NEWS AND VIEWS

Mitochondrial genome editing gets precise

A bacterial toxin has been found that allows DNA in a cellular organelle called the mitochondrion to be precisely altered. This development could help to combat diseases caused by mutations in mitochondrial DNA.
Magomet Aushev is in the Wellcome Centre for Mitochondrial Research, Biosciences Institute, Centre for Life, Newcastle upon Tyne NE1 4EP, UK.
Contact

Search for this author in:

Mary Herbert is in the Wellcome Centre for Mitochondrial Research, Biosciences Institute, Centre for Life, Newcastle upon Tyne NE1 4EP, UK.
Contact

Search for this author in:

The DNA in a cellular organelle called the mitochondrion encodes just 13 proteins, all of which are involved in generating the cell’s energy supply. Mutations in mitochondrial DNA (mtDNA) can cause a range of incurable, life-limiting metabolic diseases in humans1. The development of tools for editing mtDNA has therefore been a long-sought goal in mitochondrial genetics. Writing in Nature, Mok et al.2 report a molecular tool that for the first time enables precise editing of mtDNA. Key to this achievement was the discovery of a toxin secreted by bacteria to kill neighbouring bacteria.

The bacterial toxin discovered by Mok et al. is a cytidine deaminase enzyme called DddA, which catalyses the conversion of the nucleotide base cytosine (C) to another base, uracil (U). A remarkable feature of DddA is that it targets double-stranded DNA, whereas all previously identified3 cytidine deaminases target single-stranded DNA. Crucially, although conventional genome-editing approaches involve nuclease enzymes that act as molecular scissors to cut DNA on both strands, DddA converts C to U without inducing double-strand DNA breaks. This makes it particularly well suited to editing the mitochondrial genome, which lacks efficient mechanisms for repairing double-strand DNA breaks4.

The researchers had to overcome several challenges to repurpose DddA for mitochondrial genome editing. Chief among these is the fact that cytidine deaminase is toxic to mammalian cells. Mok et al. split the toxin domain of DddA into two inactive parts called split-DddAtox halves. They fused these halves to TALE proteins, which can be engineered to bind to specified DNA sequences. Binding of the two TALEs to mtDNA brings together, and so activates, the split-DddAtox halves.

To reach mtDNA in the mitochondrial matrix, TALE–split-DddAtox must cross two mitochondrial membranes. Mok and colleagues therefore tagged the construct with an amino-acid sequence that acts as a mitochondrial-targeting signal. The ability to exploit existing protein-import machinery5 gives this approach a major advantage over RNA-guided systems for genome editing such as CRISPR–Cas9. CRISPR methods do not work efficiently on mtDNA, possibly because the cell has no mechanisms for importing RNA into mitochondria6.

Another challenge arises from the fact that cytidine deaminase converts C to U, rather than to the DNA-specific base thymine (T). Although U has the same base-pairing properties as does T, it belongs in RNA. The base is normally cut from DNA with the help of an enzyme called uracil-DNA glycosylase and replaced with C (ref. 7)7.

Mok et al. therefore fused the TALE–split-DddAtox halves with a uracil glycosylase inhibitor (UGI). This protects U from the glycosylase until the next round of DNA replication or repair occurs, at which point the guanine (G) base from the complementary strand — which was paired with C before editing — is replaced by adenine (A), the base that pairs with T. Incorporation of the UGI increased the efficiency of cytosine base editing about eightfold.

The final construct, dubbed a DddA-derived cytosine base editor (DdCBE), therefore consists of a mitochondrial-targeting signal, a TALE protein, a split-DddAtox half and a UGI (Fig. 1). Mok et al. demonstrated that the construct is efficiently imported into mitochondria in human cells and can modify a selection of mitochondrial genes. The edit, from a C–G base pair to T–A, occurred about 5–50% of the time. The efficiency of editing was influenced by various factors: the spacing between the two DdCBE subunits; TALE design; orientation of the split-DddAtox halves; and the position of the target cytosine relative to the TALE bindings sites.

Figure 1

A major consideration for all genome-editing tools is whether they modify DNA at unintended sites. Mok and colleagues compared treated and untreated cells, and found no off-target effects in the nuclear genome. Off-target activity in mtDNA was low, except in the case of one gene, in which off-target edits were linked to the TALE design.

Next, Mok et al. examined the therapeutic potential of DdCBE. The authors reported that cytosine base editing has the potential to correct 49% of known harmful mtDNA mutations. However, in its current form, DdCBE can efficiently edit only C bases that are preceded in the genome by a T, narrowing its range.

The reliance of DdCBE on DNA replication to implement the C–G to T–A conversion implies a theoretical maximum editing efficiency of 50%. To explain, the two newly replicated mtDNAs each receive a parental DNA strand, one of which will be unedited, containing G, which becomes paired with a C. However, Mok et al. find that the activity of DdCBE persists over several days, potentially offering the opportunity for further editing during subsequent replication events. Whether off-target effects increase during prolonged exposure to DdCBE will be a key consideration for the future.

These caveats mean that DdCBE might cause a reduction in — rather than complete elimination of — mtDNA mutations. But given that the severity of the symptoms of mtDNA diseases increases with mutation load8, the ability to reduce the mutation level in itself holds therapeutic promise.

Mitochondrion-targeted nucleases have previously been used to eliminate specific mtDNA mutations in mice9,10. This is possible because the double-strand breaks they create lead to mtDNA degradation. Cells contain many copies of their mtDNA, and only the copies that carry the harmful mutation are degraded. But there is a risk that, in cases of high mutation load, elimination of mutated mtDNA could reduce the mtDNA copy number to harmfully low levels. And the nuclease approach could not be used if all copies of mtDNA carry the same mutation. By contrast, base editing could reduce the fraction of mtDNA that carries a mutation without reducing the copy number. It might therefore be the preferred (or the only) option when the mutation load is high.

Does DdCBE have the potential to prevent the transmission of mtDNA disease? MtDNA is typically inherited only from mothers, and current mitochondrial-replacement pro-cedures reduce the transmission of mtDNA mutations by transplanting the nuclear genome from the egg of a woman who carries the mutated mtDNA into an unaffected donor egg11. Base editing to reduce the mutation load in eggs or early embryos could theoretically be an alternative approach. However, mtDNA replication is thought not to occur during the first five to six days of human development12, and so success might hinge on prolonged protection of U.

Mok and colleagues’ work is a key advance towards the development of gene therapies for mtDNA diseases. In addition, by using the tool to experimentally alter the mitochondrial genome, we could gain a better understanding of the relevance of mtDNA mutations in complex diseases, cancer and age-related cellular dysfunction. The study is also likely to inspire further developments in protein engineering and evolution that increase the range and efficiency of DdCBE, and to intensify the search for other promising candidate base editors.

Nature 583, 521-522 (2020)

doi: 10.1038/d41586-020-01974-6

References

  1. 1.

    Russell, O. M., Gorman, G. S., Lightowlers, R. N. & Turnbull, D. M. Cell 181, 168–188 (2020).

  2. 2.

    Mok, B. Y. et al. Nature 583, 631–637 (2020).

  3. 3.

    Salter, J. D. & Smith, H. C. Trends Biochem. Sci. 43, 606–622 (2018).

  4. 4.

    Moretton, A. et al. PLoS ONE 12, e0176795 (2017).

  5. 5.

    Schmidt, O., Pfanner, N. & Meisinger, C. Nature Rev. Mol. Cell Biol. 11, 655–667 (2010).

  6. 6.

    Gammage, P. A., Moraes, C. T. & Minczuk, M. Trends Genet. 34, 101–110 (2018).

  7. 7.

    Kunz, C., Saito, Y. & Schär, P. Cell. Mol. Life Sci. 66, 1021–1038 (2009).

  8. 8.

    Hellebrekers, D. M. E. I. et al. Hum. Reprod. Update 18, 341–349 (2012).

  9. 9.

    Bacman, S. R. et al. Nature Med. 24, 1696–1700 (2018).

  10. 10.

    Gammage, P. A. et al. Nature Med. 24, 1691–1695 (2018).

  11. 11.

    Greenfield, A. et al. Nature Biotechnol. 35, 1059–1068 (2017).

  12. 12.

    St. John, J. C., Facucho-Oliveira, J., Jiang, Y., Kelly, R. & Salah, R. Hum. Reprod. Update 16, 488–509 (2010).

Download references

Nature Briefing

An essential round-up of science news, opinion and analysis, delivered to your inbox every weekday.