- Methodology article
- Open Access
Seamless editing of the chloroplast genome in plants
© The Author(s). 2016
Received: 27 April 2016
Accepted: 20 July 2016
Published: 29 July 2016
Gene editing technologies enable the precise insertion of favourable mutations and performance enhancing trait genes into chromosomes whilst excluding all excess DNA from modified genomes. The technology gives rise to a new class of biotech crops which is likely to have widespread applications in agriculture. Despite progress in the nucleus, the seamless insertions of point mutations and non-selectable foreign genes into the organelle genomes of crops have not been described. The chloroplast genome is an attractive target to improve photosynthesis and crop performance. Current chloroplast genome engineering technologies for introducing point mutations into native chloroplast genes leave DNA scars, such as the target sites for recombination enzymes. Seamless editing methods to modify chloroplast genes need to address reversal of site-directed point mutations by template mediated repair with the vast excess of wild type chloroplast genomes that are present early in the transformation process.
Using tobacco, we developed an efficient two-step method to edit a chloroplast gene by replacing the wild type sequence with a transient intermediate. This was resolved to the final edited gene by recombination between imperfect direct repeats. Six out of 11 transplastomic plants isolated contained the desired intermediate and at the second step this was resolved to the edited chloroplast gene in five of six plants tested. Maintenance of a single base deletion mutation in an imperfect direct repeat of the native chloroplast rbcL gene showed the limited influence of biased repair back to the wild type sequence. The deletion caused a frameshift, which replaced the five C-terminal amino acids of the Rubisco large subunit with 16 alternative residues resulting in a ~30-fold reduction in its accumulation. We monitored the process in vivo by engineering an overlapping gusA gene downstream of the edited rbcL gene. Translational coupling between the overlapping rbcL and gusA genes resulted in relatively high GUS accumulation (~0.5 % of leaf protein).
Editing chloroplast genomes using transient imperfect direct repeats provides an efficient method for introducing point mutations into chloroplast genes. Moreover, we describe the first synthetic operon allowing expression of a downstream overlapping gene by translational coupling in chloroplasts. Overlapping genes provide a new mechanism for co-ordinating the translation of foreign proteins in chloroplasts.
Methods to edit genes based on programmable nucleases have revolutionised the manipulation of nuclear genomes in multicellular eukaryotes [1, 2]. They allow precise targeted changes ranging from single nucleotide alterations to the seamless insertion of exogenous genes into nuclear chromosomes [3–5]. Successful editing gives rise to organisms with precise genome modifications, which can be free of all excess DNA such as marker genes and vector backbone sequences. Technologies to edit genomes address concerns associated with the imprecision of standard transformation technologies  including the contribution of excess DNA to phenotype. These advantages of genome editing have raised questions on the need to change the regulatory landscape for crops improved by transformation .
Outside the nucleus, important sets of genes are present in mitochondria and chloroplasts . These extra-nuclear genes play essential roles in respiration, photosynthesis and development [8, 9] and are targets for improving crop productivity to ensure global food security . Whilst programmable nucleases have been imported into mitochondria to induce double strand DNA breaks , genome editing requires the additional step of introducing a nucleic acid template into organelles to repair and introduce the desirable changes at the break sites. This requires methods that lead to the isolation of stable organelle transformants. In multicellular eukaryotes, these protocols are available for chloroplasts [12–14] but not mitochondria. Key chloroplast editing targets include the rbcL gene encoding the catalytic large subunit of ribulose bisphosphate carboxylase/oxygenase (Rubisco LS), the primary CO2 fixing enzyme, which is a focus for improvement [15–17]. Application of editing technologies to transgenes would allow their seamless insertion into chloroplast DNA to improve photosynthesis  and stress tolerance  as well as express industrial and health care products in chloroplasts [14, 20–22].
Homology dependent repair is a key component of genome editing and was used without programmable nucleases in early approaches to edit complex eukaryotic genomes . The process was relatively inefficient due to low rates of homologous recombination . The predominance of homologous recombination in chloroplasts  is a considerable advantage for developing genome editing technologies. It removes the need for making double strand breaks at editing sites with programmable nucleases [1, 2] to stimulate homologous recombination. This allows seamless insertion of selectable antibiotic and herbicide resistance genes [12, 13, 24–26] into chloroplast genomes (cp genomes). However, existing genome engineering methods to introduce point mutations or non-selectable foreign genes into the chloroplasts of wild type (WT) crops leave excess DNA associated with the transformation process, such as marker genes, or following marker excision, the target sites of site-specific recombinases and ectopic direct repeats [12–14, 24]. Seamless chloroplast genome editing methods would allow, in principle, the isolation of transplastomic derivatives that differ from the parental crop used for transformation by a single base mutation in a key chloroplast gene. Such methods need to overcome the dual challenges of the high copy number of cp genomes, which are present in thousands of copies per cell [23, 27], and reversion of edited changes by copy correction  with the vast excess of unedited genomes resident in WT chloroplasts. These issues have raised questions on the feasibility of isolating plants with a uniform (homoplasmic) population of edited cp genomes . The possibility of using gene drive technologies  in organelles to address the problem of editing multi-copy genomes raises safety concerns related to containment .
Here we describe a two-step method to edit chloroplast genes that involves replacing the unedited WT sequence with a transient editing intermediate, which was then resolved by homologous recombination to the final edited gene. The method is applicable to angiosperm cp genomes and was exemplified in tobacco, which contains a typical 156 kb cp genome [8, 13, 31] and is the model plant for transplastomic research. The tobacco cp genome encodes about 80 polypeptides, many of which are expressed from operon-like gene clusters [8, 32, 33]. The versatility of the method was illustrated by deleting a single nucleotide from the C-terminal coding region of the rbcL gene in a construct containing overlapping reading frames for the rbcL and gusA  genes. The recombination event involved in the protocol provided a powerful tool to examine the effect of switching upstream sequences on overlapping gene expression within a single transplastomic line. Efficient translation of gusA demonstrated the capacity of the chloroplast translational apparatus to express overlapping foreign genes in planta.
Chloroplast genome editing scheme
C-terminal rbcL frameshift mutation
Step one: isolation of transplastomic plants containing the iDR intermediate cp genome
Step 2: isolation of marker-free transplastomic plants homoplasmic for the edited cp genome
Whilst Hind III digests confirmed homoplasmy of the predicted edited cp genome in five of the marker-free T2 plants tested (Fig. 6a-b), they could not be used to provide a reliable estimate of the amount of edited marker-free cp genomes present in the T0 plants due to the similar sizes of the Hind III bands binding to the rbcL probe. The small fraction of edited marker-free genomes in uniformly green T0 transplastomic plants containing the iDR intermediate was determined by blot analyses using a gusA gene probe against DNA digested with NotI (N) and SacI (S). Maps of the iDR intermediate and edited genome are shown in Fig. 6e. DNA from a homoplasmic marker-free edited plant provided a control lane and gave rise to a single 4.8 kb gusA band diagnostic of the edited genome as predicted (Fig. 6f, lane 6). DNA digests from iDR plants showed a predominant 2.9 kb gusA band (Fig. 6f, lanes 3–5) diagnostic of the cp genome with the iDR intermediate (Fig. 6e). The 4.8 kb band corresponding to the edited cp genome was barely detectable in these lanes and represented less than 5 % of the signal intensity of the 2.9 kb band by phosphorimage analysis. This demonstrates the effectiveness of selection in suppressing the accumulation of edited cp genomes following spontaneous recombination between iDRs in the T0 plants containing the intermediate cp genome.
Accumulation of rbcL-gusA transcripts
Translational coupling between rbcL and gusA
Protein blot analyses with a GUS-specific antibody showed a prominent 68 kDa GUS band in GUS+ transplastomic plants (Fig. 8a lane 3) expressing gusA under the control of chloroplast rrn promoter and the bacteriophage T7 gene 10 ribosome binding site . A GUS band was not detected in gel-fractionated total leaf protein from intermediate iDR plants on protein blots (Fig. 8a, lanes 5–12) or the ΔrbcL and WT negative controls (Fig. 8a, lanes 1 and 4). In total leaf protein from edited plants, the GUS protein was detected as the major band on protein blots (Fig. 8b, lanes 3–8). GUS accumulated to 5 % of total leaf protein in the GUS+ transplastomic plants. Dilutions of leaf protein from these plants showed that GUS was present at ~0.5 % of total leaf protein in plants with edited cp genomes (Fig. 8c). Co-migration of the GUS protein band in the control (Fig. 8c, lanes 2–5) and edited lanes (Fig. 8c, lanes 7 and 9) was consistent with translation initiation at the predicted ATG start codon (Fig. 2). GUS expression mediated by ribosomal frame shifting  was ruled out by the lack of detection of a 120 kDa Rubisco LS-GUS fusion protein. To address low GUS expression in the iDR intermediate plants, a more sensitive β-glucuronidase fluorescence assay was performed. The assay showed a ~50-fold increase in GUS activity in plants with edited cp genomes relative to iDR intermediate plants (Fig. 8d), which equates to GUS levels of ~0.01 % of total leaf protein.
A two-step genome engineering scheme provided a precise and efficient method for editing the cp genome in angiosperms. The challenge of editing multi-copy organelle genomes was addressed by including a selection step to replace resident WT cp genomes with transient intermediate cp genomes. Spontaneous resolution of the iDRs in the intermediate gave rise to edited cp genomes which accumulated after release of antibiotic selection. The procedure allows the seamless insertion of point mutations and foreign genes into cp genomes. Here we deleted a single nucleotide from the rbcL gene which replaced the five C-terminal amino acids of Rubisco LS with 16 unrelated residues. This reduced Rubisco LS accumulation by ~30-fold relative to the WT polypeptide. The editing procedure provided a recombination switch to examine conditions required to express an overlapping gusA gene within the same transplastomic line. GUS accumulated to ~0.5 % of total leaf protein provided the upstream overlapping rbcL translation unit was complete.
The overall efficiency of our cp genome editing method was dependent on integration of the iDR intermediate into the cp genome, followed by resolution to the final edited genome triggered by internal recombination events between the iDRs. Approximately half of the transplastomic lines isolated after transformation incorporated the iDR with the point mutation. Maintenance of the iDR in transplastomic plants showed that copy correction back to the WT sequence does not take place at a frequency that prevents the isolation of edited cp genomes. The conversion of the iDR intermediate to the final edited cp genome was mediated by native chloroplast DNA recombination enzymes. The recombination event excised an unstable DNA circle containing aadA, which was lost, making the process unidirectional. The procedure is efficient and does not require the use of negative selection [46, 47] to promote marker excision. Following resolution of the iDR intermediate, over 80 % of the resulting marker-free plants contained the edited cp genome. Combining both steps gave an overall success rate of 40 % desirable lines isolated per total number of transplastomic lines screened. This compares favourably with nuclear genome editing where efficiencies above 0.5 % were considered successful in human cell lines . The use of chloroplast deletion mutants that lack the editing target, in this case the rbcL gene [42, 48], increase the efficiency by two-fold by eliminating undesirable integration events.
The C-terminal mutation studied here reduced Rubisco LS accumulation by ~30-fold and may have affected biogenesis of the holoenzyme, which follows a complex pathway involving chaperones . By comparison, addition of a C-terminal His-tag had little impact on Rubisco accumulation . Reduction in Rubisco accumulation was associated with a light green phenotype, which allowed the recombination process to be monitored by the appearance of pale sectors in leaves (Fig. 5a). Whilst we used the rbcL gene, which is a focus for improvement [15, 16], to illustrate the method, the procedure is applicable to a wide selection of chloroplast genes. Our results show that recombination based editing enables deleterious mutations that reduce plant fitness to be introduced into chloroplast genes. This suggests it should be possible to introduce a wide variety of point mutations into chloroplast genes by our genome editing method. Loss of function mutations would be restricted to non-essential chloroplast genes, whose dysfunction can be rescued by growing plants on sucrose medium [14, 51]. Homologous recombination is the predominant pathway of gene integration in all species in which chloroplast transformation has been reported [12, 14]. This indicates that the two-step editing procedure described here will be applicable to cp genomes in a broad range of plant species. Moreover, because the method works on WT cells it provides a route for editing the cp genomes of obligate phototrophic algae amenable to chloroplast transformation .
The dependence of gusA expression on a complete upstream rbcL gene was consistent with translational coupling between the two genes. Translational coupling has been described in bacteria [35, 36, 53], bacteriophages , animal viruses [36, 53, 55] and appears to operate in chloroplasts, although it has only been demonstrated in vitro [37, 38, 56]. Additional file 2: Figure S2 shows the four overlapping gene pairs found in the tobacco cp genome: atpB-atpE, ndhC-ndhK, psbD-psbC and rpl22-rps3 gene . The results from experiments using chloroplast lysates support translational coupling at psbD-psbC , ndhC-ndhK [38, 56] but not atpB-atpE , which was consistent with ribosome profiling  but conflicts with an earlier study ; rpl22-rps3 remains untested. Analysis of bacterial genes found limited conservation of the sequences required for translational coupling . The overlap tested here is a synthetic sequence not found in chloroplasts. Only weak similarities between the overlapping sequences present in rbcL-gusA (Fig. 2) and the four pairs of native chloroplast genes (Additional file 2: Figure S2) were found. Shared features between rbcL-gusA and ndhC-ndhK include: termination of the upstream coding sequence in reading frame one by a TAG codon, and the presence of a GTC valine codon following the ATG start codon of the downstream ORF in reading frame 3. However, the rbcL-gusA overlap is six nucleotides longer than the ten nucleotide overlap between ndhC and ndhK (Additional file 2: Figure S2) but is the same length as the overlap found in rpl22-rps3.
In bacteria, a number of mechanisms influence translational coupling including the rate at which terminating ribosomes re-initiate translation at the upstream AUG and the influence of mRNA structure on translation [35, 36, 60, 61]. A change in RNA structure could explain the results observed here. In the uncoupled state the gusA start codon is sequestered by local base pairing in a folded structure (Fig. 2). Following rbcL translation, this folded RNA structure would be unwound allowing ribosomes to bind the region containing the gusA start codon and initiate translation. Absence of secondary structure appears to be a sufficient condition for recognition of start codons and initiation of translation in prokaryotic systems . Other explanations could involve initiation of gusA translation at alternative start sites. However, no in-frame AUG start codons were found in the region upstream of gusA, which was preceded by a UAA stop codon located 48 nucleotides upstream of the gusA initiation codon. The first in-frame AUG codon within the gusA coding region would give rise to a shorter polypeptide of 56 kDa, which was not detected. The possibility that gusA was translated at similar rates in marker-free edited T2 plants and intermediate T0 plants but that the resulting GUS protein was only stable in T2 plants appears unlikely given the many reports of stable GUS expression in chloroplasts [63, 64]. Further insights into the detailed mechanism of translational coupling will require an analysis of gusA translational activity, through methods such as ribosome profiling , radiolabelling of translation products  and analysis of mRNA bound to polysomes .
To-date multiple proteins have been expressed in chloroplasts from constructs containing non-overlapping genes [67, 68]. Translational coupling provides a tightly controlled mechanism to regulate the stoichiometry of proteins expressed from overlapping genes . Successful expression of an overlapping gusA transgene in chloroplasts provides a new approach for expressing multiple proteins from polycistronic transcripts in chloroplasts and is applicable to expressing multi-subunit complexes, such as carboxysomes [17, 69] and novel metabolic pathways , in chloroplasts.
An important set of genes is located in chloroplasts including those essential for photosynthesis such as rbcL. These genes are key targets for improving crop productivity to address global food security in the era of climate change but are beyond the reach of current nuclear genome editing technologies. Here we have described an efficient and versatile method to edit angiosperm chloroplast genomes. It is based on the native homologous recombination pathway acting on transient imperfect direct DNA repeats. The method unlocks the potential of organelle transformation to produce a new class of biotech crops, which differ from their parental cultivars by single base mutations in the chloroplast. The method was used to show that the C-terminal residues of Rubisco LS are important for its accumulation. Using the bacterial gusA gene we have shown, for the first time that a foreign protein can be expressed from overlapping chloroplast genes in planta. Sequestration of the initiation codon of the downstream gusA gene in secondary structure predicted by RNA fold  provided a mechanism for explaining the observed translational coupling between gusA and the upstream rbcL gene. The overlapping sequence used was entirely synthetic indicating that translational coupling is not restricted to native sequences found in chloroplasts. Translational coupling and overlapping genes provide a new approach for co-ordinating the expression of foreign proteins in chloroplasts.
Recombinant DNA procedures
Standard procedures for manipulation of plasmids and transformation of Escherichia coli Solo Pack Gold (Agilent technologies, Stockport, UK) were used to construct pLSm^GUS. The 618 bp rbcL DR sequence was amplified as a 0.64 kb product with primers 410-F (5′GGGGGGATTCACCGCAAATA) and 418-R (5′CCATGGCACGACCTTCAATTCCAAGCTTATCCAAAACGTCCACTGCT) using pATB27-link template  and inserted into pGEM-T easy (Promega, Madison, USA). A deletion of a C (under-lined) in the 418-R primer binding region in a PCR product cloned into pGEM-T created the frameshift mutation. The 0.66 kb insert with the rbcL iDR was released with NotI and NcoI from pGEM-T easy and ligated to the 5′ end of a plasmid containing gusA linked to the 3′ UTR of Chlamydomonas reinhardtii rbcL. The resulting 2.9 kb rbcL iDR repeat-gusA-3′UTR sequence was excised with NotI and used to replace the TGFβ3 expression cassette in p201  giving rise to pLSm˄GUS. Following chloroplast transformation, the 4.2 kb foreign sequence containing aadA and gusA genes was integrated after base 59,328 of the 155,943 nucleotide N. tabacum cp genome (Accession Z00044.2).
Isolation and propagation of chloroplast transformants
Nicotiana tabacum cv. Wisconsin 38 was used for all experiments. WT seeds were obtained from Mr. Thurston Heaton (Firs Experimental Gardens, Manchester, UK) and the ΔrbcL mutant derived from WT plants as described in Kode et al., 1986 . Chloroplast transformation experiments on WT plants were carried out as previously described  using three cycles of regeneration of resistant shoots on medium containing spectinomycin (500 mg/L) and streptomycin (500 mg/L). Only one cycle of regeneration on both antibiotics was required when using leaves from the Nicotiana tabacum cv. Wisconsin 38 ΔrbcL mutant . Plants were grown in a 12 h day at 25 °C with light intensities of 130–200 μE m−2 s−1 at 25 °C. For low light conditions, plants were grown in 30 μE m−2 s−1 light at 25 °C. Marker-free seedlings identified by bleaching on 100 mg/L spectinomycin MS medium were transferred promptly to antibiotic free MS medium to recover.
PCR amplification and sequencing
Total leaf DNA was used as template with primers EXTrbcLOutDR-F (5′-CCGAAGCACTTTATAAAGCACAGGCTGA) and EXTrbcLOutDR-R (5′- AATCCATAACCCCAATTGCTACGG), to amplify a 4.6 kb PCR product from edited lines and a 2.3 kb PCR product from DR intermediate lines (see Fig. 3). Gel purified PCR products were sequenced using primer INTrbcLmut-F (5′-TGTAAAAGCTCGTAATGAAGGACGTGA the BigDye® Terminator 3.1 Cycle Sequencing Kit (Applied Biosystems) and fractionating ladders on a 3730 Genetic Analyser (Applied Biosystems) in the DNA Sequencing Facility at The University of Manchester. Primers  CGTCATCGAGCGCCATCTCGAA (aadA-F) and TGGCTCGAAGATACCTGCAAGAAT (aadA-R), GCGTTACAAGAAAGCCGGGCAAT (gusA-F) and TTGGCCACCACCTGCCAGTCAA (gusA-R), GTATCTCACCGGCGGATTTA (petB-F) and CACTGCCCAATAACCGACTTT (petB-R) were used to detect aadA, gusA and petB genes in total DNA from plants by PCR using Biomix Red (Bioline, London) with conditions of 95 °C for 60 s followed by 26 cycles of: 94 °C, 30 s; 58 °C, 30 s, 72 °C 45 s.
Nucleic acid analyses
Total leaf DNA and RNA extractions and blot analyses were carried out as previously described  and digested with restriction enzymes according to the supplier (New England Biolabs). Hybridization probes were gel purified PCR products using the following plasmid templates and primers: 1.4 kb rbcL probe, TOBrbcL-F (5′- ATGTCACCACAAACAGAGACTA) and TOBrbcL-R (5′- TTACTTATCCAAAACGTCCACT) with pATB27-link ; a 0.6 kb aadA probe, ELLE-aadA-F (5′- GAAGCGGTTATCGCCGAAGTATCGAC) and ELLE-aadA-R (5′-GATTTTGCCGGTTACTGCGCTGTA) with pUC atpX aadA ; a 1.8 kb gusA probe, GUSAprobeF (5′-TCCGTCCTGTAGAAACCCCAACCC) and GUSAprobeR (5′-TTCATTGTTTGCCTCCCTGCTGCG) with pJD330 . Following hybridization with [α32P]-dCTP labelled DNA probes, band intensities were quantified by phosphorimage analysis (FLA-3000 Image Analyzer, Fuji). RNA fold was used to predict secondary structures using the default parameters .
Total leaf protein was fractioned by SDS-PAGE, transferred to Hybond-ECL nitrocellulose membranes and incubated with monoclonal anti-Rubisco LS , anti-α tubulin  and polyclonal anti-GUS (rabbit IgG, from Molecular Probes) antibodies as described [21, 70]. Bands were visualised by using secondary antibodies conjugated to alkaline phosphatase and staining with 5-bromo-4-chloro-3-indolyl phosphate/nitro blue tetrazolium (BCIP/NBT) (Sigma-Aldrich, Poole, UK). GUS enzyme activities  were quantified with 4-methylumbelliferyl-β-D-glucuronide (Sigma-Aldrich) using a Synergy HT Multi-Mode Microplate Reader (BioTek Instruments). 5-bromo-4-chloro-3-indolyl β-D-glucuronide was used for histochemical staining of GUS activities in leaves.
cp genome, chloroplast genome; DR, direct repeat; GUS, β-Glucuronidase; iDR, imperfect direct repeat; LS, large subunit; Rubisco, ribulose bisphosphate carboxylase/oxygenase; SM, selectable marker; ΔrbcL, rbcL deletion mutant
We thank EA Mudd and anonymous reviewers for their critical and constructive comments on the manuscript, and the DNA sequencing facility for support.
Supported in part by the Biotechnology and Biological Sciences Research Council (BB/I011552/1) and University of Manchester (investment in success award) to AD and Biotechnology and Biological Sciences Research Council PhD studentships to EMA and MFG. The funding bodies had no roles in the design of the study and collection, analysis, and interpretation of data, and in writing the manuscript.
Availability of data and materials
Data supporting the findings are to be found in the manuscript and Supplementary Figures S1 and S2.
EMA, MFG and AD conceived and designed the experiments. MFG constructed the vector. EMA isolated and performed all experiments on the transplastomic plants. EMA and AD analyzed the data and wrote the paper. All authors read and approved the final manuscript.
The authors declare that they have no competing interests.
Consent to publish
Ethics (and consent to participate)
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Doudna JA, Charpentier E. The new frontier of genome engineering with CRISPR-Cas9. Science. 2014;346:1077.View ArticleGoogle Scholar
- Kim H, Kim JS. A guide to genome engineering with programmable nucleases. Nat Rev Genet. 2014;15:321–34.View ArticlePubMedGoogle Scholar
- Liu W, Yuan JS, Stewart Jr CN. Advanced genetic tools for plant biotechnology. Nat Rev Genet. 2013;14:781–93.View ArticlePubMedGoogle Scholar
- Fichtner F, Castellanos RU, Uelker B. Precision genetic modifications: a new era in molecular biology and crop improvement. Planta. 2014;239:921–39.View ArticlePubMedGoogle Scholar
- Quetier F. The CRISPR-Cas9 technology: closer to the ultimate toolkit for targeted genome editing. Plant Sci. 2016;242:65–76.View ArticlePubMedGoogle Scholar
- Yoder JI, Goldsbrough AP. Transformation systems for generating marker-free transgenic plants. Bio-Technology. 1994;12:263–7.View ArticleGoogle Scholar
- Jones HD. Regulatory uncertainty over genome editing. Nat Plants. 2014;1:14011.View ArticleGoogle Scholar
- Bock R, Knoop V, editors. Genomics of chloroplasts and mitochondria, Adv. Photosyn Resp, vol. 35. Dordrecht: Springer Netherlands; Dordrecht; 2012. p. 1–458.View ArticleGoogle Scholar
- Kode V, Mudd EA, Iamtham S, Day A. The tobacco plastid accD gene is essential and is required for leaf development. Plant J. 2005;44:237–44.View ArticlePubMedGoogle Scholar
- Ort DR, Merchant SS, Alric J, Barkan A, Blankenship RE, Bock R, Croce R, Hanson MR, Hibberd JM, Long SP, et al. Redesigning photosynthesis to sustainably meet global food and bioenergy demand. Proc Natl Acad Sci U S A. 2015;112:8529–36.View ArticlePubMedPubMed CentralGoogle Scholar
- Bacman SR, Williams SL, Pinto M, Peralta S, Moraes CT. Specific elimination of mutant mitochondrial genomes in patient-derived cells by mitoTALENs. Nat Med. 2013;19:1111–3.View ArticlePubMedPubMed CentralGoogle Scholar
- Day A, Goldschmidt-Clermont M. The chloroplast transformation toolbox: selectable markers and marker removal. Plant Biotechnol J. 2011;9:540–53.View ArticlePubMedGoogle Scholar
- Maliga P (Editor). Chloroplast biotechnology: methods and protocols, Meth Mol Biol vol. 1132. New York: Springer; 2014. pp 3–447.Google Scholar
- Bock R. Engineering plastid genomes: methods, tools, and applications in basic research and biotechnology. Ann Rev Plant Biol. 2015;66:211–41.View ArticleGoogle Scholar
- Whitney SM, Houtz RL, Alonso H. Advancing our understanding and capacity to engineer nature’s CO2-sequestering enzyme, Rubisco. Plant Physiol. 2011;155:27–35.View ArticlePubMedGoogle Scholar
- Parry MAJ, Andralojc PJ, Scales JC, Salvucci ME, Carmo-Silva AE, Alonso H, Whitney SM. Rubisco activity and regulation as targets for crop improvement. J Exp Bot. 2013;64:717–30.View ArticlePubMedGoogle Scholar
- Lin MT, Occhialini A, Andralojc PJ, Parry MAJ, Hanson MR. A faster Rubisco with potential to increase photosynthesis in crops. Nature. 2014;513:547–50.View ArticlePubMedPubMed CentralGoogle Scholar
- Whitney SM, Birch R, Kelso C, Beck JL, Kapralov MV. Improving recombinant Rubisco biogenesis, plant photosynthesis and growth by coexpressing its ancillary RAF1 chaperone. Proc Natl Acad Sci U S A. 2015;112:3564–9.View ArticlePubMedPubMed CentralGoogle Scholar
- Le Martret B, Poage M, Shiel K, Nugent GD, Dix PJ. Tobacco chloroplast transformants expressing genes encoding dehydroascorbate reductase, glutathione reductase, and glutathione-S-transferase, exhibit altered anti-oxidant metabolism and improved abiotic stress tolerance. Plant Biotechnol J. 2011;9:661–73.View ArticlePubMedGoogle Scholar
- Maliga P, Bock R. Plastid biotechnology: food, fuel, and medicine for the 21st century. Plant Physiol. 2011;155:1501–10.View ArticlePubMedPubMed CentralGoogle Scholar
- Gisby MF, Mellors P, Madesis P, Ellin M, Laverty H, O’Kane S, Ferguson MWJ, Day A. A synthetic gene increases TGFβ3 accumulation by 75-fold in tobacco chloroplasts enabling rapid purification and folding into a biologically active molecule. Plant Biotechnol J. 2011;9:618–28.View ArticlePubMedGoogle Scholar
- Jin S, Daniell H. The engineered chloroplast genome just got smarter. Trends Plant Sci. 2015;20:622–40.View ArticlePubMedGoogle Scholar
- Day A, Madesis P. DNA replication, recombination, and repair in plastids. In: Bock R, editor. Cell and molecular biology of plastids, Topics Curr Genet, vol. 19. Berlin Heidelberg: Springer; 2007. p. 65–119.View ArticleGoogle Scholar
- Iamtham S, Day A. Removal of antibiotic resistance genes from transgenic tobacco plastids. Nat Biotechnol. 2000;18:1172–6.View ArticlePubMedGoogle Scholar
- Ye GN, Colburn SM, Xu CW, Hajdukiewicz PTJ, Staub JM. Persistence of unselected transgenic DNA during a plastid transformation and segregation approach to herbicide resistance. Plant Physiol. 2003;133:402–10.View ArticlePubMedPubMed CentralGoogle Scholar
- Dufourmantel N, Dubald M, Matringe M, Canard H, Garcon F, Job C, Kay E, Wisniewski JP, Ferullo JM, Pelissier B, et al. Generation and characterization of soybean and marker-free tobacco plastid transformants over-expressing a bacterial 4-hydroxyphenylpyruvate dioxygenase which provides strong herbicide tolerance. Plant Biotechnol J. 2007;5:118–33.View ArticlePubMedGoogle Scholar
- Zoschke R, Liere K, Boerner T. From seedling to mature plant: Arabidopsis plastidial genome copy number, RNA accumulation and transcription are differentially regulated during leaf development. Plant J. 2007;50:710–22.View ArticlePubMedGoogle Scholar
- Khakhlova O, Bock R. Elimination of deleterious mutations in plastid genomes by gene conversion. Plant J. 2006;46:85–94.View ArticlePubMedGoogle Scholar
- Gantz VM, Bier E. The mutagenic chain reaction: a method for converting heterozygous to homozygous mutations. Science. 2015;348:442–4.View ArticlePubMedPubMed CentralGoogle Scholar
- Akbari BOS, Bellen HJ, Bier E, Bullock SL, Burt A, Church GM, Cook KR, Duchek P, Edwards OR, Esvelt KM, et al. Safeguarding gene drive experiments in the laboratory. Science. 2015;349:927–9.View ArticlePubMedPubMed CentralGoogle Scholar
- Yukawa M, Tsudzuki T, Sugiura M. The 2005 version of the chloroplast DNA sequence from tobacco (Nicotiana tabacum). Plant Mol Biol Report. 2005;23:359–65.View ArticleGoogle Scholar
- Zhou F, Karcher D, Bock R. Identification of a plastid intercistronic expression element (IEE) facilitating the expression of stable translatable monocistronic mRNAs from operons. Plant J. 2007;52:961–72.View ArticlePubMedPubMed CentralGoogle Scholar
- Barkan A. Expression of plastid genes: organelle-specific elaborations on a prokaryotic scaffold. Plant Physiol. 2011;155:1520–32.View ArticlePubMedPubMed CentralGoogle Scholar
- Jefferson RA, Kavanagh TA, Bevan MW. GUS fusions beta-glucuronidase as a sensitive and versatile gene fusion marker in higher-plants. EMBO J. 1987;6:3901–7.PubMedPubMed CentralGoogle Scholar
- Oppenheim DS, Yanofsky C. Translation coupling during expression of the tryptophan operon of Escherichia coli. Genetics. 1980;95:785–95.PubMedPubMed CentralGoogle Scholar
- Jackson R, Kaminski A, Pöyry TAA. Coupled termination-reinitiation events in mRNA translation. In: Mathews M, Sonenberg N, Hershey J, editors. Translational control in biology and medicine, vol. 48. New York: Cold Spring Harbor Laboratory Press; 2007. p. 197–223.Google Scholar
- Adachi Y, Kuroda H, Yukawa Y, Sugiura M. Translation of partially overlapping psbD-psbC mRNAs in chloroplasts: the role of 5 ′-processing and translational coupling. Nucleic Acids Res. 2012;40:3152–8.View ArticlePubMedGoogle Scholar
- Yukawa M, Sugiura M. Termination codon-dependent translation of partially overlapping ndhC-ndhK transcripts in chloroplasts. Proc Natl Acad Sci U S A. 2008;105:19550–4.View ArticlePubMedPubMed CentralGoogle Scholar
- Andersson I, Knight S, Schneider G, Lindqvist Y, Lundqvist T, Branden CI, Lorimer GH. Crystal structure of the active site of ribulose bisphosphate carboxylase. Nature. 1989;337:229–34.View ArticleGoogle Scholar
- van Lun M, van der Spoel D, Andersson I. Subunit interface dynamics in hexadecameric rubisco. J Mol Biol. 2011;411:1083–98.View ArticlePubMedGoogle Scholar
- Gruber AR, Lorenz R, Bernhart SH, Neuboeck R, Hofacker IL. The Vienna RNA Websuite. Nucleic Acids Res. 2008;36:W70–4.View ArticlePubMedPubMed CentralGoogle Scholar
- Kode V, Mudd EA, Iamtham S, Day A. Isolation of precise plastid deletion mutants by homology-based excision: a resource for site-directed mutagenesis, multi-gene changes and high-throughput plastid transformation. Plant J. 2006;46:901–9.View ArticlePubMedGoogle Scholar
- Kohl S, Bock R. Transposition of a bacterial insertion sequence in chloroplasts. Plant J. 2009;58:423–36.View ArticlePubMedGoogle Scholar
- Muhlbauer SK, Eichacker LA. The stromal protein large subunit of ribulose-1,5-bisphosphate carboxylase is translated by membrane-bound ribosomes. Eur J Biochem. 1999;261:784–8.View ArticlePubMedGoogle Scholar
- Yamori W, Evans JR, Von Caemmerer S. Effects of growth and measurement light intensities on temperature dependence of CO2 assimilation rate in tobacco leaves. Plant Cell Environ. 2010;33:332–43.View ArticlePubMedGoogle Scholar
- Serino G, Maliga P. A negative selection scheme based on the expression of cytosine deaminase in plastids. Plant J. 1997;12:697–701.View ArticlePubMedGoogle Scholar
- Gisby MF, Mudd EA, Day A. Growth of transplastomic cells expressing D-amino acid oxidase in chloroplasts Is tolerant to D-alanine and inhibited by D-valine. Plant Physiol. 2012;160:2219–26.View ArticlePubMedPubMed CentralGoogle Scholar
- Whitney SM, Sharwood RE. Construction of a tobacco master line to improve Rubisco engineering in chloroplasts. J Exp Bot. 2008;59:1909–21.View ArticlePubMedGoogle Scholar
- Hauser T, Popilka L, Hartl FU, Hayer-Hartl M. Role of auxiliary proteins in Rubisco biogenesis and function. Nat Plants. 2015;1:1–11.Google Scholar
- Rumeau D, Becuwe-Linka N, Beyly A, Carrier P, Cuine S, Genty B, Medgyesy P, Horvath E, Peltier G. Increased zinc content in transplastomic tobacco plants expressing a polyhistidine-tagged Rubisco large subunit. Plant Biotechnol J. 2004;2:389–99.View ArticlePubMedGoogle Scholar
- Day A. Reverse genetics in flowering plant plastids. In: Bock R, Knoop V, editors. Genomics of chloroplasts and mitochondria. Adv. Photosyn. Resp. Netherlands: Springer; 2012. p. 415–41.View ArticleGoogle Scholar
- Georgianna DR, Hannon MJ, Marcuschi M, Wu S, Botsch K, Lewis AJ, Hyun J, Mendez M, Mayfield SP. Production of recombinant enzymes in the marine alga Dunaliella tertiolecta. Algal Res. 2013;2:2–9.View ArticleGoogle Scholar
- Kozak M. Regulation of translation via mRNA structure in prokaryotes and eukaryotes. Gene. 2005;361:13–37.View ArticlePubMedGoogle Scholar
- Ivey-Hoyle M, Steege DA. Translation of phage f1 gene VII occurs from an inherently defective initiation site made functional by coupling. J Mol Biol. 1989;208:233–44.View ArticlePubMedGoogle Scholar
- Powell ML, Brown TDK, Brierley I. Translational termination re-initiation in viral systems. Biochem Soc Trans. 2008;36:717–22.View ArticlePubMedGoogle Scholar
- Yukawa M, Sugiura M. Additional pathway to translate the downstream ndhK cistron in partially overlapping ndhC-ndhK mRNAs in chloroplasts. Proc Natl Acad Sci U S A. 2013;110:5701–6.View ArticlePubMedPubMed CentralGoogle Scholar
- Suzuki H, Kuroda H, Yukawa Y, Sugiura M. The downstream atpE cistron is efficiently translated via its own cis-element in partially overlapping atpB-atpE dicistronic mRNAs in chloroplasts. Nucleic Acids Res. 2011;39:9405–12.View ArticlePubMedPubMed CentralGoogle Scholar
- Zoschke R, Watkins KP, Barkan A. A rapid ribosome profiling method elucidates chloroplast ribosome behavior in vivo. Plant Cell. 2013;25:2265–75.View ArticlePubMedPubMed CentralGoogle Scholar
- Gatenby AA, Rothstein SJ, Nomura M. Translation coupling of the maize chloroplast atpB and atpE genes. Proc Natl Acad Sci U S A. 1989;86:4066–70.View ArticlePubMedPubMed CentralGoogle Scholar
- Tian T, Salis HM. A predictive biophysical model of translational coupling to coordinate and control protein expression in bacterial operons. Nucleic Acids Res. 2015;43:7137–51.View ArticlePubMedPubMed CentralGoogle Scholar
- Spanjaard RA, van Duin J. Translational reinitiation in the presence and absence of a Shine and Dalgarno sequence. Nucleic Acids Res. 1989;17:5501–8.View ArticlePubMedPubMed CentralGoogle Scholar
- Scharff LB, Childs L, Walther D, Bock R. Local absence of secondary structure permits translation of mRNAs that lack ribosome-binding sites. PLoS Genet. 2011;7:e1002155. doi:10.1371/journal.pgen.1002155.View ArticlePubMedPubMed CentralGoogle Scholar
- Eibl C, Zou ZR, Beck A, Kim M, Mullet J, Koop HU. In vivo analysis of plastid psbA, rbcL and rpl32 UTR elements by chloroplast transformation: tobacco plastid gene expression is controlled by modulation of transcript levels and translation efficiency. Plant J. 1999;19(3):333–45.View ArticlePubMedGoogle Scholar
- Leelavathi S, Reddy VS. Chloroplast expression of His-tagged GUS-fusions: a general strategy to overproduce and purify foreign proteins using transplastomic plants as bioreactors. Mol Breeding. 2003;11:49–58.View ArticleGoogle Scholar
- Matsuoka M, Ohashi Y. Induction of pathogenesis-related proteins in tobacco leaves. Plant Physiol. 1986;80:505–10.View ArticlePubMedPubMed CentralGoogle Scholar
- Barkan A. Nuclear mutants of maize with defects in chloroplast polysome assembly have altered chloroplast RNA metabolism. Plant Cell. 1993;5:389–402.View ArticlePubMedPubMed CentralGoogle Scholar
- De Cosa B, Moar W, Lee SB, Miller M, Daniell H. Overexpression of the Bt cry2Aa2 operon in chloroplasts leads to formation of insecticidal crystals. Nat Biotechnol. 2001;19:71–4.View ArticlePubMedPubMed CentralGoogle Scholar
- Lu Y, Rijzaani H, Karcher D, Ruf S, Bock R. Efficient metabolic pathway engineering in transgenic tobacco and tomato plastids with synthetic multigene operons. Proc Natl Acad Sci U S A. 2013;110:E623–32.View ArticlePubMedPubMed CentralGoogle Scholar
- Price GD, Pengelly JJL, Forster B, Du J, Whitney SM, von Caemmerer S, Badger MR, Howitt SM, Evans JR. The cyanobacterial CCM as a source of genes for improving photosynthetic CO2 fixation in crop species. J Exp Bot. 2013;64:753–68.View ArticlePubMedGoogle Scholar
- Madesis P, Osathanunkul M, Georgopoulou U, Gisby MF, Mudd EA, Nianiou I, Tsitoura P, Mavromara P, Tsaftaris A, Day A. A hepatitis C virus core polypeptide expressed in chloroplasts detects anti-core antibodies in infected human sera. J Biotechnol. 2010;145:377–86.View ArticlePubMedGoogle Scholar
- Goldschmidt-Clermont M. Transgenic expression of aminoglycoside adenine transferase in the chloroplast: a selectable marker for site-directed transformation in Chlamydomonas. Nucleic Acids Res. 1991;19:4083–9.View ArticlePubMedPubMed CentralGoogle Scholar
- Gallie DR, Lucas WJ, Walbot V. Visualizing messenger RNA expression in plant protoplasts: factors influencing efficient messenger RNA uptake and translation. Plant Cell. 1989;1:301–11.View ArticlePubMedPubMed CentralGoogle Scholar
- Kettleborough CA, Parry MAJ, Keys AJ, Phillips AL. Chimaeras of the Rubisco large subunit from wheat and Anacystis do not assemble into active enzyme in E. coli. J Exp Bot. 1990;41:1287–92.View ArticleGoogle Scholar
- Woods A, Sherwin T, Sasse R, Macrae TH, Baines AJ, Gull K. Definition of individual components within the cytoskeleton of Trypanosoma brucei by a library of monoclonal antibodies. J Cell Sci. 1989;93:491–500.PubMedGoogle Scholar