- freely available
Mar. Drugs 2013, 11(12), 4698-4723; doi:10.3390/md11124698
Published: 28 November 2013
Abstract: Voltage-gated sodium channels (VGSCs) play a central role in the generation and propagation of action potentials in excitable neurons and other cells and are targeted by commonly used local anesthetics, antiarrhythmics, and anticonvulsants. They are also common targets of neurotoxins including shellfish toxins. Shellfish toxins are a variety of toxic secondary metabolites produced by prokaryotic cyanobacteria and eukaryotic dinoflagellates in both marine and fresh water systems, which can accumulate in marine animals via the food chain. Consumption of shellfish toxin-contaminated seafood may result in potentially fatal human shellfish poisoning. This article provides an overview of the structure, bioactivity, and pharmacology of shellfish toxins that act on VGSCs, along with a brief discussion on their pharmaceutical potential for pain management.
1. Overview of Voltage-Gated Sodium Channels
Voltage-gated sodium channels (VGSCs) are transmembrane proteins that form ion channels, conducting sodium ion (Na+) through the cell plasma membrane upon activation. VGSCs are responsible for the rising phase of action potentials in neurons, myocytes, and other excitable cells and play a key role in many electrophysiological processes [1,2]. VGSCs consist of an α-subunit (220–260 kDa) that forms the ion conduction core and one or more auxiliary β-subunits (30–40 kDa) [1,3,4,5,6,7]. The α-subunit consists of four homologous but non-identical transmembrane domains (I to IV), each of which contains six transmembrane segments (S1–S6) and a short membrane-penetrating segment (SS1 and SS2) between segments S5 and S6 (Figure 1) [1,8,9,10,11]. The α-subunit contains functional structures of the central pore (S5 and S6), ion selectivity filter (SS1 and SS2), and voltage sensors (S1 to S4) . The S4 segment contains analogous and repeated motifs in which a lysine or arginine residue is followed by two hydrophobic amino acids [8,12]. Positive charges on the lysine or arginine residues, which are called gating charges, move across the electric field when membrane potential changes, resulting in conformational changes and opening of the central pore. The inactivation gate contains three hydrophobic amino acid residues Ile-Phe-Met (IFM) and is formed by an intracellular linker between transmembrane domains III and IV. Following movement of the voltage sensors, the inactivation gate plugs the pore and prevents further Na+ flow through the channel [13,14].
In mammalian cells, four auxiliary β-subunits (β1–β4; genes, SCN1B–SCN4B) have been identified up to now. The β-subunit consists of four domains including an extracellular N-terminal signal peptide, an immunoglobulin domain, a transmembrane domain, and an intracellular C-terminal domain . Studies conducted on co-expression of α- and β-subunits have demonstrated that β-subunits modulate the kinetics and voltage-dependence of the opening and closing (gating) of the channel. More recently, β-subunits have also been reported to modulate cell adhesion and migration [7,15].
In mammalian cells, nine isoforms of VGSCs (Nav1.1–Nav1.9) have been identified and functionally expressed (Table 1) [2,16,17]. The nine isoforms are more than 50% identical in amino acid sequence in transmembrane and extracellular domains. Among the nine isoforms, Nav1.1–1.4, Nav1.6, and Nav1.7 are blocked by nanomolar concentrations of tetrodotoxin (TTX), a guanidinium toxin selectively targeting on VGSCs and generally being used as the agent to classify VGSCs, and, hence, categorized as TTX-sensitive (TTX-S) [18,19], while Nav1.5, Nav1.8, and Nav1.9 are resistant to micromolar or higher concentrations of TTX and are generally categorized as TTX-resistant (TTX-R). The nine VGSC isoforms have different tissue distributions . Nav1.1–1.3 and Nav1.6 are mainly distributed in central nervous system (CNS), Nav1.7, Nav1.8, and Nav1.9 are highly expressed in peripheral nervous system (PNS), and Nav1.4 and 1.5 are selectively expressed in adult skeletal and heart muscles, respectively. Five isoforms of VGSCs, Nav1.1 and Nav1.6–1.9 are found to be expressed in dorsal root ganglion neurones. In addition to the nine isoforms, a potential tenth isoform (Nax) has been identified. It shows approximately 50% identity to the Nav1 subfamily of VGSCs. However, Nax exhibits key structural differences in functionally important regions of the voltage sensor and the inactivation gate. In addition, Nax expressed in heterologous cells is not functionally active, suggesting that Nax may not function as a VGSC.
A variety of toxins and drugs have been found to act on VGSCs. These compounds provide invaluable pharmacological tools for the investigation of VGSCs. The mechanisms of action of these agents have been studied by site-directed mutagenesis, binding studies and electrophysiological methods [1,9]. Based on their functional effects and receptor binding sites, neurotoxins targeting VGSCs are generally classified into three groups: (1) Pore-blocking toxins such as TTX, saxitoxin (STX), and μ-conotoxins, which block Na+ conductance via binding to the outer mouth of the pore (site 1); (2) toxins which bind to intramembrane receptor site 2 (e.g., veratridine, batrachotoxin, and grayanotoxin), or 5 (e.g., brevetoxin and ciguatoxin) in the activated state of channels, or site 7 (e.g., pyrethrins), resulting in persistent activation and negative shift in voltage-dependency of activation; (3) toxins which bind to extracellular receptor site 3 (e.g., α-scorpion toxins, sea-anemone toxins, and spider toxins) or 4 (e.g., β-scorpion toxins and spider toxins), resulting in delayed inactivation and shift in voltage-dependency of activation, respectively. Conotoxin-TxVIA binding to receptor site 6 produces the same physiological effects on Na+ currents as toxins binding to receptor site 3, though the binding of conotoxin-TxVIA is voltage-independent. Both, sites 6 and 3 are allosteric binding sites [1,21].
|Table 1. Properties of the α-subunit of voltage-gated sodium channels (VGSCs) [2,16,17].|
|α-Subunits||Gene Symbol||Chromosomal Location1 ♦||TTX-S/R ♦♦||Predominant Location||Expression in DRG ♦♦♦||Effect of Mutation|
|S||CNS (embryonic)||upregulated after axotomy||None reported|
|S||skeletal muscle||−||Myotonia, periodic paralysis|
|R||heart muscle||−||Long-QT, Brugada syndrome, Progressive familial heart block|
|S||CNS, PNS, glia nodes of Ranvier||+++||Cerebellar atrophy|
|S||PNS Schwann cell||+++||Increased and decreased pain sensitivity|
|R||PNS (sensory neurons)||+++||None reported|
|R||heart, uterus, glia, PNS smooth muscle||+||−|
♦ M: mouse, H: human. ♦♦ S: sensitive, R: resistant. ♦♦♦ +++: rich, +: present, −: absent. TTX: tetrodotoxin, DRG: dorsal root ganglion.
2. Shellfish Toxins
Shellfish toxins are a variety of potent toxic secondary metabolites primarily produced by prokaryotic cyanobacteria in both marine and fresh water ecosystems and eukaryotic dinoflagellates in marine water [22,23,24,25,26]. Many novel shellfish toxins have been reported in the last two decades [27,28,29]. In recent decades, dinoflagellates, cyanobacteria, and other algae have been causing harmful algal blooms (HABs) in many regions of the world with increasing frequency and global distribution owing to human activities and water eutrophication [30,31,32]. Some HAB species produce potent toxins, which are bioaccumulated in shellfish such as clams, oysters, whelks, mussels, conch, coquinas, and other filter-feeding molluscs via the food web . Low concentrations of shellfish toxins usually produce no significantly adverse effects on shellfish, marine ecosystem, or humans. However, blooms of HAB species may result in accumulation of high concentrations of shellfish toxins in seafood, which could be fatally harmful to humans and cause a sharp downturn in seafood trade [29,30,31,32].
Shellfish toxins show diversity in structures and biological activities. Most shellfish toxins are neurotoxins which block nerve impulses via targeting specific receptors including voltage-gated Na+ , K+, and Ca2+ channels, specific nicotinic acetylcholine receptor (nAChR) subtypes, and Na+-K+ ATPase [33,34,35,36,37]. Consumption of shellfish toxin-contaminated seafood causes four major seafood-poisoning syndromes: paralytic shellfish poisoning, neurotoxic shellfish poisoning, amnesic shellfish poisoning, and diarrheic shellfish poisoning . Since STX, the first and best-known member of paralytic shellfish toxins (PSTs), was discovered in 1957, 57 STX analogs have been reported to date [38,39]. STX, and analogs, selectively targeting VGSCs are valuable tool compounds for structure and function investigation of VGSCs [40,41]. More importantly, STX as a VGSC blocker prolongs the duration of anesthesia when combined with other local anesthetics . Its analog gonyautoxin displays therapeutic potential in treatment of chronic anal fissure and chronic tension-type headache [43,44]. This review article provides an overview of chemistry, structure and bioactivity of shellfish toxins acting on VGSCs. Both widely known toxins (e.g., saxitoxins, gonyuantoxins, and brevetoxins) and recently discovered toxins (e.g., crossbyanols, hoiamide A and B, and Palmyramide A) are reviewed. We also provide a brief discussion on the pharmaceutical potential of shellfish toxins.
STX and its analogs are highly potent neurotoxins known as PSTs. PSTs are produced by marine dinoflagellates and several fresh water species of cyanobacteria [22,23,24,27]. In the marine ecology, three species of dinoflagellate produce STXs, belonging to the genera Alexandrium, Pyrodinium and Gymnodinium, while five filamentous species of cyanobacteria in freshwater environment, including Anabaena circinalis, Aphanizomenon sp., Aphanizomenon gracile, Cylindrospermopsis raciborskii, and Lyngbya wollei, have been reported to produce STXs. Blooms of these toxic species have generated lethal impact on marine and freshwater ecosystems and humans, causing paralytic shellfish poisoning in humans, mass deaths of fish, birds, and other native animals and livestock, and contamination of freshwater resources [45,46,47,48,49].
Among marine neurotoxins, STX is one of the most toxic and the most harmful to humans, which usually causes paralytic shellfish poisoning (PSP). Inadvertent ingestion of STX or its analogs quickly causes symptoms of poisoning within 30 min, including a tingling or burning sensation in the lips, tongue, and throat, and facial numbness. Additional symptoms may include perspiration, diarrhea, and vomiting [50,51,52]. In cases of acute and severe poisoning, numbness may quickly spread to the neck and extremities, and symptoms may further develop to muscular weakness, loss of motor coordination, and, eventually, paralysis. Serious neurological symptoms may culminate in respiratory arrest, cardiovascular shock, and death . The lethal oral dosage in human is 1–4 mg/person, depending on the physiological condition and gender of the victim [27,51]. There are currently no clinically approved antidotes to STX poisoning. Common treatments during early stages of PSP include removal of unabsorbed toxins with activated charcoal and artificial respiration. The half-life of STX in human is approximately 90 min. Survival opportunity significantly increases after 12 h from initial exposure [52,54]. STX and its analogs differ significantly in toxicity, with N-sulfo-carbamoyl derivatives being 10- to 100-fold less potent than the carbamate analogs [51,55]. STX and its analogs may potentially be used as biochemical weapons and have been listed as Schedule 1 chemical intoxicants by the Organization for the Prohibition of Chemical Weapons (OPCW). Their manufacture, use, transfers, and reuses are hence strictly regulated by OPCW .
STX was first isolated in pure form from Alaskan butter clam, Saxidomus gigangteus in 1957 . However, its crystal structure was not determined until 1975 due to the difficulty in finding the appropriate crystallization condition [56,57]. STX (C10H17N7O4, MW: 299 Da) is a heat-stable and water-soluble neurotoxic alkaloid. The core structure of STX and its analogs is a trialkyl tetrahydropurine, with the NH2 groups at positions 2 and 8 forming the two permanent guanidinium moieties [57,58,59,60]. STX has two pKa values, 8.22 and 11.28, for the 1, 2, 3 and 7, 8, 9 guanidinium groups, respectively [58,61]. STX and its analogs can be divided into four structural categories based on variations in functional groups at four defined positions (Figure 2): (1) Carbamate toxins containing a carbamoyl group at the R1 position, such as STX, neo-saxitoxin, and gonyautoxins 1–6; (2) N-sulfocarbamoyl toxins, such as C1–C4; (3) decarbamoyl toxins; and (4) deoxydecarbamoyl toxins [27,62].
STX was the first discovered and the most well known potent neurotoxin that selectively targets VGSCs besides TTX. STX binds to VGSCs with high affinity (Kd ~2 nM), resulting in blockade of muscle action potential and respiratory paralysis . Three models have been proposed for the mechanisms of VGSC blockage by STX . Hille et al. postulated a plugging model in 1975, in which STX penetrates the VGSC protein and binds at the bottom of the channel, forming an ion pair with an anionic site rather than deeply plugging the channel. Nonetheless, the plugging model is unsuitable for unfolded gonyautoxins owing to the lack of anticipated steric interactions . Subsequently, Kao and Walker proposed another model in which the toxin molecule binds at the outside edge of the channel with the guanidinium group on top of the channel entrance . Meanwhile, Shimizu proposed a third model called three-point binding model, in which two hydrogen bonds with the ketal OHs and ion pairing of the guanidinium group with an anionic site on the outside surface of the membrane are speculated . However, all the three models did not explain the precise action mechanism of the blockage of VGSCs by STX on molecular level until the successful cloning of VGSCs and the subsequent identification of the binding site of STX in the channel.
In 1986, Numa and Noda reported the first successful cloning of VGSCs . Later, Numa and coworkers pioneered using site-directed mutagenesis to investigate the binding site of STX in Nav1.2. Their results demonstrated that changing glutamic acid residue 387 to glutamine (E387Q) and mutations of charged amino acid residues of SS2 in the four domains strongly reduced binding sensitivity. STX was found to bind to Nav1.2 through electrostatic interactions between the 7, 8, 9-guanidinium moiety of STX and certain fixed amino acid residues in the lip of the channel pore [64,67]. These fixed amino acid residues are located in segment SS2 of the S6 transmembrane segment in all four domains, forming two rings that interact with the STX molecule [40,41]. The first ring contains D384 in domain I, E942 in domain II, K1423 in domain III, and A1714 in domain IV. The second ring contains E387 in domain I, E945 in domain II, M1425 in domain III, and D1717 in domain IV. Therefore, studies reported thus far demonstrate that STX blocks VGSCs through binding to receptor site 1 [40,41]. The specific binding mode enables STX to effectively block the inward flow of Na+ into cell. More recently, Walker et al. reported a two amino acid variation of human Nav1.7, which results in dramatic differences in the binding affinity for STX; the two residues are Thr1398 and Ile1399 of domain III, which occur as Met and Asp in other VGSC isoforms, as the critical determinants of STX binding affinity. Their findings provide possibility that selective blockers of hNav1.7 could be designed around the site 1 for the uniqueness of its outer pore structure .
STX also binds to voltage-gated K+ and Ca2+ channels, however, the binding mode is different from that with VGSCs. STX modulates the gating of human K+ channels rather than directly blocking the pore through binding to extracellular sites of the channel . For Ca2+ channels, STX was found to possibly bind to at sites located in the selectivity filter, resulting in incomplete blockage of the channel .
In marine ecosystems, dinoflagellates produce two types of lipid soluble toxins that cause neurotoxic shellfish poisoning with lethal effects on marine life including fish, sea birds, and marine mammals [49,69,70,71,72,73,74,75]. Brevetoxins are known as neurotoxic shellfish toxins, and they are mainly produced by dinoflagellate Kerenia brevis. However, brevetoxins were also recently found in other genera: Chatonella marina such as C. antiqua, Fibrocapsa japonica, Heterosigma akashiwo, K. mikimotoi, K. brevisulcata, K. selliformis, and K. papilionacea [27,29,69,70,76,77,78]. Brevetoxins are a suite of ladder-like cyclic polyether compounds with two types of backbone structures, brevetoxin B backbone (type 1: PbTx-2, 3, 5, 6, 8, and 9) and brevetoxin A backbone (type 2: PbTx-1, 7, and 10) (Figure 3) [27,62].
|PbTx-5||1||COCH3||K-ring acetate PbTx-2||936|
|PbTx-6||1||H||K-ring epoxide PbTx-2||910|
The major symptoms of severe brevetoxin poisoning are paresthesia, nausea, abdominal pain, vertigo, ataxia, diarrhea, burning pain in the rectum, headache, and bradycardia. Brevetoxins may also cause respiratory irritation syndrome . Brevetoxins are odorless, tasteless, and heat and acid stable, and, hence, not easily detectable in human food sources [27,29]. Of the ten brevetoxins identified so far, PbTx-3 was investigated more intensively compared with other ones. The LD50 of PbTx-3 in mice is 94 µg/kg body weight by intravenous injection, 170 µg/kg body weight by intraperitoneal injection, and 520 µg/kg body weight by oral administration, respectively [27,80]. Pathogenic dose of PbTx-3 in human is about 42–72 times larger than that in mice [27,80].
Brevetoxins inhibit the inactivation of TTX-S VGSCs through binding to site 5. Earlier investigations showed that brevetoxins activate VGSCs and lead to uncontrolled Na+ influx into the cell . Subsequent studies by Poli and co-workers using [3H]brevetoxin PbTx-3 as a specific probe revealed that PbTx-3 does not bind to any of the previously described sites and a new site of binding, site 5, was identified . Later studies further confirmed that brevetoxins are site 5 toxins, interacting with the α-subunit of VGSCs in a “head-down” orientation in a 1:1 stoichiometry. Binding of brevetoxins to site 5 causes conformational changes in the channel, which lead to abnormal opening of the channel and inhibited channel inactivation, resulting in persistent channel activation, membrane depolarization, Na+ current increment, and repetitive firing [27,81,82,83,84].
Antillatoxin A (C28H45N3O5; [M + H]+ at m/z 504.3436) (Figure 4), a potent ichthyotoxin and cytotoxin, was first isolated from tropical marine cyanobacterium Lyngbya majuscula in Curaçao by Gerwick et al. . It is a structurally unique cyclic lipopeptide composed of a tripeptide linked to a highly methylated lipid moiety via ester and amide bonds [85,86,87]. Antillatoxin A has been demonstrated to be one of the most ichthyotoxic metabolites isolated from marine algae up to now . Blooms of Lyngbya majuscula have been associated with adverse effects on human health, including respiratory irritation, eye inflammation and severe contact dermatitis in exposed individuals .
The earliest report about antillatoxin A provided information about its basic structure features including seven partial structures by 1D- and 2D-1H and 13C NMR [85,91]. Yokokawa et al. reported the first successful total synthesis of (4S, 5R)-antillatoxin A and presented a proposed structure of antillatoxin A . Later, Li et al. synthesized four different antillatoxin stereoisomers which are all likely C-4 and C-5 diastereomers, and identified possible stereochemistry of natural antillatoxin A through the study of the biological activities of the compound . Total synthesis of antillatoxin A and its stereoisomers were explored and finally accomplished by Yokokawa and Shioiri (1998), Yokokawa et al. (1999, 2000), and Lee and Loh [86,92,93].
Antillatoxin A is one of the most ichthyotoxic metabolites as evaluated in the goldfish toxicity assay (LD50, 0.05 μg/mL; ED50, approximately 0.01 μg/mL) . Berman et al. found that antillatoxin A showed concentration-dependent cytotoxicity to rat cerebellar granule cells with an LC50 value of 20.1 ± 6.4 nM . Antillatoxin A has been demonstrated to be an activator of VGSCs, but its precise binding site on VGSCs remains unknown [95,96,97,98]. Li and co-authors reported that the rapid increase in intracellular Ca2+ produced by antillatoxin A was antagonized by TTX; Antillatoxin A allosterically enhanced the activity of [3H]batrachotoxin ([3H]BTX), a neurotoxin acting on site 2 of VGSCs; meanwhile, antillatoxin A in combination with brevetoxin produced a strong synergistic stimulation of [3H]BTX; furthermore, antillatoxin A enhanced Na+ influx in cerebellar granule cells by acting on VGSCs . Subsequently, Cao et al. reported that high concentrations of antillatoxin A increased intracellular Na+ concentration, and this effect was abrogated by TTX . Recently, the study from the same group proved that antillatoxin A was able to promote Na+ influx in cells heterologously expressing rat Nav1.2, rat Nav1.4, or rat Nav1.5 α-subunits by using the Na+ selective fluorescent dye, sodium-binding benzofuran isophthalate. They also found that potency of antillatoxin A on the three VGSC isoforms did not differ significantly and its efficacy was quite different from those of other VGSCs activators acting on sites 2 or 5 . Taken together, these data demonstrate that antillatoxin A is an activator of VGSCs with unique pharmacological properties; decoding the molecular determinants and mechanism of action of antillatoxin A may provide further insight into gating mechanisms of VGSCs .
Antillatoxin B (C33H48N3O5 ; [M + H]+ at m/z 566.3596) (Figure 4), first isolated by Nogle et al. in 2001 from Lyngbya majuscule collected from Puerto Rico and the Dry Tortugas, is an N-methyl homophenylalanine homolog of antillatoxin A . Similar to antillatoxin A, antillatoxin B activates VGSC expressed in mouse neuro-2a neuroblastoma cells (EC50 1.77 μM) and shows strong ichthyotoxic activity (EC50 1 μM). Antillatoxin B, however, is 10-fold less potent than antillatoxin A, indicating that the substitution at the N-methyl group is critical for compound potency .
Kalkitoxin (C21H38N2OS; [M + H]+ at m/z 366.2696) (Figure 4), a thiazoline ring-containing lipopeptide, was first isolated by Wu in 1996 from organic extracts of Lyngbya majuscula collected in coasts of Curaçao using a brine shrimp toxicity guided assay. Later, Wu and coworkers reported its structure, synthesis, and biological properties . In 2003, Nogle and Gerwick also reported the isolation of this potent neurotoxin from Lyngbya majuscula specimens collected in shallow waters off the coast of Puerto Rico . Kalkitoxin is a valuable target for total synthesis for its interesting biological activities, intriguing structure, and scarcity in natural products. Wu et al. and White et al. successfully completed the total synthesis of (+)-kalkitoxin [90,100,101]. Recently, Umezawa and co-workers successfully synthesized kalkitoxin and its analogs and tested their biological activities using brine shrimp toxicity assay .
Natural kalkitoxin consists of a lipophilic chain, a 2, 4-disubstituted thiazoline, and an unsaturated CH2=CH2 unit . There are five asymmetric centers in kalkitoxin structure including a thiazoline ring and four methyl groups. The absolute stereochemistry of natural kalkitoxin was determined to be 3R, 7R, 8S, 10S, and 2′R by comparing the 13C spectrum of the natural metabolite with those of synthesized compounds with all possible configurations. In 2004, White and coworkers published the full details of their work, which was a prerequisite for successful total synthesis of natural (+)-kalkitoxin .
In 2000, Wu et al. reported that natural (+)-kalkitoxin was strongly toxic to common goldfish (Carassius auratus, LC50 700 nM) and brine shrimp (Artemia salina, LC50 170 nM) . Kalkitoxin also displayed extremely potent cytotoxicity (LC50 3.86 nM) to primary cultures of rat neurons, which was antagonized by NMDA receptor antagonists dextrorphan and MK-801 . (+)-Kalkitoxin and two synthetic precursors showed cytotoxicity to human colon cell line HCT-116, indicating that the thiazoline moiety of kalkitoxin is required for cytotoxicity .
Natural (+)-kalkitoxin is an antagonist of VGSCs. However, there have been few reports about its action mechanisms and binding site on VGSCs. Wu et al. demonstrated that kalkitoxin was a very potent blocker of VGSCs expressed in mouse neuro-2a cells (EC50 of kalkitoxin, 1 nM vs. EC50 of saxitoxin, 8 nM) . In 2005, LePage et al. found that kalkitoxin interacted with VGSCs in cerebellar granule neurons (CGN)  and eliminated elevation of [Ca2+]i induced by veratridine (a VGSCs activator) and neurotoxicity in CGN in a concentration-dependent manner (EC50 262.7 nM), providing indirect evidence that kalkitoxin may be a blocker of TTX-S VGSCs. Kalkitoxin showed no effect on basal binding of [3H]BTX to VGSCs, but it inhibited [3H]BTX binding to VGSCs in the presence of deltamethrin, a positive allosteric modulator of VGSCs. These results also suggest that kalkitoxin may be a blocker of VGSCs for that BTX binds to VGSCs only when the channel is in the open conformation [91,103].
Jamaicamides include jamaicamide A, B, and C. Jamaicamide A (C27H37O4N2ClBr; [M + H]+ at m/z 567.1625) (Figure 5) is a novel and highly functionalized lipopeptide, containing an alkynyl bromide, a vinyl chloride, a β-methoxy eneone system, and a pyrrolinone ring . It was first isolated from a dark green strain of Lyngbya majuscula (strain JHB) by Edwards et al. in 2004. Jamaicamide B (C27H37O4N2Cl) was first isolated as a pale yellow oil from the lipid extract of cultured Lyngby majuscule JHB and is slightly more polar than jamaicamide A. Jamaicamide C (C27H39O4N2Cl) was purified from the crude extract of cultured Lyngby majuscule JHB in very low yield (0.5%), and is slightly more hydrophobic than either jamaicamide A or B.
The high-resolution fast atom bombardment mass spectrometry and isotope peak analyses of the structure of jamaicamide A highlighted the presence of a chlorine atom and a bromine atom in the molecule . Its degree of unsaturation was calculated to be 10 from its molecular formula . Similarly, jamaicamide B also has a degree of unsaturation of 10, with 1H and 13C resonances very close to those of jamaicamide A. The only difference is the lack of bromine signal in jamaicamide B, suggesting that jamaicamide B is the debromo analog of jamaicamide A. The molecular formula of jamaicamide C was determined to be C27H39O4N2Cl by the high-resolution fast atom bombardment mass spectrometry with a deduced degree of unsaturation of 9. 1H and 13C NMR data indicate that jamaicamide C has two additional hydrogen atoms compared with jamaicamide B. Recently, Graf et al. published the total synthesis of jamaicamide A .
Jamaicamides have potent ichthyotoxicity and cytotoxicity . In a goldfish toxicity assay, jamaicamide B was the most active (100% lethality at 10.22 nmol after 90 min) followed by jamaicamide C (100% lethality at 20.36 nmol after 90 min), while jamaicamide A was the least active fish toxin (sublethal toxicity at 17.62 nmol after 90 min). In a brine shrimp toxicity assay, jamaicamide C was only modestly active (20.36 nmol, 25% lethality) while both jamaicamide A and B showed no significant toxicity. Moreover, jamaicamides A, B, and C exhibited similar cytotoxicity to both H-460 human lung cell line and Neuro-2a mouse neuroblastoma cell line (LC50 ~15 μM).
Jamaicamides are also antagonists of VGSCs. Edwards and coworkers reported that jamaicamides A, B, and C at 5 μM all partially blocked VGSC activity with percent inhibition about half of that by saxitoxin at 0.15 μM using an antagonism cell bioassay . In this assay, the ability of jamaicamides to antagonize the combined cytotoxic effects of ouabain (a plasma membrane Na+-K+ ATPase inhibitor) and veratridine on cerebellar granule neurons were examined, and the results were scored through visually noting morphology of a significant number of living cells .
Crossbyanols A–D are four heptabrominated polyphenolic ethers first isolated from marine cyanobacterium Leptolyngbya crossbyana collected at Honaunau reef off the island of Hawaii . The periodic extensive blooms of Leptolyngbya crossbyana in Hawaii coral reefs cause significant damage to the subtending corals, generating serious concerns. Chemical investigation of bioactive secondary metabolites of Leptolyngbya crossbyana led to the discovery of crossbyanols. Crossbyanols have a branched oligomeric structure of polybrominated diphenyl ethers . Crossbyanol A (C30H1579Br7O6, m/z: 1046.5044) possesses seven bromine atoms, three 1,2,4-trisubstituted phenyl rings, one 1,2,3,4-tetrasubstituted phenyl ring, and one 1,2,3,5-tetrasubstituted phenyl ring (Figure 6). Crossbyanol B (C30H1579Br7O12S2, m/z: 1182.4172) shows an isotope pattern similar to that of crossbyanol A with the presence of two additional sulfate groups. Interestingly, crossbyanol C and crossbyanol D showed identical molecular ion peaks at m/z values of 1102.4703 and 1102.4642 in negative-ion HRESIMS, suggesting that they share identical molecular formula of C30H1579Br7O9S. Similarly, crossbyanol C and D contain the same five substructures with substitution patterns identical to that of crossbyanol A or B. In addition, crossbyanol C and D have one sulfate group and one hydroxyl group in their structures .
Among crossbyanols, crossbyanol A activates VGSCs expressed in neuro-2a mouse neuroblastoma cells, while crossbyanols B, C, and D do not . However, how crossbyanol A activates VGSCs is largely unknown. Most studies on crossbyanols A–D are mainly about their antibacterial, ichthyotoxic, and cytotoxic activities . Crossbyanol A has weak cytotoxicity against H-460 human lung cancer cells (IC50 30 µg/mL). Crossbyanol B displays the most potent antibacterial activity (MIC value: 2.0–3.9 µg/mL) against methicillin-resistant Staphylococcus aureus. In addition, crossbyanol B is potently ichthyotoxic to brine shrimp with an IC50 value of 2.8 µg/mL. However, crossbyanols C and D show no bioactivity in all these assays at the maximum test concentration of 20 µg/mL. The observation that crossbyanols A and B have quite different bioactivities in these assays suggests that the sulfation of crossbyanols is critical for potent biological activities in this structure class. It is not clear if VGSC stimulation activity of crossbyanol A correlates with its cytotoxicity .
Hoiamides A–D are a new family of marine secondary metabolites. In 2009, the first member of hoiamides, hiamides A (C44H71N5O10S3, m/z: 926.4441) (Figure 7), was isolated from marine cyanobacteria Lyngbya majuscula and Phormidium gracile collected in Papua New Guinea . Hoiamide A, a novel cyclic depsipeptide of a highly unusual structure, displays potent cytotoxicity and neurotoxicity . In 2010, Gerwick et al. reported two additional compounds in the hoiamide family, the cyclic depsipeptide hoiamide B (C45H73N5O10S3, m/z: 940.4584) and the linear lipopeptide hoiamide C (C37H62N4O7S3, m/z: 770.3775), which were purified from two different collections of marine cyanobacteria obtained in Papua New Guinea, respectively . The fourth member, hoiamide D (C35H58N4O7S3, m/z: 743.3535) was isolated from cyanobacterium Symploca sp. collected in Kape Point, Papua New Guinea .
The hoiamides A–D are a new class of cyanobacterial compounds featuring a triheterocylic system likely derived from a mixed peptide-polyketide biogenetic origin. The hoiamides are composed of a peptidic segment with an acetated and S-adenosyl methionine modified isoleucine moiety, a central triheterocyclic core comprised of two α-methylated thiazolines and one thiazole, and a highly oxygenated and methylated C-15 polyketide substructure [108,109]. Particularly, hoiamide A and B are cyclic while hoiamide C and D are linear. Moreover, hoiamide C may be an extraction byproduct of hoiamide D given the utilization of ethanol in the isolation and storage of the biological material . The unique structures and bioactivities of hoiamides elicited extensive exploration of its synthesis and biological functions. Recently, Wang and coauthors disclosed the first successfully total synthesis of hoiamide C, which was accomplished by using a highly efficient convergent approach .
Hoiamide A shows modest cytotoxicity against H460 human lung adenocarcinoma and neuro-2a mouse neuroblastoma cells with IC50 values of 11.2 μM and 2.1 μM, respectively . Hoiamide B displays low cytotoxicity against H460 with an IC50 value of 8.3 μM, but shows no inhibition of neuro-2a neuroblastoma cells, indicating that replacing the Hiva residue in hiamide A by a Hmpa residue in hiamide B remarkably decreases cytotoxicity for neuro-2a . Moreover, the linear analog hoiamide C shows no significant inhibitory activity for either H460 or neuro-2a cell line, suggesting that the macrocyclic ring and the hydrogen bond donors at C-3, C-13, and C-37 positions in 1 and 2 are important structural features for the bioactivity of hoiamides .
Among hoiamides A–D, hoiamide A and B are site 2 activators of VGSCs. Hoiamide A produces a rapid and concentration-dependent elevation of [Na+]i with an EC50 value of 2.31 μM in neocortical neurons and TTX antagonizes hoiamide A-induced [Na+]i elevation . In comparison, BTX, another site 2 agonist of VGSCs, causes a rapid and concentration-dependent elevation of neuronal [Na+]i with an EC50 value of 11.4 nM. BTX induce the maximum elevation of [Na+]i at concentrations greater than 60 mM, whereas the maximal response for hoiamide A was less than 20 mM . Moreover, hoiamide A inhibits the specific binding of [3H]BTX A and 20-α-benzoate ([3H]BTX) to neurotoxin site 2 on VGSCs in neocortical neurons, providing direct evidence that hoiamide A is an agonist of VGSCs through interacting with the neurotoxin site 2 . In addition, deltamethrin, an agonist binding to a site distinct from sites 1–6 and allosterically coupled to sites 2, 3, and 5, enhances hoiamide A-induced elevation of [Na+]i in neocortical neurons, which is in agreement with the binding of hoiamide A to neurotoxin site 2 . Similar to hoiamide A, hoiamide B stimulates Na+ influx with an EC50 value of 3.9 µM in mouse neocortical neurons. Considering the structural similarity between hoiamide A and B, it is plausible to speculate that hoiamide B is also a site 2 activator of VGSCs .
2.8. Palmyrolide A
Palmyrolide A (C20H36O3N, m/z: 338.2690) (Figure 8) is a novel neuroactive macrolide that features a rare N-methyl enamide and t-butyl branch . In 2010, Gerwick and co-workers reported the isolation, structure determination, and biological activity of palmyrolide A. It was isolated from a cyanobacterial assemblage of Leptolyngbya cf and Oscillatoria spp. collected in the Northern Pacific at Palmyra Atoll . Palmyrolide A displays interesting bioactivities including VGSC blockage and Ca2+ oscillation inhibition . Its unique structure has attracted attentions of many researchers. In 2012, Maio and coworkers reported the first total synthesis of (+)-ent-palmyrolide A and the first asymmetric total synthesis, along with the absolute configurations of products they obtained [114,115]. Meanwhile, Brimble and coworkers accomplished a total synthesis of the initially reported and the revised structures . In 2013, Reddy et al. disclosed the shortest synthetic route for (+)-palmyrolide A and produced (−)-cis-palmyrolide A for the first time by modifying Maio’s macrocyclization conditions .
Gerwick and coauthors demonstrated that palmyrolide A acts on VGSCs in neuro-2a cells . Palmyrolide A suppresses veratridine- and ouabain-induced Na+ overload and shows cytotoxicity with an IC50 value of 5.2 µM . Moreover, palmyrolide A significantly inhibits Ca2+ oscillations in murine cerebrocortical neurons with an average IC50 value of 3.7 µM (2.29–5.98 µM, 95% CI), although it is not cytotoxic when tested against H-460 human lung adenocarcinoma cells up to 20 µM . These results indicate that palmyrolide A may be a suitable probe for pharmacological study of VGSCs.
2.9. Palmyramide A
Palmyramide A (C36H53N3O9, m/z: 672.3852) (Figure 9), a novel cyclic depsipeptide, was purified by Gerwick et al. in 2010 from a consortium of cyanobacteria and red algae collected at Palmyra Atoll . The cyclic depsipeptide is composed of three amino acids and three hydroxyl acids in an unusual arrangement. Among the three hydroxyl acids, 2,2-dimethyl-3-hydroxyhexanoic acid (Dmhha) is the most unusual which has only been reported previously in guineamides E and F . The planar structure of palmyramide A was determined by 1D and 2D NMR studies and mass spectrometry.
Palmyramide A is a VGSC blocker. It inhibits veratridine- and ouabain-induced Na+ overload in cerebrocortical neurons with an IC50 value of 17.2 µM. In addition, palmyramide A displays modest cytotoxic activities against cancer cells, inhibiting H-460 human lung carcinoma cells with an IC50 value of 39.7 µM .
3. Pharmaceutical Potential of Shellfish Toxins
The past two decades witnessed a boom in reports of secondary metabolites purified from marine and freshwater algae, among which shellfish toxins have drawn considerable attention for their structural diversity and biological activities. Particularly, the activities of shellfish toxins on VGSCs have attracted significant interest in biomedical research to explore the therapeutic potential of these compounds. Selective ion channel blockers have proved to be effective analgesics. Ziconotide (trade name Prialt®), a synthetic version of ω-conotoxin MVIIA, which selectively blocks N-type voltage-gated Ca2+ channels, reduces chronic pain in spinal cord injury and became the first marine natural product approved for pain management by the US Food and Drug Administration in 2004 [119,120,121,122]. Advances in biomedical research in recent years have demonstrated that VGSCs are involved in pain management. Loss-of-function mutations of Nav1.7 cause a complete absence of pain sensation in patients [123,124] while gain-of-function mutations lead to painful neuropathies [125,126]. In 2008, Lewis et al. demonstrated that MrVIB (μO-conotoxin) produced significant analgesic effects in neuropathic and inflammatory pain by selectively blocking Nav1.8, a VGSC specifically expressed in sensory neurons . Shellfish toxins may represent a novel class of analgesics through regulation of VGSCs activity. We hereby discuss the pharmacological potential of shellfish toxins with a focus on STX and its analogs.
STX and its analogs selectively target VGSCs and block Na+ currents via binding to site 1 with nanomolar affinity, leading to inhibition of nerve impulses, which may result in paralytic shellfish poisoning. Meanwhile, they also have significant potential as extraordinary anesthetics and analgesics. The therapeutic potential of STX as a highly selective and long lasting blocker of nerve conduction was recognized as early as 1975. However, its innate systematic toxicity has hampered its clinical development. Recent advances in drug delivery techniques may provide new strategies to facilitate the clinical development of STX. Recently, Kohane reported liposomal formulations for a mixture of STX, bupivacaine, and dexamethasone, which delivered prolonged duration of local anesthesia with minimal systemic toxicity . The formulated mixture produced sciatic nerve blockade lasting up to 7.5 days in male Sprague–Dawley rats. Systemic toxicity was only observed with high loadings of dexamethasone, which caused increased release of liposomal STX. Mild myotoxicity occurred only in formulations containing bupivacaine. There was no nerve injury on Epon-embedded sections or up-regulation of the four genes associated with nerve injury in the dorsal root ganglia. The authors thus concluded that controlled release of STX and similar compounds is capable of providing prolonged nerve blockage with minimal systemic and local toxicity .
Gonyautoxins display remarkable therapeutic effects in treatment of pain caused by anal fissures. In 2004, Garrido et al. reported that gonyautoxin 2/3 epimers effectively reduced anal tone when injected into anal sphincter of healthy adults . In this study, gonyautoxin 2/3 epimers were administered by local infiltration in the anal internal sphincter in healthy adult volunteers, and the beneficial effects were evaluated by anoscopy, electromyography, and anorectal manometry before and after toxin application. Gonyautoxin administration significantly decreased anal maximal voluntary contraction pressure, produced immediate relaxation, and brought statistically decrease in anal tone (P < 0.001). Later, Garrido et al. reported effective treatment of chronic anal fissure with repeated gonyautoxin injection. Gonyautoxin 100 units was intrasphincterically injected and infiltrated to 23 chronic anal fissure patients every four days. Anorectal pressure was recorded before and four minutes after each infiltration. Results showed that total remissions were achieved within 7–14 days with an average of 8.2 ± 2.4 days. Importantly, no relapses or side effects were observed during a 10-month follow up study . Currently gonyautoxin injections are being intensively exploited as a new therapy for pain management in anal fissure patients . In addition, gonyautoxin by local infiltration has been shown to be a safe and effective treatment of chronic tension-type headache .
Taken together, shellfish toxins such as STX and gonyautoxins may provide a new rich source for development of novel pain therapies. In the past ten years, significant progress has been made in biosynthetic route elaboration and total synthesis of cyanobacterial toxins, such as STX. With more and more new members being identified, shellfish toxins may provide great opportunity for pharmaceutical discovery and development.
Shellfish toxins exhibit novel and diverse structural features, intriguing biological activities, and significant pharmaceutical potential, which place them in the center of current studies of marine natural products. Systematic and comprehensive investigation of structure–activity relationships of shellfish toxins enables the design and synthesis of toxins with improved properties. Shellfish toxins with desirable VGSC subtype selectivity combined with suitable delivery vehicles may deliver superior therapeutic benefits with minimal toxicity.
This work was supported in part by the National Basic Research Program of China (973 Program), 2010CB529801 and 2012CB22305 and the National Science Foundation Projects, 31070699, 31170746 (to Z.L.).
Conflicts of Interest
The authors declare no conflict of interest.
- Cestèle, S.; Catterall, W.A. Molecular mechanisms of neurotoxin action on voltage-gated sodium channels. Biochimie 2000, 82, 883–892. [Google Scholar]
- Ogata, N.; Ohishi, Y. Molecular diversity of structure and function of the voltage-gated Na+ channels. Jpn. J. Pharmacol. 2002, 88, 365–377. [Google Scholar] [CrossRef]
- Isom, L.L.; DeJongh, K.S.; Patton, D.E.; Reber, B.F.; Offord, X.J.; Charbonneau, H.; Walsh, K.; Goldin, A.L.; Catterall, W.A. Primary structure and functional expression of the β1 Subunit of the rat brain sodium channel. Science 1992, 256, 839–842. [Google Scholar]
- Isom, L.L.; Ragsdale, D.S.; De Jongh, K.S.; Westenbroek, R.E.; Reber, B.F.; Scheuer, X.T.; Catterall, W.A. Structure and function of the β2 subunit of brain sodium channels, a transmembrane glycoprotein with a CAM motif. Cell 1995, 83, 433–442. [Google Scholar]
- Morgan, K.; Stevens, E.B.; Shah, B.; Cox, P.J.; Dixon, A.K.; Lee, K.; Pinnock, R.D.; Hughes, J.; Richardson, P.J.; Mizuguchi, K.; Jackson, A.P. β3: An additional auxiliary subunit of the voltage-sensitive sodium channel that modulates channel gating with distinct kinetics. Proc. Natl. Acad. Sci. USA 2000, 97, 2308–2313. [Google Scholar]
- Aman, T.K.; Grieco-Calub, T.M.; Chen, C.; Rusconi, R.; Slat, E.A.; Isom, L.L.; Raman, I.M. Regulation of persistent Na current by interactions between β subunits of voltage-gated Na channels. J. Neurosci. 2009, 29, 2027–2042. [Google Scholar]
- Patino, G.A.; Isom, L.L. Electrophysiology and beyond: multiple roles of Na+ channel β subunits in development and disease. Neurosci. Lett. 2010, 486, 53–59. [Google Scholar]
- Wang, J.; Yarov-Yarovoy, V.; Kahn, R.; Gordon, D.; Gurevitz, M.; Scheuer, M.; Catterall, W.A. Mapping the receptor site for α-scorpion toxins on a Na+ channel voltage sensor. Proc. Natl. Acad. Sci. USA 2011, 108, 15426–15431. [Google Scholar]
- Klint, J.K.; Senff, S.; Rupasinghe, D.B.; Er, S.Y.; Herzig, V.; Nicholson, G.M.; King, G.F. Spider-venom peptides that target voltage-gated sodium channels: pharmacological tools and potential therapeutic leads. Toxicon 2012, 60, 478–491. [Google Scholar]
- Catterall, W.A.; Cestèle, S.; Yarov-Yarovoy, V.; Yu, F.H.; Konoki, K.; Scheuer, T. Voltage-gated ion channels and gating modifier toxins. Toxicon 2007, 49, 124–141. [Google Scholar]
- King, G.F.; Escoubas, P.; Nicholson, G.M. Peptide toxins that selectively target insect NaV and CaV channels. Channels 2008, 2, 100–116. [Google Scholar]
- Catterall, W.A. Ion channel voltage sensors: structure, function, and pathophysiology. Neuron 2010, 67, 915–928. [Google Scholar] [CrossRef]
- Smith, M.R.; Goldin, A.L. Interaction between the sodium channel inactivation linker and domain III S4-S5. Biophys. J. 1997, 73, 1885–1895. [Google Scholar] [CrossRef]
- Catterall, W.A. From ionic currents to molecular mechanisms: The structure and function of voltage-gated sodium channels. Neuron 2000, 26, 13–25. [Google Scholar] [CrossRef]
- Brackenbury, W.J.; Isom, L.L. Voltage-gated Na+ channels: Potential for β subunits as therapeutic targets. Expert Opin. Ther. Targets 2008, 12, 1191–1203. [Google Scholar] [CrossRef]
- Mantegazza, M.; Curia, G.; Biagini, G.; Ragsdale, D.S.; Avoli, M. Voltage-gated sodium channels as therapeutic targets in epilepsy and other neurological disorders. Lancet Neurol. 2010, 9, 413–424. [Google Scholar]
- England, S.; de Groot, M.J. Subtype-selective targeting of voltage-gated sodium channels. Br. J. Pharmacol. 2009, 158, 1413–1425. [Google Scholar] [CrossRef]
- Catterall, W.A.; Goldin, A.L.; Waxman, S.G. International Union of Pharmacology. XLVII. Nomenclature and structure-function relationships of voltage-gated sodium channels. Pharmacol. Rev. 2005, 57, 397–409. [Google Scholar] [CrossRef]
- Ogta, N.; Tatebayashi, H. Kinetic analysis of two types of Na+ channels in rat dorsal root ganglia. J. Physiol. 1993, 466, 9–37. [Google Scholar]
- Goldin, A.L. Resurgence of sodium research. Annu. Rev. Physiol. 2001, 63, 871–894. [Google Scholar] [CrossRef]
- Fainzilber, M.; Kofman, O.; Zlotkin, E.; Gordon, D. A new neurotoxin receptor site on sodium channels is identified by a conotoxin that affects sodium channel inactivation in molluscs and acts as an antagonist in rat brain. J. Biol. Chem. 1994, 269, 2574–2680. [Google Scholar]
- Lefebvre, K.A.; Bill, B.D.; Erickson, A.; Baugh, K.A.; O’Rourke, L.; Costa, P.R.; Nance, S.; Trainer, V.L. Characterization of intracellular and extracellular saxitoxin levels in both field and cultured Alexandrium spp. samples from Sequim Bay, Washington. Mar. Drugs 2008, 6, 103–116. [Google Scholar]
- Usup, G.; Kulis, D.M.; Anderson, D.M. Growth and toxin production of the toxic dinoflasellate Pyodinium bahamense var. compressum in laboratory cultures. Nat. Toxins 1994, 2, 254–262. [Google Scholar]
- Oshima, Y.; Blackburn, S.I.; Hallegraeff, G.M. Comparative study on paralytic shellfish toxin of the dinoflagellate Gymnodinium catenatum from three different countries profiles. Mar. Biol. 1993, 116, 471–476. [Google Scholar]
- Daugbjerg, N.; Hansen, G.; Larsen, J.; Mosestrup, Ø. Phylogeny of some of the major genera of dinoflagellates based on ultrastructure and partial LSU rDNA sequence data, including the erection of three new genera of unarmoured dinoflagellates. Phycologia 2000, 39, 302–317. [Google Scholar] [CrossRef]
- Smith, F.M.; Wood, S.A.; Ginkel, R.V.; Broady, P.A.; Gaw, S. First report of saxitoxin production by a species of the freshwater benthic cyanobacterium, Scytonema agardh. Toxicon 2011, 57, 566–573. [Google Scholar]
- Wang, D.Z. Neurotoxins from marine dinoflagellates: A brief review. Mar. Drugs 2008, 6, 349–371. [Google Scholar] [CrossRef]
- Cusick, K.D.; Sayler, G.S. An overview on the marine neurotoxin, saxitoxin: Genetics, molecular targets, methods of detection and ecological functions. Mar. Drugs 2013, 11, 991–1018. [Google Scholar]
- Watkins, S.M.; Reich, A.; Fleming, L.E.; Hammond, R. Neurotoxic shellfish poisoning. Mar. Drugs 2008, 6, 431–455. [Google Scholar] [CrossRef]
- Van Dolah, F.M. Marine algal toxins: Origins, health effects, and their increased occurrence. Environ. Health Perspect. 2000, 108, 133–141. [Google Scholar]
- Anderson, D.M.; Glibert, P.M.; Burkholder, J.M. Harmful algal blooms and eutrophication: Nutrient sources, composition, and consequences. Estuaries 2002, 25, 704–726. [Google Scholar]
- Sellner, K.G.; Doucette, G.J.; Kirkpatrick, G.J. Harmful algal blooms: causes, impacts and detection. J. Ind. Microbiol. Biotechnol. 2003, 30, 383–406. [Google Scholar] [CrossRef]
- Rogart, R.B. High-STX-affinity vs. low-STX-affinity Na+ channel subtypes in nerve, heart, and skeletal muscle. Ann. N. Y. Acad. Sci. 1986, 479, 402–430. [Google Scholar]
- Wang, J.; Salata, J.J.; Bennett, P.B. Saxitoxin is a gating modifier of hERG K+ channels. J. Gen. Physiol. 2003, 121, 583–598. [Google Scholar]
- Su, Z.; Sheets, M.; Ishida, H.; Li, F.; Barry, W.H. Saxitoxin blocks L-type ICa. J. Pharmacol. Exp. Ther. 2004, 308, 324–329. [Google Scholar]
- Böttinger, H.; Béress, L.; Habermann, E. Involvement of (Na+ + K+)-ATPase in binding and actions of palytoxin on human erythrocytes. Biochim. Biophys. Acta Biomembr. 1986, 861, 165–176. [Google Scholar]
- Thomas, P.; Stephens, M.; Wilkie, G.; Amar, M.; Lunt, G.G.; Whiting, P.; Gallagher, T.; Pereira, E.; Alkondon, M.; Albuquerque, E.X.; Wonnacott, S. (+)-Anatoxin-a is a potent agonist at neuronal nicotinic acetylcholine receptors. J. Neurochem. 1993, 60, 2308–2311. [Google Scholar]
- Wiese, M.; D’Agostino, P.M.; Mihali, T.K.; Moffitt, M.C.; Neilan, B.A. Neurotoxic alkaloids: Saxitoxin and its analogs. Mar. Drugs 2010, 8, 2185–2211. [Google Scholar]
- Schantz, E.J.; Mold, J.D.; Stanger, D.W.; Shavel, J.; Riel, F.J.; Bowden, J.P.; Lynch, J.M.; Wyler, R.S.; Riecel, B.; Sommer, H. Paralytic shellfish poison. VI. A procedure for the isolation and purification of the poison from toxic clam and mussel tissues. J. Am. Chem. Soc. 1957, 79, 5230–5235. [Google Scholar] [CrossRef]
- Terlau, H.; Heinemann, S.H.; Stühmer, W.; Pusch, M.; Conti, F.; Imoto, K.; Numa, S. Mapping the site of block by tetrodotoxin and saxitoxin of sodium channel II. FEBS Lett. 1991, 293, 93–96. [Google Scholar] [CrossRef]
- Noda, M.; Suzuki, H.; Numa, S.; Stiihmer, W. A single point mutation confers tetrodotoxin and saxitoxin insensitivity on the sodium channel II. FEBS Lett. 1989, 259, 213–216. [Google Scholar]
- Barnet, C.S.; Tse, J.Y.; Kohane, D.S. Site 1 sodium channel blockers prolong the duration of sciatic nerve blockade from tricyclic antidepressants. Pain 2004, 110, 432–438. [Google Scholar] [CrossRef]
- Garrido, R.; Lagos, N.; Lagos, M.; Rodríguez-Navarro, A.J.; Garcia, C.; Truan, D.; Henriquez, A. Treatment of chronic anal fissure by gonyautoxin. Colorectal Dis. 2007, 9, 619–624. [Google Scholar]
- Lattes, K.; Venegas, P.; Lagos, N.; Lagos, M.; Pedraza, L.; Rodriguez-Navarro, A.J.; García, C. Local infiltration of gonyautoxin is safe and effective in treatment of chronic tension-type headache. Neurol. Res. 2009, 31, 228–233. [Google Scholar] [CrossRef]
- Negri, A.P.; Jones, G.J.; Hindmarsh, M. Sheep mortality associated with paralytic shellfish poisons from the cyanbacterium Anabaena circinalis. Toxicon 1995, 33, 1321–1329. [Google Scholar]
- Reyero, M.; Cacho, E.; Martínez, A.; Vázquez, J.; Marina, A,; Fraga, S.; Franco, J.M. Evidence of saxitoxin derivatives as causative agents in the 1997 mass mortality of monk seals in the Cape Blanc Peninsula. Nat. Toxins 1999, 7, 311–315. [Google Scholar]
- Anderson, D.M. Red tides. Sci. Am. 1994, 271, 62–68. [Google Scholar] [CrossRef]
- Stewart, I.; Seawright, A.A.; Shaw, G.R. Cyanobacterial poisoning in livestock, wild mammals and birds—an overview. In Cyanobacterial Harmful Algal Blooms: State of the Science and Research Needs; Springer Science and Business Media LLC: New York, NY, USA, 2008; pp. 613–637. [Google Scholar]
- Trainer, V.L.; Baden, D.G. High affinity binding of red tide neurotoxins to marine mammal brain. Aquat. Toxicol. 1999, 46, 139–148. [Google Scholar]
- Halsetead, B.W. Poisonous and Venomous Marine Animals of the World; Darwin Press: Princeton, NJ, USA, 1978; pp. 325–400. [Google Scholar]
- Llewellyn, L.E. Saxitoxin, a toxic marine natural product that targets a multitude of receptors. Nat. Prod. Rep. 2006, 23, 200–222. [Google Scholar] [CrossRef]
- Pearson, L.; Mihali, T.; Moffitt, M.; Kellmann, R.; Neilan, B. On the chemistry, toxicology and genetics of the cyanobacterial toxins, microcystin, nodularin, saxitoxin and cylindrospermopsin. Mar. Drugs 2010, 8, 1650–1680. [Google Scholar]
- Lagos, N.; Andrinolo, D. Paralytic shellfish poisoning (PSP): Toxicology and kinetics. In Seafood and Freshwater Toxins: Pharmacology, Physiology and Detection; Botana, L.M., Ed.; Marcel Dekker: New York, NY, USA, 2000; pp. 203–215. [Google Scholar]
- Kao, C.Y. Paralytic shellfish poisoning. In Algal Toxins in Seafood and Drinking Water; Falconer, I.R., Ed.; Academic Press: London, UK, 1993; pp. 75–86. [Google Scholar]
- Hall, S.; Strichartz, G.; Moczydlowski, E.; Ravindran, A.; Reichardt, P.B. The saxitoxins: Sources, chemistry and pharmacology. In Marine Toxins. Origin, Structure and Pharmacology; Hall, S., Reichardt, P.B., Eds.; American Chemical Society: Washington, DC, USA, 1990; pp. 29–69. [Google Scholar]
- Schantz, E.J.; Ghazarossian, V.E.; Schnoes, H.K.; Strong, F.M.; Springer, J.P.; Pezzanite, J.O.; Clardy, J. The structure of saxitoxin 1. J. Am. Chem. Soc. 1975, 97, 1238–1239. [Google Scholar]
- Bordner, J.; Thiessen, W.E.; Bates, H.A.; Rapoport, H. The structure of a crystalline derivative of saxitoxin. The structure of saxitoxin. J. Am. Chem. Soc. 1975, 97, 6008–6012. [Google Scholar]
- Rogers, S.R.; Rapport, H. The pKa’s of saxitoxin. J. Am. Chem. Soc. 1980, 102, 7335–7339. [Google Scholar] [CrossRef]
- Shimizu, Y.; Hsu, C.P.; Genenah, A. Structure of saxitoxin in solutions and stereochemistry of dihydrosaxitoxins. J. Am. Chem. Soc. 1981, 103, 605–609. [Google Scholar] [CrossRef]
- Schantz, E.J.; Lynch, J.M.; Vayvada, G.; Matsumoto, K.; Rapoport, H. The purification and characterization of the poison produced by Gonyaulax catenella in axenic culture. Biochemistry 1966, 5, 1191–1195. [Google Scholar]
- Strichartz, G. Structural determinants of the affinity of saxitoxin for neuronal sodium Channels. Electrophysiological studies on frog peripheral nerve. J. Gen. Physiol. 1984, 84, 281–305. [Google Scholar] [CrossRef]
- Van Dolah, F.M. Diversity of Marine and Freshwater Algal Toxins. In Seafood Toxicology: Pharmacology, Physiology and Detection; Botana, L., Ed.; Marcel Dekker: New York, NY, USA, 2000; pp. 19–43. [Google Scholar]
- Hille, B. The receptor for tetrodotoxin and saxitoxin. A structural hypothesis. Biophys. J. 1975, 15, 615–619. [Google Scholar] [CrossRef]
- Kao, C.Y.; Walker, S.E. Active groups of saxitoxin and tetrodotoxin as deduced from actions of saxitoxin analogues on frog muscle and squid axon. J. Physiol. 1982, 323, 619–637. [Google Scholar]
- Shiinizu, Y. Recent progress in marine toxin research. Pure Appl. Chem. 1982, 54, 1973–1980. [Google Scholar]
- Numa, S.; Noda, M. Molecular structure of sodium channels. Ann. N. Y. Acad. Sci. 1986, 479, 338–355. [Google Scholar] [CrossRef]
- Hartshorne, R.P.; Catterall, W.A. The sodium channel from rat brain. Purification and subunit composition. J. Biol. Chem. 1984, 259, 1667–1675. [Google Scholar]
- Walker, J.R.; Novick, P.A.; Parsons, W.H.; McGregor, M.; Zablocki, J.; Pande, V.S.; Du Bois, J. Marked difference in saxitoxin and tetrodotoxin affinity for the human nociceptive voltage-gated sodium channel (Nav1.7). Proc. Natl. Acad. Sci. USA 2012, 109, 18102–18107. [Google Scholar]
- Steidinger, K.A. Phytoplankton ecology: A conceptual review based on eastern. Gulf of Mexico research. Crit. Rev. Microbiol. 1973, 3, 49–68. [Google Scholar] [CrossRef]
- Baden, D.G. Marine food-borne dinoflagellate toxins. Int. Rev. Cytol. 1983, 82, 99–150. [Google Scholar]
- Baden, D.G.; Mende, T.J. Toxicity of two toxins from the Florida red tide marine dinoflagellate, Ptychodiscus brevis. Toxicon 1982, 20, 457–461. [Google Scholar] [CrossRef]
- Poli, M.; Mende, T.J.; Baden, D.G. Brevetoxins, unique activators of voltage-sensitive sodium channels bind to specific sites in rat brain synaptosomes. Mol. Pharmacol. 1986, 30, 129–135. [Google Scholar]
- Baden, D.; Fleming, L.E.; Bean, J.A. Marine Toxins. In Handbook of Clinical Neurology: Intoxications of the Nervous System Part H. Natural Toxins and Drugs; deWolf, F.A, Ed.; Elsevier: Amsterdam, The Nertherlands, 1995; pp. 141–175. [Google Scholar]
- Landsberg, J.H. The effects of harmful algal blooms on aquatic organisms. Rev. Fish. Sci. 2002, 10, 113–390. [Google Scholar]
- Flewelling, L.J.; Naar, J.P.; Abbott, J.P.; Baden, D.G.; Barros, N.B.; Bossart, G.D.; Bottein, M.Y.; Hammond, D.G.; Haubold, E.M.; Heil, C.A.; et al. Brevetoxicosis: Red tides and marine mammal mortalities. Nature 2005, 435, 755–756. [Google Scholar]
- Sagir Ahmed, M.D.; Arakawa, O.; Onoue, Y. Toxicity of cultured Chatonella marina. In Harmful Marine Algal Blooms; Lassus, P., Arzul, G., Erhard, E., Gentien, P., Marcaillou, C., Eds.; Lavoisier: Paris, France, 1995; pp. 499–504. [Google Scholar]
- Khan, S.; Arakawa, O.; Onoue, Y. Neurotoxins in a toxic red tide of Heterosigma akashiwo (Raphidophyceae) in Kagoshima Bay, Japan. Aquac. Res. 1997, 28, 9–14. [Google Scholar] [CrossRef]
- Hallegraeff, G.M.; Munday, B.L.; Baden, D.G.; Whitney, P.L. Chatonnella maria raphidophyte bloom associated with mortality of cultured bluefin tuna (Thunnus maccoyii) in south Australia. In Harmful Algae; Reguera, B., Blanco, J., Ferandz, M.L., Wyatt, T., Eds.; Xunta de Galacia and IOC: Santiago de Compostela, Spain, 1998; pp. 93–96. [Google Scholar]
- Morris, P.D.; Campbell, D.S.; Taylor, T.J.; Freeman, J.I. Clinical and epidemiological features of neurotoxic shellfish poisoning in North Carolina. Am. J. Public Health 1991, 81, 471–474. [Google Scholar]
- Kirkpatrick, B.; Fleming, L.E.; Squicciarini, D.; Backer, L.C.; Clark, R.; Abraham, W.; Benson, J.; Chenge, Y.S.; Johnson, D.; Pierce, R.; et al. Literature review of Florida red tide: Implications for human health effects. Harmful Algae 2004, 3, 99–115. [Google Scholar] [CrossRef]
- Gallagher, J.P.; Shinnick-Gallaqher, P. Effect of Gymnodinium breve toxin in the rat phrenic nerve diaphragm preparation. Br. J. Pharmacol. 1980, 69, 367–372. [Google Scholar]
- Trainer, V.L.; Thomsen, W.J.; Catterall, W.A.; Baden, D.G. Photoaffinity labeling of the brevetoxin receptor on sodium channels in rat brain synaptosomes. Mol. Pharmacol. 1991, 40, 988–994. [Google Scholar]
- Rein, K.S.; Baden, D.G.; Gawley, R.E. Conformational analysis of the sodium channel modulator, brevetoxin A, comparison with brevetoxin B conformations, and a hypothesis about the common pharmacophore of the “site 5” toxins. J. Org. Chem. 1994, 59, 2101–2106. [Google Scholar] [CrossRef]
- Baden, D.G.; Bourdelais, A.J.; Jacocks, H.; Michelliza, S.; Naar, J. Natural and derivative brevetoxins: Historical background, multiplicity, and effects. Environ. Health Perspect. 2005, 113, 621–625. [Google Scholar]
- Orjala, J.; Nagle, D.G.; Hsu, V.L.; Gerwick, W.H. Antillatoxin: An exceptionally ichthyotoxic cyclic lipopeptide from the tropical cyanobacterium Lyngbya majuscula. J. Am. Chem. Soc. 1995, 117, 8281–8282. [Google Scholar]
- Yokokawa, F.; Fujiwara, H.; Shioiri, T. Total synthesis and revision of absolute stereochemistry of antillatoxin, an ichthyotoxic cyclic lipopeptide from marine cyanobacterium Lyngbya majuscula. Tetrahedron 2000, 56, 1759–1775. [Google Scholar] [CrossRef]
- Li, W.I.; Marquez, B.L.; Okino, T.; Yokokawa, F.; Shioiri, T.; Gerwick, W.H.; Murray, T.F. Characterization of the preferred stereochemistry for the neuropharmacologic actions of antillatoxin. J. Nat. Prod. 2004, 67, 559–568. [Google Scholar]
- Osborne, N.J.; Webb, P.M.; Shaw, G.R. The toxins of Lyngbya majuscula and their human and ecological health effects. Environ. Int. 2001, 27, 381–392. [Google Scholar] [CrossRef]
- Nogle, L.M.; Okino, T.; Gerwick, W.H. Antillatoxin B, a neurotoxic lipopeptide from the marine cyanobacterium lyngbya majuscule. J. Nat. Prod. 2001, 64, 983–985. [Google Scholar] [CrossRef]
- Wu, M.; Okino, T.; Nogle, L.M.; Marquez, B.L.; Williamson, R.T.; Sitachitta, N.; Berman, F.W.; Murray, T.F.; McGough, K.; Jacobs, R.; et al. Structure, synthesis, and biological properties of kalkitoxin, a novel neurotoxin from the marine cyanobacterium Lyngbya majuscula. J. Am. Chem. Soc. 2000, 122, 12041–12042. [Google Scholar]
- Aráoz, R.; Molgó, J.; Tandeau de Marsac, N. Neurotoxic cyanobacterial toxins. Toxicon 2010, 56, 813–828. [Google Scholar] [CrossRef]
- Yokokawa, F.; Fujiwara, H.; Shioiri, T. Total synthesis and revision of absolute configuration of antillatoxin, an ichthyotoxic cyclic lipopeptide of marine origin. Tetrahedron Lett. 1999, 40, 1915–1916. [Google Scholar] [CrossRef]
- Yokokawa, F.; Shioiri, T. Total synthesis of antillatoxin, an ichthyotoxic cyclic lipopeptide, having the proposed structure. What is the real structure of antillatoxin? J. Org. Chem. 1998, 63, 8638–8639. [Google Scholar] [CrossRef]
- Berman, F.W.; Gerwick, W.H.; Murray, T.F. Antillatoxin and kalkitoxin, ichthyotoxins from the tropical cyanobacterium Lyngbya majuscula, induce distinct temporal patterns of NMDA receptor-mediated neurotoxicity. Toxicon 1999, 37, 1645–1648. [Google Scholar] [CrossRef]
- Li, W.I.; Berman, F.W.; Okino, T.; Yokokawa, F.; Shioiri, T.; Gerwick, W.H.; Murray, T.F. Antillatoxin is a marine cyanobacterial toxin that potently activates voltage-gated sodium channels. Proc. Natl. Acad. Sci. USA 2001, 98, 7599–7604. [Google Scholar]
- Cao, Z.; George, J.; Gerwick, W.H.; Baden, D.G.; Rainier, J.D.; Murray, T.F. Influence of lipid-soluble gating modifier toxins on sodium influx in neocortical neurons. J. Pharmacol. Exp. Ther. 2008, 326, 604–613. [Google Scholar]
- Jabba, S.V.; Prakash, A.; Dravid, S.M.; Gerwick, W.H.; Murray, T.F. Antillatoxin, a novel lipopeptide, enhances eeurite outgrowth in immature cerebrocortical neurons through activation of voltage-gated sodium channels. J. Pharmacol. Exp. Ther. 2010, 332, 698–709. [Google Scholar]
- Cao, Z.; Gerwick, W.H.; Murray, T.F. Antillatoxin is a sodium channel activator that displays unique efficacy in heterologously expressed rNav1.2, rNav1.4 and rNav1.5 alpha subunits. BMC Neurosci. 2010, 11, 1–13. [Google Scholar]
- Nogle, L.M.; Gerwick, W.H. Diverse secondary metabolites from a Puerto Rican collection of Lyngbya majuscula. J. Nat. Prod. 2003, 66, 217–220. [Google Scholar] [CrossRef]
- White, J.D.; Lee, C.S.; Xu, Q. Total synthesis of (+)-kalkitoxin. Chem. Commun. (Camb.) 2003, 16, 2012–2013. [Google Scholar]
- White, J.D.; Xu, Q.; Lee, C.S.; Valeriote, F.A. Total synthesis and biological evaluation of (+)-kalkitoxin, a cytotoxic metabolite of the cyanobacterium Lyngbya majuscule. Org. Biomol. Chem. 2004, 2, 2092–2102. [Google Scholar]
- Umezawa, T.; Sueda, M.; Kamura, T.; Kawahara, T.; Han, X.; Okino, T.; Matsuda, F. Synthesis and biological activity of kalkitoxin and its analogues. J. Org. Chem. 2012, 77, 357–370. [Google Scholar]
- LePage, K.T.; Goeger, D.; Yokokawa, F.; Asano, T.; Shioiri, T.; Gerwick, W.H.; Murray, T.F. The neurotoxic lipopeptide kalkitoxin interacts with voltage-sensitive sodium channels in cerebellar granule neurons. Toxicol. Lett. 2005, 158, 133–139. [Google Scholar]
- Edwards, D.J.; Marquez, B.L.; Nogle, L.M.; McPhail, K.; Goeger, D.E.; Roberts, M.A.; Gerwick, W.H. Structure and biosynthesis of the jamaicamides, new mixed polyketide-peptide neurotoxins from the marine cyanobacterium Lyngbya majuscule. Chem. Biol. 2004, 11, 817–833. [Google Scholar]
- Graf, K.M.; Tabor, M.G.; Brown, M.L.; Paige, M. Synthesis of (s)-jamaicamide C carboxylic acid. Org. Lett. 2009, 11, 5382–5385. [Google Scholar] [CrossRef]
- Manger, R.L.; Leja, L.S.; Lee, S.Y.; Hungerford, J.M.; Hokama, Y.; Dickey, R.W.; Granade, H.R.; Lewis, R.; Yasumoto, T.; Wekell, M.M. Detection of sodium channel toxins: Directed cytotoxicity assays of purified ciguatoxins, brevetoxins, saxitoxins, and seafood extracts. J. AOAC Int. 1995, 78, 521–527. [Google Scholar]
- Choi, H.; Engene, N.; Smith, J.E.; Preskitt, L.B.; Gerwick, W.H. Crossbyanols A–D, toxic brominated polyphenyl ethers from the Hawai’ian bloom-forming cyanobacterium Leptolyngbya crossbyana. J. Nat. Prod. 2010, 73, 517–522. [Google Scholar]
- Pereira, A.; Cao, Z.; Murray, T.F.; Gerwick, W.H. Hoiamide A, a sodium channel activator of unusual architecture from a consortium of two papua new Guinea Cyanobacteria. Chem. Biol. 2009, 16, 893–906. [Google Scholar]
- Choi, H.; Pereira, A.R.; Cao, Z.; Shuman, C.F.; Engene, N.; Byrum, T.; Matainaho, T.; Murray, T.F.; Mangoni, A.; Gerwick, W.H. The hoiamides, structurally intriguing neurotoxic lipopeptides from Papua New Guinea marine cyanobacteria. J. Nat. Prod. 2010, 73, 1411–1421. [Google Scholar]
- Malloy, K.L.; Choi, H.; Fiorilla, C.; Valeriote, F.A.; Matainaho, T.; Gerwick, W.H. Hoiamide D, a marine cyanobacteria-derived inhibitor of p53/MDM2 interaction. Bioorg. Med. Chem. Lett. 2012, 22, 683–688. [Google Scholar]
- Wang, L.; Xu, Z.; Ye, T. Total synthesis of hoiamide C. Org. Lett. 2011, 13, 2506–2509. [Google Scholar]
- Philkhana, S.C.; Seetharamsingh, B.; Dangat, Y.B.; Vanka, K.; Reddy, D.S. Synthesis of palmyrolide A and its cis-isomer and mechanistic insight into trans–cis isomerisation of the enamide macrocycle. Chem. Commun. 2013, 49, 3342–3344. [Google Scholar]
- Pereira, A.R.; Cao, Z.; Engene, N.; Soria-Mercado, I.E.; Murray, T.F.; Gerwick, W.H. Palmyrolide A, an unusually stabilized neuroactive macrolide from palmyra atoll cyanobacteria. Org. Lett. 2010, 12, 4490–4493. [Google Scholar]
- Tello-Aburto, R.; Newar, T.D.; Maio, W.A. Evolution of a protecting-group-free total synthesis: Studies en route to the neuroactive marine macrolide (−)-palmyrolide A. J. Org. Chem. 2012, 77, 6271–6289. [Google Scholar]
- Tello-Aburto, R.; Johnson, E.M.; Valdez, C.K.; Maio, W.A. Asymmetric total synthesis and absolute stereochemistry of the neuroactive marine macrolide palmyrolide A. Org Lett. 2012, 14, 2150–2153. [Google Scholar]
- Wadsworth, A.D.; Furkert, D.P.; Sperry, J.; Brimble, M.A. Total synthesis of the initially reported and revised structures of the neuroprotective agent palmyrolide A. Org. Lett. 2012, 14, 5374–5377. [Google Scholar]
- Taniguchi, M.; Nunnery, J.K.; Engene, N.; Esquenazi, E.; Byrum, T.; Dorrestein, P.C.; Gerwick, W.H. Palmyramide A, a cyclic depsipeptide from a palmyra atoll collection of the marine cyanobacterium Lyngbya majuscule. J. Nat. Prod. 2010, 73, 393–398. [Google Scholar]
- Tan, L.T.; Sitachitta, N.; Gerwick, W.H. The guineamides, novel cyclic depsipeptides from a Papua New Guinea collection of the marine cyanobacterium Lyngbya majuscule. J. Nat. Prod. 2003, 66, 764–771. [Google Scholar]
- Glaser, K.B.; Mayer, A.M.S. A renaissance in marine pharmacology: from preclinical curiosity to clinical reality. Biochem. Pharmacol. 2009, 78, 440–448. [Google Scholar]
- Olivera, B.M.; Cruz, L.J.; de Santos, V.; LeCheminant, G.W.; Griffin, D.; Zeikus, R.; McIntosh, J.M.; Galyean, R.; Varga, J.; Gray, W.R.; et al. Neuronal calcium channel antagonists. Discrimination between calcium channel cubtypes using ω-conotoxin from Conus magus venom. Biochemistry 1987, 26, 2086–2090. [Google Scholar]
- Molinski, T.F.; Dalisay, D.S.; Lievens, S.L.; Saludes, J.P. Drug development from marine natural products. Nat. Rev. Drug Discov. 2009, 8, 69–85. [Google Scholar]
- Klotz, U. Ziconotide—a novel neuron-specific calcium channel blocker for the Intrathecal treatment of severe chronic pain—a short review. Int. J. Clin. Pharmacol. Ther. 2006, 44, 478–483. [Google Scholar] [CrossRef]
- Goldberg, Y.P.; MacFarlane, J.; MacDonald, M.L.; Thompson, J.; Dube, M.P.; Mattice, M.; Fraser, R.; Young, C.; Hossain, S.; Pape, T.; et al. Loss-of-function mutations in the Nav1.7 gene underlie congenital indifference to pain in multiple human populations. Clin. Genet. 2007, 71, 311–319. [Google Scholar] [CrossRef]
- Cox, J.J.; Reimann, F.; Nicholas, A.K.; Thornton, G.; Roberts, E.; Springell, K.; Karbani, G.; Jafri, H.; Mannan, J.; Raashid, Y.; et al. An SCN9A channelopathy causes congenital inability to experience pain. Nature 2006, 444, 894–898. [Google Scholar]
- Fertleman, C.R.; Baker, M.D.; Parker, K.A.; Moffatt, S.; Elmslie, F.V.; Abrahamsen, B.; Ostman, J.; Klugbauer, N.; Wood, J.N.; Gardiner, R.M.; et al. SCN9A mutations in paroxysmal extreme pain disorder: Allelic variants underlie distinct channel defects and phenotypes. Neuron 2006, 52, 767–774. [Google Scholar] [CrossRef]
- Han, C.; Rush, A.M.; Dib-Hajj, S.D.; Li, S.; Xu, Z.; Wang, Y.; Tyrrell, L.; Wang, X.; Yang, Y.; Waxman, S.G. Sporadic onset of erythermalgia: A gain-of-function mutation in Nav1.7. Ann. Neurol. 2006, 59, 553–558. [Google Scholar] [CrossRef]
- Ekberg, J.; Jayamanne, A.; Vaughan, C.W.; Aslan, S.; Thomas, L.; Mould, J.; Drinkwater, R.; Baker, M.D.; Abrahamsen, B.; Wood, J.N.; et al. μO-conotoxin MrVIB selectively blocks Nav1.8 sensory neuron specific sodium channels and chronic pain behavior without motor deficits. Proc. Natl. Acad. Sci. USA 2006, 103, 17030–17035. [Google Scholar]
- Epstein-Barash, H.; Shichor, I.; Kwon, A.H.; Hall, S.; Lawlor, M.W.; Langer, R.; Kohane, D.S. Prolonged duration local anesthesia with minimal toxicity. Proc. Natl. Acad. Sci. USA 2009, 106, 7125–7130. [Google Scholar]
- Garrido, R.; Laqos, N.; Lattes, K.; Azolas, C.G.; Bocic, G.; Cuneo, A.; Chiong, H.; Jensen, C.; Heríandez, A.; Fernández, C. The Gonyautoxin 2/3 epimers reduces anal tone when injected in the anal sphincter of healthy adults. Biol. Res. 2004, 37, 395–403. [Google Scholar]
- Poh, A.; Tan, K.Y.; Seow-Choen, F. Innovations in chronic anal fissure treatment: A systematic review. World J. Gastrointest. Surg. 2010, 2, 231–241. [Google Scholar] [CrossRef]
© 2013 by the authors; licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution license (http://creativecommons.org/licenses/by/3.0/).