Abstract
Microtubule drugs such as paclitaxel, colchicine, vinblastine, trifluralin, or oryzalin form a chemically diverse group that has been reinforced by a large number of novel compounds over time. They all share the ability to change microtubule properties. The profound effects of disrupted microtubule systems on cell physiology can be used in research as well as anticancer treatment and agricultural weed control. The activity of microtubule drugs generally depends on their binding to α- and β-tubulin subunits. The microtubule drugs are often effective only in certain taxonomic groups, while other organisms remain resistant. Available information on the molecular basis of this selectivity is summarized. In addition to reviewing published data, we performed sequence data mining, searching for kingdom-specific signatures in plant, animal, fungal, and protozoan tubulin sequences. Our findings clearly correlate with known microtubule drug resistance determinants and add more amino acid positions with a putative effect on drug-tubulin interaction. The issue of microtubule network properties in plant cells producing microtubule drugs is also addressed.
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Introduction
Microtubule drugs (also known as mitotic poisons) constitute a variable group of compounds targeted against the microtubular cytoskeleton, an intricate intracellular system of hollow cylindrical polymers composed of αβ-tubulin dimers. They have been intensely studied for their actions in animal cells (reviewed in Jordan and Wilson (2004); Ganguly and Cabral (2011)), and some of them are widely used in anticancer treatment. Although several compounds have been exploited in agriculture for their herbicidal effects, their actions on plant cells are known to a lesser extent. Molecular effects of these compounds on fungi and protozoa have also been rarely studied.
The principal building blocks of microtubules are α- and β-tubulin subunits. Knowledge of their structure is crucial to understanding the binding of microtubule-active drugs. Both α- and β-tubulins are globular proteins consisting of approximately 450 amino acids each (Downing and Nogales 1998a) with ~40 % amino acid identity among α- and β-tubulins of each species, as determined from a wide array of tubulin sequences (Little and Seehaus 1988). Their 3D structures consist of two internal β-sheets surrounded by several α-helices (Nogales et al. 1998). This compact model of a tubulin subunit can still be dissected into several domains with diverse functions. The N-terminal domain, made of several closely packed α-helical and β-sheet units, binds GTP. The amino acid chain continues by a smaller intermediate domain. This is then followed by two antiparallel α-helices running along the two domains and thus forming an additional C-terminal domain. The C-terminal domain is the most variable part of the tubulin molecule and plays an important role in tubulin interactions with other proteins (Downing and Nogales 1998b; Lefèvre et al. 2011; Amos 2011).
Tubulin genes are present in all known eukaryotes, often in multiple copies (isotypes). Plants may have as many as 13 α- and 20 β-tubulin genes (Breviario et al. 2013), while there are 8 functional α- and 7 β-tubulin genes in humans (Verdier-Pinard et al. 2009). Both animal and plant tubulin isotypes are differentially expressed in various tissues (Radchuk 2009; Leandro-García et al. 2010).
α- and β-Tubulin subunits form stable heterodimers in the cell. In favorable conditions, the heterodimers assemble into microtubules, long hollow cylinders of 24 nm in diameter. They consist of a variable number of protofilaments—often 13 in mammals, but microtubules with 8–19 protofilaments have been observed in other organisms (Chrétien et al. 1992; Breviario et al. 2013). The protofilaments are arranged in a circle and run lengthwise from one end of the microtubule to the other. The C-terminal tubulin domains face the outer microtubule surface, whereas the N-terminal GTPase domains are exposed to the inner space and GTP is always bound between the neighboring subunits (Downing and Nogales 1998a; Amos 2011). One end of microtubules (called the “minus end”) is typically anchored, while the plus end grows into the surrounding cytoplasm by adding subunits with bound GTP. Periods of growth alternating with periods of rapid shortening constitute the basis for microtubule dynamics (Jordan 2002).
The overall arrangement of microtubular cytoskeleton inside eukaryotic cells is very diverse. Animal microtubules emanate from the centrosome, a microtubule organizing center (MTOC) where minus ends of microtubules are typically anchored. Vascular plants lack a centrosome, having instead a rather dispersed system of microtubules attached to various membranes (Wasteneys 2002; Brown and Lemmon 2007). The centrosome is also missing in cells of many fungi, as well as unicellular eukaryotes, i.e., protists (Adl et al. 2005). Protists also possess many intricate microtubule-based structures such as flagella, cilia, or axostyles. These structures have a precisely arranged heritable system of microtubules and often contain unusual types of tubulin (Gull 2001). Despite the differences, the overall structure and function of microtubules remain the same. Common and distinct features of various microtubular systems are reflected in their affinity towards an array of tubulin-binding compounds.
Microtubule drugs and mechanism of their action
The list of microtubule-active natural compounds is enormous and still continues to grow. The canonical drugs used in medicine include colchicine, paclitaxel (and related taxanes), and vinblastine (or other vinca alkaloids), but several hundred of other similarly acting compounds have been discovered, such as podophyllotoxin, cryptophycins, dolastatins, epothilones, discodermolides, halichondrin, and many others. Moreover, a significant proportion of known herbicides directly or indirectly act on microtubules (Vaughn and Lehnen 1991). This group is chiefly represented by dinitroaniline herbicides (oryzalin, trifluralin, benefin, ethylfluralin, pendimethalin, and prodiamine) and pyridine-based compounds such as dithiopyr and thiazopyr (Mallory-Smith 2003). Despite their diverse chemical structures (Fig. 1), most of them bind directly to a common substrate, tubulin, or microtubules. General characteristics of key microtubule drugs are shown in Table 1.
The compounds fall into two major groups according to their origin. Oryzalin and trifluralin are synthetic compounds of the dinitroaniline group, formerly manufactured as dyes in chemical industry. However, many other microtubule drugs are naturally occurring compounds, produced by plants, animals, or microbes to mimic endogenous microtubule regulators. They have probably evolved to prevent predation or herbivory (Dumontet and Jordan 2010) or to defend the organisms against parasites and pathogens (Wagner 1994). For instance, vinblastine was isolated from Madagascar periwinkle (Catharanthus roseus, formerly known as Vinca rosea), colchicine was obtained from meadow saffron (Colchicum autumnale), while paclitaxel originates from the bark of Pacific yew tree (Taxus brevifolia). Because of its efficiency, microtubule poison-based strategy of defense is a widespread phenomenon and can serve as an example of evolutionary convergence (Goodin et al. 2004).
The mechanism of action of microtubule drugs has been a hot topic of cell biology for decades. Still, the majority of our knowledge is derived from studies in animals or animal cell cultures. The compounds usually show affinity to one of three principal binding sites of tubulin (Fig. 2). The luminal side of β-subunit binds taxanes; the interdimer space between the β-subunit of one dimer and α-subunit of the following dimer binds vinca alkaloids; and the intradimeric space between the α- and β-subunits of one heterodimer, adjacent to the GTP of the α-subunit, binds colchicine (Jordan and Wilson 2004). Podophyllotoxin binds to the colchicine-binding site or at least overlaps with it (ter Haar et al. 1996; Sharma et al. 2010). The binding site of dinitroanilines (such as oryzalin) likely resides on the α-subunit, close to the dimer-dimer interface, although the exact location remains unknown (Dempsey et al. 2013). Drug binding typically leads to intricate conformational changes in the tubulin molecule and/or whole microtubules, as reviewed in Stanton et al. (2011).
Microtubule drugs are thought to act on cells by increasing (e.g., paclitaxel) or decreasing (e.g., colchicine and vinblastine) the mass of polymerized tubulin (Dumontet and Jordan 2010). However, as reviewed in Correia and Lobert (2001), microtubule drugs often also decrease duration and rate of microtubule growth or shortening and often increase the time that microtubules spend in the pause state, which reduces the microtubule dynamics. Importantly, the effects on microtubule dynamics generally occur at even very low drug concentrations at which the polymer mass remains largely unchanged (Jordan et al. 1992). The relevance of these two effects to the actual drug potency is a matter of debate (Jordan and Wilson 2004; Ganguly et al. 2010), and both mechanisms may apply.
Spindle microtubules are thought to be the ultimate target of these compounds, and investigators generally concentrate on the effects in proliferating cells such as those in tumors. On the other hand, only a small percentage of cells are dividing at any time in the tumor, calling the true target of microtubule drugs into question. Several scenarios have been presented to explain the discrepancies (Komlodi-Pasztor 2011; Mitchison 2012). Additionally, some studies point to a structural similarity between certain domains of tubulin and Bcl2 protein and show that paclitaxel may have more than one binding partner in the cell (Rodi et al. 1999; Ferlini et al. 2009), a phenomenon that could have functional consequences because Bcl2 is an important member of the apoptotic pathway. Whether such knowledge acquired from animal cells (and especially from cancer studies) is transferable to other kingdoms of life is an open question with no experimental data available.
Kingdom-specific effects: plants, animals, fungi, and protozoa
Both α- and β-tubulins are highly conserved proteins, and the evolutionary stability of their genes best resembles the conservative nature of histones. Tubulins are so conservative that a mix of tubulin heterodimers isolated from a chick brain and Chlamydomonas reinhardtii flagella easily copolymerizes into microtubules in vitro (Binder et al. 1975; Little et al. 1982). This would suggest that the effects of microtubule-binding drugs will be uniform in organisms belonging to distinct evolutionary groups. In reality, though, the ability to induce effects differs among the eukaryotic kingdoms (Table 2). The sensitivity of various eukaryotic groups towards particular microtubule drugs can be mapped on a cladogram of eukaryotes (Fig. 3).
Resistance to microtubule drugs is attributable to many biological and biochemical phenomena. These include alterations in apoptotic pathways and changes in interactions with microtubule-associated proteins (MAPs) or tubulin isotype expression as well as an increased efflux of microtubule drugs by transmembrane proteins from the family of ATP-binding cassette (ABC) transporters, which are often associated with multidrug resistance (Fojo and Menefee 2005). The role of conserved tubulin posttranslational modifications—such as acetylations, phosphorylations, or glutamylations—in the resistance to microtubule drugs has not been evaluated to our knowledge. These modifications have a strong influence on microtubule stability (Wloga and Gaertig 2010), an important factor in resistance to microtubule drugs, but the data regarding tubulin posttranslational modifications among eukaryotic kingdoms are rather insufficient. Finally, mutations in tubulin sequence constitute an important cause of resistance (Fojo and Menefee 2005). The relevance of such mutations and their connection to effects of microtubule drugs in various kingdoms of eukaryotic organisms are summarized below.
Colchicine
Colchicine is one of the oldest known and most notorious microtubule drugs, effectively blocking microtubule assembly in animal cells. Upon administration, the disrupted microtubular cytoskeleton leads to a mitotic arrest, decreased cell motility, and impaired exocytosis and endocytosis. Accumulation of pathological effects can result in multiorgan failure and death (Finkelstein et al. 2010). Unfortunately, colchicine’s anticancer action is difficult to achieve in safe dosage. However, the drug is prescribed for the treatment of gout—its antiinflammatory action has been explained by inhibition of both neutrophil migration and superoxide production (Nuki 2008). Why colchicine’s action on microtubules often leads to such harmful effects on health, compared with other safer anticancer microtubule drugs, remains an open question.
In plants, colchicine working concentrations are generally much higher than in animals (Table 2). These have enabled scientists to use colchicine for the induction of polyploidy in plant cells, although sometimes in concentrations as high as 6 mM (Berger and Witkus 1943; Siddiqi and Marwat 1983). The drug is reported to be effective on plants at 250 μM or even higher (Kramers and Stebbings 1977; Gunning and Hardham 1982; Morejohn and Fosket 1984; Caperta et al. 2006). However, lower concentrations (25–250 μM) were shown to affect plant cell viability in a dose-dependent manner; weakly induce mixoploidy (Ascough et al. 2008); and, in one case, change the normal phenotype of mitotic cells (Schmit and Lambert 1988). Protozoa and fungi are also highly resistant to colchicine, with affinity constants ∼10,000× weaker than in animals (Bode et al. 2002; Banerjee et al. 2007). TION of the colchicine solution. Alternatively, the sentece can be chaged as follows:"The growth of Physarum polycephalum amoebae was not inhibited by 100 uM colchicine (Quinlan et al. 1981),....."uM means micromolar, unfortunately greek letter (mi:) is missing in the "insert special character" feature.<br Type="_moz"/>"?>One hundred micromolar colchicine did not inhibit growth of Physarum polycephalum amoebae (Quinlan et al. 1981), and Tetrahymena pyriformis tubulin shows very low binding affinity towards colchicine (Kovács and Csaba 2006). Colchicine is apparently selectively directed against animal predators.
The relatively high affinity of colchicine towards animal tubulin has been associated with two animal-specific amino acid residues in the colchicine-binding region—Ala 248β and Pro 268β. They are substituted by Ser 248β and Val or Ile 268β in plants, fungi, and protists (α and β symbols denote positions in α- and β-tubulin, respectively). These substitutions probably lead to complex rearrangements in the tubulin molecule that are thought to disrupt hydrogen bonding of tubulin with colchicine (Banerjee et al. 2007). Protozoan β-tubulin was also modeled using Leishmania sp. sequence aligned to a known crystallographic structure, indicating that the colchicine-binding site is hindered by an extension and torsion of an α-helix and a displacement of a β-sheet, preventing colchicine access (Luis et al. 2013).
Taxanes
Taxanes are a group of microtubule drugs best represented by paclitaxel (Taxol) and several related semisynthetic compounds with a common mechanism of action. Paclitaxel disrupts microtubular cytoskeleton in animal cells by decreasing microtubule dynamics and (in higher concentrations) by causing tubulin to assemble into superfluous stable structures (Jordan 2002). Treatment with paclitaxel has been successful in several types of cancer although the action on tumor is associated with several adverse effects. Neutropenia (a decrease in the number of neutrophils, a subset of rapidly dividing white blood cells) is symptomatic of the antiproliferative effects of paclitaxel (Mitchison 2012). Similarly, peripheral neuropathy has been linked to disruption of microtubule-associated transport in sensory neurons and neuronal cell death in the tissues of cancer patients (Komlodi-Pasztor 2011).
Paclitaxel differs from many other microtubule drugs because it is almost equally effective in plant and animal cells (Vaughn and Vaughan 1988). It is claimed that the paclitaxel-binding site is more conserved among all eukaryotes than the colchicine-binding site (Morejohn and Fosket 1984). A compelling explanation for this observation is that paclitaxel is an “unknown” molecule for both animal and plant cells because this compound is synthesized by the endosymbiotic fungi, such as Taxomyces sp., colonizing the bark of Pacific yew tree (Stierle et al. 1993). Indeed, several species of fungi (representatives of basidiomycetes, ascomycetes, and deuteromycetes) were found to be resistant to taxane treatment (Wagner 1994). Wildtype Saccharomyces cerevisiae tubulin does not bind paclitaxel either (Foland et al. 2005). However, a thorough metabolic assay found no traces of taxanes in the Taxomyces sp. cells, although paclitaxel biosynthesis genes were initially detected in their genome (Staniek et al. 2009), possibly by means of horizontal gene transfer. Taxomyces sp. genome was later completely sequenced, and an extensive search yielded no paclitaxel biosynthesis genes whatsoever (Heinig et al. 2013). In the light of these studies, the proposed explanation for the paclitaxel-binding site conservation does not seem valid anymore.
It is noteworthy that Phytophthora sp. and Pythium sp. oomycetes were found to be sensitive to paclitaxel (Wagner 1994; Mu et al. 1999) in times when oomycetes were considered to be a class of fungi. The current placement of oomycetes in the kingdom Chromista, far from fungi, creates a more logical image of paclitaxel selectivity. Otherwise, trypanosomatid protozoa, such as Leishmania and Trypanosoma, are now known to be susceptible to paclitaxel in micromolar concentrations and in a dose-dependent manner (Baum et al. 1981; Kapoor et al. 1999; Havens et al. 2000).
A closer look on S. cerevisiae β-tubulin led to important insights concerning its resistance to paclitaxel. By comparing fungal and animal β-tubulin, five key amino acid residues were found that could confer tubulin resistance towards paclitaxel: yeast residues Ala 19β, Thr 23β, Gly 26β, Asn 227β, and Tyr 270β; they all locate to paclitaxel-binding regions. When these residues were artificially replaced by their animal counterparts (Lys 19β, Val 23β, Asp 26β, His 227β, and Phe 270β), the yeast became paclitaxel-sensitive (Gupta et al. 2003). All five substitutions were later discussed in terms of their effect on paclitaxel binding; some of them cause a loss of contact between paclitaxel and tubulin, and others prevent the structural distortions of tubulin that are required for binding of paclitaxel (Das et al. 2012). A molecular modelling study by Akbari et al. (2011) came to similar conclusions and stressed residue 227β as a key to fungal resistance to paclitaxel.
Dinitroanilines
Dinitroanilines represent a group of potent microtubule drugs used as preemergent herbicides, applied to seeds before germination. Oryzalin and trifluralin are the most commonly used compounds from this class.
Oryzalin (Surflan) has been called the “colchicine of the plant kingdom” (Bajer and Molè-Bajer 1986) because its effects on plants are similar to those of colchicine, decreasing the mass of polymerized microtubules. Plant bodies and tissues show a characteristic response to mitotic disruption, symptomatic of microtubular damage. In Arabidopsis thaliana treated with oryzalin, cell division is inhibited and deposition of cellulose is impaired, leading to malformation in the proliferating shoot and root meristem regions. Both effects are known consequences of microtubule disruption: inhibition of mitosis results from interference with mitotic spindle, and deposition of cellulose requires microtubules to achieve correct orientation of microfibrils. Interestingly, the cells do not enter apoptosis after oryzalin treatment and rather continue to increase their volume (Corson et al. 2009). This is unlike the typical behavior of similarly treated animal cells. On a subcellular level, chromosomes enter a prometaphase arrest in a so-called colchicine (C) mitosis (Vaughn and Lehnen 1991), reminiscent of the mitotic arrest seen in animal cells. Oryzalin treatment, like that with colchicine, can elicit polyploidy in plants in vitro (Yemets and Blume 2008).
Oryzalin acts mainly on grasses and a few broad-leafed plants (Altland et al. 2003); therefore, it can be safely applied to control weeds in field nurseries or in certain crops such as soybean. Soybean (Glycine max) is approximately 110× more resistant to oryzalin in the seed germination test than oat (Avena sativa) and 10× more resistant than ryegrass (Lolium sp.), a weed commonly eliminated by oryzalin. Systematically, monocots are the most sensitive to oryzalin while rosids (including cucumber, soybean, cabbage, and other crops as well as many wild plants) are usually the most resistant (Feutz 1992). These differences still wait for a satisfactory explanation; they might be attributed to shifted expression ratio of plant tubulin isotypes or to subtle changes in their sequence. Position 253α is believed to play an important role, influencing the strength of dimer-dimer contacts. Asn 253α of sensitive plants is often substituted by Thr 253α in resistant plant species, animals, and fungi. Positions 16α, 136α, 239α, and 252α are other examples of residues which follow this distribution pattern distinguishing sensitive and resistant species (Délye et al. 2004).
While oryzalin is generally a potent inhibitor of plant microtubules (10 nM oryzalin is enough to affect the course of anaphase in Haemanthus sp. endosperm cells), Xenopus endothelial primary culture was found to be highly resistant to oryzalin—concentrations as high as 50 μM caused only slight disturbances to the normal cell physiology and proliferation (Bajer and Molè-Bajer 1986; Dow et al. 2002). Rust Melampsora lini was observed to be also resistant to oryzalin, compared to its host plant (Kobayashi et al. 1997). Fungi, close relatives of animals (Baldauf and Palmer 1993), are generally believed to be resistant to oryzalin (Lyons-Abbott et al. 2010; Lopes et al. 2012). In contrast, many protozoa are sensitive to oryzalin treatment such as Plasmodium falciparum (Fennell et al. 2006; Dempsey et al. 2013), a plastid-carrying parasite that is evolutionarily closer to plants than it is to animals (Cavalier-Smith 2010). Similarly, oomycetes, which are now classified into Chromista, are susceptible to oryzalin (Utkhede 1982; Walker and Morey 1999).
The mechanism of oryzalin susceptibility and resistance has been covered in several studies. One of the first explanations was proposed by Anthony et al. (1998) who discovered a point mutation in a strain of goosegrass (Eleusine indica) responsible for oryzalin resistance. Nowadays, a number of point mutations have been identified which cause the acquisition of oryzalin resistance in plants or protozoa. These mutations sometimes localize to the proposed dinitroaniline-binding site (e.g., 136α Leu → Phe) or the GTPase activating domain (252α Val → Leu). Importantly, some of the known important substitution sites can elicit the same effect in both plants and protozoa. Moreover, 29 amino acid residues were found to be characteristic for both trypanosomatid and plant α-tubulins. These residues are not conserved in animal tubulins and thus could potentially be implicated in sensitivity (Traub-Cseko et al. 2001; Lyons-Abbott et al. 2010).
Trifluralin is the second most studied dinitroaniline compound currently in use as a herbicide. Like oryzalin, it causes microtubule disassembly in the cells, disrupts the correct course of mitosis, and inhibits root growth. In Chlamydomonas sp. algae, it blocks the regeneration of flagella (Hess and Bayer 1977). The drug has also been shown to be effective against various protozoan parasites such as Toxoplasma, Trypanosoma, Leishmania, and Cryptosporidium (Traub-Cseko et al. 2001). Cross-resistance to oryzalin has been reported from trifluralin-resistant strains of various organisms (Vaughn et al. 1987; Stokkermans et al. 1996). Conversely, animal cells are generally immune to the antimicrotubule effects of trifluralin; it does not bind to animal tubulin nor does it affect the cell culture growth in a saturated solution of trifluralin (Hess and Bayer 1977). However, trifluralin toxicity has been reported in various animals including carp (Poleksić and Karan 1999) and millipedes (Merlini et al. 2012). Mechanism of this toxicity remains unknown and there is no evidence of trifluralin binding to animal tubulin. Trifluralin effects on the growth of fungi have not been studied yet.
Vinca alkaloids
Vinca alkaloids (vinblastine, vincristine, vinflunine, and others) are natural or semisynthetic compounds first discovered in periwinkle C. roseus. They have profound effects on mammalian microtubules, inhibiting their dynamics and, in higher concentrations, promoting the microtubule disassembly (Ngan et al. 2000). Only limited information is available regarding the action of vinca alkaloids in nonmammalian organisms. They were shown to have antiparasitic effects against Trypanosoma cruzi, inhibiting its mitosis and affecting its cell shape (Grellier et al. 1999). The compounds also bind to Leishmania mexicana tubulin and interfere with its assembly at low micromolar concentrations (Werbovetz et al. 1999) and affect growth of T. pyriformis ciliates (Kovács and Csaba 2006). Plants are, to a very limited extent, susceptible to the effects of vinca alkaloids (Degraeve and Gilot-Delhalle 1972; Hillmann and Ruthmann 1982), but there is a general lack of more recent reports on the subject. Root tip cells of garden cress (Lepidium sativum) and broad bean (Vicia faba) show metaphase arrest at 100 μM concentration of vinblastine (Kramers and Stebbings 1977; Hillmann and Ruthmann 1982). Aspergillus nidulans mutant with hyperstable microtubules was not rescued by vinblastine, indicating a lack of activity in fungi (Kiso et al. 2004). Vinblastine elicits no effects in S. cerevisiae either (Bode et al. 2002).
Novel compounds
Traditional classes of microtubule drugs have been reinforced by many newer compounds of synthetic or natural origin (reviewed in Kingston (2009)). The latter include epothilones discovered in bacterium Sorangium cellulosum, combrestatins isolated from Cape Bushwillow tree (Combretum caffrum), and dolastatins from a sea slug Dolabella auricularia (Bollag et al. 1995; Pettit et al. 1989; Pettit et al. 1981). Additionally, bodies of marine sponges are a rich source of novel compounds, including discodermolide from Discodermia dissoluta, halichondrins from Halichondria okadai, and hemiasterlins from Hemiasterella minor (Gunasekera et al. 1990; Hirata and Uemura 1986; Talpir et al. 1994).
Very little information is available on the activity of these compounds apart from their antiproliferative effects on cancer cells. Some of them may have exploited new target positions on the tubulin molecule. Other novel compounds share their binding site with the traditional classes of microtubule drugs—such as epothilones, targeting the paclitaxel-binding region (Akbari et al. 2011). Still, epothilones have markedly different binding properties. In contrast to paclitaxel, epothilones bind to yeast S. cerevisiae tubulin and promote its assembly (Bode et al. 2002). This is explained by the fact that the two compounds are chemically very different even though they share a common binding site. Key residues for epothilone binding are conserved in fungi, and epothilone can withstand certain substitutions as its 3D structure is more flexible than that of paclitaxel (Akbari et al. 2011).
As more knowledge is acquired, the relative affinity of these compounds in diverse eukaryotes will prove enormously interesting. Notably, many of the compounds are of animal origin but act potently on growth of animal cancer cells. Such high potency of the compounds on representatives of “their own” kingdom is not seen in colchicine or vinblastine but can be compared to that of paclitaxel.
Tubulin comparisons: shedding light on differences in drug action
Microtubule drugs show distinct activity patterns among the various systematic groups of eukaryotes. To understand these differences, it is useful to compare amino acid sequences of α- and β-tubulin proteins of animals, plants, fungi, and various protists and search for outstanding substitutions. These often constitute the underlying cause of drug resistance.
Many tubulin mutations conferring resistance to microtubule drugs have been described to date, and two general mechanisms have been proposed to explain their impact. Firstly, the amino acid substitutions can localize to the binding sites of the microtubule drugs or to their immediate proximity. Alternatively, resistance to microtubule drugs can be caused by any mutation which alters the microtubule dynamics: for instance, drugs which stabilize microtubules are likely to be less potent in mutants with intrinsically higher microtubule dynamics. The spatial distribution of resistance-conferring mutations in tubulin was reviewed by Nyporko and Blume (2009). However, these are almost exclusively mutations conferring drug resistance in representatives of taxonomical groups that are normally sensitive to it—exceptions to the rules, so as to say.
Literature dealing with kingdom-specific differences in tubulin sequences, i.e., mutations typically yet exclusively found in some eukaryotic kingdoms, is much more limited. Older articles, using comparisons of electrophoretic mobility of tubulins, can be traced back to the pregenomic era (Little et al. 1981; Little et al. 1982; Little et al. 1984). Intriguingly, one of these articles was describing a fundamental difference between chromist and plant tubulin on one hand and animal tubulin on the other hand (Little et al. 1982). Fungi were not included in these comparisons. Nowadays, phylogenetic data can be used together with the known location of several drug-binding sites: high-resolution model paclitaxel-binding site (Löwe et al. 2001) or paclitaxel-, colchicine-, and vinblastine-binding regions defined by 6-ångström (Å) radiuses around the bound drug molecules (Huzil et al. 2006) as well as the most recent estimation of the dinitroaniline-binding site (Nyporko et al. 2009). Sequence analysis has elucidated several kingdom-specific mutations in tubulin (Traub-Cseko et al. 2001; Banerjee et al. 2007; Luis et al. 2013) which were mentioned in the previous chapter.
Hunting for the kingdom-specific tubulin mutations
Thanks to the progress in sequencing, virtually all important groups of eukaryotes are now represented by at least a partially known genome sequence in the databases. The ever-growing list of sequenced tubulins can be used to extract the outstanding substitutions from their sequences “across” the eukaryotic kingdoms. A data set of 88 α-tubulin and 73 β-tubulin polypeptide sequences (partially adapted from Banerjee et al. (2007)) was carefully aligned in search for common features and differences. These can subsequently be visualized with a sequence logo, which is, in its simplest design, a graphical representation of amino acids present in the polypeptide positions. The size of amino acid symbols in the figure reflects the frequency of the corresponding amino acids at the specific position.
In the analyzed collection of sequences, approximately half of all amino acid positions are identical in at least 95 % (225 amino acid residues in α-tubulin and 248 in β-tubulin). Conserved regions are distributed along the whole length of tubulin. They include, among others, the residues in the proximity of a bound GTP or a magnesium ion and at the longitudinal contacts between subunits. β-Tubulin is generally richer in long unbroken conserved regions than α-tubulin. The most prominent variable region is the acidic C-terminal domain. The unique conservativeness of tubulin has been explained by the immense functional constraints inflicted on the tubulin molecule, which has evolved to bind GTP and assemble into intricate dynamic polymers (Ludueña 2013).
Not all positions are conserved and a careful analysis of the sequences yields a number of kingdom-specific mutations. A total of 69 α-tubulin and 51 β-tubulin kingdom-specific substitutions were recovered (see Electronic Supplementary Figs. 1 and 2), including both conservative and nonconservative substitutions as even a change in one methyl group of a residue can influence the binding properties of tubulin to microtubule drugs (Burns 1992). Some of these changes can be so consistently conserved that they provide hints to specific evolutionary events; for instance, a closer look on positions 22β or 248β reveals that substitutions probably occurred in the common ancestor of subdivision Pezizomycotina, the crown group of ascomycete fungi which does not include “lower” ascomycetes such as Saccharomyces or Pneumocystis.
The recovered substitutions include not only many previously published positions but also some new ones which might deserve further investigation. Several examples are shown in Fig. 4. Among those already known are positions 19β, 23β, and 26β implicated in S. cerevisiae resistance to paclitaxel (Gupta et al. 2003); 248β and 268β responsible for colchicine affinity in animals (Banerjee et al. 2007); and 313β and others, hypothesized to confer resistance to colchicine in kinetoplastid protozoa such as Leishmania or Trypanosoma (Luis et al. 2013). Residue 268α was also proposed to be responsible for the selective action of dinitroanilines by (Anthony et al. 1998). Many others were reported by Traub-Cseko et al. (2001) to account for the selectivity pattern of dinitroanilines. Noticeably, position 248β has been described in three of the articles mentioned above (Traub-Cseko et al. 2001; Banerjee et al. 2007; Luis et al. 2013); it may indeed prove to be a hallmark of microtubule drug sensitivity in general. In contrast, a putative importance of residues 227β and 231β for fungal resistance to paclitaxel (Akbari et al. 2011) can be questioned as S. cerevisiae substitutions 227β His → Asn and 231β Ala → Ser are not kingdom-specific in any way. All kingdom-specific positions described in the cited literature are marked yellow in the Electronic Supplementary Figs. 1 and 2.
A few kingdom-specific positions reside in the vicinity of the proposed drug-binding sites, offering the most straightforward way of explaining selectivity of microtubule drugs. These include positions 23β and 26β in the paclitaxel-binding site (Löwe et al. 2001; Gupta et al. 2003), potentially responsible for fungal resistance to paclitaxel; the same may be true for 279β and 280β glutamines (shown in Fig. 4), located in the 6-Å area around the bound paclitaxel. Residue 232β is also a part of the 6-Å area around paclitaxel. Residues 238β, 248β, 257β, 350β, 351β, and 352β are located in the colchicine 6-Å area, but only 248β is specific for animals and thus could be accounted for colchicine selectivity. Residues 221β and 222β are found in the 6-Å vicinity of bound vinblastine (Huzil et al. 2006). Finally, 252α and 253α probably form a part of the proposed dinitroaniline-binding site (Nyporko et al. 2009). Previously undescribed kingdom-specific positions which reside in drug-binding sites or their surroundings include 252α (dinitroaniline site); 22β, 279β, and 280β (paclitaxel site); and 221β (vinblastine site). These have been marked blue in the Electronic Supplementary Figs. 1 and 2.
Some of the discovered kingdom-specific differences coincide with tubulin mutations known to cause resistance to microtubule drugs in various species of animals, plants, fungi, and protists (reviewed in Nyporko and Blume (2009)). Those could potentially be the sites which allowed drug-producing organisms to target the drug to their predators. Namely, it is the case of 268α Met → Thr mutation recorded in goosegrass and accounting for its resistance to dinitroanilines (Yamamoto et al. 1998), 383α Ala → Val in Chinese hamster cells leading to cross-resistance to vinblastine and colcemid (Hari et al. 2003), 26β Asp → Glu in KB-3-1 human cell line conferring resistance to taxanes (Hari et al. 2006), and 350β mutated Lys → Glu in C. reinhardtii and conferring resistance to colchicine and dinitroanilines (Lee and Huang 1990) or 350β Lys → Asn in human cell lines leading to resistance to indanocine, a synthetic colchicine site binding agent (Hua et al. 2001). None of these mutations simulate precisely the known kingdom-specific differences, but it is conceivable that resistance depends on a mere presence/absence of a key residue or chemical group. Overall, new point mutations rarely reside in the kingdom-specific positions, suggesting that the resistant lineages rarely “choose” from the pool of kingdom-specific sites. One notable exception are mutations in α-tubulin of Toxoplasma gondii lines which were selected for resistance to oryzalin; out of 17 identified mutation sites (Morrissette et al. 2004), 7 coincided with kingdom-specific mutations.
The outstanding conservation of tubulin, together with the presence of kingdom-specific substitutions, constitutes a living proof of the protein’s crucial role in the life of eukaryotic organisms. A gradually emerging concept will once be able to map regions of the protein that are important for resistance to various microtubule drugs.
Drug-producing species: a taste of their own medicine
Several plants produce their own antimicrotubule compounds in order to protect themselves from their herbivores, and these plant species are thus naturally subjected to high concentrations of their “own” poisons. In any case, the producer plants clearly must have a mechanism to escape the effects of microtubule-active drugs. Considering the importance of this phenomenon which might help us develop more powerful or more selective drugs, it comes as a surprise that the understanding of this topic is fragmentary and only a handful of articles have been published to date.
First, relatively little is known about the kinetics and dynamics of microtubule-active compounds inside the plant bodies. Endogenous alkaloids are produced in a certain plant organ or structure (seeds, bark, leaves) but can sometimes be transported to another organ where they often accumulate in the cell vacuoles. Some alkaloids can freely pass the vacuolar membrane (tonoplast), but, once inside this acidic compartment, they are protonated and effectively trapped (Shitan and Yazaki 2007). While this may apply to vinblastine and other alkaloids, paclitaxel has no ionizable side groups (Mahoney et al. 2003) and cannot be easily trapped inside the vacuole. High amounts of paclitaxel are therefore found in the plant cell wall (Choi et al. 2001).
The first mitotic poison to be discovered—and subsequently studied—was colchicine. Very soon, scientists began to wonder why Colchicum is unaffected even though the plant itself contains as much as 0.4 % colchicine by dry weight (Blakeslee 1939). Blakeslee compared the situation to the “snake and snake’s venom” conundrum and expressed a belief that Colchicum contains an antidote, which, although theoretically possible, has never been found in the plant. Further studies have shown that the resistance to colchicine is very specific—Colchicum is sensitive to acenaphthene, a different mitotic poison (Levan 1940). The biochemical mechanism for Colchicum resistance to colchicine is not known (Vaughn and Vaughan 1988), and no relevant publications have been published to date.
Several instances show that the plant resistance to its poison can be conferred by pharmacokinetic and pharmacodynamic characteristics of the drug inside the tissues of drug-producing plants. In the case of vinblastine-producing C. roseus, which is at least 100–1,000× less sensitive to its drug vinblastine than a control species (garden cress—Lepidium, family Brassicaceae), it is hypothesized that intracellular vinblastine is in its inactive form, which is secreted from the cells, and, during or after secretion, modified to become the active vinblastine molecule (Kramers and Stebbings 1977). This hypothesis, however, fails to explain why the active vinblastine would not reenter the cells. A similar yet more sophisticated scenario has been suggested for the resistance of Podophyllum peltatum to its microtubule-binding drug podophyllotoxin. This compound is present in the plant vacuoles as an inactive glucoside (podophyllotoxin-4-O-β-d-glucopyranoside) and thus cannot harm the plant. At the same time, however, a highly specific β-glucosidase is present in the cytosol but is practically inactive because its pH optimum lies in acidic values (5.0, compared with pH ∼7.0 in the cytosol). Only when insects feed on the Podophyllum plant, the cells are damaged, vacuolar membrane is disrupted and the enzyme comes into contact with its substrate. The acidic pH of the mix leads to rapid deglucosidation and activation of the podophyllotoxin, effectively poisoning the herbivorous insects (Dayan et al. 2003).
There are other solutions to being resistant to one’s own poisons. One of them is to alter the molecular target of the drug and thus escape its deleterious effects. One of the possible explanations for C. roseus resistance to vinblastine is that the vinca-binding site in tubulin is mutated to prevent the vinblastine from binding to it (Kramers and Stebbings 1977). This has, however, never been proven for vinblastine or, until recently, for any other tubulin-binding compound. As a part of the 1000 Plants Initiative (1KP), European yew tree (Taxus baccata) transcriptome was sequenced and its tubulin gene has recently been analyzed to allow comparison with other tubulins. Results show that the yew tree tubulin is highly mutated in the paclitaxel-binding region when compared with a homologous human tubulin gene. Sixty-five percent of all substitutions in α- and β-tubulins are located on the surface of β-tubulin. Moreover, 95 % of these are substitutions on the luminal side of β-tubulin, where paclitaxel-binding site is found. Some of the mutations are located adjacent to the nanopores which form in the microtubule wall and allow diffusion of paclitaxel towards the lumen of the microtubule, but subsequent analysis has shown that the size of these openings is not significantly altered by these substitutions (Tuszynski et al. 2012). Large-scale analyses are currently conducted on other plants such as Colchicum sp. (J. A. Tuszynski, University of Alberta, personal communication).
The resistance of the drug-producing marine sponges (Porifera) is as enigmatic as it is neglected in research. Thousands of new and promising compounds have been isolated from these marine invertebrates (Sipkema et al. 2005). Microtubule drugs constitute only a fraction of these, suggesting that their ability to produce drugs—while not causing harm to themselves—is a more general phenomenon. The production of toxic compounds by marine sponges may relate to their unusual body composition: up to 50–60 % of the sponge biomass is composed of endosymbiotic microorganisms such as actinobacteria and fungi. These microbes have sometimes been made responsible for the actual production of bioactive compounds (Thomas et al. 2010; Waters et al. 2010). In soil, actinobacteria are known to produce diverse bioactive compounds to compete with other microbes while being completely resistant to them (Hopwood 2007). Similar phenomenon might well explain the production of microtubule drugs by microbes living in the crowded sponge microenvironment. It will be very interesting to determine whether the compounds, produced by these endosymbionts, exert their activity against fungi or other competitors of drug-producing microbes inside marine sponges.
While marine sponges are presumably resistant to their toxins, their tubulin displays typical animal features including its sequence in the predicted drug-binding sites. Most importantly, the vinca-binding site of Halichondria sp., where halichondrin binds (Bai et al. 1991), is almost identical to the tubulin of vertebrates (unpublished data). It still remains a mystery why these compounds do not kill their host sponges while remaining active against human cancer cells—especially when taking into account that such drugs can often be produced in one cell and elicit their effect elsewhere (Waters et al. 2010).
Concluding remarks
We have summarized available information on two kinds of interspecies differences responsible for variable potency of microtubule drugs: changes specific for the various kingdoms of life (“kingdom-specific”) and changes in drug-producing organisms. Although it was shown that both phenomena can be connected to changes in general behavior of microtubule drugs (spatial separation, pharmacokinetic parameters), they have usually been attributed to differences in tubulin sequence. These phenomena enable us to inspect pharmacologically interesting processes. The nature of changes, altering the sensitivity to drugs, offers an inspiration for a more precise drug delivery and selectivity and might provide hints at the problem of drug resistance. The data may thus prove relevant to anticancer therapy and herbicide research.
Why some of the differences in tubulins are so conserved and kingdom-specific remains an open question. Tubulin has very similar functions in all the kingdoms of eukaryotes, and adaptive mutations posing an evolutionary advantage for their carrier are presumably rare. Conceivably, some mutations could be adaptations to the need of more dynamic or, conversely, rigid microtubules in various kingdoms of life. Some of the known differences on the surface of tubulin might well be explained by the presence of specific MAP-binding sites. In contrast, it is highly unlikely that the observed interkingdom differences are adaptations to microtubule drugs: these drugs did not exist at the moment of divergence of all the major eukaryotic clades. Rather, the selective nature of many microtubule drugs suggests that the drugs themselves evolved to exploit the preexisting differences in tubulins. This was achieved by, for instance, mimicking MAPs to bind to ancient binding sites as there was a selective pressure on compounds that would harm the natural enemies but not the producing species. This takes us to the examination of tubulins in drug-producing organisms which should be especially tolerant to high concentrations of their microtubule drugs. We have seen that, apart from altering the tubulin structure, they have also exploited other ways of achieving resistance.
Many differences in sensitivity to microtubule drugs could potentially be explained by the evolution of tubulin paralogs, i.e., tubulin isotypes. Information on the relative importance, distribution, and function of tubulin isotypes in various eukaryotes is, to a large extent, missing. Some aspects of drug sensitivity and resistance could hypothetically be attributed to differences in drug efflux (expression of drug transporters) or metabolism. There is also a complete lack of data on many drug-producing plants and their unexplained resistance to their own toxins. Several plant stories might be uncovered soon, but other microtubule drug-producing organisms, such as marine sponges (Porifera) should not be missed out of focus either.
References
Adl SM, Simpson AGB, Farmer MA, Andersen RA, Anderson OR, Barta JR, Bowser SS et al (2005) The new higher level classification of eukaryotes with emphasis on the taxonomy of protists. J Eukaryot Microbiol 52(5):399–451. doi:10.1111/j.1550-7408.2005.00053.x
Akbari V, Moghim S, Reza Mofid M (2011) Comparison of epothilone and taxol binding in yeast tubulin using molecular modeling. Avicenna J Med Biotechnol 3(4):167–175
Altland JE, Gilliam CH, Wehtje G (2003) Weed control in field nurseries. HortTechnology 13(1):9–14
Amos LA (2011) What tubulin drugs tell us about microtubule structure and dynamics. Semin Cell Dev Biol 22(9):916–926. doi:10.1016/j.semcdb.2011.09.014
Anthony RG, Waldin TR, Ray JA, Bright SWJ, Hussey PJ (1998) Herbicide resistance caused by spontaneous mutation of the cytoskeletal protein tubulin. Nature 393(6682):260–263
Ascough GD, van Staden J, Erwin JE (2008) Effectiveness of colchicine and oryzalin at inducing polyploidy in Watsonia lepida N.E. Brown. HortSci 43(7):2248–2251
Bai RL, Paull KD, Herald CL, Malspeis L, Pettit GR, Hamel E (1991) Halichondrin B and homohalichondrin B, marine natural products binding in the vinca domain of tubulin. Discovery of tubulin-based mechanism of action by analysis of differential cytotoxicity data. J Biol Chem 266(24):15882–15889
Bajer AS, Molè-Bajer J (1986) Drugs with colchicine-like effects that specifically disassemble plant but not animal microtubules. Ann N Y Acad Sci 466:767–784
Baldauf SL, Palmer JD (1993) Animals and fungi are each other’s closest relatives: congruent evidence from multiple proteins. Proc Natl Acad Sci U S A 90(24):11558–11562
Banerjee M, Roy D, Bhattacharyya B, Basu G (2007) Differential colchicine-binding across eukaryotic families: the role of highly conserved Pro268beta and Ala248beta residues in animal tubulin. FEBS Lett 581(26):5019–5023. doi:10.1016/j.febslet.2007.09.047
Baum SG, Wittner M, Nadler JP, Horwitz SB, Dennis JE, Schiff PB, Tanowitz HB (1981) Taxol, a microtubule stabilizing agent, blocks the replication of Trypanosoma cruzi. Proc Natl Acad Sci U S A 78(7):4571–4575
Berger CA, Witkus ER (1943) A cytological study of c-mitosis in the polysomatic plant Spinacia oleracea, with comparative observations on Allium cepa. Bull Torrey Bot Club 70(5):457. doi:10.2307/2481391
Binder LI, Dentler WL, Rosenbaum JL (1975) Assembly of chick brain tubulin onto flagellar microtubules from Chlamydomonas and sea urchin sperm. Proc Natl Acad Sci U S A 72(3):1122–1126
Blakeslee AF (1939) The present and potential service of chemistry to plant breeding. Am J Bot 26(3):163. doi:10.2307/2436533
Bode CJ, Gupta ML Jr, Reiff EA, Suprenant KA, Georg GI, Himes RH (2002) Epothilone and paclitaxel: unexpected differences in promoting the assembly and stabilization of yeast microtubules. Biochemistry (Mosc) 41(12):3870–3874
Bollag DM, McQueney PA, Zhu J, Hensens O, Koupal L, Liesch J, Goetz M et al (1995) Epothilones, a new class of microtubule-stabilizing agents with a taxol-like mechanism of action. Cancer Res 55(11):2325–2333
Breviario D, Gianì S, Morello L (2013) Multiple tubulins: evolutionary aspects and biological implications. Plant J Cell Mol Biol 75(2):202–218. doi:10.1111/tpj.12243
Brown RC, Lemmon BE (2007) The pleiomorphic plant MTOC: an evolutionary perspective. J Integr Plant Biol 49(8):1142–1153. doi:10.1111/j.1672-9072.2007.00538.x
Burns RG (1992) Analysis of the colchicine-binding site of β-tubulin. FEBS Lett 297(3):205–208. doi:10.1016/0014-5793(92)80538-R
Caperta AD, Delgado M, Ressurreicao F, Meister A, Jones RN, Ressurreição F, Viegas W et al (2006) Colchicine-induced polyploidization depends on tubulin polymerization in c-metaphase cells. Protoplasma 227(2–4):147–153. doi:10.1007/s00709-005-0137-z
Cavalier-Smith T (2010) Kingdoms Protozoa and Chromista and the eozoan root of the eukaryotic tree. Biol Lett 6(3):342–345. doi:10.1098/rsbl.2009.0948
Choi H-K, Kim S-I, Song J-Y, Son J-S, Hong S-S, Durzan DJ, Lee HJ (2001) Localization of paclitaxel in suspension culture of Taxus chinensis. J Microbiol Biotechnol 11(3):458–462
Chrétien D, Metoz F, Verde F, Karsenti E, Wade RH (1992) Lattice defects in microtubules: protofilament numbers vary within individual microtubules. J Cell Biol 117(5):1031–1040
Correia JJ, Lobert S (2001) Physiochemical aspects of tubulin-interacting antimitotic drugs. Curr Pharm Des 7(13):1213–1228
Corson F, Hamant O, Bohn S, Traas J, Boudaoud A, Couder Y (2009) Turning a plant tissue into a living cell froth through isotropic growth. Proc Natl Acad Sci 106(21):8453–8458. doi:10.1073/pnas.0812493106
Crooks GE, Hon G, Chandonia J-M, Brenner SE (2004) WebLogo: a sequence logo generator. Genome Res 14(6):1188–1190. doi:10.1101/gr.849004
Das L, Bhattacharya B, Basu G (2012) Rationalization of paclitaxel insensitivity of yeast β-tubulin and human βIII-tubulin isotype using principal component analysis. BMC Res Notes 5(1):395. doi:10.1186/1756-0500-5-395
Dayan FE, Kuhajek JM, Canel C, Watson SB, Moraes RM (2003) Podophyllum peltatum possesses a beta-glucosidase with high substrate specificity for the aryltetralin lignan podophyllotoxin. Biochim Biophys Acta 1646(1–2):157–163
Degraeve N, Gilot-Delhalle J (1972) Cytological effects of vinblastine in plants. Experientia 28(5):581–582. doi:10.1007/BF01931891
Délye C, Menchari Y, Michel S, Darmency H (2004) Molecular bases for sensitivity to tubulin-binding herbicides in green foxtail. Plant Physiol 136(4):3920–3932. doi:10.1104/pp. 103.037432
Dempsey E, Prudêncio M, Fennell BJ, Gomes-Santos CS, Barlow JW, Bell A (2013) Antimitotic herbicides bind to an unidentified site on malarial parasite tubulin and block development of liver-stage Plasmodium parasites. Mol Biochem Parasitol 188(2):116–127. doi:10.1016/j.molbiopara.2013.03.001
Dhamodharan R, Jordan MA, Thrower D, Wilson L, Wadsworth P (1995) Vinblastine suppresses dynamics of individual microtubules in living interphase cells. Mol Biol Cell 6(9):1215–1229
Dow GS, Armson A, Boddy MR, Itenge T, McCarthy D, Parkin JE, Thompson RCA et al (2002) Plasmodium: assessment of the antimalarial potential of trifluralin and related compounds using a rat model of malaria, Rattus norvegicus. Exp Parasitol 100(3):155–160. doi:10.1016/S0014-4894(02)00016-4
Downing KH, Nogales E (1998a) Tubulin and microtubule structure. Curr Opin Cell Biol 10(1):16–22
Downing KH, Nogales E (1998b) Tubulin structure: insights into microtubule properties and functions. Curr Opin Struct Biol 8(6):785–791
Dumontet C, Jordan MA (2010) Microtubule-binding agents: a dynamic field of cancer therapeutics. Nat Rev Drug Discov 9(10):790–803. doi:10.1038/nrd3253
Fennell BJ, Naughton JA, Dempsey E, Bell A (2006) Cellular and molecular actions of dinitroaniline and phosphorothioamidate herbicides on Plasmodium falciparum: tubulin as a specific antimalarial target. Mol Biochem Parasitol 145(2):226–238. doi:10.1016/j.molbiopara.2005.08.020
Ferlini C, Cicchillitti L, Raspaglio G, Bartollino S, Cimitan S, Bertucci C, Mozzetti S et al (2009) Paclitaxel directly binds to Bcl-2 and functionally mimics activity of Nur77. Cancer Res 69(17):6906–6914. doi:10.1158/0008-5472.CAN-09-0540
Feutz E (1992) Evaluating the effects of oryzalin on the germination, emergence, and vegetative vigor of non-target terrestrial plants: Lab Project Number: 40292; ABC Labs, Inc. 155 p.; MRID# 42602401. http://www.epa.gov/oppsrrd1/REDs/0186.pdf. Accessed 10 Jan 2014
Filho SA, Pereira de Almeida ER, Gander ES (1978) The influence of hydroxyurea and colchicine on growth and morphology of Trypanosoma cruzi. Acta Trop 35(3):229–237
Finkelstein Y, Aks SE, Hutson JR, Juurlink DN, Nguyen P, Dubnov-Raz G, Pollak U et al (2010) Colchicine poisoning: the dark side of an ancient drug. Clin Toxicol Phila Pa 48(5):407–414. doi:10.3109/15563650.2010.495348
Fojo AT, Menefee M (2005) Microtubule targeting agents: basic mechanisms of multidrug resistance (MDR). Semin Oncol 32:3–8. doi:10.1053/j.seminoncol.2005.09.010
Foland TB, Dentler WL, Suprenant KA, Gupta ML Jr, Himes RH (2005) Paclitaxel-induced microtubule stabilization causes mitotic block and apoptotic-like cell death in a paclitaxel-sensitive strain of Saccharomyces cerevisiae. Yeast Chichester Engl 22(12):971–978. doi:10.1002/yea.1284
Ganguly A, Cabral F (2011) New insights into mechanisms of resistance to microtubule inhibitors. Biochim Biophys Acta 1816(2):164–171. doi:10.1016/j.bbcan.2011.06.001
Ganguly A, Yang H, Cabral F (2010) Paclitaxel dependent cell lines reveal a novel drug activity. Mol Cancer Ther 9(11):2914–2923. doi:10.1158/1535-7163.MCT-10-0552
Gigant B, Ravelli R, Wang C, Knossow M, Roussi F, Steinmetz MO, Curmi PA et al (2005) Structural basis for the regulation of tubulin by vinblastine. Nature 435(7041):519–522. doi:10.1038/nature03566
Goodin S, Kane MP, Rubin EH (2004) Epothilones: mechanism of action and biologic activity. J Clin Oncol 22(10):2015–2025. doi:10.1200/JCO.2004.12.001
Grellier P, Sinou V, Garreau-de Loubresse N, Bylèn E, Boulard Y, Schrével J (1999) Selective and reversible effects of vinca alkaloids on Trypanosoma cruzi epimastigote forms: blockage of cytokinesis without inhibition of the organelle duplication. Cell Motil Cytoskeleton 42(1):36–47. doi:10.1002/(SICI)1097-0169(1999)42:1<36::AID-CM4>3.0.CO;2-G
Gull K (2001) Protist tubulins: new arrivals, evolutionary relationships and insights to cytoskeletal function. Curr Opin Microbiol 4(4):427–432. doi:10.1016/S1369-5274(00)00230-7
Gunasekera SP, Gunasekera M, Longley RE, Schulte GK (1990) Discodermolide: a new bioactive polyhydroxylated lactone from the marine sponge Discodermia dissoluta. J Org Chem 55(16):4912–4915. doi:10.1021/jo00303a029
Gunning BES, Hardham AR (1982) Microtubules. Annu Rev Plant Physiol 33(1):651–698. doi:10.1146/annurev.pp. 33.060182.003251
Gupta ML Jr, Bode CJ, Georg GI, Himes RH (2003) Understanding tubulin–Taxol interactions: mutations that impart Taxol binding to yeast tubulin. Proc Natl Acad Sci U S A 100(11):6394–6397. doi:10.1073/pnas.1131967100
Haber JE, Peloquin JG, Halvorson HO, Borisy GG (1972) Colcemid inhibition of cell growth and the characterization of a colcemid-binding activity in Saccharomyces cerevisiae. J Cell Biol 55(2):355–367
Hari M, Wang YQ, Veeraraghavan S, Cabral F (2003) Mutations in alpha- and beta-tubulin that stabilize microtubules and confer resistance to colcemid and vinblastine. Mol Cancer Ther 2(7):597–605
Hari M, Loganzo F, Annable T, Tan XZ, Musto S, Morilla DB, Nettles JH et al (2006) Paclitaxel-resistant cells have a mutation in the paclitaxel-binding region of beta-tubulin (AsP(26)Glu) and less stable microtubules. Mol Cancer Ther 5(2):270–278. doi:10.1158/1535-7163.MCT-05-0190
Hart JW, Sabnis DD (1976) Colchicine binding activity in extracts of higher plants. J Exp Bot 27(6):1353–1360. doi:10.1093/jxb/27.6.1353
Havens CG, Bryant N, Asher L, Lamoreaux L, Perfetto S, Brendle JJ, Werbovetz KA (2000) Cellular effects of leishmanial tubulin inhibitors on L. donovani. Mol Biochem Parasitol 110(2):223–236. doi:10.1016/S0166-6851(00)00272-3
Heinig U, Scholz S, Jennewein S (2013) Getting to the bottom of Taxol biosynthesis by fungi. Fungal Divers 60(1):161–170. doi:10.1007/s13225-013-0228-7
Hess FD, Bayer DE (1977) Binding of the herbicide trifluralin to Chlamydomonas flagellar tubulin. J Cell Sci 24(1):351–360
Hillmann G, Ruthmann A (1982) Effect of mitotic inhibitors on the ultrastructure of root meristem cells. Planta 155(2):124–132. doi:10.1007/BF00392542
Hirata Y, Uemura D (1986) Halichondrins—antitumor polyether macrolides from a marine sponge. Pure Appl Chem 58(5):701–710. doi:10.1351/pac198658050701
Hopwood DA (2007) How do antibiotic-producing bacteria ensure their self-resistance before antibiotic biosynthesis incapacitates them? Mol Microbiol 63(4):937–940. doi:10.1111/j.1365-2958.2006.05584.x
Hua XQH, Genini D, Gussio R, Tawatao R, Shih H, Kipps TJ, Carson DA et al (2001) Biochemical genetic analysis of indanocine resistance in human leukemia. Cancer Res 61(19):7248–7254
Huzil JT, Ludueña RF, Tuszynski J (2006) Comparative modelling of human β tubulin isotypes and implications for drug binding. Nanotechnology 17(4):S90–S100. doi:10.1088/0957-4484/17/4/014
Jordan MA (2002) Mechanism of action of antitumor drugs that interact with microtubules and tubulin. Curr Med Chem Anti-Cancer Agents 2(1):1–17
Jordan MA, Wilson L (2004) Microtubules as a target for anticancer drugs. Nat Rev Cancer 4(4):253–265. doi:10.1038/nrc1317
Jordan MA, Thrower D, Wilson L (1992) Effects of vinblastine, podophyllotoxin and nocodazole on mitotic spindles. Implications for the role of microtubule dynamics in mitosis. J Cell Sci 102:401–416
Jordan MA, Toso RJ, Thrower D, Wilson L (1993) Mechanism of mitotic block and inhibition of cell proliferation by taxol at low concentrations. Proc Natl Acad Sci U S A 90(20):9552–9556
Kapoor P, Sachdeva M, Madhubala R (1999) Effect of the microtubule stabilising agent taxol on leishmanial protozoan parasites in vitro. FEMS Microbiol Lett 176(2):429–435
Kingston DGI (2009) Tubulin-interactive natural products as anticancer agents. J Nat Prod 72(3):507–515. doi:10.1021/np800568j
Kiso T, Fujita K-I, Ping X, Tanaka T, Taniguchi M (2004) Screening for microtubule-disrupting antifungal agents by using a mitotic-arrest mutant of Aspergillus nidulans and novel action of phenylalanine derivatives accompanying tubulin loss. Antimicrob Agents Chemother 48(5):1739–1748. doi:10.1128/AAC.48.5.1739-1748.2004
Kobayashi I, Kobayashi Y, Hardham AR (1997) Inhibition of rust-induced hypersensitive response in flax cells by the microtubule inhibitor oryzalin. Aust J Plant Physiol 24(6):733–740
Komlodi-Pasztor E (2011) Mitosis is not a key target of microtubule agents in patient tumors. Nat Rev Clin Oncol 8(4):244–250
Kovács P, Csaba G (2006) Effect of drugs affecting microtubular assembly on microtubules, phospholipid synthesis and physiological indices (signalling, growth, motility and phagocytosis) in Tetrahymena pyriformis. Cell Biochem Funct 24(5):419–429. doi:10.1002/cbf.1238
Kramers MR, Stebbings H (1977) The insensitivity of Vinca rosea to vinblastine. Chromosoma 61(3):277–287
Leandro-García LJ, Leskelä S, Landa I, Montero-Conde C, López-Jiménez E, Letón R, Cascón A et al (2010) Tumoral and tissue-specific expression of the major human beta-tubulin isotypes. Cytoskeleton Hoboken NJ 67(4):214–223. doi:10.1002/cm.20436
Lee V, Huang B (1990) Missense mutations at lysine-350 in beta-2-tubulin confer altered sensitivity to microtubule inhibitors in Chlamydomonas. Plant Cell 2(11):1051–1057
Lefèvre J, Chernov KG, Joshi V, Delga S, Toma F, Pastré D, Curmi PA et al (2011) The C terminus of tubulin, a versatile partner for cationic molecules: binding of Tau, polyamines, and calcium. J Biol Chem 286(4):3065–3078. doi:10.1074/jbc.M110.144089
Levan A (1940) The effect of acenaphthene and colchicine on mitosis of Allium and Colchicum. Hereditas 26(3–4):262–276. doi:10.1111/j.1601-5223.1940.tb03236.x
Liebmann JE, Cook JA, Lipschultz C, Teague D, Fisher J, Mitchell JB (1993) Cytotoxic studies of paclitaxel (Taxol) in human tumour cell lines. Br J Cancer 68(6):1104–1109
Little M, Seehaus T (1988) Comparative analysis of tubulin sequences. Comp Biochem Physiol B Comp Biochem 90(4):655–670. doi:10.1016/0305-0491(88)90320-3
Little M, Ludueña RF, Langford GM, Asnes CF, Farrell K (1981) Comparison of proteolytic cleavage patterns of α-tubulins and β-tubulins from taxonomically distant species. J Mol Biol 149(1):95–107. doi:10.1016/0022-2836(81)90262-X
Little M, Ludueña RF, Keenan R, Asnes CF (1982) Tubulin evolution: two major types of α-tubulin. J Mol Evol 19(1):80–86. doi:10.1007/BF02100226
Little M, Luduena R, Morejohn L, Asnes C, Hoffman E (1984) The tubulins of animals, plants, fungi and protists implications for metazoan evolution. Orig Life Evol Biosph 13(3–4):169–176. doi:10.1007/BF00927168
Lopes R, Eleutério CV, Gonçalves LMD, Cruz MEM, Almeida AJ (2012) Lipid nanoparticles containing oryzalin for the treatment of leishmaniasis. Eur J Pharm Sci Off J Eur Fed Pharm Sci 45(4):442–450. doi:10.1016/j.ejps.2011.09.017
Löwe J, Li H, Downing KH, Nogales E (2001) Refined structure of alpha beta-tubulin at 3.5 A resolution. J Mol Biol 313(5):1045–1057. doi:10.1006/jmbi.2001.5077
Ludueña RF (2013) Chapter Two—A hypothesis on the origin and evolution of tubulin. In: Kwang W. Jeon (ed) Int. Rev. Cell Mol. Biol. Academic Press, pp 41–185
Luis L, Serrano ML, Hidalgo M, Mendoza-León A (2013) Comparative analyses of the β-tubulin gene and molecular modeling reveal molecular insight into the colchicine resistance in kinetoplastids organisms. BioMed Res Int. doi: 10.1155/2013/843748
Lyons-Abbott S, Sackett DL, Wloga D, Gaertig J, Morgan RE, Werbovetz KA, Morrissette NS (2010) α-Tubulin mutations alter oryzalin affinity and microtubule assembly properties to confer dinitroaniline resistance. Eukaryot Cell 9(12):1825–1834. doi:10.1128/EC.00140-10
Mahoney BP, Raghunand N, Baggett B, Gillies RJ (2003) Tumor acidity, ion trapping and chemotherapeutics. I. Acid pH affects the distribution of chemotherapeutic agents in vitro. Biochem Pharmacol 66(7):1207–1218
Mallory-Smith CA (2003) Revised classification of herbicides by site of action for weed resistance management strategies. Weed Technol 17(3):605–617
Merlini VV, Nogarol LR, Marin-Morales MA, Fontanetti CS (2012) Toxicity of trifluralin herbicide in a representative of the edaphic fauna: histopathology of the midgut of Rhinocricus padbergi (Diplopoda). Microsc Res Technol 75(10):1361–1369. doi:10.1002/jemt.22075
Mitchison TJ (2012) The proliferation rate paradox in antimitotic chemotherapy. Mol Biol Cell 23(1):1–6. doi:10.1091/mbc.E10-04-0335
Molè Bajer J, Bajer AS (1983) Action of taxol on mitosis: modification of microtubule arrangements and function of the mitotic spindle in Haemanthus endosperm. J Cell Biol 96(2):527–540. doi:10.1083/jcb.96.2.527
Morejohn LC, Fosket DE (1984) Taxol-induced rose microtubule polymerization in vitro and its inhibition by colchicine. J Cell Biol 99(1 Pt 1):141–147
Morejohn LC, Fosket DE (1991) The biochemistry of compounds with anti-microtubule activity in plant cells. Pharmacol Ther 51(2):217–230. doi:10.1016/0163-7258(91)90078-Z
Morrissette NS, Mitra A, Sept D, Sibley LD (2004) Dinitroanilines bind α-tubulin to disrupt microtubules. Mol Biol Cell 15(4):1960–1968. doi:10.1091/mbc.E03-07-0530
Mu JH, Bollon AP, Sidhu RS (1999) Analysis of beta-tubulin cDNAs from taxol-resistant Pestalotiopsis microspora and taxol-sensitive Pythium ultimum and comparison of the taxol-binding properties of their products. Mol Gen Genet 262(4–5):857–868
Ngan VK, Bellman K, Panda D, Hill BT, Jordan MA, Wilson L (2000) Novel actions of the antitumor drugs vinflunine and vinorelbine on microtubules. Cancer Res 60(18):5045–5051
Nogales E, Wolf SG, Downing KH (1998) Structure of the alpha beta tubulin dimer by electron crystallography. Nature 391(6663):199–203. doi:10.1038/34465
Nuki G (2008) Colchicine: its mechanism of action and efficacy in crystal-induced inflammation. Curr Rheumatol Rep 10(3):218–227
Nyporko AY, Blume YB (2009) Spatial distribution of tubulin mutations conferring resistance to antimicrotubular compounds. In: Blume YB, Baird WV, Yemets AI, Breviario D (eds) Plant cytoskelet. Key tool agro-biotechnol. Springer, Netherlands, pp 397–417
Nyporko AY, Yemets AI, Brytsun VN, Lozinsky MO, Blume YB (2009) Structural and biological characterization of the tubulin interaction with dinitroanilines. Cytol Genet 43(4):267–282. doi:10.3103/S0095452709040082
Pettit GR, Kamano Y, Fujii Y, Herald CL, Inoue M, Brown P, Gust D et al (1981) Marine animal biosynthetic constituents for cancer chemotherapy. J Nat Prod 44(4):482–485
Pettit GR, Singh SB, Hamel E, Lin CM, Alberts DS, Garcia-Kendall D (1989) Isolation and structure of the strong cell growth and tubulin inhibitor combretastatin A-4. Experientia 45(2):209–211
Poleksić V, Karan V (1999) Effects of trifluralin on carp: biochemical and histological evaluation. Ecotoxicol Environ Saf 43(2):213–221. doi:10.1006/eesa.1999.1790
Quinlan RA, Roobol A, Pogson CI, Gull K (1981) A correlation between in vivo and in vitro effects of the microtubule inhibitors colchicine, parbendazole and nocodazole on myxamoebae of Physarum polycephalum. J Gen Microbiol 122(1):1–6
Radchuk VV (2009) The transcriptome of the tubulin gene family in plants. In: Blume YB, Baird WV, Yemets AI, Breviario D (eds) Plant cytoskelet. Key tool agro-biotechnol. Springer Netherlands, Dordrecht, pp 219–241
Ravelli RBG, Gigant B, Curmi PA, Jourdain I, Lachkar S, Sobel A, Knossow M (2004) Insight into tubulin regulation from a complex with colchicine and a stathmin-like domain. Nature 428(6979):198–202. doi:10.1038/nature02393
Rodi DJ, Janes RW, Sanganee HJ, Holton RA, Wallace B, Makowski L (1999) Screening of a library of phage-displayed peptides identifies human Bcl-2 as a taxol-binding protein. J Mol Biol 285(1):197–203. doi:10.1006/jmbi.1998.2303
Rosenbaum JL, Carlson K (1969) Cilia regeneration in Tetrahymena and its inhibition by colchicine. J Cell Biol 40(2):415–425. doi:10.1083/jcb.40.2.415
Schmit AC, Lambert AM (1988) Plant actin filament and microtubule interactions during anaphase–telophase transition: effects of antagonist drugs. Biol Cell Auspices Eur Cell Biol Organ 64(3):309–319
Sharma S, Poliks B, Chiauzzi C, Ravindra R, Blanden AR, Bane S (2010) Characterization of the colchicine binding site on avian tubulin isotype βVI. Biochemistry (Mosc) 49(13):2932–2942. doi:10.1021/bi100159p
Shitan N, Yazaki K (2007) Accumulation and membrane transport of plant alkaloids. Curr Pharm Biotechnol 8(4):244–252
Siddiqi SH, Marwat KB (1983) Cytomorphological effects of colchicine on wheat (Triticum aestivum). Pak J Agric Res 4(2):120–125
Sipkema D, Franssen MCR, Osinga R, Tramper J, Wijffels RH (2005) Marine sponges as pharmacy. Mar Biotechnol N Y N 7(3):142–162. doi:10.1007/s10126-004-0405-5
Staniek A, Woerdenbag HJ, Kayser O (2009) Taxomyces andreanae: a presumed paclitaxel producer demystified? Planta Med 75(15):1561–1566. doi:10.1055/s-0029-1186181
Stanton RA, Gernert KM, Nettles JH, Aneja R (2011) Drugs that target dynamic microtubules: a new molecular perspective. Med Res Rev 31(3):443–481. doi:10.1002/med.20242
Stierle A, Strobel G, Stierle D (1993) Taxol and taxane production by Taxomyces andreanae, an endophytic fungus of Pacific yew. Science 260(5105):214–216
Stokkermans TJ, Schwartzman JD, Keenan K, Morrissette NS, Tilney LG, Roos DS (1996) Inhibition of Toxoplasma gondii replication by dinitroaniline herbicides. Exp Parasitol 84(3):355–370. doi:10.1006/expr.1996.0124
Talpir R, Benayahu Y, Kashman Y, Pannell L, Schleyer M (1994) Hemiasterlin and geodiamolide TA: two new cytotoxic peptides from the marine sponge Hemiasterella minor (Kirkpatrick). Tetrahedron Lett 35(25):4453–4456. doi:10.1016/S0040-4039(00)73382-X
Ter Haar E, Rosenkranz HS, Hamel E, Day BW (1996) Computational and molecular modeling evaluation of the structural basis for tubulin polymerization inhibition by colchicine site agents. Bioorg Med Chem 4(10):1659–1671
Thomas TRA, Kavlekar DP, LokaBharathi PA (2010) Marine drugs from sponge–microbe association—a review. Mar Drugs 8(4):1417–1468. doi:10.3390/md8041417
Traub-Cseko YM, Ramalho-Ortigão JM, Dantas AP, de Castro SL, Barbosa HS, Downing KH (2001) Dinitroaniline herbicides against protozoan parasites: the case of Trypanosoma cruzi. Trends Parasitol 17(3):136–141. doi:10.1016/S1471-4922(00)01834-1
Tuszynski JA, Craddock TJA, Mane JY, Barakat K, Tseng C-Y, Gajewski M, Winter P et al (2012) Modeling the yew tree tubulin and a comparison of its interaction with paclitaxel to human tubulin. Pharm Res 29(11):3007–3021. doi:10.1007/s11095-012-0829-y
Utkhede RS (1982) Effects of six herbicides on the growth of Phytophthora cactorum and a bacterial antagonist. Pestic Sci 13(6):693–695. doi:10.1002/ps.2780130617
Vaughn K, Lehnen L (1991) Mitotic disrupter herbicides. Weed Sci 39(3):450–457
Vaughn K, Vaughan M (1988) Mitotic disrupters from higher plants—effects on plant cells. Acs Symp Ser 380:273–293
Vaughn KC, Marks MD, Weeks DP (1987) A dinitroaniline-resistant mutant of Eleusine indica exhibits cross-resistance and supersensitivity to antimicrotubule herbicides and drugs. Plant Physiol 83(4):956–964
Verdier-Pinard P, Pasquier E, Xiao H, Burd B, Villard C, Lafitte D, Miller LM et al (2009) Tubulin proteomics: towards breaking the code. Anal Biochem 384(2):197–206. doi:10.1016/j.ab.2008.09.020
Wagner LJ (1994) Effect of taxol and related compounds on growth of plant pathogenic fungi. Phytopathology 84:1173–1178
Walker GE, Morey BG (1999) Effects of chemicals and microbial antagonists on nematodes and fungal pathogens of citrus roots. Aust J Exp Agric 39(5):629–637
Wasteneys GO (2002) Microtubule organization in the green kingdom: chaos or self-order? J Cell Sci 115(7):1345–1354
Waters AL, Hill RT, Place AR, Hamann MT (2010) The expanding role of marine microbes in pharmaceutical development. Curr Opin Biotechnol 21(6):780–786. doi:10.1016/j.copbio.2010.09.013
Werbovetz KA, Brendle JJ, Sackett DL (1999) Purification, characterization, and drug susceptibility of tubulin from Leishmania. Mol Biochem Parasitol 98(1):53–65
Williams NE, Williams RJ (1976) Macronuclear division with and without microtubules in Tetrahymena. J Cell Sci 20(1):61–77
Wloga D, Gaertig J (2010) Post-translational modifications of microtubules. J Cell Sci 123(20):3447–3455. doi:10.1242/jcs.063727
Yamamoto E, Zeng LH, Baird WV (1998) Alpha-tubulin missense mutations correlate with antimicrotubule drug resistance in Eleusine indica. Plant Cell 10(2):297–308. doi:10.1105/tpc.10.2.297
Yemets AI, Blume YB (2008) Progress in plant polyploidization based on antimicrotubular drugs. Open Hortic J 1:15–20
Acknowledgments
This work was partially supported by project UNCE204013. We would like to thank Dr. Vladimír Hampl, Dr. Marian Novotný, and Dr. Marie Macůrková for their helpful comments.
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The authors declare that they have no conflicts of interest.
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Dostál, V., Libusová, L. Microtubule drugs: action, selectivity, and resistance across the kingdoms of life. Protoplasma 251, 991–1005 (2014). https://doi.org/10.1007/s00709-014-0633-0
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DOI: https://doi.org/10.1007/s00709-014-0633-0