Oligonucleotide-directed construction of mutations: a gapped duplex DNA procedure without enzymatic reactions in vitro.

The gapped duplex DNA approach to oligonucleotide-directed construction of mutations (Kramer et al. 1984, Nucl. Acids Res. 12, 9441-9456) has been developed further. A procedure is described that makes in vitro DNA polymerase/DNA ligase reactions dispensable. Direct transfection of host bacteria with gdDNA molecules of recombinant phage M13 plus mutagenic oligonucleotide results in marker yields in excess of 50% (gap size 1640 nucleotides). An important feature incorporated into the mutagenic oligonucleotide is the presence of one or two internucleotidic phosphorothioate linkages immediately adjacent to the 5'-terminus. Automated preparation and biochemical properties of such compounds are described as well as their performance in oligonucleotide-directed mutagenesis. A systematic study of the following parameters influencing marker yield is reported: Gap size, length of oligonucleotide, chemical nature of oligonucleotide termini and heatshock temperature during transformation.     

EcoK selection vectors for shotgun cloning into M13 and deletion mutagenesis.

For shotgun cloning into M13 vectors, a double-stranded cassette of synthetic oligonucleotides containing a SmaI site within the two halves of an EcoK site, has been introduced into the vector M13mp8. Cloning of blunt end DNA into the SmaI site destroys the EcoK site, and recombinants are therefore preferentially selected on transfection into a K strain of E.coli. For deletion mutagenesis using synthetic oligonucleotides, an M13 vector with four copies of the EcoK cassette has been made to facilitate the joining of lacZ or a Factor Xa cleavage site to any protein reading frame.     

Oligonucleotide directed mutagenesis of the human beta-globin gene: a general method for producing specific point mutations in cloned DNA.

A nonadecanucleotide has been used both as a site specific mutagen to introduce a T leads to A transversion mutation in the human beta-globin gene cloned in pBR322 as well as a probe to screen transformed colonies for the desired mutant. The specificity of the oligonucleotide as a mutagen and as a hybridization probe provide a general method for producing site specific mutations in DNA cloned in plasmid vectors such as pBR322.     

Half-site editing: an in vitro mutagenesis procedure for truncating a DNA fragment and introducing a new restriction site

Half-site editing is an in vitro mutagenesis procedure designed for use in making precise plasmid constructions. Like many in vitro mutagenesis techniques, this procedure involves hybridization of a mutagenic oligonucleotide primer to single-stranded template DNA followed by polymerization with DNA polymerase I (Klenow). Half-site editing differs from other techniques in two main ways. First, T4 DNA polymerase treatment truncates the target DNA at a point determined by the primer and repairs any mismatches to the sequence specified by the primer. Second, a blunt-end ligation step is included. This ligation exploits the symmetry inherent in most restriction sites to create a desired restriction site at the truncated end of the target DNA fragment. Half-site editing has been used to place ClaI restriction sites at the 3' end of the yeast pyruvate kinase promoter and at two positions at the 5' end of the yeast acetolactate synthase coding sequence.     

Improvement in the alkaline stability of subtilisin using an efficient random mutagenesis and screening procedure

An efficient random mutagenesis procedure coupled to a replica plate screen facilitated the isolation of mutant subtilisins from Bacillus amyloliquefaciens that had altered autolytic stability under alkaline conditions. Out of about 4000 clones screened, approximately 70 produced subtilisins with reduced stability (negatives). Two clones produced a more stable subtilisin (positives) and were identified as having a single mutation, either Ile107Val or Lys213Arg (the wild-type amino acid is followed by the codon position and the mutant amino acid). One of the negative mutants, Met50Val, was at a site where other homologous subtilisins contained a Phe. When the Met50Phe mutation was introduced into the B. amyloliquefaciens gene, the mutant subtilisin was more alkaline stable. The double mutant (Ile107Val/Lys213Arg) was more stable than the isolated single mutant parents. The triple mutant (Met50Phe/Ile107Val/Lys213Arg) was even more stable than Ile107Val/Lys213Arg (up to two times the autolytic half-time of wild-type at pH 12). These studies demonstrate the feasibility for improving the alkaline stability of proteins by random mutagenesis and identifying potential sites where substitutions from homologous proteins can improve alkaline stability.     

Rapid synthesis and cloning of complementary DNA from any RNA molecule into plasmid and phage M13 vectors

We describe several modifications of the Gubler and Hoffman procedure [Gene 25 (1983) 263-269] for complementary DNA (cDNA) synthesis that expand the versatility of this method for the rapid synthesis and cloning of double-stranded (ds) cDNA. These modifications include: (1) The combination of first and second strand synthesis into a single two-step reaction, which reduces the time for synthesis of blunt-ended ds-cDNA to less than 4 h. (2) The use of random hexadeoxyribonucleotide primers (RP) for the synthesis of ds-cDNA, which allows the synthesis of cDNA from any RNA template. (3) The combined use of random primers and DNA ligase treatment of cDNA/RNA hybrids prior to second-strand synthesis, which promotes the production of nearly full length ds-cDNA molecules. (4) The use of gel filtration to size-fractionate ds-cDNA, which allows the selection of specific size classes of ds-cDNA for cloning. (5) The use of blunt-end ligation to insert the ds-cDNA into the vector, which reduces the total time required for the construction of cDNA libraries to less than 24 h.     

Variants of phage M13 DNA containing a fragment of the beta-galactosidase gene--a convenient mutation system for the study of oligonucleotide-directed mutagenesis

A model system is developed to test oligonucleotide-directed mutations: T----C transition, T and C deletions (delta T and delta C), C insertion, double mutations (A----G, delta T), (T----C, A----G), and large oligonucleotide deletions (36 or 44 nucleotides). The system includes 9 variants of the phage M13 DNA carrying fragment of beta-galactosidase gene, and oligodeoxyribonucleotides partially noncomplementary to DNA sequence of this gene. Six variants are obtained by the site-localized mutagenesis, the other were described earlier. Induced mutations are easily tested by phenotype change of transformed bacteria (Lac+----Lac-); by formation or loss of the sites for BamHI and EcoRI restrictases; by DNA hybridization with 32P-labeled oligonucleotides; and by DNA sequencing by the Sanger method. The system is used to study the role of some factors, such as completeness of RF DNA synthesis, thermal stability of the oligonucleotide: DNA complex, quality of enzymes and substrates used in polymerase reaction, mutation type or the efficiency of mutagenesis. A number of unexpected mutations were observed in the course of oligonucleotide-directed mutagenesis. Lower yields of some mutants induced by oligonucleotides are shown to be due to the action of repair systems of bacteria.     

Cassette mutagenesis: an efficient method for generation of multiple mutations at defined sites

A method is described for the efficient insertion of mutagenic oligodeoxynucleotide cassettes which allow saturation of a target amino acid codon with multiple mutations. Restriction sites are introduced by oligonucleotide-directed mutagenesis procedures to flank closely the target codon in the plasmid containing the gene. The restriction sites to be introduced are chosen based on their uniqueness to the plasmid, proximity to the target codon and conservation of the final amino acid coding sequence. The flanking restriction sites in the plasmid are digested with the cognate restriction enzymes, and short synthetic duplex DNA cassettes (10-25 bp) are inserted. The mutagenic cassette is designed to restore fully the wild-type coding sequence, except over the target codon, and to eliminate one or both restriction sites. Elimination of a restriction site facilitates selection of clones containing the mutagenic oligodeoxynucleotide cassette. To make the cassettes, single-stranded oligodeoxynucleotides and their complements are synthesized in separate pools containing different codons over the target. This method has been successfully applied to generate 19 amino acid substitutions at position 222 in the subtilisin protein sequence.     

Deletion loop mutagenesis: a novel method for the construction of point mutations using deletion mutants

Deletion loop mutagenesis is a new, general method for site-directed mutagenesis that allows point mutations to the introduced within a sequence of DNA defined by a previously isolated deletion mutant. Wild type and deletion mutant DNA are cloned into a bacterial plasmid and each is cleaved with a different single cut restriction enzyme. Heteroduplexes are formed between the two DNAs to produce circular molecules containing a nick in each strand and a single-stranded deletion loop. The deletion loops are mutagenised using sodium bisulphite and the DNA transfected directly into a uracil repair deficient strain of Escherichia coli. Up to half of the resultant clones contain DNA produced by replication of the wild-type length strand and bear mutations exclusively within the target area. An example is given in which a deletion mutant lacking 21 nucleotides from the region coding for SV40 large-T was used. Eight of the possible nine target cytosine residues were mutagenised. The method described is specific, efficient and simple.     

EMS mutagenesis and qPCR-HRM prescreening for point mutations in an embryogenic cell suspension of grapevine

Key message

Embryogenic suspension cultures are suitable for EMS mutagenesis in grapevine, and HRM prescreening of EMS-treated somatic embryo clusters allows rapid detection of point mutations before plant regeneration.

Abstract

Somatic embryogenesis is an excellent system for induced mutagenesis and clonal propagation in woody plants. Our work was focused on establishing a procedure for inducing ethyl methanesulfonate (EMS) mutagenesis in grapevine. Embryogenic cell aggregates (ECAs) growing in liquid medium were treated with increasing concentrations of EMS. We found that EMS dramatically affects the viability of ECAs at concentrations above 20 mM (25.5 ± 2.9 % survival), whereas concentrations above 10 mM affect embryogenic potential (22.1 ± 1.7 % of ECAs gave rise to embryos). Embryo masses generated from EMS-treated embryogenic cell aggregates were prescreened by quantitative PCR-High Resolution Melting (qPCR-HRM) to detect single nucleotide polymorphisms (SNPs) in a 1,000-bp VvNCED1-encoding DNA fragment, which served as the target gene. Detected mutations were verified in regenerated plants by PCR and sequencing. qPCR-HRM analysis of the difference plots for the fluorescence signals allowed detection of a mutation in a sample from an embryogenic aggregate treated with 10 mM EMS. To confirm the nature of the mutation, embryos from this aggregate were recovered and germinated, and leaves were collected for PCR and sequencing analysis. The alignment of sequences from regenerated plants with the wild-type sequence revealed a transitional mutation (G/C to A/T) in the 1,000-bp VvNCED1-encoding region. To our knowledge, this is the first time that EMS mutagenesis has been performed using an embryogenic cell suspension of grapevine.     

A simple and efficient method for chemical mutagenesis of DNA.

A simple and efficient procedure for the generation of random GC to AT transition mutations in a specific DNA segment is described. A restriction fragment is inserted in each orientation into an M13 vector, single-stranded virion DNA from each recombinant phage is treated with methoxylamine, and, after reannealing of the mutagenized strands, a double-stranded restriction fragment is obtained. This methoxylamine-derivatized DNA segment is then joined with linearized M13 RF DNA, competent E. coli is transfected, and mutations are directly identified by sequencing of the phage DNA. Using this technique, single and double nucleotide substitutions were generated at a frequency greater than 50% in a 56-base pair segment of the signal codons of the TEM beta-lactamase.     

Improved M13 phage cloning vectors and host strains: nucleotide sequences of the M13mp18 and pUC19 vectors

Three kinds of improvements have been introduced into the M13-based cloning systems. (1) New Escherichia coli host strains have been constructed for the E. coli bacteriophage M13 and the high-copy-number pUC-plasmid cloning vectors. Mutations introduced into these strains improve cloning of unmodified DNA and of repetitive sequences. A new suppressorless strain facilitates the cloning of selected recombinants. (2) The complete nucleotide sequences of the M13mp and pUC vectors have been compiled from a number of sources, including the sequencing of selected segments. The M13mp18 sequence is revised to include the G-to-T substitution in its gene II at position 6 125 bp (in M13) or 6967 bp in M13mp18. (3) M13 clones suitable for sequencing have been obtained by a new method of generating unidirectional progressive deletions from the polycloning site using exonucleases HI and VII.     

A simple and efficient method for the oligodeoxyribonucleotide-directed mutagenesis of double-stranded plasmid DNA.

A method for the oligodeoxyribonucleotide-directed mutagenesis of double-stranded DNA without the necessity for phenotypic selection is described. Plasmids denatured with alkali and purified by adsorption to and elution from nitrocellulose have single-stranded regions where primers can hybridize and serve as templates for a T7 DNA polymerase-catalyzed synthesis of complementary mutant DNA strands. When this procedure was carried out such that the original nonmutant strand contained uracil [method of Kunkel, Proc. Natl. Acad. Sci. USA 82(1985)488-492], mutation frequencies of between 30% and 40% were obtained. The technique has been used to generate mutant genes in plasmids of a wide variety of sizes. The largest plasmid manipulated and successfully mutagenized was 22 kb. The method is rapid and efficient and is not dependent upon either f1 phage vectors or the presence of restriction sites in the vicinity of the sequence targeted for mutation.     

Specificity of ionizing radiation-induced mutagenesis in the lac region of single-stranded phage M13 mp10 DNA.

M13 mp10 single-stranded phage DNA was irradiated with 60 Co gamma-rays, and transfected into Escherichia coli. One hundred and sixteen mutant clones having lesions in the lac insert were selected, and mutational sites were examined by DNA sequence analysis. Fourteen out of the 15 nucleotide changes thus detected were base substitutions, and the rest was a base addition. Transitions and transversions were almost equal in number. Mutational events were observed at cytosine residues more frequently than at other residues, and the predominant base change was a C ---- T transition. Possible roles in gamma-ray-induced mutagenesis played by the misincorporation of dAMP owing to radiolytic derivatives of cytosine residues and/or formation of apurinic/apyrimidinic sites are discussed.     

A simple and efficient method for the oligonucleotide-directed mutagenesis using plasmid DNA template and phosphorothioate-modified nucleotide

We have developed a simple and efficient method for oligonucleotide-directed mutagenesis with double-stranded (plasmid) DNA as a template. The template was simply and rapidly prepared by cell lysis and the following DNA denaturation with alkali. The chain elongation was performed with phosphorothioate-modified nucleotide at 37 degrees C. After the selective digestion of original DNA with NciI and exonuclease III, the desired mutated gene was obtained at a high frequency (about 70%).     

Efficient point mutagenesis in mycobacteria using single-stranded DNA recombineering: characterization of antimycobacterial drug targets

Construction of genetically isogenic strains of mycobacteria is complicated by poor recombination rates and the lack of generalized transducing phages for Mycobacterium tuberculosis . We report here a powerful method for introducing single point mutations into mycobacterial genomes using oligonucleotide-derived single-stranded DNA recombineering and mycobacteriophage-encoded proteins. Phage Che9c gp61-mediated recombination is sufficiently efficient that single base changes can be introduced without requirement for direct selection, with isogenic mutant strains identified simply by PCR. Efficient recombination requires only short (50 nucleotide) oligonucleotides, but there is an unusually strong strand bias and an oligonucleotide targeting lagging strand DNA synthesis can recombine more than 10 000-fold efficiently than its complementary oligonucleotide. This ssDNA recombineering provides a simple assay for comparing the activities of related phage recombinases, and we find that both Escherichia coli RecET and phage λ Red recombination proteins function inefficiently in mycobacteria, illustrating the utility of developing recombineering in new bacterial systems using host-specific bacteriophage recombinases. ssDNA mycobacterial recombineering provides a simple approach to characterizing antimycobacterial drug targets, and we have constructed and characterized single point mutations that confer resistance to isoniazid, rifampicin, ofloxacin and streptomycin.