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Review

Host-Defense Activities of Cyclotides

by
David J. Craik
Institute for Molecular Bioscience, The University of Queensland, Brisbane, QLD 4072, Australia
Toxins 2012, 4(2), 139-156; https://doi.org/10.3390/toxins4020139
Submission received: 22 November 2011 / Revised: 25 January 2012 / Accepted: 31 January 2012 / Published: 15 February 2012
(This article belongs to the Special Issue Insecticidal Toxins)
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Abstract

:
Cyclotides are plant mini-proteins whose natural function is thought to be to protect plants from pest or pathogens, particularly insect pests. They are approximately 30 amino acids in size and are characterized by a cyclic peptide backbone and a cystine knot arrangement of three conserved disulfide bonds. This article provides an overview of the reported pesticidal or toxic activities of cyclotides, discusses a possible common mechanism of action involving disruption of biological membranes in pest species, and describes methods that can be used to produce cyclotides for potential applications as novel pesticidal agents.

1. Introduction

Cyclotides [1] are a plant-derived family of small proteins characterized by their head-to-tail cyclic backbone and a cystine knot arrangement of three conserved disulfide bonds. They were first discovered in plants from the Rubiaceae (coffee) and Violaceae (violet) families but have since been reported in a range of other plants from the Cucurbitaceae (cucurbit) and Fabaceae (legume) families and it has been predicted that they are widely distributed within the plant kingdom [2]. Cyclotides are notable for their exceptional stability and their diverse range of bioactivities, as well as for their expression in a wide range of plant tissues, including leaves, stems, flowers, dormant seeds and roots [3]. There have been a number of recent reviews on the discovery [4,5,6], structures [4,7,8], and applications [9,10,11,12] of cyclotides, to which the reader is referred for more background but here the focus is on their pesticidal and/or toxic activities.
The structure of the prototypical cyclotide, kalata B1, is shown in Figure 1 [13], highlighting that cyclotides are around 30 amino acids in size with a cyclic peptide backbone. They fold into compact three-dimensional shapes that incorporate a small β-sheet structure and a series of turns built around the cystine knot core. This compact structure and elaborate cross-bracing by disulfide bonds is a main contributing factor that makes cyclotides exceptionally stable. They are highly resistant to chemical, thermal and enzymatic treatments that would typically destroy conventional proteins [14].
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Figure 1. Schematic illustration of (a) the sequence and (b) the structure of the prototypical cyclotide, kalata B1 showing the head-to-tail cyclic backbone and six conserved cysteine residues (numbered using Roman numerals) that are connected together in a I–IV, II–V and III–VI connectivity leading to a cystine knot [15]. This connectivity has been established by a range of chemical and NMR methods [16,17]. The structure folds up into a compact three-dimensional shape that contains a β-sheet motif (indicated by the broad arrows) as well as a series of turns. The backbone segments between cysteine residues are referred to as loops and are numbered 1–6. Some loops, e.g. loops 1 and 4, are relatively highly conserved, whereas others are typically hypervariable in cyclotides from different plants, leading to the description of cyclotides as a natural combinatorial template [18]; (c) Space-filling view of the surface of kalata B1 showing the location of a surface-exposed patch of hydrophobic residues.
Figure 1. Schematic illustration of (a) the sequence and (b) the structure of the prototypical cyclotide, kalata B1 showing the head-to-tail cyclic backbone and six conserved cysteine residues (numbered using Roman numerals) that are connected together in a I–IV, II–V and III–VI connectivity leading to a cystine knot [15]. This connectivity has been established by a range of chemical and NMR methods [16,17]. The structure folds up into a compact three-dimensional shape that contains a β-sheet motif (indicated by the broad arrows) as well as a series of turns. The backbone segments between cysteine residues are referred to as loops and are numbered 1–6. Some loops, e.g. loops 1 and 4, are relatively highly conserved, whereas others are typically hypervariable in cyclotides from different plants, leading to the description of cyclotides as a natural combinatorial template [18]; (c) Space-filling view of the surface of kalata B1 showing the location of a surface-exposed patch of hydrophobic residues.
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Individual plants express a suite of cyclotides, sometimes comprising more than 100 different sequences. Based on the reported discovery rates for cyclotides in the Violaceae and Rubiaceae and the large number of unique cyclotides per plant species it has been predicted that there might be ~50,000 cyclotide sequences in nature [2] but this is probably an underestimate based on recent discoveries in the Fabaceae [19,20]. Table 1 shows a representative selection of cyclotides from the three major subfamilies that have so far been identified. The Möbius and bracelet subfamilies are the largest subfamilies of cyclotides and are so named because of the presence or absence of a conceptual 180° twist in the peptide backbone brought about by a cis X-Pro peptide bond in the Möbius class and the lack of this “twist” in the circular ribbon of the bracelet class [1]. A smaller subfamily of cyclotides known as the trypsin inhibitor cyclotides has quite different sequences than the other two subfamilies and is also routinely classified as “cyclic knottins” based on their sequence homology to conventional (acyclic) cystine knot proteins from the knottin family [21]. The cyclotides shown in Table 1 have been structurally characterized and their relevant PDB ID codes are given in the table, along with their sequences and some biophysical characteristics, including net charge and size (numbers of amino acids).
Table
Table 1. Representative cyclotides from the Möbius, bracelet and trypsin inhibitor subfamilies.
Table 1. Representative cyclotides from the Möbius, bracelet and trypsin inhibitor subfamilies.
Cyclotide aAA bCh cSequence dPDB eRef.
Möbius subfamily
kalata B130+2GLPVCGETCVGGTCNTPGCTCSWPVCTRN1NB1[13]
kalata B229−1GLPVCGETCFGGTCNTPGCSCTWPICTRD1PT4[22,23]
kalata B729+1GLPVCGETCTLGTCYTQGCTCSWPICKRN2JWM[24]
kalata B1228−2GSLCGDTCFVLGCNDSSCSCNYPICVKD2KVX[25]
cycloviolacin O1431+3GSIPACGESCFKGKCYTPGCSCSKYPLCAKN2GJ0[26]
varv F290GVPICGETCTLGTCYTAGCSCSWPVCTRN3E4H[27]
Bracelet subfamily
circulin A30+2GIPCGESCVWIPCISAALGCSCKNKVCYRN1BH4[28,29]
circulin B31+2GVIPCGESCVFIPCISTLLGCSCKNKVCYRN2ERI[29]
cycloviolacin O1300GIPCAESCVYIPCTVTALLGCSCSNRVCYN1NBJ[26]
cycloviolacin O230+2GIPCGESCVWIPCISSAIGCSCKSKVCYRN2KNM[26]
kalata B530−1GTPCGESCVYIPCISGVIGCSCTDKVCYLN2KUX[30,31]
kalata B831+1GSVLNCGETCLLGTCYTTGCTCNKYRVCTKD2B38[32]
tricyclon A33−1GGTIFDCGESCFLGTCYTKGCSCGEWKLCYGTN1YP8[33]
palicourein37−1GDPTFCGETCRVIPVCTYSAALGCTCDDRSDGLCKRN1R1F[34,35]
vhl-1310SISCGESCAMISFCFTEVIGCSCKNKVCYLN1ZA8[36]
vhl-230−1GLPVCGETCFTGTCYTNGCTCDPWPVCTRN2KUK[36,37]
vhr1300GIPCAESCVWIPCTVTALLGCSCSNKVCYN1VB8[3]
Trypsin inhibitor subfamily
MCoTI-II34+3GGVCPKILKKCRRDSDCPGACICRGNGYCGSGSD1IB9[38,39]
a Selected examples only are shown. For a full listing of cyclotides see CyBase [40]; b AA refers to the number of amino acids in the sequence; c Ch refers to the net charge of the cyclotide; d shows the sequences using one-letter amino acid codes, with the conserved Glu (E) bolded; e PDB ID code for 3D coordinates.
Cyclotides were originally discovered based on their observed bioactivities. The prototypical member of the family, kalata B1, was identified as the active uterotonic agent in a medicinal tea used by women in Africa to accelerate child birth. The plant used to make the tea is Oldenlandia affinis, a member of the Rubiaceae family of plants [41]. The first cyclotide discovered from the violet family, violapeptide 1, was fortuitously discovered while looking for haemolytic activity of saponins [42]. In one of the most significant early reports, a series of circular peptides was discovered in a screening program searching for anti-HIV molecules [29,43,44]. Similarly, cyclopsychotride A [45] was discovered during a screen for neurotensin antagonists. These initial bioassay-guided discoveries led to systematic searches for cyclotides based on their structural properties and this eventually led to the discovery of a wide range of other activities for cyclotides, including antimicrobial [46], insecticidal [22,47] and other pesticidal activities. I will describe these biological activities in more detail in Section 3, after making some brief comments on the biosynthesis and artificial synthesis of cyclotides.
Cyclotides are biosynthesized ribosomally as precursor proteins that encode one or more cyclotide domains [48,49]. Figure 2 shows the generic arrangement of a typical cyclotide precursor protein, which comprises an endoplasmic reticulum (ER) signal sequence, a pro-domain, a mature cyclotide domain and a C-terminal region. Although the excision and cyclization processes that yield cyclic mature peptides from these precursors are not fully understood, it is believed that asparaginyl endoproteinase (AEP) enzyme activity plays an important role [50,51]. This hypothesis is consistent with the presence of an absolutely conserved Asn (or Asp) residue that at the C-terminus of the cyclotide domain within the precursor proteins. (e.g., see cyclotide sequences in Table 1). It is further supported by studies involving expression of mutated cyclotides in transgenic plants that have identified residues important for processing. For example mutation of the conserved Asn to Ala abolishes production of cyclic peptides in planta [51].
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Figure 2. Schematic illustration of the architecture of cyclotide precursor proteins from the Violaceae and Rubiaceae. They comprise an ER signal sequence, an N-terminal prodomain, the mature peptide sequence and a C-terminal pro-peptide. Some precursors contain multiple copies (i.e., up to three copies) of the cyclotide domain flanked by short pro-peptide regions. Recent studies of cyclotides from the Fabaceae family have suggested that they are produced from what appears to be an ancestral albumin gene [20,52], suggesting that plants have evolved several alternative mechanisms for the biosynthesis of cyclotides.
Figure 2. Schematic illustration of the architecture of cyclotide precursor proteins from the Violaceae and Rubiaceae. They comprise an ER signal sequence, an N-terminal prodomain, the mature peptide sequence and a C-terminal pro-peptide. Some precursors contain multiple copies (i.e., up to three copies) of the cyclotide domain flanked by short pro-peptide regions. Recent studies of cyclotides from the Fabaceae family have suggested that they are produced from what appears to be an ancestral albumin gene [20,52], suggesting that plants have evolved several alternative mechanisms for the biosynthesis of cyclotides.
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2. Pesticidal and/or Toxic Activities

The natural function of cyclotides is thought to be for the protection of plants against pests, a suggestion prompted by the discovery that cyclotides potently inhibit the growth and development of certain insect larvae [47]. It is not known why an individual plant species can express so many different cyclotides. This phenomenon might have evolved to counter the development of resistance of pests to an individual defense molecule, or it might reflect that fact that cyclotides have an array of functions in plants that have so far not been identified. For example, some host defense peptides in animals have direct antimicrobial activity but also function as signaling molecules and immune modulators. Similar multifunctional roles might be possible for cyclotides but have so far not been reported. In this article the focus is on toxic activities of cyclotides. Table 2 summarizes examples of pesticidal and/or toxic activities of cyclotides. They include hemolytic, cytotoxic, antimicrobial, insecticidal, antifouling, molluscicidal and nematocidal activities.
Table
Table 2. Pesticidal and/or toxic activities reported for selected cyclotides.
Table 2. Pesticidal and/or toxic activities reported for selected cyclotides.
CyclotideActivityRef.
Möbius subfamily
kalata B1Insecticidal, molluscicidal, hemolytic, nematocidal, antibacterial, anti-HIV[47,53,54,55,56]
kalata B2Insecticidal, molluscicidal, nematocidal, antibacterial[22,56,57]
kalata B5Molluscicidal[56]
cycloviolacin O14Nematocidal, anti-HIV, hemolytic[26]
varv A & FCytotoxic[27,58]
Bracelet subfamily
circulin A & BHemolytic, anti-bacterial, anti-HIV[29]
cycloviolacin O1Nematocidal, molluscicidal[26,56,59,60]
cycloviolacin O2Nematocidal, cytotoxicity, hemolytic, anti-barnacle, antibacterial[57,61]
Cycloviolacin Y1Hemolytic, anti-HIV[62]
vhl-1Nematocidal, anti-HIV[36]
Trypsin inhibitor subfamily
MCoTI-IIProtease inhibition[63,64,65]

2.1. Hemolytic and Cytotoxic Activities

Hemolytic activity, i.e., the ability to cause lysis of erythrocytes, was one of the first activities reported for cyclotides and indeed led to the discovery of violapeptide-I [42]. Overall, cyclotides are only mildly hemolytic, with median hemolytic doses (HD50 values) of 10–1000 μM [66] which is weak compared to the potent hemolytic agent melittin from bee venom with a HD50 of ~1 μM. Interestingly, hemolytic activity is lost on linearization of cyclotides [67], showing that the intact cyclic backbone is important for this activity, as also appears to be the case for a number of other cyclotide activities, including anti-HIV activity.
So far there have been no reports describing a functional role for this hemolytic activity in a specific host defense interaction. Most investigations of the hemolytic activity of cyclotides have been more concerned with engineering out this activity for cases where a cyclotide framework is targeted for use as a pharmaceutical template. For example, an alanine scan identified a region of the kalata B1 surface in which substitution of any one of nine resides with Ala significantly reduced the hemolytic activity [68].
Various cyclotides have been reported to be cytotoxic to other human cell lines aside from erythrocytes. Cycloviolacin O2, a bracelet cyclotide, has been a particular focus of these studies and of most interest is a small degree of selective toxicity to cancer cell lines relative to normal cells, opening the possibility of uses of cyclotides in anti-cancer activity [58,69,70,71]. This activity however did not hold-up to be useful in a mouse tumor model [72]. The reasons for a lack of in vivo activity are not fully understood, but could include high clearance rates or poor distribution to the site of action in a poorly vascularized tumor model [72]. Also of concern from a pharmaceutical perspective is the finding that cycloviolacin O2 has a very abrupt toxicity profile, with lethality in mice at a single injection of 2 mg/kg but no signs of discomfort to the animals at 1.5 mg/kg [72].
Overall the cytotoxic activities of cyclotides appear to be confined to members of the Möbius and bracelet subfamilies and toxic activities have not been reported for members of the trypsin inhibitor subfamily.

2.2. Antimicrobial Activity

Antimicrobial activity of several synthetically produced cyclotides was first reported in 1999 [46] and there have only been a few other primary reports of this activity since then [20,73,74]. Overall, it appears that not all cyclotides are antimicrobial and that the positive examples have activity typically only under low salt conditions. In the initial study [46] four synthetically produced cyclotides, kalata B1, circulin A, circulin B and cyclopsychotride A, were tested against a range of human pathogenic bacteria, including E. coli and Staphylococcus aureus. The most potent example was circulin A against S. aureus, which had a minimum inhibitory concentration (MIC) of 0.19 µM, but kalata B1 was also reported to be highly potent (MIC = 0.26 µM) against S. aureus. Kalata B1 was inactive against E.coli under either high or low salt conditions but a later study reported conflicting data in E.coli. [73] Recent studies have confirmed antimicrobial activity for cycloviolacin O2, [74] and hedyotide B1 [20]. These studies have focused on testing against human pathogenic bacteria and it appears that there have been no systematic studies of the effect of cyclotides on plant-pathogenic bacteria. A recent report [57] did however examine the toxic effects of cyclotides against soil bacteria, and against several plants and algae, to determine the environmental effects of cyclotides, as further described in Section 6.

2.3. Insecticidal Activity

The first report of insecticidal activities of cyclotides was in 2001 where kalata B1 was shown to inhibit the growth and development and increase the mortality of Helicoverpa larvae presented with an artificial diet containing cyclotides [47]. When present in a diet at approximately the same concentration as it occurs in natural leaf tissue (~0.8 µmol/g), kalata B1 was found to be a potent insecticidal agent. These findings have since been reproduced in studies of kalata B2 [22] from O. affinis and Cter M from Clitoria ternatea. [19]. The mechanism of the insecticidal activity appears to be by disruption of the mid-gut membranes of larvae that have ingested cyclotides, as judged from electron microscopy studies [75]. Although insecticidal activity is presumed to be the primary natural biological function of cyclotides [76] there have not yet been systematic reports of their testing against a range of insect species, nor have there been studies of possible synergistic effects of cyclotides, given that a single plant often expresses a large number of cyclotides in any one tissue [12].

2.4. Anti-Fouling Activities

Cycloviolacin O2 has been reported to have activity against the barnacle Balanus improvisus in the sub-micromolar range [61]. Although there potentially could be applications of this activity in defouling ship hulls, the cost of cyclotides is likely to be a limiting factor in precluding such applications, unless considerably cheaper production methods for cyclotides can be developed than are currently available. It is interesting that cycloviolacin O2 is a member of the bracelet subfamily of cyclotides and that in general this subfamily tends to be more active in toxic properties against many organisms relative to the Möbius subclass.

2.5. Molluscicidal Activities

Cyclotides tested against Pomacea canaliculata, the Golden Apple snail, a major pest of rice in South East Asia have shown promising activities. This snail was originally imported into Taiwan from South America in the 1980s and has now spread widely in agricultural wetlands in Japan, the Philippines and Taiwan where it has caused crop damage estimated to have cost billions of dollars. The cyclotides cycloviolacin O1, kalata B1 and kalata B2 were found to be more toxic to Pomacea canaliculata than the commercially used molluscicide metaldehyde, whereas kalata B7 and B8 were significantly less toxic [56]. These assays showed that there was a dose dependent effect on snail mortality when cyclotides were introduced into the aquatic environment of the snails. The LC50 (median lethal concentration) was 53 µM for kalata B2 and 133 µM for metaldehyde. Tests of kalata B2 against a non-target fish species, Oreochromis niloticus, which has been used as a biological control agent in rice fields, revealed toxicity lower than rotenone, a naturally occurring commercial piscicidal agent. However, further detailed investigations on the relative toxicities of cyclotides against target and non-target species are required before cyclotides could be used to develop natural molluscicides.

2.6. Nematocidal Activities

The nematocidal activity of cyclotides has been extensively studied over the last few years, particularly against livestock pest nematodes [55,59,60]. In the first study [55] the in vitro effects of kalata B1, B2, B3, B5, B6 and B7 on the viability of egg, larval, and adult life stages of two species of economically important gastrointestinal nematode parasites of livestock, Hemonchus contortus and Trichostrongylus colubriformis were examined. The cyclotides showed significant activity in inhibiting development of nematode larvae and motility of adult worms, with activities comparable to some commercially used anthelmintic compounds. For example, kalata B6 was the most potent of the natural cyclotides tested, having a larvicidal activity (IC50) of 2.6 µg/mL against H. contortus. [55]. Alanine mutants of kalata B1 were assayed against larvae to determine residues responsible for activity and it was found that the anthelmintic activity was dramatically reduced as a consequence of the mutation of a series of residues clustered on one face of the molecule. Activities toward larvae were equivalent in the naturally occurring L-isomer of kalata B1 and a synthetic all-D-isomer, indicating that there is no chiral requirement for anthelmintic activity [55]. The clustering of “bioactive” residues and the lack of chiral selectivity supported a proposed mode of action of cyclotides that involves a membrane-based interaction rather than interaction with a stereospecific receptor. The cyclotide-induced leakage of a fluorescent dye from vesicles used as a model membrane mimetic further confirmed the membrane lytic ability of cyclotides. The relative potency of kalata B1 and kalata B2 in causing membrane leakage was consistent with the order of their anthelmintic activity.
This initial study was followed by a series of investigations that led to improved anthelmintic activity against these livestock pests [59,77], and also demonstrated activity against canine and human hookworms [60]. Overall, the results demonstrate that the cyclotides show potential for use in the control of nematode parasites of both agricultural and medical importance.

3. Mechanisms of Action

Although the range of biological activities of cyclotides might seem diverse, in fact they all appear to be accounted for by a common mechanism involving interactions of cyclotides with membranes and their subsequent disruption. In an early biophysical study NMR chemical shifts and diffusion measurements were used to demonstrate a specific interaction between a model membrane in the form of dodecylphosphocholine (DPC) micelles and the cyclotide kalata B1 [78]. This was followed by similar studies on B7 [79], which confirmed that a hydrophobic patch on the surface of the cyclotides (shown in Figure 1c) was the primary interaction face with membranes. The orientation of kalata B1 binding to the DPC surface is shown in Figure 3a. The precise orientation varies with different cyclotides, dependent on the location of the surface-exposed hydrophobic patch [80].
Independent studies showed that the membrane binding was functional, in that cyclotides were able to induce leakage of contents from phospholipid vesicles (Figure 3b) and form large pores in lipid bilayers [81], and that membrane binding modulated cytotoxicity [69]. Surface plasmon resonance studies [82,83] also established a specific interaction between cyclotides and phospholipid bilayers, as shown in Figure 3c [83]. These various studies have provided details on the selectivity of particular cyclotides for particular lipid subtypes. Overall, cyclotides appear to have a preference for phosphatidylethanolamine (PE) as opposed to phosphatidylcholine lipids (PC). Furthermore, for membranes of a given PE content kalata B1 has a higher affinity for membranes in a liquid disordered phase (i.e., more rigid membranes rich in cholesterol (Chol) and sphingomyelin (SM) that are raft-like domains [83]).
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Figure 3. Schematic illustration of studies done to establish membrane binding of cyclotides. Panel (a) shows preferred binding mode of kalata B1 to DPC micelles as deduced from NMR studies, indicating binding via the hydrophobic patch [78,80]; (b) shows vesicle leakage studies in which the addition of cyclotides to phospholipid vesicles causes leakage of vesicle contents in a dose dependent manner, with differential effects for different lipid compositions made up of palmitoyloleoylethanolamine (POPC), palmitoyloleoylethanolamine (POPE), cholesterol (Chol) and sphingomyelin (SM) [83]; (c) shows surface plasmon resonance studies indicating preferential binding to PE compared to PC lipids [83].
Figure 3. Schematic illustration of studies done to establish membrane binding of cyclotides. Panel (a) shows preferred binding mode of kalata B1 to DPC micelles as deduced from NMR studies, indicating binding via the hydrophobic patch [78,80]; (b) shows vesicle leakage studies in which the addition of cyclotides to phospholipid vesicles causes leakage of vesicle contents in a dose dependent manner, with differential effects for different lipid compositions made up of palmitoyloleoylethanolamine (POPC), palmitoyloleoylethanolamine (POPE), cholesterol (Chol) and sphingomyelin (SM) [83]; (c) shows surface plasmon resonance studies indicating preferential binding to PE compared to PC lipids [83].
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The ability to chemically synthesize or modify cyclotides has been important in establishing structure-activity relationships. As noted earlier, chemically modified cyclotide derivatives in which individual residues are successively replaced by alanine established that there was a patch of residues clustered on the surface of cyclotides that is important for biological activity [68]. This bioactive patch is not co-located with the hydrophobic patch implicated in membrane binding, which led to the suggestion that self-association may be involved in the mediation of cyclotide activity. Chemical modification studies have also established the importance of a key glutamic acid in regulating the activity of cyclotides. Esterification of this residue causes a marked drop in biological activity [84]. This residue is at the centre of the bioactive patch of residues on the kalata B1 cyclotide surface. The Glu residue is conserved in all but one of the currently known naturally occurring cyclotides, with the exception being kalata B12, where it is replaced with the conservative Asp residue. However, the precise role of the Glu in determining cyclotide activity is yet to be delineated.
In another example of the value of chemistry in determining structure-activity relationships of cyclotides a recent study used a chemically synthesized all-D kalata molecule to confirm the membrane binding hypothesis [83]. The insecticidal, anti-HIV and hemolytic activity of all-D and all-L mirror image forms of kalata B1 were similar, suggesting that a stereospecific receptor is not involved in the interaction. The slightly lower activity for the all-D peptide can be attributed to the slight chirality associated with membranes.
In summary, although cyclotides have a diverse range of activities, including antimicrobial, anti-HIV and hemolytic, and insecticidal, all these activities can be attributed to membrane binding interactions. In the case of insecticidal activity electron microscopy studies have shown clear disruption to the surface cells in the midgut of Lepidopteran larvae fed on a cyclotide-containing diet [75].

4. Methods of Production of Cyclotides

To commercially exploit cyclotides as pesticidal agents it will be necessary to develop cost-effective approaches for delivering them to target plants. Synthetic methods to produce cyclotides have been developed over the last decade, and include solid phase peptide synthesis approaches [46,85,86,87,88] as well as chemo-enzymatic [64,65,89,90] and biological approaches involving modified inteins [91,92,93]. So far, most of the proof-of-concept work on the structure-activity relationships of cyclotides has been done using chemically synthesized cyclotides analogues. Solid phase chemistry is the preferred method here and typically the ligation of the N and the C terminus is achieved using an adaptation of “native chemical ligation” chemistry [94,95]. This requires that the peptide chain be assembled linked to the resin with a thioester and the linear precursor sequence assembled in such an order that the N-terminal residue is a cysteine. This allows a trans-thioesterification reaction to achieve the cyclization, as highlighted in Figure 4.
This technology works well for Möbius trypsin inhibitor subfamily cyclotides although in the past the folding of the bracelet cyclotides has been problematic [96]. Several approaches have recently been developed to overcome this limitation and further improvement seems likely in the future [97,98].
Another approach to making cyclotides is to assemble them as conventional linear peptides and then achieve the cyclization enzymatically. This chemo-enzymatic approach can be done by engineering, for example, a trypsin active site into the linear cyclotide precursor and using trypsin to achieve the ligation. Proof-of-concept for this approach was established early for the cyclic peptide SFTI-I [99] and then adapted to the trypsin inhibitor cyclotide MCoTI-II [64,65,89,90]. One advantage of this approach is that the enzyme can be immobilized on a column and the cyclization achieved while the substrate flows through the column, thus leading to easy purification.
Toxins 04 00139 g004 1024
Figure 4. Schematic illustration of synthetic chemical approach for the production of cyclotides. The peptide chain is assembled using solid phase peptide chemistry (SPPS) with the C-terminal residue (aa1) linked to the resin using a thioester linker. Amino acids are added sequentially and the chain completed with an N-terminal cysteine. Since cyclotides contain six cysteines there are thus six possible linear cyclotide designs that could be used to produce a given cyclotide [87]. The linear cyclotide is cleaved from the solid-phase resin under acidic conditions. Cyclization occurs under basic conditions through a trans-esterification reaction and spontaneous S, N-acyl shift.
Figure 4. Schematic illustration of synthetic chemical approach for the production of cyclotides. The peptide chain is assembled using solid phase peptide chemistry (SPPS) with the C-terminal residue (aa1) linked to the resin using a thioester linker. Amino acids are added sequentially and the chain completed with an N-terminal cysteine. Since cyclotides contain six cysteines there are thus six possible linear cyclotide designs that could be used to produce a given cyclotide [87]. The linear cyclotide is cleaved from the solid-phase resin under acidic conditions. Cyclization occurs under basic conditions through a trans-esterification reaction and spontaneous S, N-acyl shift.
Toxins 04 00139 g004
Biological approaches to cyclotide synthesis have also been developed using E. coli as the host cells and modified inteins for activation of linear cyclotide precursors. This approach has been demonstrated for a range of cyclotides, including kalata B1 and MCoTI-II and has been used to produce small libraries of cyclotides and other cyclic peptides [11,91,92,93,100,101]. Although at this stage the yields are still relatively low compared to solid phase peptide synthesis approaches the biological approach has the potential to be less expensive.
In another biological approach, significant progress has been made in using plant cell culture methods for the production of native cyclotides. Specifically, Dörnenburg et al. [102,103,104,105] have developed a plant cell fermentation system and demonstrated excellent yields of native cyclotides in cultured O. affinis cells. Interestingly, the cultured cells not only produced cyclotides that had been identified in whole plant extracts of O. affinis but also produced some novel cyclotides not previously seen.
Despite the promise seen with SPPS or whole-cell-based approaches to cyclotide production, it seems likely that for large scale pesticidal applications of cyclotides a transgenic approach in which cyclotide genes are inserted directly into target plants is likely to be the most cost effective method. The main advantage of this approach is that the cyclotides are expressed only in the target organism thus potentially minimizing environmental impacts seen with traditional pesticidal applications through spraying. Proof-of-concept that cyclotides can be produced in model plants (tobacco and Arabidopsis) has been obtained in studies aimed at understanding the mechanistic basis of cyclotide processing [50,51].

5. Safety and Breakdown

The potential applications of cyclotides as pesticidal and/or pharmaceutical agents, merit safely evaluations of their effects in the environment. In a recent study [57] it was found that cyclotides were toxic to a range of test organisms, with EC50 values ranging from 12 to 140 µM against algae, 9–40 µM against duckweed, 4–50 µM against lettuce and 7–26 µM against soil bacteria. It was concluded that cyclotides might adversely affect solid and aquatic environments and that this should be taken into account in future risk assessments for cropping systems producing cyclotides. However, it also needs to be noted that cyclotides appear to be widely present naturally in a wide range of plants from the Rubiaceae, Violaceae, Cucurbitaceae and Fabaceae families and there are so far no reports of toxic effects in the environments associated with these naturally occurring cyclotides.
There have only been two studies that have reported chemical breakdown products of cyclotides [31,84] and it seems that more work in understanding cyclotide turnover is warranted to assess how stable these molecules are in their natural environment.

6. Conclusions

Although cyclotides were discovered only 15 years ago, they have developed into an exciting field of research and display a wide range of biological activities. At this stage it would appear that these activities are all associated with membrane interactions and given a demonstrated preference for cyclotides for some phospholipids over others it seems likely that cyclotides are targeted to specific cell types based on membrane composition to exert their biological activity. The rate of cyclotides discovery is rapidly evolving and the prediction of at around 50,000 members of the family may turn out to be an underestimate. Significant progress has been made in the chemistry for synthesizing cyclotides as well as in their biological synthesis. Thus there are now available an array of tools for the chemical production and modification of cyclotides, allowing further refinement of structure-activity relationships. Significant progress has also been made in the production of transgenic plants expressing cyclotides and so there appears to be great potential for the use of cyclotides as pesticidal agents, and indeed for modified cyclotides as medicines.

Acknowledgments

Work in my laboratory is funded by grants from the Australian Research Council (DP0984390) and the National Health and Medical Research Council (APP1009267). DJC is a NHMRC Professorial Fellow (569603). I thank David Wilson for assistance with drawing the figures and am very grateful to the many valuable contributions to cyclotide research by my students and colleagues as documented in the references.

Conflict of Interest

The author declares no conflict of interest other than being an inventor on patents associated with the pharmaceutical and agricultural uses of cyclotides.

References

  1. Craik, D.J.; Daly, N.L.; Bond, T.; Waine, C. Plant cyclotides: A unique family of cyclic and knotted proteins that defines the cyclic cystine knot structural motif. J. Mol. Biol. 1999, 294, 1327–1336. [Google Scholar]
  2. Gruber, C.W.; Elliott, A.G.; Ireland, D.C.; Delprete, P.G.; Dessein, S.; Goransson, U.; Trabi, M.; Wang, C.K.; Kinghorn, A.B.; Robbrecht, E.; Craik, D.J. Distribution and evolution of circular miniproteins in flowering plants. Plant Cell 2008, 20, 2471–2483. [Google Scholar]
  3. Trabi, M.; Craik, D.J. Tissue-specific expression of head-to-tail cyclized miniproteins in Violaceae and structure determination of the root cyclotide Viola hederacea root cyclotide1. Plant Cell 2004, 16, 2204–2216. [Google Scholar]
  4. Craik, D.J.; Daly, N.L.; Mulvenna, J.; Plan, M.R.; Trabi, M. Discovery, structure and biological activities of the cyclotides. Curr. Protein Pept. Sci. 2004, 5, 297–315. [Google Scholar]
  5. Göransson, U.; Svangard, E.; Claeson, P.; Bohlin, L. Novel strategies for isolation and characterization of cyclotides: The discovery of bioactive macrocyclic plant polypeptides in the Violaceae. Curr. Protein Pept. Sci. 2004, 5, 317–329. [Google Scholar]
  6. Gran, L.; Sandberg, F.; Sletten, K. Oldenlandia affinis (R&S) DC. A plant containing uteroactive peptides used in African traditional medicine. J. Ethnopharmacol. 2000, 70, 197–203. [Google Scholar] [CrossRef]
  7. Daly, N.L.; Rosengren, K.J.; Craik, D.J. Discovery, structure and biological activities of cyclotides. Adv.Drug Deliv. Rev. 2009, 61, 918–930. [Google Scholar]
  8. Pelegrini, P.B.; Quirino, B.F.; Franco, O.L. Plant cyclotides: An unusual class of defense compounds. Peptides 2007, 28, 1475–1481. [Google Scholar]
  9. Craik, D.J.; Cĕmažar, M.; Daly, N.L. The cyclotides and related macrocyclic peptides as scaffolds in drug design. Curr. Opin. Drug Discov. Dev. 2006, 9, 251–260. [Google Scholar]
  10. Craik, D.J.; Clark, R.J.; Daly, N.L. Potential therapeutic applications of the cyclotides and related cystine knot mini-proteins. Expert Opin. Investig. Drugs 2007, 16, 595–604. [Google Scholar]
  11. Sancheti, H.; Camarero, J.A. “Splicing up” drug discovery. Cell-based expression and screening of genetically-encoded libraries of backbone-cyclized polypeptides. Adv. Drug Deliv. Rev. 2009, 61, 908–917. [Google Scholar] [CrossRef]
  12. Gruber, C.W.; Cemazar, M.; Anderson, M.A.; Craik, D.J. Insecticidal plant cyclotides and related cystine knot toxins. Toxicon 2007, 49, 561–575. [Google Scholar]
  13. Saether, O.; Craik, D.J.; Campbell, I.D.; Sletten, K.; Juul, J.; Norman, D.G. Elucidation of the primary and three-dimensional structure of the uterotonic polypeptide kalata B1. Biochemistry 1995, 34, 4147–4158. [Google Scholar]
  14. Colgrave, M.L.; Craik, D.J. Thermal, chemical, and enzymatic stability of the cyclotide kalata B1: The importance of the cyclic cystine knot. Biochemistry 2004, 43, 5965–5975. [Google Scholar] [CrossRef]
  15. Craik, D.J.; Daly, N.L.; Waine, C. The cystine knot motif in toxins and implications for drug design. Toxicon 2001, 39, 43–60. [Google Scholar]
  16. Göransson, U.; Craik, D.J. Disulfide mapping of the cyclotide kalata B1. Chemical proof of the cyclic cystine knot motif. J. Biol. Chem. 2003, 278, 48188–48196. [Google Scholar]
  17. Rosengren, K.J.; Daly, N.L.; Plan, M.R.; Waine, C.; Craik, D.J. Twists, knots, and rings in protein. Structural definition of the cyclotide framework. J. Biol. Chem. 2003, 278, 8606–8616. [Google Scholar]
  18. Craik, D.J.; Cemazar, M.; Wang, C.K.; Daly, N.L. The cyclotide family of circular miniproteins: Nature’s combinatorial peptide template. Biopolymers 2006, 84, 250–266. [Google Scholar]
  19. Poth, A.G.; Colgrave, M.L.; Philip, R.; Kerenga, B.; Daly, N.L.; Anderson, M.A.; Craik, D.J. Discovery of cyclotides in the fabaceae plant family provides new insights into the cyclization, evolution, and distribution of circular proteins. ACS Chem. Biol. 2011, 6, 345–355. [Google Scholar] [CrossRef]
  20. Nguyen, G.K.; Zhang, S.; Nguyen, N.T.; Nguyen, P.Q.; Chiu, M.S.; Hardjojo, A.; Tam, J.P. Discovery and characterization of novel cyclotides originated from chimeric precursors consisting of albumin-1 chain a and cyclotide domains in the fabaceae family. J. Biol. Chem. 2011, 286, 24275–24287. [Google Scholar]
  21. Chiche, L.; Heitz, A.; Gelly, J.C.; Gracy, J.; Chau, P.T.; Ha, P.T.; Hernandez, J.F.; Le-Nguyen, D. Squash inhibitors: From structural motifs to macrocyclic knottins. Curr. Protein Pept. Sci. 2004, 5, 341–349. [Google Scholar]
  22. Jennings, C.V.; Rosengren, K.J.; Daly, N.L.; Plan, M.; Stevens, J.; Scanlon, M.J.; Waine, C.; Norman, D.G.; Anderson, M.A.; Craik, D.J. Isolation, solution structure, and insecticidal activity of kalata B2, a circular protein with a twist: Do Mobius strips exist in nature? Biochemistry 2005, 44, 851–860. [Google Scholar]
  23. Nair, S.S.; Romanuka, J.; Billeter, M.; Skjeldal, L.; Emmett, M.R.; Nilsson, C.L.; Marshall, A.G. Structural characterization of an unusually stable cyclic peptide, kalata B2 from Oldenlandia affinis. Biochim. Biophys.Acta 2006, 1764, 1568–1576. [Google Scholar]
  24. Craik, D.J. Plant cyclotides: Circular, knotted peptide toxins. Toxicon 2001, 39, 1809–1813. [Google Scholar]
  25. Wang, C.K.L.; Clark, R.J.; Cemazar, M.; Craik, D.J. Role of conserved Glu in cyclotide stability and activity: A structural and functional study of kalata B12, a naturally occurring Glu to Asp mutant. Biochemistry 2011, 50, 4077–4086. [Google Scholar]
  26. Ireland, D.C.; Colgrave, M.L.; Craik, D.J. A novel suite of cyclotides from Viola odorata: Sequence variation and the implications for structure, function and stability. Biochem. J. 2006, 400, 1–12. [Google Scholar]
  27. Wang, C.K.; Hu, S.H.; Martin, J.L.; Sjogren, T.; Hajdu, J.; Bohlin, L.; Claeson, P.; Goransson, U.; Rosengren, K.J.; Tang, J.; Tan, N.H.; Craik, D.J. Combined X-ray and NMR analysis of the stability of the cyclotide cystine knot fold that underpins its insecticidal activity and potential use as drug scaffold. J. Biol. Chem. 2009, 284, 10672–10683. [Google Scholar]
  28. Daly, N.L.; Koltay, A.; Gustafson, K.R.; Boyd, M.R.; Casas-Finet, J.R.; Craik, D.J. Solution structure by NMR of circulin A: A macrocyclic knotted peptide having anti-HIV activity. J. Mol. Biol. 1999, 285, 333–345. [Google Scholar]
  29. Gustafson, K.R.; Sowder, R.C.I.; Henderson, L.E.; Parsons, I.C.; Kashman, Y.; Cardellina, J.H.I.; McMahon, J.B.; Buckheit, R.W.J.; Pannell, L.K.; Boyd, M.R. Circulins A and B: Novel HIV-inhibitory macrocyclic peptides from the tropical tree Chassalia parvifolia. J. Am. Chem. Soc. 1994, 116, 9337–9338. [Google Scholar]
  30. Plan, M.R.; Rosengren, K.J.; Sando, L.; Daly, N.L.; Craik, D.J. Structural and biochemical characteristics of the cyclotide kalata B5 from Oldenlandia affinis. Biopolym. Pept. Sci. 2010, 94, 647–658. [Google Scholar]
  31. Plan, M.R.R.; Göransson, U.; Clark, R.J.; Daly, N.L.; Colgrave, M.L.; Craik, D.J. The cyclotide fingerprint in Oldenlandia affinis: Elucidation of chemically modified, linear and novel macrocyclic peptides. ChemBioChem 2007, 8, 1001–1011. [Google Scholar]
  32. Daly, N.L.; Clark, R.J.; Plan, M.R.; Craik, D.J. Kalata B8, a novel antiviral circular protein, exhibits conformational flexibility in the cystine knot motif. Biochem. J. 2006, 393, 619–626. [Google Scholar] [CrossRef]
  33. Mulvenna, J.P.; Sando, L.; Craik, D.J. Processing of a 22 kDa precursor protein to produce the circular protein tricyclon A. Structure 2005, 13, 691–701. [Google Scholar]
  34. Barry, D.G.; Daly, N.L.; Bokesch, H.R.; Gustafson, K.R.; Craik, D.J. Solution structure of the cyclotide palicourein: Implications for the development of a pharmaceutical framework. Structure 2004, 12, 85–94. [Google Scholar]
  35. Bokesch, H.R.; Pannell, L.K.; Cochran, P.K.; Sowder, R.C., II; McKee, T.C.; Boyd, M.R. A novel anti-HIV macrocyclic peptide from Palicourea condensata. J. Nat. Prod. 2001, 64, 249–250. [Google Scholar] [CrossRef]
  36. Chen, B.; Colgrave, M.L.; Daly, N.L.; Rosengren, K.J.; Gustafson, K.R.; Craik, D.J. Isolation and characterization of novel cyclotides from Viola hederaceae: Solution structure and anti-HIV activity of vhl-1, a leaf-specific expressed cyclotide. J. Biol. Chem. 2005, 280, 22395–22405. [Google Scholar]
  37. Chen, B.; Colgrave, M.L.; Wang, C.; Craik, D.J. Cycloviolacin H4, a hydrophobic cyclotide from Viola hederaceae. J. Nat. Prod. 2006, 69, 23–28. [Google Scholar]
  38. Felizmenio-Quimio, M.E.; Daly, N.L.; Craik, D.J. Circular proteins in plants: Solution structure of a novel macrocyclic trypsin inhibitor from Momordica cochinchinensis. J. Biol. Chem. 2001, 276, 22875–22882. [Google Scholar]
  39. Heitz, A.; Hernandez, J.F.; Gagnon, J.; Hong, T.T.; Pham, T.T.; Nguyen, T.M.; Le-Nguyen, D.; Chiche, L. Solution structure of the squash trypsin inhibitor MCoTI-II. A new family for cyclic knottins. Biochemistry 2001, 40, 7973–7983. [Google Scholar]
  40. Wang, C.K.; Kaas, Q.; Chiche, L.; Craik, D.J. CyBase: A database of cyclic protein sequences and structures, with applications in protein discovery and engineering. Nucleic Acids Res. 2008, 36, D206–D210. [Google Scholar]
  41. Gran, L. An oxytocic principle found in Oldenlandia affinis DC. Medd. Nor. Farm. Selsk. 1970, 12, 173–180. [Google Scholar]
  42. Schöpke, T.; Hasan Agha, M.I.; Kraft, R.; Otto, A.; Hiller, K. Hämolytisch aktive komponenten aus Viola tricolor L. und Viola arvensis Murray. Sci. Pharm. 1993, 61, 145–153. [Google Scholar]
  43. Gustafson, K.R.; McKee, T.C.; Bokesch, H.R. Anti-HIV cyclotides. Curr. Protein Pept. Sci. 2004, 5, 331–340. [Google Scholar]
  44. Gustafson, K.R.; Walton, L.K.; Sowder, R.C.I.; Johnson, D.G.; Pannell, L.K.; Cardellina, J.H.I.; Boyd, M.R. New circulin macrocyclic polypeptides from Chassalia parvifolia. J. Nat. Prod. 2000, 63, 176–178. [Google Scholar]
  45. Witherup, K.M.; Bogusky, M.J.; Anderson, P.S.; Ramjit, H.; Ransom, R.W.; Wood, T.; Sardana, M. Cyclopsychotride A, A biologically active, 31-residue cyclic peptide isolated from Psychotria longipes. J. Nat. Prod. 1994, 57, 1619–1625. [Google Scholar] [CrossRef]
  46. Tam, J.P.; Lu, Y.A.; Yang, J.L.; Chiu, K.W. An unusual structural motif of antimicrobial peptides containing end-to-end macrocycle and cystine-knot disulfides. Proc. Natl. Acad. Sci. USA 1999, 96, 8913–8918. [Google Scholar]
  47. Jennings, C.; West, J.; Waine, C.; Craik, D.; Anderson, M. Biosynthesis and insecticidal properties of plant cyclotides: The cyclic knotted proteins from Oldenlandia affinis. Proc. Natl. Acad. Sci. USA 2001, 98, 10614–10619. [Google Scholar]
  48. Craik, D.J.; Anderson, M.A.; Barry, D.G.; Clark, R.J.; Daly, N.L.; Jennings, C.V.; Mulvenna, J. Discovery and structures of the cyclotides: Novel macrocyclic peptides from plants. Lett. Pep. Sci. 2002, 8, 119–128. [Google Scholar]
  49. Dutton, J.L.; Renda, R.F.; Waine, C.; Clark, R.J.; Daly, N.L.; Jennings, C.V.; Anderson, M.A.; Craik, D.J. Conserved structural and sequence elements implicated in the processing of gene-encoded circular proteins. J. Biol. Chem. 2004, 279, 46858–46867. [Google Scholar]
  50. Saska, I.; Gillon, A.D.; Hatsugai, N.; Dietzgen, R.G.; Hara-Nishimura, I.; Anderson, M.A.; Craik, D.J. An asparaginyl endopeptidase mediates in vivo protein backbone cyclisation. J. Biol. Chem. 2007, 282, 29721–29728. [Google Scholar]
  51. Gillon, A.D.; Saska, I.; Jennings, C.V.; Guarino, R.F.; Craik, D.J.; Anderson, M.A. Biosynthesis of circular proteins in plants. Plant J. 2008, 53, 505–515. [Google Scholar]
  52. Poth, A.G.; Colgrave, M.L.; Lyons, R.E.; Daly, N.L.; Craik, D.J. From the cover: Discovery of an unusual biosynthetic origin for circular proteins in legumes. Proc. Natl. Acad. Sci. USA 2011, 108, 10127–10132. [Google Scholar]
  53. Daly, N.L.; Gustafson, K.R.; Craik, D.J. The role of the cyclic peptide backbone in the anti-HIV activity of the cyclotide kalata B1. FEBS Lett. 2004, 574, 69–72. [Google Scholar]
  54. Gran, L. Oxytocic principles of Oldenlandia affinis. Lloydia 1973, 36, 174–178. [Google Scholar]
  55. Colgrave, M.L.; Kotze, A.C.; Huang, Y.H.; O’Grady, J.; Simonsen, S.M.; Craik, D.J. Cyclotides: Natural, circular plant peptides that possess significant activity against gastrointestinal nematode parasites of sheep. Biochemistry 2008, 47, 5581–5589. [Google Scholar]
  56. Plan, M.R.; Saska, I.; Cagauan, A.G.; Craik, D.J. Backbone cyclised peptides from plants show molluscicidal activity against the rice pest Pomacea canaliculata (golden apple snail). J. Agric. Food Chem. 2008, 56, 5237–5241. [Google Scholar]
  57. Ovesen, R.G.; Brandt, K.K.; Göransson, U.; Nilesen, J.; Hansen, H.C.B.; Cedergreen, N. Biomedicine in the environment: Cyclotides constitute potent natural toxins in plants and soil bacteria. Environ. Toxinol. Chem. 2011, 30, 119–1196. [Google Scholar]
  58. Lindholm, P.; Göransson, U.; Johansson, S.; Claeson, P.; Gullbo, J.; Larsson, R.; Bohlin, L.; Backlund, A. Cyclotides: A novel type of cytotoxic agents. Mol. Cancer Ther. 2002, 1, 365–369. [Google Scholar]
  59. Colgrave, M.L.; Kotze, A.C.; Ireland, D.C.; Wang, C.K.; Craik, D.J. The anthelmintic activity of the cyclotides: Natural variants with enhanced activity. ChemBioChem 2008, 9, 1939–1945. [Google Scholar]
  60. Colgrave, M.L.; Kotze, A.C.; Kopp, S.; McCarthy, J.S.; Coleman, G.T.; Craik, D.J. Anthelmintic activity of cyclotides: In vitro studies with canine and human hookworms. Acta Trop. 2009, 109, 163–166. [Google Scholar]
  61. Göransson, U.; Sjogren, M.; Svangard, E.; Claeson, P.; Bohlin, L. Reversible antifouling effect of the cyclotide cycloviolacin O2 against barnacles. J. Nat. Prod. 2004, 67, 1287–1290. [Google Scholar]
  62. Wang, C.K.; Colgrave, M.L.; Gustafson, K.R.; Ireland, D.C.; Göransson, U.; Craik, D.J. Anti-HIV cyclotides from the Chinese medicinal herb Viola yedoensis. J. Nat. Prod. 2008, 71, 47–52. [Google Scholar]
  63. Hernandez, J.F.; Gagnon, J.; Chiche, L.; Nguyen, T.M.; Andrieu, J.P.; Heitz, A.; Trinh Hong, T.; Pham, T.T.; le Nguyen, D. Squash trypsin inhibitors from Momordica cochinchinensis exhibit an atypical macrocyclic structure. Biochemistry 2000, 39, 5722–5730. [Google Scholar]
  64. Thongyoo, P.; Bonomelli, C.; Leatherbarrow, R.J.; Tate, E.W. Potent inhibitors of beta-tryptase and human leukocyte elastase based on the MCoTI-II scaffold. J. Med. Chem. 2009, 52, 6197–6200. [Google Scholar]
  65. Thongyoo, P.; Roque-Rosell, N.; Leatherbarrow, R.J.; Tate, E.W. Chemical and biomimetic total syntheses of natural and engineered MCoTI cyclotides. Org. Biomol. Chem. 2008, 6, 1462–1470. [Google Scholar]
  66. Daly, N.L.; Craik, D.J. Acyclic permutants of naturally occurring cyclic proteins. Characterization of cystine knot and beta -sheet formation in the macrocyclic polypeptide kalata B1. J. Biol. Chem. 2000, 275, 19068–19075. [Google Scholar]
  67. Barry, D.G.; Daly, N.L.; Clark, R.J.; Sando, L.; Craik, D.J. Linearization of a naturally occurring circular protein maintains structure but eliminates hemolytic activity. Biochemistry 2003, 42, 6688–6695. [Google Scholar]
  68. Simonsen, S.M.; Sando, L.; Rosengren, K.J.; Wang, C.K.; Colgrave, M.L.; Daly, N.L.; Craik, D.J. Alanine scanning mutagenesis of the prototypic cyclotide reveals a cluster of residues essential for bioactivity. J. Biol. Chem. 2008, 283, 9805–9813. [Google Scholar]
  69. Svangard, E.; Burman, R.; Gunasekera, S.; Lovborg, H.; Gullbo, J.; Goransson, U. Mechanism of action of cytotoxic cyclotides: Cycloviolacin O2 disrupts lipid membranes. J. Nat. Prod. 2007, 70, 643–647. [Google Scholar]
  70. Svangard, E.; Göransson, U.; Hocaoglu, Z.; Gullbo, J.; Larsson, R.; Claeson, P.; Bohlin, L. Cytotoxic cyclotides from Viola tricolor. J. Nat. Prod. 2004, 67, 144–147. [Google Scholar]
  71. Svangard, E.; Göransson, U.; Smith, D.; Verma, C.; Backlund, A.; Bohlin, L.; Claeson, P. Primary and 3-D modelled structures of two cyclotides from Viola odorata. Phytochemistry 2003, 64, 135–142. [Google Scholar]
  72. Burman, R.; Svedlund, E.; Felth, J.; Hassan, S.; Herrmann, A.; Clark, R.J.; Craik, D.J.; Bohlin, L.; Claeson, P.; Goransson, U.; Gullbo, J. Evaluation of toxicity and anti-tumour activity of cycloviolacin O2 in mice. Biopolym. Pept. Sci. 2010, 94, 626–634. [Google Scholar]
  73. Gran, L.; Sletten, K.; Skjeldal, L. Cyclic peptides from Oldenlandia affinis DC. Molecular and biological properties. Chem. Biodivers. 2008, 5, 2014–2022. [Google Scholar] [CrossRef]
  74. Pranting, M.; Loov, C.; Burman, R.; Goransson, U.; Andersson, D.I. The cyclotide cycloviolacin O2 from Viola odorata has potent bactericidal activity against Gram-negative bacteria. J. Antimicrob. Chemoth. 2010, 65, 1964–1971. [Google Scholar]
  75. Barbeta, B.L.; Marshall, A.T.; Gillon, A.D.; Craik, D.J.; Anderson, M.A. Plant cyclotides disrupt epithelial cells in the midgut of lepidopteran larvae. Proc. Natl. Acad. Sci. USA 2008, 105, 1221–1225. [Google Scholar]
  76. Craik, D.J. Circling the enemy: Cyclic proteins in plant defence. Trends Plant Sci. 2009, 14, 328–335. [Google Scholar]
  77. Huang, Y.H.; Colgrave, M.L.; Clark, R.J.; Kotze, A.C.; Craik, D.J. Lysine-scanning mutagenesis reveals an amendable face of the cyclotide kalata B1 for the optimization of nematocidal activity. J. Biol. Chem. 2010, 285, 10797–10805. [Google Scholar]
  78. Shenkarev, Z.O.; Nadezhdin, K.D.; Sobol, V.A.; Sobol, A.G.; Skjeldal, L.; Arseniev, A.S. Conformation and mode of membrane interaction in cyclotides. Spatial structure of kalata B1 bound to a dodecylphosphocholine micelle. FEBS J. 2006, 273, 2658–2672. [Google Scholar] [CrossRef]
  79. Shenkarev, Z.O.; Nadezhdin, K.D.; Lyukmanova, E.N.; Sobol, V.A.; Skjeldal, L.; Arseniev, A.S. Divalent cation coordination and mode of membrane interaction in cyclotides: NMR spatial structure of ternary complex Kalata B7/Mn2+/DPC micelle. J. Inorg. Biochem. 2008, 102, 1246–1256. [Google Scholar]
  80. Wang, C.K.; Colgrave, M.L.; Ireland, D.C.; Kaas, Q.; Craik, D.J. Despite a conserved cystine knot motif, different cyclotides have different membrane binding modes. Biophys. J. 2009, 97, 1471–1481. [Google Scholar]
  81. Huang, Y.H.; Colgrave, M.L.; Daly, N.L.; Keleshian, A.; Martinac, B.; Craik, D.J. The biological activity of the prototypic cyclotide Kalata B1 is modulated by the formation of multimeric pores. J. Biol. Chem. 2009, 284, 20699–20707. [Google Scholar]
  82. Kamimori, H.; Hall, K.; Craik, D.J.; Aguilar, M.I. Studies on the membrane interactions of the cyclotides kalata B1 and kalata B6 on model membrane systems by surface plasmon resonance. Anal. Biochem. 2005, 337, 149–153. [Google Scholar]
  83. Henriques, S.T.; Huang, Y.-H.; Rosengren, K.J.; Franquelim, H.G.; Carvalho, F.A.; Johnson, A.; Sonza, S.; Tachedjian, G.; Castanha, M.A.R.B.; Daly, N.L.; Craik, D.J. Decoding the membrane activity of the cyclotide kalata B1: The importance of phosphatidylethanolamine phospholipids and lipid organization hemolytic and anti-HIV activities. J. Biol. Chem. 201, 286, 24231–24241. [Google Scholar]
  84. Herrmann, A.; Svangard, E.; Claeson, P.; Gullbo, J.; Bohlin, L.; Goransson, U. Key role of glutamic acid for the cytotoxic activity of the cyclotide cycloviolacin O2. Cell. Mol. Life Sci. 2006, 63, 235–245. [Google Scholar]
  85. Tam, J.P.; Lu, Y.-A. Synthesis of large cyclic cystine-knot peptide by orthogonal coupling strategy using unprotected peptide precursors. Tetrahedron Lett. 1997, 38, 5599–5602. [Google Scholar]
  86. Tam, J.P.; Lu, Y.-A. A biomimetic strategy in the synthesis and fragmentation of cyclic protein. Protein Sci. 1998, 7, 1583–1592. [Google Scholar]
  87. Clark, R.J.; Daly, N.L.; Craik, D.J. Structural plasticity of the cyclic-cystine-knot framework: Implications for biological activity and drug design. Biochem. J. 2006, 394, 85–93. [Google Scholar]
  88. Daly, N.L.; Love, S.; Alewood, P.F.; Craik, D.J. Chemical synthesis and folding pathways of large cyclic polypeptides: Studies of the cystine knot polypeptide kalata B1. Biochemistry 1999, 38, 10606–10614. [Google Scholar]
  89. Thongyoo, P.; Jaulent, A.M.; Tate, E.W.; Leatherbarrow, R.J. Immobilized protease-assisted synthesis of engineered cysteine-knot microproteins. ChemBioChem 2007, 8, 1107–1109. [Google Scholar]
  90. Thongyoo, P.; Tate, E.W.; Leatherbarrow, R.J. Total synthesis of the macrocyclic cysteine knot microprotein MCoTI-II. Chem. Commun. (Camb) 2006, 2848–2850. [Google Scholar]
  91. Kimura, R.H.; Tran, A.-T.; Camarero, J.A. Biosynthesis of the cyclotide kalata B1 by using protein splicing. Angew. Chem. Int. Ed. 2006, 118, 987–990. [Google Scholar]
  92. Austin, J.; Wang, W.; Puttamadappa, S.; Shekhtman, A.; Camarero, J.A. Biosynthesis and biological screening of a genetically encoded library based on the cyclotide MCoTI-I. ChemBioChem 2009, 10, 2663–2670. [Google Scholar]
  93. Camarero, J.A.; Kimura, R.H.; Woo, Y.-H.; Shekhtman, A.; Cantor, J. Biosynthesis of a fully functional cyclotide inside living bacterial cells. ChemBioChem 2007, 8, 1363–1366. [Google Scholar]
  94. Dawson, P.E.; Muir, T.W.; Clark-Lewis, I.; Kent, S.B. Synthesis of proteins by native chemical ligation. Science 1994, 266, 776–779. [Google Scholar]
  95. Kent, S.B. Total chemical synthesis of proteins. Chem. Soc. Rev. 2009, 38, 338–351. [Google Scholar]
  96. Gunasekera, S.; Daly, N.L.; Anderson, M.A.; Craik, D.J. Chemical synthesis and biosynthesis of the cyclotide family of circular proteins. IUBMB Life 2006, 58, 515–524. [Google Scholar]
  97. Leta Aboye, T.; Clark, R.J.; Craik, D.J.; Goransson, U. Ultra-stable peptide scaffolds for protein engineering-synthesis and folding of the circular cystine knotted cyclotide cycloviolacin O2. ChemBioChem 2008, 9, 103–113. [Google Scholar]
  98. Gunasekera, S.; Daly, N.L.; Clark, R.J.; Craik, D.J. Dissecting the oxidative folding of circular cystine knot miniproteins. Antioxid. Redox Signal. 2009, 11, 971–980. [Google Scholar]
  99. Marx, U.C.; Korsinczky, M.L.; Schirra, H.J.; Jones, A.; Condie, B.; Otvos, L., Jr.; Craik, D.J. Enzymatic cyclization of a potent Bowman-Birk protease inhibitor, sunflower trypsin inhibitor-1, and solution structure of an acyclic precursor peptide. J. Biol. Chem. 2003, 278, 21782–21789. [Google Scholar]
  100. Austin, J.; Kimura, R.H.; Woo, Y.H.; Camarero, J.A. In vivo biosynthesis of an Ala-scan library based on the cyclic peptide SFTI-1. Amino Acids 2010, 38, 1313–1322. [Google Scholar]
  101. Jagadish, K.; Camarero, J.A. Cyclotides, a promising molecular scaffold for peptide-based therapeutics. Biopolymers 2010, 94, 611–616. [Google Scholar]
  102. Dörnenburg, H. Plant cell culture technology-harnessing a biological approach for competitive cyclotides production. Biotechnol. Lett. 2008, 30, 1311–1321. [Google Scholar]
  103. Dörnenburg, H. Progress in kalata peptide production via plant cell bioprocessing. Biotechnol. J. 2009, 4, 632–645. [Google Scholar]
  104. Dörnenburg, H.; Frickinger, P.; Seydel, P. Plant cell-based processes for cyclotides production. J. Biotechnol. 2008, 135, 123–126. [Google Scholar]
  105. Seydel, P.; Dörnenburg, H. Establishment of in vitro plants, cell and tissue cultures from Oldenlandia affinis for the production of cyclic peptides. Plant Cell Tissue Organ Cult. 2006, 85, 247–255. [Google Scholar]

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Craik, D.J. Host-Defense Activities of Cyclotides. Toxins 2012, 4, 139-156. https://doi.org/10.3390/toxins4020139

AMA Style

Craik DJ. Host-Defense Activities of Cyclotides. Toxins. 2012; 4(2):139-156. https://doi.org/10.3390/toxins4020139

Chicago/Turabian Style

Craik, David J. 2012. "Host-Defense Activities of Cyclotides" Toxins 4, no. 2: 139-156. https://doi.org/10.3390/toxins4020139

APA Style

Craik, D. J. (2012). Host-Defense Activities of Cyclotides. Toxins, 4(2), 139-156. https://doi.org/10.3390/toxins4020139

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