Nucleic Acids Research Advance Access originally published online on August 28, 2007
Nucleic Acids Research 2007 35(17):e114; doi:10.1093/nar/gkm640
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Nucleic Acids Research, 2007, Vol. 35, No. 17 e114
© 2007 The Author(s)
This is an Open Access article distributed under the terms of the Creative Commons Attribution Non-Commercial License (http://creativecommons.org/licenses/by-nc/2.0/uk/) which permits unrestricted non-commercial use, distribution, and reproduction in any medium, provided the original work is properly cited.
Methods Online |
A rapid high-throughput method for the detection and quantification of RNA editing based on high-resolution melting of amplicons
ARC Centre of Excellence for Plant Energy Biology, 4th Floor MCS Building, M316, University of Western Australia, 35 Stirling Highway, Crawley 6009, Western Australia
*To whom correspondence should be addressed. Email: iansmall{at}cyllene.uwa.edu.au
Received July 1, 2007. Revised August 1, 2007. Accepted August 1, 2007.
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ABSTRACT |
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 TOP ABSTRACT INTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
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We describe a rapid, high-throughput method to scan for new RNA editing sites. This method is adapted from high-resolution melting (HRM) analysis of amplicons, a technique used in clinical research to detect mutations in genomes. The assay was validated by the discovery of six new editing sites in different chloroplast transcripts of Arabidopsis thaliana. A screen of a collection of mutants uncovered a mutant defective for editing of one of the newly discovered sites. We successfully adapted the technique to quantify editing of partially edited sites in different individuals or different tissues. This new method will be easily applicable to RNA from any organism and should greatly accelerate the study of the role of RNA editing in physiological processes as diverse as plant development or human health.
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INTRODUCTION |
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TOPABSTRACTINTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
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RNA editing is a process reported in a wide range of organisms from viruses to mammals and plants where it has different functions such as regulating gene expression, increasing protein diversity or reversing the effect of mutations in the genome (1). RNA editing is defined as a site-specific modification of RNA molecules, occurring by nucleotide insertion/deletion, nucleotide substitution or nucleotide modification, usually by deamination of A to I or C to U. Occurring via several molecular mechanisms, different types of editing have been described generally involving a specificity factor (RNA or protein) that recognizes the editing site, an enzyme catalyzing the reaction and sometimes other accessory factors. RNA editing alters the sequence of different types of mRNAs but also tRNAs, rRNAs and small regulatory RNAs (2) (microRNAs). The number of site-specific editing sites varies considerably between organisms. While about a thousand have been reported in some early diverging land plants (3), only a few are known in humans. In many cases, RNA editing is essential for correct production of the protein encoded by the RNA, such as in trypanosomatid and plant organelles or in humans, where this process is essential for the absorption of dietary fats in small intestine by producing the lipid-carrying protein apolipoprotein B48 (4). In other cases, RNA editing modulates the functional properties of the encoded protein as in the case of the glutamate and serotonin receptors in the central nervous system (5,6).
RNA editing events result in a single nucleotide polymorphism between genomic DNA and the corresponding RNA sequence. Partial editing is common and results in a mixed edited and unedited RNA population. The unpredictability of RNA editing and the possibility of editing frequency varying with tissue, development and environmental conditions have made it extremely difficult to effectively screen systematically for editing events or for mutants that are affected in the RNA editing processes. Computational approaches have suggested that editing is much more prevalent than previously realized, particularly in primates (7–9), but few of the predicted sites have been experimentally verified. Previously used methods such as cDNA sequencing, primer extension or pyrosequencing are either too expensive, not sensitive enough or too labor intensive for high-throughput screens (10–12). A one-step, high-throughput method that allows both the scanning of transcripts for new editing sites (without any prior knowledge of their nature or location) and the quantification of editing would greatly accelerate RNA editing research.
We reasoned that techniques used in clinical and genetics research to detect mutations and determine allele frequency should be suitable for detecting new editing sites and quantifying editing. High resolution melting (HRM) of PCR amplicons is used as a closed-tube method for mutation scanning and genotyping that does not require probes or labeled oligonucleotides, and no purification step is needed (13–18). A PCR is performed using a fluorescent double-stranded DNA dye that can be used in fully saturating conditions. The amplicon is analyzed by melting—the change in fluorescence caused by the release of the intercalating dye from a DNA duplex as it is denatured by increasing temperature is precisely monitored. The presence of heteroduplexes (containing one or more mismatches), that melt at lower temperature, alter the shape of the melting curve.
Here, we report the successful adaptation of HRM analysis to scan transcripts for new editing sites and to quantify editing variability in different individuals under various conditions. Our model is the plant Arabidopsis thaliana which displays a moderate frequency of C-to-U editing in mitochondrial and chloroplast transcripts, but the approach would be easily applicable to RNA samples from any organism and to any type of nucleotide substitution or modification editing that results in a different base being incorporated by reverse transcriptase.
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MATERIAL AND METHODS |
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TOPABSTRACTINTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
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Template preparation
DNA was isolated from leaves of Arabidopsis Col-0 as described in Edwards et al. (19). Total RNA was extracted with an RNeasy minikit (Qiagen Pty Ltd, Clifton Hill, VIC, Australia) and treated with a DNA-free kit (Ambion, Austin, TX, USA). DNA-free RNA (3 µg) was reverse transcribed for 1 h at 50°C with the SuperScript III Reverse Transcriptase (Invitrogen Australia Pty, Mount Waverley, VIC, Australia) using random hexamers. PCR and RT-PCR products were cloned in the pGEM-T easy vector (Promega, Madison, WI, USA).
HRM: amplification and melting conditions
The primers used to scan Arabidopsis plastid transcripts are given in Supplementary Table S1. They allow the amplification of fragments of an average size of 500 bp (ranging from 350 to 1330 bp). The intercalating dye used was LCGreen Plus (Idaho Technology Inc., Salt Lake City, UT, USA).
(i) One nanogram of gDNA, (ii) 25 pg of plasmid DNA and (iii) 3 µl of a 1/100 dilution of cDNA or a mixture of (i) and (iii) were amplified in a volume of 10 µl using the LightCycler 480 Probes Master mix (Roche Diagnostics GmbH, Mannheim, Germany) and 200 nM of each primer. All PCR reactions were performed in duplicate. PCR cycling and HRM analysis was performed on an LC480 machine (Roche). The exact amount of cDNA used was not determined, but was adjusted empirically in preliminary experiments to give similar rates of amplification for a wide range of amplicons to those measured using genomic DNA template. The approach is very robust to large differences in cDNA/gDNA ratio.
Short amplicons (60–200 pb) were produced with the following conditions; one cycle of 95°C for 10 min; 40 cycles of 95°C, 20 s; 60°C, 20 s and 72°C, 20 s. For longer amplicons, extension time was increased to 30 s. The amplicons were then denaturated at 95°C for 30 s, renaturated at 70°C for 30 s and melted from 70 to 90°C with 30 signal acquisitions per degree.
The cost per data point for the HRM results was approximately $0.79 AUD, including the cost of primers, amplification mix, fluorescent dye and multiwell plates.
Primer pairs which gave PCR fragments with candidate editing sites were used to re-amplify, clone and sequence cDNAs (sequencing by Macrogen Inc., Seoul, Korea), at a cost of approximately $5.60 AUD per sample.
Amplification and HRM analyses
Amplicons were analyzed with the LightCycler 480 software package. First, an absolute quantification analysis was performed to check the amplification curve and the Crossing Point (CP) value. Then, a Tm calling analysis was done to generate melting curves representing the fluorescence signal (at 450–500 nm) with increasing temperature, melting peaks corresponding to the negative derivative (–d/dT) of the fluorescence signal, and to calculate Tm values.
Transcript scanning
To detect sequence variation between genomic and cDNA we used the Gene Scanning Software. This software analyzes the high-resolution melting curve data to identify changes in the shape of the curve that indicate sequence polymorphisms. The melting curves of different samples are normalized using the fluorescence intensity before and after melting, and temperature shifted to superimpose the curves and better compare their shapes. The Gene Scanning Software generates a difference plot by subtracting the curves from a reference curve and automatically groups samples with similar melting curves. To detect editing events, we compared the amplification product obtained from gDNA and a mix of gDNA and cDNA, and used the Auto Group mode with the highest sensitivity value.
Quantitative assay using short amplicons
The editing efficiency of a particular site was determined by comparing the shape of the melting peaks and Tm values of RT-PCR products to known dilution mixes of edited and unedited plasmids containing the same site.
Poisoned primer extension assay
PPE of RT-PCR products and determination of editing efficiency were performed essentially as described in Peeters and Hanson (11) except that the oligonucleotides used were fluorescently labeled at the 5' end using 6-carboxyfluorescein (FAM) (Sigma Genosys, Sigma-Aldrich Pty Ltd, Castle Hill, NSW, Australia). PCR templates were generated using the primers listed in Supplementary Table S1. Unincorporated primers and nucleotides were removed using ExoSAP-IT (USB Corporation, Cleveland, OH, USA) treatment following the manufacturer's instructions.
The 5' FAM oligonucleotide (0.5 pmol) was extended using 1U of Thermosequenase (ThermoSequenase Cycle Sequencing kit, USB) in a 20 µl reaction containing the thermosequenase buffer, 100 nM of 3 out of 4 dNTP and 100 nM of the fourth ddNTP in a thermocycler for 35 cycles (30 s at 94°C, 30 s at 55°C, 10 s at 72°C). PPE products were resolved on 12% acrylamide sequencing gels (Sequagel, National Diagnostics, Atlanta, GA, USA) at 55W. Following electrophoresis, gels were scanned at 200 µm resolution using a Typhoon Trio imager (GE Healthcare, Amersham, UK) with the emission filter 520 BP 40. FAM fluorescence was collected at 488 nm with a photomultiplier tube voltage set at 500 V.
The cost of a single PPE reaction came to approximately $5.00 AUD including labeled primer, enzymes and sequencing gel.
Scans were analyzed using ImageQuantTL 1D gel analysis software (Amersham Biosciences, Piscataway, NJ, USA). The bands corresponding to edited or unedited products were manually defined. The software gives raw volume data corresponding to fluorescence intensity. A background volume was subtracted from edited and unedited band volumes, by defining as a band the location of either edited or unedited product in the unedited plasmid and edited plasmid control, respectively. The editing efficiency (% edited product) for every lane was calculated as 100*(edited band volume—background volume for edited band)/(edited band volume—background volume for edited band) + (unedited band volume—background volume for unedited band).
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RESULTS |
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TOPABSTRACTINTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
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HRM detects single nucleotide polymorphisms between DNA and RNA with high throughput
Until recently, special apparatus was required to perform HRM analysis that was not designed for high-throughput analyses. However, the latest generation of real-time PCR machines (e.g. Roche LC480) offers the possibility of analyzing 384 samples in parallel on a machine not specifically designed for HRM but with sufficiently resolutive melting curves to attempt the analysis. We tested the ability of the LC480 to detect C to U editing events in transcripts. As we planned to compare amplification products from genomic DNA with a C at the editing sites and RT-PCR products with a T at the same position, we assayed the detection of C/T heteroduplexes, by mixing plasmid DNA containing a C and plasmid DNA containing a T at the same site in various ratios. We were able to convincingly detect single base-pair mismatch heteroduplexes that alter the melting curve shape in amplicons up to 700 bp (data not shown).
To scan transcripts for editing sites, we compared the melting curves of amplification products from genomic DNA (homoduplexes) to amplification products from a mix of genomic (gDNA) and cDNA (containing heteroduplexes if the cDNA has been reverse transcribed from an edited mRNA). The procedure is described in Figure 1a. Our interest was to gain a complete description of the editing sites in chloroplast transcripts of the model plant A. thaliana as an important step towards characterizing editing factors in plants. To generate amplicons to be analyzed by HRM, primers originally designed to screen chloroplast transcripts for transcription, processing and splicing defects were used (Charles Andrés, Andéol Falcon de Longevialle, ALCB, Claire Lurin and IS, in preparation). This primer set comprises 320 pairs spanning the entire Arabidopsis plastid genome with an average amplicon size of 
500 bp.
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Among these primer pairs, 21 couples flank all 28 of the known editing sites (20). Four of these pairs flank multiple editing sites. All these pairs were tested and all 21 amplicons were flagged as containing heteroduplexes by the HRM assay, demonstrating the sensitivity of the technique (Table 1).
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Discovery of six new editing sites in Arabidopsis chloroplasts
Out of the full set of 320 amplicons, besides the 21 known to contain editing sites, 18 other amplicons were found to give different melting curve shapes from gDNA alone versus a mix of gDNA and cDNA. The amplification products were checked by gel electrophoresis and those presenting more than one band (5 out of the 18) were not considered further as multiple PCR products obviously interfere with the melting analysis. To confirm the remaining 13 candidates, we sequenced cloned RT-PCR products. For 6 candidates, no difference in the sequence was found indicating that they are false positives. The remaining 7 candidate amplicons contained single C to T changes consistent with RNA editing, covering six new sites not previously identified in Arabidopsis (Figure 2, Table 1). One of these new sites was covered by two amplicons in the screen and detected in both. Five of the six new sites could be further confirmed by analysis of public EST databases that revealed sequences containing the same C/T polymorphisms. No publicly available ESTs exist for the sixth transcript, accD.
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Identifying mutants impaired in editing
The factors involved in RNA editing in plants are still elusive. Two pentatricopeptide repeat (PPR) proteins have been reported to be essential for the editing of specific sites in the chloroplast transcript ndhD of Arabidopsis (21,22), raising the possibility that this large family of RNA-binding proteins could constitute the specificity factors recognizing the sequence around the target C and recruiting the enzyme to catalyze editing (23).
We are undertaking extensive HRM screening of Arabidopsis mutant lines lacking different proteins of the PPR family, to check for defects in RNA editing. One mutant, clb19, with an insertion in the gene At1g05750 was found to be impaired in the editing of two sites in the transcripts rpoA and clpP (Figure 3). This mutant will be described more fully elsewhere (Charles Andrés, ALCB, Maricela Ramos Vega, Arturo Guevara-García, María de la Luz Gutiérrez-Nava, Araceli Cantero, Luis Felipe Jiménez, Claire Lurin, IS and Patricia León, in preparation). The site in rpoA is one of the six new sites discovered in the screen developed during this study.
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HRM to quantify RNA editing
HRM has been used to detect mutations in heterogeneous DNA populations and proved reasonably sensitive (15). We decided to adapt this type of sensitivity test to quantify editing (the procedure is shown in Figure 1b and differs primarily from the screens described previously in that the cDNA is not mixed with genomic DNA before amplification and that much shorter amplicons are required for the best results). We first calibrated the test with mixes of plasmid DNA containing a range of ratios of C to T at known editing sites. In short amplicons of 70 bp, as little as 2.5% T was easily detected and melting peak profiles for amplicons differing by only a few percent in C/T could be distinguished (Figure 4). In plant organelles, the extent of RNA editing of some sites can vary according to the genotype, the tissue or in different growth conditions (11,24–26). No systematic survey has been published so far concerning such changes, which may well have physiological relevance. To gauge the efficacy of the HRM assay for such a survey, we prepared cDNA samples from different Arabidopsis genotypes, different organs, or from plants grown in different conditions. The cDNAs were amplified, subjected to HRM analysis and their melting peak profiles were compared to the ones from plasmid mixes with increasing ratios of T as compared to C. Five primer pairs flanking four different sites in the transcripts clpP, accD, ndhG and rpoA were tested. The results obtained with the HRM assay were compared to those obtained by a widely used, but much more labor-intensive poisoned primer extension (PPE) assay (11). In all, 24 comparisons were made (6 samples x 4 editing sites). In 18 of the 24 comparisons, the editing efficiency measured by HRM matched that measured by PPE (Table 2). In the cases where the two approaches gave different values, the values were reasonably close, generally within 10%.
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DISCUSSION |
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TOPABSTRACTINTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
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Following optimization of the procedures, we employed HRM to analyze chloroplast transcripts from A. thaliana, already extensively analyzed by previous groups (20,27). This screen covered a total of 126 kb of Arabidopsis chloroplast transcripts in four amplification plates and took only 4 days to complete. The screen detected 34 editing sites in total, including all 28 known sites, whilst discovering 6 new editing sites (Figure 2 and Table 1). Four of these sites in are coding sequences (rpoA, rpoC1, psbZ, rpl23) and change the protein sequence translated from these mRNAs. The other two sites are the first to be identified in Arabidopsis chloroplast non-coding sequences (in the 3' UTR of accD and the intron of rps12). Despite the sensitivity of the screen, only 11 false candidates needed to be eliminated (a false positive rate of 11/292 or 3.8%), and 5 of those could be ruled out simply by electrophoresis of the amplicons. This high sensitivity coupled with a low false positive rate, the simplicity of use and the affordability of the approach (6 times cheaper per data point than bulk sequencing of RT-PCR products) make HRM screening an extremely attractive new tool for studying RNA editing. We demonstrated that this method is highly suitable for systematically screening mutants for a defect in editing by discovering that the Arabidopsis mutant clb19 fails to edit two sites, in clpP and rpoA.
Furthermore, using small amplicons, HRM is sensitive and accurate enough to detect < 2.5% editing and to easily quantify partially edited sites, the editing extent of which can vary in different genotypes, different organs and different conditions. Previous quantification techniques such as poisoned primer extension or pyrosequencing were much more labor intensive, low throughput and prohibitively expensive for large-scale surveys.
One of the few drawbacks of the approach is that HRM analysis alone cannot easily detect how many editing sites are present, or where within the amplified region the editing site is positioned. For this, sequencing of the amplified product is required.
In conclusion, we have demonstrated that a method originally designed to detect DNA mutations and genotype individuals in clinical research and diagnostics can be simply adapted to research on RNA editing. Currently research in this area is limited by the lack of cheap, effective approaches for screening for new editing sites or for mutants affected in the editing process. The approach described here can be simply and directly applied to samples from any organism, so this breakthrough should stimulate research in many laboratories.
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SUPPLEMENTARY DATA |
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TOPABSTRACTINTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
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Supplementary Data are available at NAR Online.
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ACKNOWLEDGEMENTS |
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This work was funded by Australian Research Council (CE0561495 to I.S.), the State Government of Western Australia and the University of Western Australia. Funding to pay the Open Access publication charges for this article was provided by XXX.
Conflict of interest statement. None declared.
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REFERENCES |
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TOPABSTRACTINTRODUCTIONMATERIAL AND METHODSRESULTSDISCUSSIONSUPPLEMENTARY DATAREFERENCES |
|---|
- Gott JM, Emeson RB. Functions and mechanisms of RNA editing. Annu. Rev. Genet. (2000) 34:499–531.[CrossRef][ISI][Medline]
- Kawahara Y, Zinshteyn B, Sethupathy P, Iizasa H, Hatzigeorgiou AG, Nishikura K. Redirection of silencing targets by adenosine-to-inosine editing of miRNAs. Science (2007) 315:1137–1140.
[Abstract/Free Full Text] - Kugita M, Yamamoto Y, Fujikawa T, Matsumoto T, Yoshinaga K. RNA editing in hornwort chloroplasts makes more than half the genes functional. Nucleic Acids Res. (2003) 31:2417–2423.
[Abstract/Free Full Text] - Young SG. Recent progress in understanding apolipoprotein B. Circulation (1990) 82:1574–1594.[ISI][Medline]
- Burns CM, Chu H, Rueter SM, Hutchinson LK, Canton H, Sanders-Bush E, Emeson RB. Regulation of serotonin-2C receptor G-protein coupling by RNA editing. Nature (1997) 387:303–308.[CrossRef][Medline]
- Seeburg PH, Higuchi M, Sprengel R. RNA editing of brain glutamate receptor channels: mechanism and physiology. Brain Res. Brain Res. Rev. (1998) 26:217–229.[CrossRef][Medline]
- Athanasiadis A, Rich A, Maas S. Widespread A-to-I RNA editing of Alu-containing mRNAs in the human transcriptome. PLoS Biol. (2004) 2:e391.[CrossRef][Medline]
- Kim DD, Kim TT, Walsh T, Kobayashi Y, Matise TC, Buyske S, Gabriel A. Widespread RNA editing of embedded alu elements in the human transcriptome. Genome Res. (2004) 14:1719–1725.
[Abstract/Free Full Text] - Levanon EY, Eisenberg E, Yelin R, Nemzer S, Hallegger M, Shemesh R, Fligelman ZY, Shoshan A, Pollock SR, et al. Systematic identification of abundant A-to-I editing sites in the human transcriptome. Nat. Biotechnol. (2004) 22:1001–1005.[CrossRef][ISI][Medline]
- Iwamoto K, Bundo M, Kato T. Estimating RNA editing efficiency of five editing sites in the serotonin 2C receptor by pyrosequencing. RNA (2005) 11:1596–1603.
[Abstract/Free Full Text] - Peeters NM, Hanson MR. Transcript abundance supercedes editing efficiency as a factor in developmental variation of chloroplast gene expression. RNA (2002) 8:497–511.[Abstract]
- Sasaki T, Yukawa Y, Wakasugi T, Yamada K, Sugiura M. A simple in vitro RNA editing assay for chloroplast transcripts using fluorescent dideoxynucleotides: distinct types of sequence elements required for editing of ndh transcripts. Plant J. (2006) 47:802–810.[CrossRef][ISI][Medline]
- Herrmann MG, Durtschi JD, Bromley LK, Wittwer CT, Voelkerding KV. Amplicon DNA melting analysis for mutation scanning and genotyping: cross-platform comparison of instruments and dyes. Clin. Chem. (2006) 52:494–503.
[Abstract/Free Full Text] - Herrmann MG, Durtschi JD, Bromley LK, Wittwer CT, Voelkerding KV. Instrument comparison for heterozygote scanning of single and double heterozygotes: a correction and extension of Herrmann et al. Clin Chem 2006;52:494–503. Clin. Chem. (2007) 53:150–152.
[Free Full Text] - Krypuy M, Newnham GM, Thomas DM, Conron M, Dobrovic A. High resolution melting analysis for the rapid and sensitive detection of mutations in clinical samples: KRAS codon 12 and 13 mutations in non-small cell lung cancer. BMC Cancer (2006) 6:295.[CrossRef][Medline]
- Liew M, Pryor R, Palais R, Meadows C, Erali M, Lyon E, Wittwer C. Genotyping of single-nucleotide polymorphisms by high-resolution melting of small amplicons. Clin. Chem. (2004) 50:1156–1164.
[Abstract/Free Full Text] - Reed GH, Wittwer CT. Sensitivity and specificity of single-nucleotide polymorphism scanning by high-resolution melting analysis. Clin. Chem. (2004) 50:1748–1754.
[Abstract/Free Full Text] - Wittwer CT, Reed GH, Gundry CN, Vandersteen JG, Pryor RJ. High-resolution genotyping by amplicon melting analysis using LCGreen. Clin. Chem. (2003) 49:853–860.
[Abstract/Free Full Text] - Edwards K, Johnstone C, Thompson C. A simple and rapid method for the preparation of plant genomic DNA for PCR analysis. Nucleic Acids Res. (1991) 19:1349.
[Free Full Text] - Tillich M, Funk HT, Schmitz-Linneweber C, Poltnigg P, Sabater B, Martin M, Maier RM. Editing of plastid RNA in Arabidopsis thaliana ecotypes. Plant J. (2005) 43:708–715.[CrossRef][ISI][Medline]
- Kotera E, Tasaka M, Shikanai T. A pentatricopeptide repeat protein is essential for RNA editing in chloroplasts. Nature (2005) 433:326–330.[CrossRef][Medline]
- Okuda K, Myouga F, Motohashi R, Shinozaki K, Shikanai T. Conserved domain structure of pentatricopeptide repeat proteins involved in chloroplast RNA editing. Proc. Natl Acad. Sci. USA (2007) 104:8178–8183.
[Abstract/Free Full Text] - Lurin C, Andres C, Aubourg S, Bellaoui M, Bitton F, Bruyere C, Caboche M, Debast C, Gualberto J, et al. Genome-wide analysis of Arabidopsis pentatricopeptide repeat proteins reveals their essential role in organelle biogenesis. Plant Cell (2004) 16:2089–2103.
[Abstract/Free Full Text] - Bentolila S, Chateigner-Boutin AL, Hanson MR. Ecotype allelic variation in C-to-U editing extent of a mitochondrial transcript identifies RNA-editing quantitative trait loci in Arabidopsis. Plant Physiol. (2005) 139:2006–2016.
[Abstract/Free Full Text] - Chateigner-Boutin AL, Hanson MR. Developmental co-variation of RNA editing extent of plastid editing sites exhibiting similar cis-elements. Nucleic Acids Res. (2003) 31:2586–2594.
[Abstract/Free Full Text] - Nakajima Y, Mulligan RM. Heat stress results in incomplete C-to-U editing of maize chloroplast mRNAs and correlates with changes in chloroplast transcription rate. Curr. Genet. (2001) 40:209–213.[CrossRef][ISI][Medline]
- Lutz KA, Maliga P. Lack of conservation of editing sites in mRNAs that encode subunits of the NAD(P)H dehydrogenase complex in plastids and mitochondria of Arabidopsis thaliana. Curr. Genet. (2001) 40:214–219.[CrossRef][ISI][Medline]
- Zeng WH, Liao SC, Chang CC. Identification of RNA editing sites in chloroplast transcripts of Phalaenopsis aphrodite and comparative analysis with those of other seed plants. Plant Cell Physiol. (2007) 48:362–368.
[Abstract/Free Full Text] - Inada M, Sasaki T, Yukawa M, Tsudzuki T, Sugiura M. A systematic search for RNA editing sites in pea chloroplasts: an editing event causes diversification from the evolutionarily conserved amino acid sequence. Plant Cell Physiol. (2004) 45:1615–1622.
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