustacean cardiac ganglia. In: Neural Origin of Rhythmic Movements, vol. 37, Symp. Soc. Exp. Biol., edited by Roberts A and Roberts B. Cambridge, UK: Cambridge Univ. Press, 1983b, p. 129–157.
Tazaki K and Cooke IM. Characterization of Ca current underlying burst formation in lobster cardiac ganglion neurons. J Neurophysiol 63: 370–384, 1990.
Tierney AJ, Kim T, and Abrams R. Dopamine in crayfish and other crustaceans: distribution in the central nervous system and physiological functions. Microsc Res Tech 60: 325–335, 2003.[CrossRef][Web of Science][Medline]
Weiss KR, Brezina V, Cropper EC, Hooper SL, Miller MW, Probst WC, Vilim FS, and Kupfermann I. Peptidergic co-transmission in Aplysia: functional implications for rhythmic behaviors. Experientia 48: 456–463, 1992.[CrossRef][Web of Science][Medline]
Welsh JH and Maynard DM. Electrical activity of a simple ganglion. Fed Proc 10: 145, 1951.
Wood DE. Neuromodulation of rhythmic motor patterns in the blue crab Callinectes sapidus by amines and the peptide proctolin. J Comp Physiol A Sens Neural Behav Physiol 177: 335–349, 1995.[Medline]
Wood DE and Derby CD. Distribution of dopamine-like immunoreactivity suggests a role for dopamine in the courtship display behavior of the blue crab, Callinectes sapidus. Cell Tissue Res 285: 321–330, 1996.[CrossRef][Web of Science][Medline]
Wood DE, Nishikawa M, and Derby CD. Proctolin-like immunoreactivity and identified neurosecretory cells as putative substrates for modulation of courtship display behavior in the blue crab, Callinectes sapidus. J Comp Neurol 368: 153–163, 1996.[CrossRef][Web of Science][Medline]
Worden MK. Modulation of vertebrate and invertebrate neuromuscular junctions. Curr Opin Neurobiol 8: 740–745, 1998.[CrossRef][Web of Science][Medline]
Xin Y, Hurwitz I, Perrins R, Evans CG, Alexeeva V, Weiss KR, and Kupfermann I. Actions of a pair of identified cerebral-buccal interneurons (CBI-8/9) in Aplysia that contain the peptide myomodulin. J Neurophysiol 81: 507–520, 1999.
Yazawa T and Kuwasawa K. Dopaminergic acceleration and GABAergic inhibition in extrinsic neural control of the hermit crab heart. J Comp Physiol A Sens Neural Behav Physiol 174: 65–75, 1994.
Yazawa T, Takaka K, Yasumatsu M, Otokawa M, Aihara Y, Ohsuga K, and Kuwawawa K. A pharmacological and HPLC analysis of the excitatory transmitter of the cardiac ganglion in the heart of the isopod crustacean Bathynomus doederleini. Can J Physiol Pharmacol 76: 599–604, 1998.[CrossRef][Web of Science][Medline]
This article has been cited by other articles:
|
|
 |
|
  D. M. Blitz, R. S. White, S. R. Saideman, A. Cook, A. E. Christie, F. Nadim, and M. P. Nusbaum A newly identified extrinsic input triggers a distinct gastric mill rhythm via activation of modulatory projection neurons J. Exp. Biol., March 15, 2008; 211(6): 1000 - 1011. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 T. J. Fort, V. Brezina, and M. W. Miller Regulation of the Crab Heartbeat by FMRFamide-Like Peptides: Multiple Interacting Effects on Center and Periphery J Neurophysiol, November 1, 2007; 98(5): 2887 - 2902. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
N. D. Cruz-Bermudez and E. Marder Multiple modulators act on the cardiac ganglion of the crab, Cancer borealis J. Exp. Biol., August 15, 2007; 210(16): 2873 - 2884. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
G. E. Serrano, C. Martinez-Rubio, and M. W. Miller Endogenous Motor Neuron Properties Contribute to a Program-Specific Phase of Activity in the Multifunctional Feeding Central Pattern Generator of Aplysia J Neurophysiol, July 1, 2007; 98(1): 29 - 42. [Abstract] [Full Text] [PDF]
|
|
|
|
|
|
T. J. Fort, K. Garcia-Crescioni, H.-J. Agricola, V. Brezina, and M. W. Miller Regulation of the Crab Heartbeat by Crustacean Cardioactive Peptide (CCAP): Central and Peripheral Actions J Neurophysiol, May 1, 2007; 97(5): 3407 - 3420. [Abstract] [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| Visit Other APS Journals Online |
TOP
ABSTRACT
INTRODUCTION
