Patent Application
20120317681
Humans grow corn for food and energy applications. Humans also grow many other crops, including soybeans and cotton. Insects eat and damage plants and thereby undermine these human efforts. Billions of dollars are spent each year to control insect pests and additional billions are lost to the damage they inflict. Synthetic organic chemical insecticides have been the primary tools used to control insect pests but biological insecticides, such as the insecticidal proteins derived from Bacillus thuringiensis (Bt), have played an important role in some areas. The ability to produce insect-resistant plants through transformation with Bt insecticidal protein genes has revolutionized modern agriculture and heightened the importance and value of insecticidal proteins and their genes.
Several Bt proteins have been used to create the insect-resistant transgenic plants that have been successfully registered and commercialized to date. These include Cry1Ab, Cry1Ac, Cry1F and Cry3Bb in corn, Cry1Ac and Cry2Ab in cotton, and Cry3A in potato.
The commercial products expressing these proteins express a single protein except in cases where the combined insecticidal spectrum of 2 proteins is desired (e.g., Cry1Ab and Cry3Bb in corn combined to provide resistance to lepidopteran pests and rootworm, respectively) or where the independent action of the proteins makes them useful as a tool for delaying the development of resistance in susceptible insect populations (e.g., Cry1Ac and Cry2Ab in cotton combined to provide resistance management for tobacco budworm).
That is, some of the qualities of insect-resistant transgenic plants that have led to rapid and widespread adoption of this technology also give rise to the concern that pest populations will develop resistance to the insecticidal proteins produced by these plants. Several strategies have been suggested for preserving the utility of Bt-based insect resistance traits which include deploying proteins at a high dose in combination with a refuge, and alternation with, or co-deployment of, different toxins (McGaughey et al. (1998), “B.t. Resistance Management,” Nature Biotechnol. 16:144-146).
The proteins selected for use in an IRM stack need to exert their insecticidal effect independently so that resistance developed to one protein does not confer resistance to the second protein (i.e., there is not cross resistance to the proteins). If, for example, a pest population selected for resistance to “Protein A” is sensitive to “Protein B”, one would conclude that there is not cross resistance and that a combination of Protein A and Protein B would be effective in delaying resistance to Protein A alone.
In the absence of resistant insect populations, assessments can be made based on other characteristics presumed to be related to mechanism of action and cross-resistance potential. The utility of receptor-mediated binding in identifying insecticidal proteins likely to not exhibit cross resistance has been suggested (van Mellaert et al. 1999). The key predictor of lack of cross resistance inherent in this approach is that the insecticidal proteins do not compete for receptors in a sensitive insect species.
In the event that two Bt toxins compete for the same receptor, then if that receptor mutates in that insect so that one of the toxins no longer binds to that receptor and thus is no longer insecticidal against the insect, it might be the case that the insect will also be resistant to the second toxin (which competitively bound to the same receptor). That is, the insect is said to be cross-resistant to both Bt toxins. However, if two toxins bind to two different receptors, this could be an indication that the insect would not be simultaneously resistant to those two toxins.
Cry1Fa is useful in controlling many lepidopteran pests species including the European corn borer (ECB; Ostrinia nubilalis (Hübner)) and the fall armyworm (FAW; Spodoptera frugiperda), and is active against the sugarcane borer (SCB; Diatraea saccharalis).
The Cry1Fa protein, as produced in corn plants containing event TC1507, is responsible for an industry-leading insect resistance trait for FAW control. Cry1Fa is further deployed in the Herculex®, SmartStax™, and WideStrike™ products.
The ability to conduct (competitive or homologous) receptor binding studies using Cry1Fa protein is limited because the most common technique available for labeling proteins for detection in receptor binding assays inactivates the insecticidal activity of the Cry1Fa protein.
Additional Cry toxins are listed at the website of the official B.t. nomenclature committee (Crickmore et al.; lifesci.sussex.ac.uk/home/Neil_Crickmore/Bt/). See Appendix A, attached. There are currently nearly 60 main groups of “Cry” toxins (Cry1-Cry59), with additional Cyt toxins and VIP toxins and the like. Many of each numeric group have capital-letter subgroups, and the capital letter subgroups have lower-cased letter sub-subgroups. (Cry1 has A-L, and Cry1A has a-i, for example).
The subject invention relates in part to the surprising discovery that a fall armyworm (Spodoptera frugiperda; FAW) population selected for resistance to the insecticidal activity of the Cry1Fa protein is not resistant to the insecticidal activity of the Cry1Ca protein. As one skilled in the art will recognize with the benefit of this disclosure, plants expressing these two insecticidal proteins, or insecticidal portions thereof, will be useful in delaying or preventing the development of resistance to either of these insecticidal proteins alone.
The subject invention is also supported by the discovery that Cry1Fa and Cry1Ca do not compete with each other for binding gut receptors from FAW (or from Diatraea saccharalis (sugarcane borer; SCB)).
The subject invention also relates in part to triple stacks or “pyramids” of three (or more) toxins, with Cry1Fa and Cry1C toxins being the base pair. One preferred pyramid provides at least two proteins providing non-cross-resistant activity against two pests—the FAW and the ECB (European corn borer; Ostrinia nubilalis): Cry1Fa plus Cry1Ca plus one or more anti-ECB toxins such as Cry1Ab. In some preferred pyramid embodiments, the selected toxins have three separate modes of action against FAW. Preferred pyramid combinations are Cry1Fa plus Cry1Ca plus another toxin/gene selected from the group consisting of Vip3Ab, Cry1D, Cry1Be, and Cry1E. Plants (and acreage planted with such plants) that produce these three toxins are included within the scope of the subject invention. Additional toxins/genes can also be added, but these particular triple stacks would, according to the subject invention, advantageously and surprisingly provide three modes of action against FAW. This can help to reduce or eliminate the requirement for refuge acreage. The subject invention also relates generally to the use of three insecticidal proteins (Cry proteins in some preferred embodiments) that do not compete with each other against a single target pest.
SEQ ID NO:1 Cry1Ca core/Cry1Ab protoxin chimeric protein 1164 aa (DIG-152) (pMYC2547 version)
SEQ ID NO:2 second Cry1Ca core/Cry1Ab protoxin chimeric protein 1164 aa (DIG-109) (maize version)
SEQ ID NO:3 maize-optimized CDS encoding DIG-109 3492 bp
SEQ ID NO:4 is a Cry1Fa core toxin.
SEQ ID NO:5 is a Cry1Ca core toxin.
As reported herein, Cry1Ca toxin produced in transgenic corn and other plants (cotton and soybeans, for example) is very effective in controlling fall armyworm (FAW; Spodoptera frugiperda) that have developed resistance to Cry1Fa activity. Thus, the subject invention relates in part to the surprising discovery that fall armyworm resistant to Cry1Fa are susceptible (i.e., are not cross-resistant) to Cry1Ca.
The subject invention also relates in part to the surprising discovery that Cry1Ca toxin is effective at protecting plants (such as maize plants) from damage by Cry1Fa-resistant fall armyworm. For a discussion of this pest See e.g. Tabashnik, PNAS (2008), vol. 105 no. 49, 19029-19030.
The subject invention includes the use of Cry1Ca toxin to protect corn and other economically important plant species from damage and yield loss caused by fall armyworm feeding or to fall armyworm populations that have developed resistance to Cry1Fa.
The subject invention thus teaches an IRM stack to prevent or mitigate against the development of resistance by fall armyworm to Cry1Fa and/or Cry1Ca.
The present invention provides compositions for controlling lepidopteran pests comprising cells that produce a Cry1Fa core toxin-containing protein and a Cry1Ca core toxin-containing protein.
The invention further comprises a host transformed to produce both a Cry1Fa core toxin-containing protein and a Cry1Ca core toxin-containing protein, wherein said host is a microorganism or a plant cell. The subject polynucleotide(s) are preferably in a genetic construct under control (operably linked to/comprising) of a non-Bacillus-thuringiensis promoter. The subject polynucleotides can comprise codon usage for enhanced expression in a plant.
It is additionally intended that the invention provides a method of controlling lepidopteran pests comprising contacting said pests or the environment of said pests with an effective amount of a composition that contains a Cry1Fa core toxin-containing protein and further contains a Cry1Ca core toxin-containing protein.
An embodiment of the invention comprises a maize plant (and other plants—cotton and soybeans, for example) comprising a plant-expressible gene encoding a Cry1Ca core toxin-containing protein and a plant-expressible gene encoding a Cry1Fa core toxin-containing protein, and seed of such a plant.
A further embodiment of the invention comprises a maize plant (and other plants—cotton and soybeans, for example) wherein a plant-expressible gene encoding a Cry1Ca core toxin-containing protein and a plant-expressible gene encoding a Cry1Fa core toxin-containing protein have been introgressed into said maize plant, and seed of such a plant.
(For a review of Cry1C as a potential bioinsecticide in plants, see Avisar et al. 2009). Avisar D, Eilenberg H, Keller M, Reznik N, Segal M, Sneh B, Zilberstein A (2009) The Bacillus thuringiensis delta-endotoxin Cry1C as a potential bioinsecticide in plants. Plant Science 176:315-324.)
Insect Receptors.
As described in the Examples, competitive receptor binding studies using radiolabeled Cry1Ca core toxin protein show that the Cry1Fa core toxin protein does not compete for the high affinity binding site present in FAW insect tissues to which Cry1Ca binds. These results indicate that the combination of Cry1Fa and Cry1Ca proteins is an effective means to mitigate the development of resistance in FAW populations to Cry1Fa (and likewise, the development of resistance to Cry1Ca), and would likely increase the level of resistance to this pest in corn plants expressing both proteins.
Thus, based in part on the data described above and elsewhere herein, it is thought that co-production (stacking) of the Cry1Ca and Cry1Fa proteins can be used to produce a high dose IRM stack for FAW. Other proteins can be added to this combination to expand insect-control spectrum. For example in corn, the addition of Cry1Ab would create an IRM pyramid for control of European corn borer.
Another deployment option would be to use one or both of the Cry1Fa and Cry1Ca proteins in combination with the Cry1Ab protein to mitigate the development of resistance. Thus, another deployment option of the subject invention would be to use one or both of the Cry1Fa and Cry1Ca proteins in crop-growing regions where deployment of the Cry1Ab protein has become ineffective in controlling sugarcane borer due to the development of resistance populations. Accordingly, a preferred “triple stack” or “pyramid” combination for use according to the subject invention is Cry1F plus Cry1C plus Cry1Ab.
The subject invention also relates in part to triple stacks or “pyramids” of three (or more) toxins, with Cry1Fa and Cry1C toxins being the base pair. One preferred pyramid provides at least two proteins providing non-cross-resistant activity against two pests—the FAW and the ECB (European corn borer; Ostrinia nubilalis): Cry1Fa plus Cry1Da plus one or more ECB toxins such as Cry1Ab (see US 2008 0311096), as Cry1F is active against both insects. Other ECB toxins include Cry1Be (see U.S. Ser. No. 61/284,290; filed Dec. 16, 2009), Cry1I (see U.S. Ser. No. 61/284,278; filed Dec. 16, 2009), Cry2Aa (see U.S. Ser. No. 61/284,278; filed Dec. 16, 2009) and DIG-3 (see US 2010 00269223). In some preferred pyramid embodiments, the selected toxins have three separate modes of action against FAW; these preferred pyramid combinations are Cry1Fa plus Cry1Ca plus another toxin/gene selected from the group consisting of Vip3Ab, Cry1D (see U.S. Ser. No. 61/284,252; filed Dec. 16, 2009), Cry1Be, and Cry1E (see U.S. Ser. No. 61/284,278; filed Dec. 16, 2009). Plants (and acreage planted with such plants) that produce these three toxins are included within the scope of the subject invention. Additional toxins/genes can also be added, but these particular triple stacks would, according to the subject invention, advantageously and surprisingly provide three modes of action against FAW. This can help to reduce or eliminate the requirement for refuge acreage. A field thus planted of over 10 acres is thus included within the subject invention.
Other Vip3 toxins, for example, are listed in the attached Appendix A. Those GENBANK numbers can also be used to obtain the sequences for any of the genes and proteins disclosed or mentioned herein.
U.S. Pat. No. 5,188,960 and U.S. Pat. No. 5,827,514 describe Cry1Fa core toxin containing proteins suitable for use in carrying out the present invention. U.S. Pat. No. 6,218,188 describes plant-optimized DNA sequences encoding Cry1Fa core toxin-containing proteins that are suitable for use in the present invention.
Combinations of the toxins described in the subject invention can be used to control lepidopteran pests. Adult lepidopterans, for example, butterflies and moths, primarily feed on flower nectar and are a significant effector of pollination. Nearly all lepidopteran larvae, i.e., caterpillars, feed on plants, and many are serious pests. Caterpillars feed on or inside foliage or on the roots or stem of a plant, depriving the plant of nutrients and often destroying the plant's physical support structure. Additionally, caterpillars feed on fruit, fabrics, and stored grains and flours, ruining these products for sale or severely diminishing their value. As used herein, reference to lepidopteran pests refers to various life stages of the pest, including larval stages.
Some chimeric toxins of the subject invention comprise a full N-terminal core toxin portion of a Bt toxin and, at some point past the end of the core toxin portion, the protein has a transition to a heterologous protoxin sequence. The N-terminal, insecticidally active, toxin portion of a Bt toxin is referred to as the “core” toxin. The transition from the core toxin segment to the heterologous protoxin segment can occur at approximately the toxin/protoxin junction or, in the alternative, a portion of the native protoxin (extending past the core toxin portion) can be retained, with the transition to the heterologous protoxin portion occurring downstream.
As an example, one chimeric toxin of the subject invention, is a full core toxin portion of Cry1Fa (amino acids 1 to 601) and a heterologous protoxin (amino acids 602 to the C-terminus). In one preferred embodiment, the portion of a chimeric toxin comprising the protoxin is derived from a Cry1Ab protein toxin. As a second Example, a second chimeric toxin of the subject invention, as disclosed in SEQ ID NO:1 has the full core toxin portion of Cry1Ca (amino acids 1 to 619) and a heterologous protoxin (amino acids 620 to the C-terminus). In a preferred embodiment, the portion of a chimeric toxin comprising the protoxin is derived from a Cry1Ab protein toxin.
A person skilled in this art will appreciate that Bt toxins, even within a certain class such as Cry1F, will vary to some extent in length and the precise location of the transition from core toxin portion to protoxin portion. Typically, the Cry1Ca and Cry1Fa toxins are about 1150 to about 1200 amino acids in length. The transition from core toxin portion to protoxin portion will typically occur at between about 50% to about 60% of the full length toxin. The chimeric toxin of the subject invention will include the full expanse of this N-terminal core toxin portion. Thus, the chimeric toxin will comprise at least about 50% of the full length of the Cry1Fa Bt toxin protein or at least about 50% of the full length of the Cry1Ca Bt toxin protein. This will typically be at least about 590 amino acids. With regard to the protoxin portion, the full expanse of the Cry1Ab protoxin portion extends from the end of the core toxin portion to the C-terminus of the molecule.
Genes and Toxins.
The genes and toxins useful according to the subject invention include not only the full length sequences disclosed but also fragments of these sequences, variants, mutants, and fusion proteins which retain the characteristic pesticidal activity of the toxins specifically exemplified herein. As used herein, the terms “variants” or “variations” of genes refer to nucleotide sequences which encode the same toxins or which encode equivalent toxins having pesticidal activity. As used herein, the term “equivalent toxins” refers to toxins having the same or essentially the same biological activity against the target pests as the claimed toxins.
As used herein, the boundaries represent approximately 95% (Cry1Fa's and 1Ca's), 78% (Cry1F's and Cry1C's), and 45% (Cry1's) sequence identity, per “Revision of the Nomenclature for the Bacillus thuringiensis Pesticidal Crystal Proteins,” N. Crickmore, D. R. Zeigler, J. Feitelson, E. Schnepf, J. Van Rie, D. Lereclus, J. Baum, and D. H. Dean. Microbiology and Molecular Biology Reviews (1998) Vol 62: 807-813. These cut offs can also be applied to the core toxins only (for Cry1F and Cry1C toxins).
It should be apparent to a person skilled in this art that genes encoding active toxins can be identified and obtained through several means. The specific genes or gene portions exemplified herein may be obtained from the isolates deposited at a culture depository. These genes, or portions or variants thereof, may also be constructed synthetically, for example, by use of a gene synthesizer. Variations of genes may be readily constructed using standard techniques for making point mutations. Also, fragments of these genes can be made using commercially available exonucleases or endonucleases according to standard procedures. For example, enzymes such as Bal31 or site-directed mutagenesis can be used to systematically cut off nucleotides from the ends of these genes. Genes that encode active fragments may also be obtained using a variety of restriction enzymes. Proteases may be used to directly obtain active fragments of these protein toxins.
Fragments and equivalents which retain the pesticidal activity of the exemplified toxins would be within the scope of the subject invention. Also, because of the redundancy of the genetic code, a variety of different DNA sequences can encode the amino acid sequences disclosed herein. It is well within the skill of a person trained in the art to create these alternative DNA sequences encoding the same, or essentially the same, toxins. These variant DNA sequences are within the scope of the subject invention. As used herein, reference to “essentially the same” sequence refers to sequences which have amino acid substitutions, deletions, additions, or insertions which do not materially affect pesticidal activity. Fragments of genes encoding proteins that retain pesticidal activity are also included in this definition.
A further method for identifying the genes encoding the toxins and gene portions useful according to the subject invention is through the use of oligonucleotide probes. These probes are detectable nucleotide sequences. These sequences may be detectable by virtue of an appropriate label or may be made inherently fluorescent as described in International Application No. WO93/16094. As is well known in the art, if the probe molecule and nucleic acid sample hybridize by forming a strong bond between the two molecules, it can be reasonably assumed that the probe and sample have substantial homology. Preferably, hybridization is conducted under stringent conditions by techniques well-known in the art, as described, for example, in Keller, G. H., M. M. Manak (1987) DNA Probes, Stockton Press, New York, N.Y., pp. 169-170. Some examples of salt concentrations and temperature combinations are as follows (in order of increasing stringency): 2×SSPE or SSC at room temperature; 1×SSPE or SSC at 42° C.; 0.1×SSPE or SSC at 42° C.; 0.1×SSPE or SSC at 65° C. Detection of the probe provides a means for determining in a known manner whether hybridization has occurred. Such a probe analysis provides a rapid method for identifying toxin-encoding genes of the subject invention. The nucleotide segments which are used as probes according to the invention can be synthesized using a DNA synthesizer and standard procedures. These nucleotide sequences can also be used as PCR primers to amplify genes of the subject invention.
Variant Toxins.
Certain toxins of the subject invention have been specifically exemplified herein. Since these toxins are merely exemplary of the toxins of the subject invention, it should be readily apparent that the subject invention comprises variant or equivalent toxins (and nucleotide sequences coding for equivalent toxins) having the same or similar pesticidal activity of the exemplified toxin. Equivalent toxins will have amino acid homology with an exemplified toxin. This amino acid homology will typically be greater than 75%, preferably be greater than 90%, and most preferably be greater than 95%. The amino acid homology will be highest in critical regions of the toxin which account for biological activity or are involved in the determination of three-dimensional configuration which ultimately is responsible for the biological activity. In this regard, certain amino acid substitutions are acceptable and can be expected if these substitutions are in regions which are not critical to activity or are conservative amino acid substitutions which do not affect the three-dimensional configuration of the molecule. For example, amino acids may be placed in the following classes: non-polar, uncharged polar, basic, and acidic. Conservative substitutions whereby an amino acid of one class is replaced with another amino acid of the same type fall within the scope of the subject invention so long as the substitution does not materially alter the biological activity of the compound. Table 1 provides a listing of examples of amino acids belonging to each class.
In some instances, non-conservative substitutions can also be made. The critical factor is that these substitutions must not significantly detract from the biological activity of the toxin.
Recombinant Hosts.
The genes encoding the toxins of the subject invention can be introduced into a wide variety of microbial or plant hosts. Expression of the toxin gene results, directly or indirectly, in the intracellular production and maintenance of the pesticide. Conjugal transfer and recombinant transfer can be used to create a Bt strain that expresses both toxins of the subject invention. Other host organisms may also be transformed with one or both of the toxin genes then used to accomplish the synergistic effect. With suitable microbial hosts, e.g., Pseudomonas, the microbes can be applied to the situs of the pest, where they will proliferate and be ingested. The result is control of the pest. Alternatively, the microbe hosting the toxin gene can be treated under conditions that prolong the activity of the toxin and stabilize the cell. The treated cell, which retains the toxic activity, then can be applied to the environment of the target pest.
Where the Bt toxin gene is introduced via a suitable vector into a microbial host, and said host is applied to the environment in a living state, it is essential that certain host microbes be used. Microorganism hosts are selected which are known to occupy the “phytosphere” (phylloplane, phyllosphere, rhizosphere, and/or rhizoplane) of one or more crops of interest. These microorganisms are selected so as to be capable of successfully competing in the particular environment (crop and other insect habitats) with the wild-type microorganisms, provide for stable maintenance and expression of the gene expressing the polypeptide pesticide, and, desirably, provide for improved protection of the pesticide from environmental degradation and inactivation.
A large number of microorganisms are known to inhabit the phylloplane (the surface of the plant leaves) and/or the rhizosphere (the soil surrounding plant roots) of a wide variety of important crops. These microorganisms include bacteria, algae, and fungi. Of particular interest are microorganisms, such as bacteria, e.g., genera Pseudomonas, Erwinia, Serratia, Klebsiella, Xanthomonas, Streptomyces, Rhizobium, Rhodopseudomonas, Methylophilius, Agrobactenum, Acetobacter, Lactobacillus, Arthrobacter, Azotobacter, Leuconostoc, and Alcaligenes; fungi, particularly yeast, e.g., genera Saccharomyces, Cryptococcus, Kluyveromyces, Sporobolomyces, Rhodotorula, and Aureobasidium. Of particular interest are such phytosphere bacterial species as Pseudomonas syringae, Pseudomonas fluorescens, Serratia marcescens, Acetobacter xylinum, Agrobactenium tumefaciens, Rhodopseudomonas spheroides, Xanthomonas campestris, Rhizobium melioti, Alcaligenes entrophus, and Azotobacter vinlandii; and phytosphere yeast species such as Rhodotorula rubra, R. glutinis, R. marina, R. aurantiaca, Cryptococcus albidus, C. diffluens, C. laurentii, Saccharomyces rosei, S. pretoriensis, S. cerevisiae, Sporobolomyces roseus, S. odorus, Kluyveromyces veronae, and Aureobasidium pollulans. Of particular interest are the pigmented microorganisms.
A wide variety of methods are available for introducing a Bt gene encoding a toxin into a microorganism host under conditions which allow for stable maintenance and expression of the gene. These methods are well known to those skilled in the art and are described, for example, in U.S. Pat. No. 5,135,867, which is incorporated herein by reference.
Treatment of Cells.
Bacillus thuringiensis or recombinant cells expressing the Bt toxins can be treated to prolong the toxin activity and stabilize the cell. The pesticide microcapsule that is formed comprises the Bt toxin or toxins within a cellular structure that has been stabilized and will protect the toxin when the microcapsule is applied to the environment of the target pest. Suitable host cells may include either prokaryotes or eukaryotes, normally being limited to those cells which do not produce substances toxic to higher organisms, such as mammals. However, organisms which produce substances toxic to higher organisms could be used, where the toxic substances are unstable or the level of application sufficiently low as to avoid any possibility of toxicity to a mammalian host. As hosts, of particular interest will be the prokaryotes and the lower eukaryotes, such as fungi.
The cell will usually be intact and be substantially in the proliferative form when treated, rather than in a spore form, although in some instances spores may be employed.
Treatment of the microbial cell, e.g., a microbe containing the B.t. toxin gene or genes, can be by chemical or physical means, or by a combination of chemical and/or physical means, so long as the technique does not deleteriously affect the properties of the toxin, nor diminish the cellular capability of protecting the toxin. Examples of chemical reagents are halogenating agents, particularly halogens of atomic no. 17-80. More particularly, iodine can be used under mild conditions and for sufficient time to achieve the desired results. Other suitable techniques include treatment with aldehydes, such as glutaraldehyde; anti-infectives, such as zephiran chloride and cetylpyridinium chloride; alcohols, such as isopropyl and ethanol; various histologic fixatives, such as Lugol iodine, Bouin's fixative, various acids and Helly's fixative (See: Humason, Gretchen L., Animal Tissue Techniques, W. H. Freeman and Company, 1967); or a combination of physical (heat) and chemical agents that preserve and prolong the activity of the toxin produced in the cell when the cell is administered to the host environment. Examples of physical means are short wavelength radiation such as gamma-radiation and X-radiation, freezing, UV irradiation, lyophilization, and the like. Methods for treatment of microbial cells are disclosed in U.S. Pat. Nos. 4,695,455 and 4,695,462, which are incorporated herein by reference.
The cells generally will have enhanced structural stability which will enhance resistance to environmental conditions. Where the pesticide is in a proform, the method of cell treatment should be selected so as not to inhibit processing of the proform to the mature form of the pesticide by the target pest pathogen. For example, formaldehyde will crosslink proteins and could inhibit processing of the proform of a polypeptide pesticide. The method of treatment should retain at least a substantial portion of the bio-availability or bioactivity of the toxin.
Characteristics of particular interest in selecting a host cell for purposes of production include ease of introducing the B.t. gene or genes into the host, availability of expression systems, efficiency of expression, stability of the pesticide in the host, and the presence of auxiliary genetic capabilities. Characteristics of interest for use as a pesticide microcapsule include protective qualities for the pesticide, such as thick cell walls, pigmentation, and intracellular packaging or formation of inclusion bodies; survival in aqueous environments; lack of mammalian toxicity; attractiveness to pests for ingestion; ease of killing and fixing without damage to the toxin; and the like. Other considerations include ease of formulation and handling, economics, storage stability, and the like.
Growth of cells. The cellular host containing the B.t. insecticidal gene or genes may be grown in any convenient nutrient medium, where the DNA construct provides a selective advantage, providing for a selective medium so that substantially all or all of the cells retain the B.t. gene. These cells may then be harvested in accordance with conventional ways. Alternatively, the cells can be treated prior to harvesting.
The B.t. cells producing the toxins of the invention can be cultured using standard art media and fermentation techniques. Upon completion of the fermentation cycle the bacteria can be harvested by first separating the B.t. spores and crystals from the fermentation broth by means well known in the art. The recovered B.t. spores and crystals can be formulated into a wettable powder, liquid concentrate, granules or other formulations by the addition of surfactants, dispersants, inert carriers, and other components to facilitate handling and application for particular target pests. These formulations and application procedures are all well known in the art.
Formulations.
Formulated bait granules containing an attractant and spores, crystals, and toxins of the B.t. isolates, or recombinant microbes comprising the genes obtainable from the B.t. isolates disclosed herein, can be applied to the soil. Formulated product can also be applied as a seed-coating or root treatment or total plant treatment at later stages of the crop cycle. Plant and soil treatments of B.t. cells may be employed as wettable powders, granules or dusts, by mixing with various inert materials, such as inorganic minerals (phyllosilicates, carbonates, sulfates, phosphates, and the like) or botanical materials (powdered corncobs, rice hulls, walnut shells, and the like). The formulations may include spreader-sticker adjuvants, stabilizing agents, other pesticidal additives, or surfactants. Liquid formulations may be aqueous-based or non-aqueous and employed as foams, gels, suspensions, emulsifiable concentrates, or the like. The ingredients may include rheological agents, surfactants, emulsifiers, dispersants, or polymers.
As would be appreciated by a person skilled in the art, the pesticidal concentration will vary widely depending upon the nature of the particular formulation, particularly whether it is a concentrate or to be used directly. The pesticide will be present in at least 1% by weight and may be 100% by weight. The dry formulations will have from about 1-95% by weight of the pesticide while the liquid formulations will generally be from about 1-60% by weight of the solids in the liquid phase. The formulations will generally have from about 102 to about 104 cells/mg. These formulations will be administered at about 50 mg (liquid or dry) to 1 kg or more per hectare.
The formulations can be applied to the environment of the lepidopteran pest, e.g., foliage or soil, by spraying, dusting, sprinkling, or the like.
Plant Transformation.
A preferred recombinant host for production of the insecticidal proteins of the subject invention is a transformed plant. Genes encoding Bt toxin proteins, as disclosed herein, can be inserted into plant cells using a variety of techniques which are well known in the art. For example, a large number of cloning vectors comprising a replication system in Escherichia coli and a marker that permits selection of the transformed cells are available for preparation for the insertion of foreign genes into higher plants. The vectors comprise, for example, pBR322, pUC series, M13mp series, pACYC184, inter alia. Accordingly, the DNA fragment having the sequence encoding the Bt toxin protein can be inserted into the vector at a suitable restriction site. The resulting plasmid is used for transformation into E. coli. The E. coli cells are cultivated in a suitable nutrient medium, then harvested and lysed. The plasmid is recovered. Sequence analysis, restriction analysis, electrophoresis, and other biochemical-molecular biological methods are generally carried out as methods of analysis. After each manipulation, the DNA sequence used can be cleaved and joined to the next DNA sequence. Each plasmid sequence can be cloned in the same or other plasmids. Depending on the method of inserting desired genes into the plant, other DNA sequences may be necessary. If, for example, the Ti or Ri plasmid is used for the transformation of the plant cell, then at least the right border, but often the right and the left border of the Ti or Ri plasmid T-DNA, has to be joined as the flanking region of the genes to be inserted. The use of T-DNA for the transformation of plant cells has been intensively researched and sufficiently described in EP 120 516, Lee and Gelvin (2008), Hoekema (1985), Fraley et al., (1986), and An et al., (1985), and is well established in the art.
Once the inserted DNA has been integrated in the plant genome, it is relatively stable. The transformation vector normally contains a selectable marker that confers on the transformed plant cells resistance to a biocide or an antibiotic, such as Bialaphos, Kanamycin, G418, Bleomycin, or Hygromycin, inter alia. The individually employed marker should accordingly permit the selection of transformed cells rather than cells that do not contain the inserted DNA.
A large number of techniques is available for inserting DNA into a plant host cell. Those techniques include transformation with T-DNA using Agrobacterium tumefaciens or Agrobacterium rhizogenes as transformation agent, fusion, injection, biolistics (microparticle bombardment), or electroporation as well as other possible methods. If Agrobacteria are used for the transformation, the DNA to be inserted has to be cloned into special plasmids, namely either into an intermediate vector or into a binary vector. The intermediate vectors can be integrated into the Ti or Ri plasmid by homologous recombination owing to sequences that are homologous to sequences in the T-DNA. The Ti or Ri plasmid also comprises the vir region necessary for the transfer of the T-DNA. Intermediate vectors cannot replicate themselves in Agrobacteria. The intermediate vector can be transferred into Agrobacterium tumefaciens by means of a helper plasmid (conjugation). Binary vectors can replicate themselves both in E. coli and in Agrobacteria. They comprise a selection marker gene and a linker or polylinker which are framed by the Right and Left T-DNA border regions. They can be transformed directly into Agrobacteria (Holsters et al., 1978). The Agrobacterium used as host cell is to comprise a plasmid carrying a vir region. The vir region is necessary for the transfer of the T-DNA into the plant cell. Additional T-DNA may be contained. The bacterium so transformed is used for the transformation of plant cells. Plant explants can advantageously be cultivated with Agrobacterium tumefaciens or Agrobacterium rhizogenes for the transfer of the DNA into the plant cell. Whole plants can then be regenerated from the infected plant material (for example, pieces of leaf, segments of stalk, roots, but also protoplasts or suspension-cultivated cells) in a suitable medium, which may contain antibiotics or biocides for selection. The plants so obtained can then be tested for the presence of the inserted DNA. No special demands are made of the plasmids in the case of injection and electroporation. It is possible to use ordinary plasmids, such as, for example, pUC derivatives.
The transformed cells grow inside the plants in the usual manner. They can form germ cells and transmit the transformed trait(s) to progeny plants. Such plants can be grown in the normal manner and crossed with plants that have the same transformed hereditary factors or other hereditary factors. The resulting hybrid individuals have the corresponding phenotypic properties.
In a preferred embodiment of the subject invention, plants will be transformed with genes wherein the codon usage has been optimized for plants. See, for example, U.S. Pat. No. 5,380,831, which is hereby incorporated by reference. While some truncated toxins are exemplified herein, it is well-known in the Bt art that 130 kDa-type (full-length) toxins have an N-terminal half that is the core toxin, and a C-terminal half that is the protoxin “tail.” Thus, appropriate “tails” can be used with truncated/core toxins of the subject invention. See e.g. U.S. Pat. No. 6,218,188 and U.S. Pat. No. 6,673,990. In addition, methods for creating synthetic Bt genes for use in plants are known in the art (Stewart and Burgin, 2007). One non-limiting example of a preferred transformed plant is a fertile maize plant comprising a plant expressible gene encoding a Cry1Fa protein, and further comprising a second plant expressible gene encoding a Cry1Ca protein.
Transfer (or introgression) of the Cry1Fa- and Cry1Ca-determined trait(s) into inbred maize lines can be achieved by recurrent selection breeding, for example by backcrossing. In this case, a desired recurrent parent is first crossed to a donor inbred (the non-recurrent parent) that carries the appropriate gene(s) for the Cry1F- and Cry1C-determined traits. The progeny of this cross is then mated back to the recurrent parent followed by selection in the resultant progeny for the desired trait(s) to be transferred from the non-recurrent parent. After three, preferably four, more preferably five or more generations of backcrosses with the recurrent parent with selection for the desired trait(s), the progeny will be heterozygous for loci controlling the trait(s) being transferred, but will be like the recurrent parent for most or almost all other genes (see, for example, Poehlman & Sleper (1995) Breeding Field Crops, 4th Ed., 172-175; Fehr (1987) Principles of Cultivar Development, Vol. 1: Theory and Technique, 360-376).
Insect Resistance Management (IRM) Strategies.
Roush et al., for example, outlines two-toxin strategies, also called “pyramiding” or “stacking,” for management of insecticidal transgenic crops. (The Royal Society. Phil. Trans. R. Soc. Lond. B. (1998) 353, 1777-1786).
On their website, the United States Environmental Protection Agency (epa.gov/oppbppd1/biopesticides/pips/bt_corn_refuge—2006.htm) publishes the following requirements for providing non-transgenic (i.e., non-B.t.) refuges (a section or block of non-Bt crops/corn) for use with transgenic crops producing a single Bt protein active against target pests.
In addition, the National Corn Growers Association, on their website:
also provides similar guidance regarding the refuge requirements. For example:
As stated by Roush et al. (on pages 1780 and 1784 right column, for example), stacking or pyramiding of two different proteins each effective against the target pests and with little or no cross-resistance can allow for use of a smaller refuge. Roush suggests that for a successful stack, a refuge size of less than 10% refuge, can provide comparable resistance management to about 50% refuge for a single (non-pyramided) trait. For currently available pyramided Bt corn products, the U.S. Environmental Protection Agency requires significantly less (generally 5%) structured refuge of non-Bt corn be planted than for single trait products (generally 20%).
There are various ways of providing the IRM effects of a refuge, including various geometric planting patterns in the fields (as mentioned above) and in-bag seed mixtures, as discussed further by Roush et al. (supra), and U.S. Pat. No. 6,551,962.
The above percentages, or similar refuge ratios, can be used for the subject double or triple stacks or pyramids. For triple stacks with three modes of action against a single target pest, a goal would be zero refuge (or less than 5% refuge, for example). This is particularly true for commercial acreage—of over 10 acres for example.
All patents, patent applications, provisional applications, and publications referred to or cited herein are incorporated by reference in their entirety to the extent they are not inconsistent with the explicit teachings of this specification.
Following are examples that illustrate procedures for practicing the invention. These examples should not be construed as limiting. All percentages are by weight and all solvent mixture proportions are by volume unless otherwise noted. All temperatures are in degrees Celsius.
Unless specifically indicated or implied, the terms “a”, “an”, and “the” signify “at least one” as used herein.
Chimeric Toxins. Chimeric proteins utilizing the core toxin domain of one Cry toxin fused to the protoxin segment of another Cry toxin have previously been reported, for example, in U.S. Pat. No. 5,593,881 and U.S. Pat. No. 5,932,209. A Cry1Ca3 delta endotoxin protein sequence is deposited as GenBank Accession Number AAA22343 under an obsolete terminology of CryIC(b).
Cry1Ca chimeric protein variants of this invention include chimeric toxins comprising an N-terminal core toxin segment derived from a Cry1Ca3 insecticidal toxin fused to a heterologous delta endotoxin protoxin segment at some point past the end of the core toxin segment. The transition from the core toxin to the heterologous protoxin segment can occur at approximately the native core toxin/protoxin junction or, in the alternative, a portion of the native protoxin (extending past the core toxin segment) can be retained, with the transition to the heterologous protoxin occurring downstream. In variant fashion, the core toxin and protoxin segments may comprise exactly the amino acid sequence of the native toxins from which they are derived, or may include amino acid additions, deletions, or substitutions that do not diminish, and may enhance, the biological function of the segments when fused to one another.
For example, a chimeric toxin of the subject invention comprises a core toxin segment derived from Cry1Ca3 and a heterologous protoxin. In a preferred embodiment of the invention, the core toxin segment derived from Cry1Ca3 (619 amino acids) is fused to a heterologous segment comprising a protoxin segment derived from a Cry1Ab delta-endotoxin (545 amino acids). The 1164 amino acid sequence of the chimeric protein, herein referred to as DIG-152, is disclosed as SEQ ID NO:1. A second preferred embodiment of the invention comprises a chimeric protein in which the Cry1Ca core toxin segment (619 amino acids) is joined to a second 545 amino acid protoxin segment derived from Cry1Ab The 1164 amino acid sequence of the second chimeric protein, referred to as DIG-109, is disclosed as SEQ ID NO:2 (maize optimized version). It is to be understood that other chimeric fusions comprising Cry1Ca core toxin variants and protoxins derived from Cry1Ab are within the scope of this invention.
It is noted that the DIG-152 and DIG-109 chimeric proteins are essentially functional equivalents of one another, differing in sequence only at a single position (amino acid 620, which joins the Cry1Ca core toxin segment to the Cry1Ab protoxin segment).
Standard cloning methods (as described in, for example, Sambrook et al., (1989) and Ausubel et al., (1995), and updates thereof) were used in the construction of Pseudomonas fluorescens (Pf) expression construct pMYC2547 engineered to produce a full-length DIG-152 chimeric protein (as disclosed in SEQ ID NO:1). Protein production was performed in Pseudomonas fluorescens strain MB214 (a derivative of strain MB101; P. fluorescens biovar I), having an insertion of a modified lac operon as disclosed in U.S. Pat. No. 5,169,760. The basic cloning strategy entailed subcloning a DNA fragment encoding DIG-152 into plasmid vectors, whereby it is placed under the expression control of the Ptac promoter and the rrnBT1T2 terminator from plasmid pKK223-3 (PL Pharmacia, Milwaukee, Wis.). One such plasmid was named pMYC2547, and the MB214 isolate harboring this plasmid is named Dpf108.
Growth and Expression Analysis in Shake Flasks
Production of DIG-152 protein for characterization and insect bioassay was accomplished by shake-flask-grown P. fluorescens strain Dpf108. DIG-152 protein production driven by the Ptac promoter was conducted as described previously in U.S. Pat. No. 5,527,883. Details of the microbiological manipulations are available in Squires et al., (2004), US Patent Application 20060008877, US Patent Application 20080193974, and US Patent Application 20080058262, incorporated herein by reference. Expression was induced by addition of isopropyl-β-D-1-thiogalactopyranoside (IPTG) after an initial incubation of 24 hours at 30° with shaking. Cultures were sampled at the time of induction and at various times post-induction. Cell density was measured by optical density at 600 nm (OD600).
Cell Fractionation and SDS-PAGE Analysis of Shake Flask Samples
At each sampling time, the cell density of samples was adjusted to OD600=20 and 1 mL aliquots were centrifuged at 14000×g for five minutes. The cell pellets were frozen at −80°. Soluble and insoluble fractions from frozen shake flask cell pellet samples were generated using EasyLyse™ Bacterial Protein Extraction Solution (EPICENTRE® Biotechnologies, Madison, Wis.). Each cell pellet was resuspended in 1 mL EasyLyse™ solution and further diluted 1:4 in lysis buffer and incubated with shaking at room temperature for 30 minutes. The lysate was centrifuged at 14,000 rpm for 20 minutes at 4° and the supernatant was recovered as the soluble fraction. The pellet (insoluble fraction) was then resuspended in an equal volume of phosphate buffered saline (PBS; 11.9 mM Na2HPO4, 137 mM NaCl, 2.7 mM KCl, pH7.4).
Samples were mixed 1:1 with 2× Laemmli sample buffer containing β-mercaptoethanol (Sambrook et al., supra.) and boiled for 5 minutes prior to loading onto Criterion XT Bis-Tris 12% gels (Bio-Rad Inc., Hercules, Calif.). Electrophoresis was performed in the recommended XT MOPS buffer. Gels were stained with Bio-Safe Coomassie Stain according to the manufacturer's (Bio-Rad) protocol and imaged using the Alpha Innotech Imaging system (San Leandro, Calif.).
Inclusion Body Preparation.
DIG-152 protein inclusion body (IB) preparations were performed on cells from P. fluorescens fermentations that produced insoluble Bt insecticidal protein, as demonstrated by SDS-PAGE and MALDI-MS (Matrix Assisted Laser Desorption/Ionization Mass Spectrometry). P. fluorescens fermentation pellets were thawed in a 37° water bath. The cells were resuspended to 25% w/v in lysis buffer [50 mM Tris, pH 7.5, 200 mM NaCl, 20 mM EDTA disodium salt (Ethylenediaminetetraacetic acid), 1% Triton X-100, and 5 mM Dithiothreitol (DTT); 5 mL/L of bacterial protease inhibitor cocktail (Catalog #P8465; Sigma-Aldrich, St. Louis, Mo.) were added just prior to use]. The cells were suspended using a hand-held homogenizer at lowest setting (Tissue Tearor, BioSpec Products, Inc., Bartlesville, Okla.). Lysozyme (25 mg of Sigma L7651, from chicken egg white) was added to the cell suspension by mixing with a metal spatula, and the suspension was incubated at room temperature for one hour. The suspension was cooled on ice for 15 minutes, then sonicated using a Branson Sonifier 250 (two 1-minute sessions, at 50% duty cycle, 30% output). Cell lysis was checked by microscopy. An additional 25 mg of lysozyme were added if necessary, and the incubation and sonication were repeated. Following confirmation of cell lysis via microscopy, the lysate was centrifuged at 11,500×g for 25 minutes (4°) to form the IB pellet, and the supernatant was discarded. The IB pellet was resuspended with 100 mL lysis buffer, homogenized with the hand-held mixer and centrifuged as above. The IB pellet was repeatedly washed by resuspension (in 50 mL lysis buffer), homogenization, sonication, and centrifugation until the supernatant became colorless and the IB pellet became firm and off-white in color. For the final wash, the IB pellet was resuspended in sterile-filtered (0.22 μm) distilled water containing 2 mM EDTA, and centrifuged. The final pellet was resuspended in sterile-filtered distilled water containing 2 mM EDTA, and stored in 1 mL aliquots at −80°.
SDS-PAGE analysis and quantitation of protein in IB preparations was done by thawing a 1 mL aliquot of IB pellet and diluting 1:20 with sterile-filtered distilled water. The diluted sample was then boiled with 4× reducing sample buffer [250 mM Tris, pH6.8, 40% glycerol (v/v), 0.4% Bromophenol Blue (w/v), 8% SDS (w/v) and 8% β-mercaptoethanol (v/v)] and loaded onto a Novex® 4-20% Tris-Glycine, 12+2 well gel (Invitrogen) run with 1× Tris/Glycine/SDS buffer (BioRad). The gel was run for 60 min at 200 volts then stained with Coomassie Blue (50% G-250/50% R-250 in 45% methanol, 10% acetic acid), and destained with 7% acetic acid, 5% methanol in distilled water. Quantification of target bands was done by comparing densitometric values for the bands against Bovine Serum Albumin (BSA) standard samples run on the same gel to generate a standard curve.
Solubilization of Inclusion Bodies.
Six mL of DIG-152 inclusion body suspension from Pf clone DPf108 were centrifuged on the highest setting of an Eppendorf model 5415C microfuge (approximately 14,000×g) to pellet the inclusions. The storage buffer supernatant was removed and replaced with 25 mL of 100 mM sodium carbonate buffer, pH11, in a 50 mL conical tube. Inclusions were resuspended using a pipette and vortexed to mix thoroughly. The tube was placed on a gently rocking platform at 4° overnight to extract the target protein. The extract was centrifuged at 30,000×g for 30 min at 4°, and the resulting supernatant was concentrated 5-fold using an Amicon Ultra-15 regenerated cellulose centrifugal filter device (30,000 Molecular Weight Cutoff; Millipore). The sample buffer was then changed to 10 mM CAPS [3-(cyclohexamino)1-propanesulfonic acid] pH 10 using disposable PD-10 columns (GE Healthcare, Piscataway, N.J.).
Solubilization and Trypsin Activation of Inclusion Body Protein.
In some instances, DIG-152 inclusion body suspension from Pf clone DPf108 was centrifuged on the highest setting of an Eppendorf model 5415C microfuge (approximately 14,000×g) to pellet the inclusions. The storage buffer supernatant was removed and replaced with 100 mM CAPS, pH 11 to provide a protein concentration of approximately 50 mg/mL. The tube was rocked at room temperature for three hours to completely solubilize the protein. Trypsin was added at an amount equal to 5% to 10% (w:w, based on the initial weight of IB powder) and digestion was accomplished by incubation while rocking overnight at 4° or by rocking 90-120 minutes at room temperature. Insoluble material was removed by centrifugation at 10,000×g for 15 minutes, and the supernatant was applied to a MonoQ anion exchange column (10 mm by 10 cm). Activated DIG-152 protein was eluted (as determined by SDS-PAGE, see below) by a 0% to 100% 1 M NaCl gradient over 25 column volumes. Fractions containing the activated protein were pooled and, when necessary, concentrated to less than 10 mL using an Amicon Ultra-15 regenerated cellulose centrifugal filter device as above. The material was then passed through a Superdex 200 column (16 mm by 60 cm) in buffer containing 100 mM NaCl. 10% glycerol, 0.5% Tween-20 and 1 mM EDTA. It was determined by SDS-PAGE analysis that the activated (enzymatically truncated) protein elutes at 65 to 70 mL. Fractions containing the activated protein were pooled and concentrated using the centrifugal concentrator as above.
Gel Electrophoresis.
The concentrated protein preparations were prepared for electrophoresis by diluting 1:50 in NuPAGE® LDS sample buffer (Invitrogen) containing 5 mM DTT as a reducing agent and heated at 95° for 4 minutes. The sample was loaded in duplicate lanes of a 4-12% NuPAGE® gel alongside five BSA standards ranging from 0.2 μg to 2 μg/lane (for standard curve generation). Voltage was applied at 200 V using MOPS SDS running buffer (Invitrogen) until the tracking dye reached the bottom of the gel. The gel was stained with 0.2% Coomassie Blue G-250 in 45% methanol, 10% acetic acid, and destained, first briefly with 45% methanol, 10% acetic acid, and then at length with 7% acetic acid, 5% methanol until the background cleared. Following destaining, the gel was scanned with a BioRad Fluor-S MultiImager. The instrument's Quantity One Software v.4.5.2 was used to obtain background-subtracted volumes of the stained protein bands and to generate the BSA standard curve that was used to calculate the concentration of chimeric DIG-152 protein in the stock solution.
Insecticidal activity of the DIG-152 protein was demonstrated on larvae of the fall armyworm (FAW, Spodoptera frugiperda (J. E. Smith)) and on larvae of Cry1F-resistant FAW (rFAW).
Sample Preparation and Bioassays.
Inclusion body preparations (native full length protein or trypsin activated protein) were transferred to 10 mM CAPS pH10 buffer by exchange methods such as dialysis or PD-10 columns. The samples were then diluted appropriately in 10 mM CAPS pH 10, and all bioassays contained a control treatment consisting of this buffer, which served as a background check for mortality or growth inhibition.
Protein concentrations in bioassay buffer were estimated by gel electrophoresis using BSA to create a standard curve for gel densitometry, which was measured using a BioRad imaging system as above. Proteins in the gel matrix were stained with Coomassie Blue-based stain and destained before reading.
Purified proteins were tested for insecticidal activity in bioassays conducted with neonate Lepidopteran larvae on artificial insect diet. Larvae of FAW were hatched from eggs obtained from a colony maintained by a commercial insectary (Benzon Research Inc., Carlisle, Pa.). Larvae of rFAW were hatched from eggs harvested from a non-commercial colony (Dow AgroSciences, Indianapolis, Ind.).
The bioassays were conducted in 128-well plastic trays specifically designed for insect bioassays (C-D International, Pitman, N.J.). Each well contained 1.0 mL of multi-species Lepidoptera diet (Southland Products, Lake Village, Ark.). A 40 μL aliquot of protein sample was delivered by pipette onto the 1.5 cm2 diet surface of each well (i.e. 26.7 μL/cm2). Diet concentrations were calculated as the amount (ng) of DIG-152 protein per square centimeter of surface area in the well. The treated trays were held in a fume hood until the liquid on the diet surface had evaporated or was absorbed into the diet.
Within a few hours of eclosion, individual larvae were picked up with a moistened camel hair brush and deposited on the treated diet, one larva per well. The infested wells were then sealed with adhesive sheets of clear plastic, vented to allow gas exchange (C-D International). Bioassay trays were held under controlled environmental conditions [28°, approximately 40% Relative Humidity (RH), 16 hr:8 hr (light:dark)] for 5 days, after which time the total number of insects exposed to each protein sample, the number of dead insects, and the weight of surviving insects were recorded. Percent mortality and percent growth inhibition were calculated for each treatment. Percent growth inhibition (GI) was calculated as follows:
% GI=[1−(TWIT/TNIT)/(TWIBC/TNIBC)]×100
The GI50 was determined to be the concentration of chimeric DIG-152 protein in the diet at which the % GI value was 50. The LC50 (50% Lethal Concentration) was recorded as the concentration of DIG-152 protein in the diet at which 50% of test insects were killed. Statistical analysis (One-way ANOVA) was done using JMP software (SAS, Cary, N.C.).
Table 2 presents the results of ingestion bioassays of DIG-152 protein on fall armyworm insect larvae.
It is a feature of the DIG-152 protein of the subject invention that the growth of neonate larvae of fall armyworm (Spodoptera frugiperda) is inhibited following ingestion of the DIG-152 protein. Further, fall armyworm larvae that are resistant to intoxication by Cry1Fa are as susceptible to DIG-152 activity as are wild-type fall armyworm larvae. The significance of the susceptibility of these Cry1Fa resistant insects to Cry1Ca is discussed in more detail above.
One skilled in the art of plant molecular biology will understand that multiple DNA sequences may be designed to encode a single amino acid sequence. A common means of increasing the expression of a coding region for a protein of interest is to tailor the coding region in such a manner that its codon composition resembles the overall codon composition of the host in which the gene is destined to be expressed. Guidance regarding the design and production of synthetic genes can be found in, for example, WO 1997/13402 and U.S. Pat. No. 5,380,831.
A DNA sequence having a maize codon bias was designed and synthesized to produce the DIG-109 chimeric insecticidal protein in transgenic monocot plants. A codon usage table for maize (Zea mays L.) was calculated from 706 protein coding sequences obtained from sequences deposited in GenBank (world wide web: ncbi.nlm.nih.gov). A weighted-average maize codon set was calculated after omitting any redundant codon used less than about 10% of total codon uses for that amino acid. The Weighted Average representation for each codon was calculated using the formula:
Weighted Average % of C1=1/(% C1+% C2+% C3+ etc.)×% C1×100
To derive a maize-codon-optimized DNA sequence encoding the 1164 amino acid DIG-109 protein of SEQ ID NO:2, codon substitutions to the native cry1Ca DNA sequence encoding the Cry1Ca core toxin segment were made such that the resulting DNA sequence had the overall codon composition of the maize-optimized codon bias table. In similar fashion, codon substitutions to the native cry1Ab DNA sequence encoding the Cry1Ab protoxin segment were made such that the resulting DNA sequence had the overall codon composition of the maize-optimized codon bias table. Further refinements to the sequences were made to eliminate undesirable restriction enzyme recognition sites, potential plant intron splice sites, long runs of A/T or C/G residues, and other motifs that might interfere with RNA stability, transcription, or translation of the coding region in plant cells. Other changes were made to introduce desired restriction enzyme recognition sites, and to eliminate long internal Open Reading Frames (frames other than +1). These changes were all made within the constraints of retaining approximately the maize-biased codon composition. A complete maize-codon-optimized sequence (encoding the DIG-109 protein) is disclosed as SEQ ID NO:3. Synthesis of the DNA fragment was performed by a commercial vendor (DNA2.0, Menlo Park, Calif.).
The Agrobacterium superbinary system (Japan Tobacco, Tokyo, JP) is conveniently used for transformation of monocot plant hosts. The superbinary system employs the pSB11 shuttle vector plasmid which contains the sequences for the Right T-DNA border repeat (RB) and Left T-DNA border repeat (LB) separated by multiple cloning sites. A derivative of pSB11 (called pDAB7691) was prepared by standard DNA cloning methods. Plasmid pDAB7691 contains the maize-optimized DIG-109 coding sequence (CDS; i.e., SEQ ID NO:3) under the transcriptional control of the maize ubiquitin1 promoter with associated intron1 (U.S. Pat. No. 5,510,474) and the maize Per5 3′ Untranslated Region (3′ UTR) (U.S. Pat. No. 7,179,902). Further, pDAB7691 contains a plant selectable marker gene comprising the Dow AgroSciences DSM2 CDS (WO 2008/070845 A2) under the transcriptional control of the rice actin1 promoter with associated intron1 (U.S. Pat. No. 5,641,876) and the maize Lipase 3′ UTR (U.S. Pat. No. 7,179,902). The physical arrangement of the components of the pDAB7691 T-region is conveniently illustrated as:
A second derivative of pSB11 (called pDAB100276) was prepared by standard DNA cloning methods. Plasmid pDAB100276 contains the maize-optimized DIG-109 coding sequence (CDS; i.e., SEQ ID NO:3) under the transcriptional control of the maize ubiquitin1 promoter with associated intron1 and the maize Per5 3′ UTR. Further, pDAB100276 contains a plant selectable marker gene comprising the Dow AgroSciences AAD1 CDS (US Patent Application No. 20090093366), under the transcriptional control of the maize ubiquitin1 promoter with associated intron1 and the maize Lipase 3′ UTR. The physical arrangement of the components of the pDAB100276 T-region is conveniently illustrated as:
To prepare for Agrobacterium transformation, cells of Escherichia coli cloning strain DH5α harboring plasmid pDAB7691 or plasmid pDAB100276 were grown at 37° overnight on LB agar medium (g/L: Bacto Tryptone, 10; Bacto Yeast Extract, 5; NaCl, 10; agar, 15) in containing Spectinomycin (100 μg/mL). Strain DH5α cells containing the conjugal mobilizing plasmid pRK2013 were grown on LB agar containing Kanamycin (50 μg/mL). After incubation the plates were placed at 4° to await the availability of the Agrobacterium tumefaciens strain LBA4404 containing plasmid pSB1.
The Agrobacterium superbinary system, which employs Agrobacterium tumefaciens strain LBA4404 containing plasmid pSB1, is conveniently used for transformation of monocot plant hosts. Methodologies for constructing and validating superbinary vectors are well established as provided in the Operating Manual for pSB1 (Japan Tobacco). Standard microbiological and molecular biological methods were used to generate and validate the superbinary plasmid pDAS5162, which is a cointegrant plasmid comprising plasmids pSB1 and pDAB7691, and superbinary plasmid pDAS5848, which is a cointegrant plasmid comprising plasmids pSB1 and pDAB100276.
Agrobacterium-Mediated Transformation of Maize
Seeds from a Hi-II F1 cross (Armstrong et al., 1991) were planted into 5-gallon-pots containing a mixture of 95% Metro-Mix 360 soilless growing medium (Sun Gro Horticulture, Bellevue, Wash.) and 5% clay/loam soil. The plants were grown in a greenhouse using a combination of high pressure sodium and metal halide lamps with a 16 hr light:8 hr dark photoperiod. Controlled sib-pollinations were performed to obtain immature F2 embryos for transformation. Maize ears were harvested at approximately 8-10 days post-pollination when immature embryos were between 1.0 mm and 2.0 mm in size.
Infection and Co-Cultivation.
Maize ears were dehusked and surface sterilized by scrubbing with liquid soap, immersing in 20% commercial bleach (containing 5% sodium hypochlorite) for about 20 minutes, then rinsing three times with sterile water. A suspension of Agrobacterium tumefaciens cells containing pDAS5162, a superbinary vector harboring a gene encoding the DIG-109 protein and containing the DSM2 plant selectable marker gene, was prepared by transferring 1 or 2 loops of bacteria [grown for 2-3 days at 28° on YEP solid medium (g/L: Bacto Yeast Extract, 10; Bacto Peptone, 10; NaCl, 5; agar, 15) containing 100 mg/L Spectinomycin, 10 mg/L Tetracycline, and 250 mg/L Streptomycin] into 5 mL of liquid infection medium [LS Basal Medium (Linsmaier and Skoog, 1965), N6 vitamins (Chu et al., 1975), 1.5 mg/L 2,4-Dichlorophenoxyacetic acid (2,4-D), 68.5 g/L sucrose, 36.0 g/L glucose, 6 mM L-proline, pH 5.2] containing 100 μM acetosyringone.
Alternatively, a suspension of Agrobacterium tumefaciens cells containing pDAS5848, a superbinary vector harboring a gene encoding the DIG-109 protein and containing the AAD-1 plant selectable marker gene, was prepared by transferring 1 or 2 loops of bacteria grown as above into 5 mL of liquid infection medium containing 100 to 200 μM acetosyringone.
In both cases, the solution was vortexed until a uniform suspension was achieved, and the concentration was adjusted to a final density of 200 Klett units using a Klett-Summerson colorimeter with a purple filter (for pDAS5162 transformations), or to an optical density of 1.2 at 550 nm (for pDAS5848 transformations). Immature embryos were isolated directly into a microcentrifuge tube containing 2 mL of the infection medium. The medium was removed and replaced with 1 mL of the Agrobacterium solution and the Agrobacterium/embryo solution was incubated for 5 to 10 minutes at room temperature. Embryos were then transferred to cocultivation medium [LS Basal Medium, N6 vitamins, 1.5 mg/L 2,4-D, 30.0 g/L sucrose, 6 mM L-proline, 0.85 mg/L AgNO3, 2.8 g/L Gellan gum (PhytoTechnology Laboratories, Lenexa, Kans.), pH 5.8] containing 100 μM acetosyringone (for pDAS5162 transformants) or containing 100 to 200 μM acetosyringone (for pDAS5848 transformants), and cocultivated for 3-4 days at 20° in the dark.
After cocultivation, the embryos were transferred to resting medium containing MS salts and vitamins, 6 mM L-proline, 100 mg/L myo-inositol, 500 mg/L MES, 30 g/L sucrose, 1.5 mg/L 2,4-D, 0.85 mg/L AgNO3, 250 mg/L Cefotaxime, 2.8 g/L Gellan gum, pH 5.8. Approximately 7 days later, embryos were transferred to the same medium supplemented with 3 mg/L Bialaphos (for pDAS5162 transformants) or supplemented with 100 nM haloxyfop (for pDAS5848 transformants) (selection medium). Transformed isolates were identified after approximately 8 weeks and were bulked up by transferring to fresh selection medium at 2-week intervals for regeneration and analysis.
Regeneration and Seed Production.
For regeneration, the cultures were transferred to “28” induction medium (MS salts and vitamins, 30 g/L sucrose, 5 mg/L Benzylaminopurine, 0.25 mg/L 2,4-D, 250 mg/L Cefotaxime, 2.5 g/L Gellan gum, pH 5.7) supplemented with 3 mg/L Bialaphos (for pDAS5162 transformants) or supplemented with 100 nM haloxyfop (for pDAS5848 transformants). Incubation was for 1 week under low-light conditions (14 μEm−2s−1), then 1 week under high-light conditions (approximately 89 μEm−2s−1). Tissues were subsequently transferred to “36” regeneration medium (same as induction medium except lacking plant growth regulators). When plantlets were 3-5 cm in length, they were transferred to glass culture tubes containing SHGA medium [(Schenk and Hildebrandt (1972) salts and vitamins; PhytoTechnologies Labr.), 1.0 g/L myo-inositol, 10 g/L sucrose and 2.0 g/L Gellan gum, pH 5.8] to allow for further growth and development of the shoot and roots. Plants were transplanted to the same soil mixture as described earlier and grown to flowering in the greenhouse. Controlled pollinations for seed production were conducted.
Those skilled in the art of maize transformation will understand that other methods are available for maize transformation and for selection of transformed plants when other plant expressible selectable marker genes (e.g. herbicide tolerance genes) are used.
The production of DIG-109 protein in transgenic maize plants was examined in proteins extracted from leaves of young plants (TO generation). Two 6 mm diameter maize leaf disks were placed in a sample tube from a deep well 96 cluster tube box (Costar Cat#3957) and frozen at −80° until day of analysis. At that time, two 4.5 mm zinc-coated Daisy™ BB's were added to each (frozen) tube, along with 200 μL of extraction buffer comprised of PBS (Phosphate Buffered Saline; Fisher Cat# BP665-1) plus 0.05% Tween 20. Each tube was capped and the box was placed in a bead mill (Kleco™ 4-96 Pulverizer; Garcia Manufacturing, Visalia, Calif.) at maximum setting for three minutes. The pulverized samples were centrifuged for 5 minutes at 2,500×g and the supernatant containing soluble proteins was used in the immunoassays.
Immunoblot analyses of extracted maize leaf proteins revealed that the DIG152RPC1 polyclonal antibody (prepared from rabbits immunized with the trypsin-activated Cry1Ca core toxin protein) does not cross react with proteins extracted from leaves of nontransgenic plants. In extracts of plants transformed with pDAS5162, several protein species were detected by the DIG152PRC1 antibody.
It is apparent that, although the transgene introduced into maize via transformation with pDAS5162 encodes the full-length DIG-109 protein, proteolytic activity within the maize cells processes the nascent protein to an abundance of stable smaller molecular weight species.
The insect toxicity of leaves harvested from independently isolated transgenic maize plants transformed with the pDAS5162 construct was tested in vitro using neonate larvae of fall armyworm (FAW, Spodoptera frugiperda (J. E. Smith)) and Cry1F-resistant FAW (rFAW) larvae. FAW eggs were obtained from a commercial insectary (Benzon), and rFAW eggs came from a non-commercial population (Dow AgroSciences). Leaf segment samples were taken for insect bioassays from greenhouse-grown TO plants approximately 2 weeks after the plants were transplanted from the laboratory into the greenhouse. Two leaf pieces from each plant (each approximately 1 square inch) were placed into separate wells of a 32-well tray (CD International) on top of about 3 mL of solidified 2% agar. Eggs were hatched onto multi-species Lepidopteran diet (Southland Products) and neonate larvae were selected when less than 24 hours old. Approximately 10 larvae per leaf segment were carefully placed into each well using a camel hair paintbrush. Infested trays were sealed with the perforated lids supplied with the trays, then held at 28°, 40% RH, 16 hr light:8 hr dark for three days. Percent damage (% DAM) for each leaf piece was recorded at the conclusion of the test. Damage ratings were averaged and used to determine which plants had the least damage from each type of test insect. Tests were replicated several times for all insects.
Data were analyzed using JMP statistical software (SAS, Cary, N.C.), averaging the % DAM scores for each plant, for each insect type. The “Fit Y by X” model was used for one way ANOVA analyses. Tukey-Kramer means separation was used as needed to analyze for significant differences amongst the mean % DAM scores for each treatment. Comparisons were made to the % DAM scores obtained from control plants of similar age. Positive control plants were grown from seeds of the commercial Herculex I™ hybrid, which produces the Cry1Fa B.t. toxin. Negative controls (i.e. nontransformed plants) were represented by the Hi II and B104 lines, and a Herculex I™ Isoline (a non-Cry containing parent of the Herculex I™ hybrid).
It is understood that other insect pests of maize may be tested in similar fashion. These pests include, but are not limited to: Agromyza parvicornis (corn blot leafminer), Agrotis ipsilon (black cutworm), Anticarsia gemmatalis (velvetbean caterpillar), Diatraea grandiosella (southwestern corn borer), Diatraea saccharalis (sugarcane borer), Elasmopalpus lignosellus (lesser cornstalk borer), Helicoverpa zea (corn earworm), Heliothis virescens, (tobacco budworm), Ostrinia nubilalis (European corn borer), Cry1F-resistant O. nubilalis, Plutella xylostella (diamondback moth), Cry1-resistant P. xylostella, Spodoptera exigua (beet armyworm), and Trichoplusia ni (cabbage looper).
Transgenic maize plants transformed with pDAS5848 (TO generation) were also examined by insect bioassay and by immunoanalyses. The amount of DIG-109 protein in leaf extracts was quantitated using a commercially available Cry1C ELISA detection kit (Envirologix™, Portland, Mass.; Cat# AP007), and the level of DIG-109 protein detected was expressed as parts per million (ppm; 1 ppm represents 1 ng of DIG-109 protein per mg of total soluble protein in the extract).
Feeding damage by FAW and rFAW was codified as follows: 0=no damage or a few pinhole feeding marks, 1=25% to 50% of leaf eaten, and 2=most all of leaf consumed or no leaf left. A protected plant is one whose damage score is 0.67 or lower.
The data in Table 3 show that there is a positive correlation between the presence of DIG-109 protein species detected by ELISA in the TO plants and control of feeding damage done by fall armyworm larvae in in vitro bioassays. The plant with the highest detected level of DIG-109 protein (plant 5848-005.4) had the lowest leaf feeding damage score. Leaves from plants with lower levels of detectable DIG-109 protein in the range of 190 to 230 ppm also suffered less feeding damage than was seen with leaves from the negative control plants (i.e. nontransformed controls B104 and Hi II), which had mean damage scores of 1.7 and 1.8. In all pDAS5848 leaves examined, the predominant DIG-109 protein species detected comprised a doublet of peptides of approximate size 60 kDa and 55 kDa.
NAa
aNA = Not Applicable;
bSD = Standard Deviation of the mean
It is thus a feature of the subject invention that the DIG-109 protein, when produced in maize plants, renders the plants resistant to feeding damage by fall armyworm larvae and Cry1F-resistant fall armyworm larvae.
The following Examples evaluate the competition binding of Cry1 core toxin proteins to putative receptors in insect gut tissues. It is shown that 125I-labeled Cry1Ca core toxin protein binds with high affinity to Brush Border Membrane Vesicles (BBMV's) prepared from Spodoptera frugiperda (fall armyworm) and that Cry1Fa core toxin protein does not compete with this binding.
Purification of Cry Proteins.
A gene encoding a chimeric protein comprising the Cry1Ca core toxin and Cry1Ab protoxin was expressed in the Pseudomonas fluorescens expression strain as described in Example 2. In similar fashion, a gene encoding a chimeric protein, comprising the Cry1Fa core toxin (603 amino acids) and Cry1Ab protoxin (545 amino acids) was expressed in the Pf system. The proteins were purified by the methods of Example 2, and trypsin digestion to produce activated core toxins from the full-length proteins was performed and the products were purified by the methods of Example 2. Preparations of the trypsin processed (activated core toxin) proteins were >95% pure and had a molecular weight of approximately 65 kDa as determined experimentally by SDS-PAGE.
Standard methods of protein quantification and SDS-polyacrylamide gel electrophoresis were employed as taught, for example, in Sambrook et al. (1989) and Ausubel et al. (1995), and updates thereof.
Preparation and Fractionation of Solubilized BBMV's.
Last instar Spodoptera frugiperda larvae were fasted overnight and then dissected after chilling on ice for 15 minutes. The midgut tissue was removed from the body cavity, leaving behind the hindgut attached to the integument. The midgut was placed in a 9× volume of ice cold homogenization buffer (300 mM mannitol, 5 mM EGTA, 17 mM Tris base, pH7.5), supplemented with Protease Inhibitor Cocktail (Sigma-Aldrich P-2714) diluted as recommended by the supplier. The tissue was homogenized with 15 strokes of a glass tissue homogenizer. BBMV's were prepared by the MgCl2 precipitation method of Wolfersberger (1993). Briefly, an equal volume of a 24 mM MgCl2 solution in 300 mM mannitol was mixed with the midgut homogenate, stirred for 5 minutes and allowed to stand on ice for 15 min. The solution was centrifuged at 2,500×g for 15 min at 4°. The supernatant was saved and the pellet suspended into the original volume of 0.5× diluted homogenization buffer and centrifuged again. The two supernatants were combined and centrifuged at 27,000×g for 30 min at 4° to form the BBMV fraction. The pellet was suspended into BBMV Storage Buffer (10 mM HEPES, 130 mM KCl, 10% glycerol, pH7.4) to a protein concentration of about 3 mg/mL. Protein concentration was determined using Bovine Serum Albumin (BSA) as the standard. Alkaline phosphatase determination (a marker enzyme for the BBMV fraction) was made prior to freezing the samples using the QuantiChrom™ DALP-250 Alkaline Phosphatase Assay Kit (Gentaur Molecular Products, Kampenhout, BE) following the manufacturer's instructions. The specific activity of this enzyme typically increased 7-fold compared to that found in the starting midgut homogenate fraction. The BBMV's were aliquoted into 250 μL samples, flash frozen in liquid nitrogen and stored at −80°.
Electrophoresis.
Analysis of proteins by SDS-PAGE was conducted under reducing (i.e. in 5% β-mercaptoethanol, BME) and denaturing (i.e. heated 5 minutes at 90° in the presence of 2% SDS) conditions. Proteins were loaded into wells of a 4% to 20% Tris-Glycine polyacrylamide gel (BioRad; Hercules, Calif.) and separated at 200 volts for 60 minutes. Protein bands were detected by staining with Coomassie Brilliant Blue R-250 (BioRad) for one hour, and destained with a solution of 5% methanol in 7% acetic acid. The gels were imaged and analyzed using a BioRad Fluoro-S Multi Imager™. Relative molecular weights of the protein bands were determined by comparison to the mobilities of known molecular weight proteins observed in a sample of BenchMark™ Protein Ladder (Life Technologies, Rockville, Md.) loaded into one well of the gel.
Iodination of Cry1Ca Core Toxin Protein.
Purified Cry1Ca core toxin protein was iodinated using Pierce Iodination Beads (Thermo Fisher Scientific, Rockford, Ill.). Briefly, two Iodination Beads were washed twice with 500 μL of PBS (20 mM sodium phosphate, 0.15 M NaCl, pH7.5), and placed into a 1.5 mL centrifuge tube with 100 μL of PBS. 0.5 mCi of 125I-labeled sodium iodide was added, the components were allowed to react for 5 minutes at room temperature, then 1 μg of Cry1Ca core toxin protein was added to the solution and allowed to react for an additional 3 to 5 minutes. The reaction was terminated by pipetting the solution from the Iodination Beads and applying it to a Zeba™ spin column (Invitrogen) equilibrated in 50 mM CAPS, pH10.0, 1 mM DTT (dithiothreitol), 1 mM EDTA, and 5% glycerol. The Iodination Beads were washed twice with 10 μL of PBS and the wash solution was also applied to the Zeba™ desalting column. The radioactive solution was eluted through the spin column by centrifuging at 1,000×g for 2 min. 125I-radiolabeled Cry1Ca core toxin protein was then dialyzed against 50 mM CAPS, pH10.0, 1 mM DTT, 1 mM EDTA, and 5% glycerol.
Imaging.
Radio-purity of the iodinated Cry1Ca core toxin protein was determined by SDS-PAGE and phosphorimaging. Briefly, SDS-PAGE gels were dried using a BioRad gel drying apparatus following the manufacturer's instructions. The dried gels were imaged by wrapping them in Mylar film (12 μm thick) and exposing them under a Molecular Dynamics storage phosphor screen (35 cm×43 cm) for 1 hour. The plates were developed using a Molecular Dynamics Storm 820 phosphorimager and the image was analyzed using ImageQuant™ software.
A saturation curve was generated using 125I-radiolabeled Cry1Ac core toxin protein to determine the optimal amount of BBMV protein to use in the binding assays with Cry1Ca and Cry1Fa core toxin proteins. 0.5 nM of 125I-radiolabeled Cry1Ac core toxin protein was incubated for 1 hr at 28° in binding buffer (8 mM NaHPO4, 2 mM KH2PO4, 150 mM NaCl, 0.1% BSA, pH7.4) with amounts of BBMV protein ranging from 0 μg/mL to 500 μg/mL (total volume of 0.5 mL). 125I-labeled Cry1Ac core toxin protein bound to the BBMV proteins was separated from the unbound fraction by sampling 150 μL of the reaction mixture in triplicate into separate 1.5 mL centrifuge tubes and centrifuging the samples at 14,000×g for 8 minutes at room temperature. The supernatant was gently removed and the pellet was washed three times with ice cold binding buffer. The bottom of the centrifuge tube containing the pellet was cut off, placed into a 13×75 mm glass culture tube and the samples were counted for 5 minutes each in the gamma counter. CPM (counts per minute) obtained minus background CPM (reaction with no BBMV protein) was plotted versus BBMV protein concentration. In accordance with other results as well, the optimal concentration of BBMV protein to use in the binding assays was determined to be 150 μg/mL.
Homologous and heterologous competition binding assays were conducted using 150 μg/mL BBMV protein and 0.5 nM of the 125I-radiolabeled Cry1Ca core toxin protein. Concentrations of the competitive non-radiolabeled Cry1Fa core toxin protein added to the reaction mixture ranged from 0.045 nM to 1000 nM and were added at the same time as the radioactive Cry1Ca core toxin protein, to assure true binding competition. Incubations were carried out for 1 hr at 28° and the amount of 125I-labeled Cry1Ca core toxin protein bound to the BBMV (specific binding) was measured as described above. Non-specific binding was represented by the counts obtained in the presence of 1,000 nM of non-radiolabeled Cry1Ca core toxin protein. One hundred percent total binding was considered to be the amount of binding in the absence of any competitor Cry1Fa core toxin protein.
Receptor binding assays using 125I-labeled Cry1Ca core toxin protein determined the ability of the Cry1Fa core toxin protein to displace this radiolabeled ligand from its binding site on BBMV's from S. frugiperda. The results (
It is thus indicated that the Cry1Ca core toxin protein interacts with a binding site in S. frugiperda BBMV that does not bind the Cry1Fa core toxin protein.
See
The following Examples evaluate the competition binding of Cry1 core toxin proteins to putative receptors in insect gut tissues. It is shown that biotin-labeled Cry1Fa core toxin protein binds with high affinity to Brush Border Membrane Vesicles (BBMV's) prepared from Diatraea saccharalis (sugarcane borer) and that Cry1Ca core toxin protein does not compete with this binding.
Preparation and Fractionation of Solubilized BBMV's.
Last instar D. saccharalis larvae were fasted overnight and then dissected after chilling on ice for 15 minutes. BBMV preparations were made following the methods disclosed in Example 10.
Competition binding assay results using 125I-labeled Cry1Fa core toxin protein may have limited biological relevance, since iodination of Cry1Fa protein renders the protein inactive in insect feeding bioassays. In contrast, it has been discovered that biotinylated Cry1Fa core toxin protein retains its toxicity against insects. Further, it is possible to measure the interaction of this (biotinylated) protein with receptors in the presence of non-biotinylated (competing) Cry core toxin proteins. Such a competition experiment can detect binding of biotin-labeled Cry1Fa core toxin protein to receptors in D. saccharalis BBMV after electrophoresis of the BBMV proteins and transfer of the entire sample to a PVDF (polyvinylidene fluoride) membrane. Avidin conjugated to horseradish peroxidase, in combination with an enhanced chemical luminescence reagent, is used to visualize the biotin-labeled Cry1Fa core toxin protein.
Cry1Fa core toxin protein was labeled with biotin using a Pierce EZ-Link® Sulfo-NHS-LC Biotinylation Kit (Thermo Fisher Scientific). Briefly, 40 μL of Sulfo-NHS-LC-biotin (10 mg/mL in Dimethyl Sulfoxide) was added to 500 μL of Cry1Fa core toxin protein (2.0 mg/mL) in 0.1M sodium phosphate buffer, pH7.2. The reaction was incubated at 4° overnight, then unreacted Sulfo-NHS-LC-biotin was removed using a Zeba™ desalting column. Biotin incorporation into Cry1Fa core toxin protein was measured using the Pierce HABA-avidin displacement assay (Thermo Fisher Scientific) as described by the manufacturer.
Biotin labeled Cry1Fa core toxin protein (2.5 nM) was incubated 1 hr. at 28° with 0.2 mg of BBMV's prepared from D. saccharalis [in a total volume of 1.0 mL] in the presence or absence of a 500-fold excess of nonlabeled Cry1Fa or Cry1Ca core toxin proteins. Unbound biotin-labeled Cry1Fa core toxin protein was removed by centrifugation at 16,000×g for 10 min and the resulting pellet was washed 3 times with ice cold binding buffer. The pellet was suspended into 15 μL of 4× Laemmli sample buffer, vortexed and sonicated to assure complete solubilization, and heated to 90° for 3 min. The entire sample was loaded onto a 4% to 20% Tris glycine gel, separated by SDS-PAGE, and electro transferred onto PVDF membrane as recommended by the supplier's instructions (BioRad). 1,000 ng of Cry1Fa core toxin protein and Cry1Ca core toxin protein were also run on the gel as negative controls. Biotin-labeled Cry1Fa core toxin protein was visualized with avidin-conjugated horseradish peroxidase at 1:15,000 dilution with enhanced chemiluminescence using a 1:1 mixture of SuperSignal® West Pico Peroxide Solution with Luminal Enhancer Solution (Thermo Fisher Scientific, Catalog numbers 1859674 and 1859675). Bands were recorded using a Biorad Fluor-S MultiImager with Quantity One v.4.5.2 software.
The results demonstrated the detection of biotin-labeled Cry1Fa core toxin protein bound to receptors in D. saccharalis BBMV, and further showed that non-biotinylated Cry1Fa core toxin protein at 500-fold excess concentration completely displaced the bound biotinylated Cry1Fa core toxin protein from its receptor(s). In contrast, a 500-fold excess concentration of Cry1Ca core toxin protein was not able to displace the bound biotinylated Cry1Fa core toxin protein, indicating that Cry1Ca core toxin protein does not compete for the Cry1Fa core toxin protein binding site(s) in D. saccharalis BBMV. It is thus indicated that, analogous to the results obtained with BBMVs of S. frugiperda, the Cry1Fa core toxin protein and Cry1Ca core toxin protein bind to separate binding sites in D. saccharalis BBMVs.
| Filing Document | Filing Date | Country | Kind | 371c Date |
|---|---|---|---|---|
| PCT/US10/60817 | 12/16/2010 | WO | 00 | 8/30/2012 |
| Number | Date | Country | |
|---|---|---|---|
| 61284281 | Dec 2009 | US |
