Adeno-associated virus (AAV) vectors are the leading platform for gene delivery for the treatment of a variety of human diseases. Recent advances in developing clinically desirable AAV capsids, optimizing genome designs and harnessing revolutionary biotechnologies have contributed substantially to the growth of the gene therapy field. Preclinical and clinical successes in AAV-mediated gene replacement, gene silencing and gene editing have helped AAV gain popularity as the ideal therapeutic vector, with two AAV-based therapeutics gaining regulatory approval in Europe or the United States. Continued study of AAV biology and increased understanding of the associated therapeutic challenges and limitations will build the foundation for future clinical success.
Adeno-associated virus (AAV) was first discovered from laboratory adenovirus (AdV) preparations in the mid-1960s1,2 and found in human tissues soon after3. Driven by pure scientific curiosity and without realizing its tremendous potential as a human gene therapy platform, a few research groups embarked on a journey to understand basic AAV biology4,5,6. During the first 15–20 years of AAV research, several important aspects of AAV were characterized, including its genome configuration and composition7,8,9,10, DNA replication and transcription11,12,13, infectious latency14,15,16,17,18,19 and virion assembly20. These achievements collectively fostered the successful cloning of the wild-type AAV2 sequence into plasmids, which enabled genetic studies21,22 and sequencing of the entire AAV2 genome23. These early investigations provided fundamental knowledge that led to the use of AAV as a gene delivery vehicle (Fig. 1). Since the advent of AAV vectors, their use as a biotherapy has also advanced our understanding of virus–host interactions that govern the transduction pathway of AAV (Fig. 2).
Today, recombinant AAVs (rAAVs) are the leading platform for in vivo delivery of gene therapies. The first rAAV gene therapy product, alipogene tiparvovec (Glybera), was approved by the European Medicines Agency to treat lipoprotein lipase deficiency in 2012 (ref.24), while the approval of voretigene neparvovec-rzyl (Luxturna), the first rAAV gene therapy product licensed in the United States, followed 5 years later. Although the clinical success of rAAV gene therapy is encouraging, we must acknowledge the limitations and challenges of this gene delivery platform, which include issues with rAAV manufacturing and immunological barriers to delivery25. These challenges are being addressed by a growing field that encompasses multidisciplinary expertise.
In this article, we aim to provide an overview of the use of AAV vectors to deliver therapeutic transgenes. We briefly introduce basic AAV biology and vectorology, describe general vector design principles and summarize current therapeutic strategies and clinical progress. Existing challenges, as well as recent advances that have helped to transition these promising drug platforms to the bedside, are discussed. While other viral and non-viral vectors have also played substantial roles in the advancement of gene and cell therapy, their discussion is beyond the scope of this article, and we refer readers to relevant review articles on these topics26,27,28.
Fundamentals of AAV and vectorology
AAV as a virus
AAV belongs to the genus Dependoparvovirus within the family Parvoviridae. Its life cycle is dependent on the presence of a helper virus, such as AdV, hence its name and taxonomy classification. AAV is found in multiple vertebrate species, including human and non-human primates (NHPs). The current consensus is that AAV does not cause any human diseases. It is composed of an icosahedral protein capsid of ~26 nm in diameter and a single-stranded DNA genome of ~4.7 kb that can either be the plus (sense) or minus (anti-sense) strand29. The capsid comprises three types of subunit, VP1, VP2 and VP3, totalling 60 copies in a ratio of 1:1:10 (VP1:VP2:VP3). The genome is flanked by two T-shaped inverted terminal repeats (ITRs) at the ends that largely serve as the viral origins of replication and the packaging signal. The rep gene encodes four proteins required for viral replication; they are named after their molecular masses: Rep78, Rep68, Rep52 and Rep40. The cap gene encodes the three capsid subunits through alternative splicing and translation from different start codons. In addition, a third gene, which encodes assembly activating protein (AAP), is encoded within the cap coding sequence in a different reading frame and has been shown to promote virion assembly30,31. The AAV genome can integrate into a genomic locus known as AAVS1 in human cells to establish latency16,17,18,19,32,33,34. This phenomenon is in part due to the sequence similarity found within AAVS1 and the ITR and Rep activity. As discussed below, because rAAV is devoid of the rep gene, rAAV genome integration is greatly reduced.
AAV as a vector for in vivo gene delivery
In practical terms, rAAVs are composed of the same capsid sequence and structure as found in wild-type AAVs (wtAAVs). However, rAAVs encapsidate genomes that are devoid of all AAV protein-coding sequences and have therapeutic gene expression cassettes designed in their place. The only sequences of viral origin are the ITRs, which are needed to guide genome replication and packaging during vector production. The complete removal of viral coding sequences maximizes the packaging capacity of rAAVs and contributes to their low immunogenicity and cytotoxicity when delivered in vivo. The ITR-flanked rAAV genome can be cloned into plasmids and can be conveniently manipulated using standard molecular cloning techniques. Because rAAVs optimally accommodate genomes that are under 5.0 kb (ref.35), the payload must be carefully designed to consider not only the therapeutic transgene sequence but also the inclusion of regulatory elements necessary for gene expression (for example, promoter and polyadenylation signal).
It is now increasingly appreciated that host factors impacting the potency of gene delivery come into play as soon as the rAAV is administered to the patient. For example, new findings indicate that different serotypes interact with serum proteins in different ways36. Nonetheless, the effectiveness of rAAV is in large part determined by the molecular interactions between the capsid and target cell surface receptors37,38 and subsequent downstream events following particle internalization39 (Fig. 2). The prevailing serotypes are presumed to recognize distinct cell receptors, such as glycoproteins, and therefore display different tissue-type and cell-type tropism profiles. Combinatorial recognition of co-receptors may also participate in cell surface binding and internalization39. AAVR was identified as an essential AAV receptor for multiple serotypes40,41. Intriguingly, AAVR may play a larger role in facilitating intracellular trafficking of the virus42. The receptor-interacting regions of several serotypes have been determined and collectively provide a roadmap for the rational engineering of capsids with desired properties43. Successful receptor recognition may lead to internalization by endocytosis44,45,46. Intact rAAV particles in endosomes undergo a series of pH-dependent structural changes necessary for transduction47 and traffic through the cytosol via the cytoskeletal network48. After endosomal escape, rAAV enters the nucleus through the nuclear pore complex49,50,51, where it undergoes capsid uncoating to release the genome. It is important to note that intracellular trafficking involves multiple cellular events and may abort at any step, resulting in unsuccessful gene delivery. Therefore, identifying the key cellular host factors and underpinningmechanisms that regulate this process holds great potential for improving rAAV transduction efficiency.
The single-stranded rAAV genome that is released in the nucleus is not immediately ready for gene expression until it is converted to a double-stranded form — a requirement of transcription and a rate-limiting step for transduction52,53 (Fig. 2). Second strand synthesis is initiated from the self-primed ITR at the 3ʹ-end of the genome54,55. Additionally, double-stranded genomes can be achieved by strand annealing, whereby plus-stranded and minus-stranded genomes that are packaged into separate virions anneal by Watson–Crick base pairing once in the nucleus56. An elegant rAAV genome design utilizes a mutated ITR to generate a self-complementary genome configuration, allowing for faster and higher gene expression than a conventional single-stranded AAV genome57,58. However, the packaging capacity is halved. The double-stranded genome then undergoes circularization via intra-molecular or inter-molecular genome recombination at the ITRs59,60. This circularization and concatemerization process stabilizes the rAAV genome as episomal DNA, leading to gene expression that persists in postmitotic cells.
Replication and packaging of rAAV is dependent on host cell factors and elements provided by helper viruses, such as herpes simplex virus (HSV) and AdV. Therefore, cell-free systems for producing rAAV remain elusive given the present technologies. The development of methods to enhance rAAV production has been a continual challenge for human applications. Current platforms for rAAV production and purification are discussed in Box 1.
The engineering of novel AAV capsids to gain new properties and characteristics has been a constant pursuit from the time when rAAVs were shown to exhibit clinical promise more than 20 years ago. Strategies for developing new capsids have evolved with technological advancements. For example, cryogenic electron microscopy (cryo-EM) has provided insights into the effect of structure and function of capsid residues on stability61 and how antibodies recognize and dock onto capsids62. This has accelerated the characterization and validation of new capsids. Capsid development approaches can be divided into three main categories: natural discovery, rational design and directed evolution (Fig. 3). With recent improvements to computational power and bioinformatic prediction methods, a new branch of AAV capsid design has emerged: in silico discovery. The pros and cons of these approaches and some seminal studies that exemplify the basis of these methods are discussed below.
As discussed above, AAV was originally discovered as a cell culture contaminant, as was the most widely characterized and used serotype, AAV2. Notably, the most clinically promising vectorized serotypes have been those that were isolated from natural sources. This notion is best epitomized by AAV9, which was isolated from human liver tissue63. AAV9 is a clade F serotype and demonstrates the capacity to bypass the blood–brain barrier (BBB), making it a leading capsid for the transduction of the central nervous system (CNS) via systemic administration. Livers and spleens are the predominant sites of natural AAV infection in both humans and NHPs, although proviral sequences can be isolated from a range of tissues63,64,65,66,67. For instance, other human-derived clade F capsids that have recently gained attention are those isolated from CD34+ human peripheral blood haematopoietic stem cells, which demonstrate the capacity to confer nuclease-free gene editing68,69.
Epidemiological analyses have shown that 40–80% of the human population are seropositive for antibodies against AAV70, suggesting that human-derived capsids may not be ideal for gene therapy vectors owing to pre-existing AAV capsid immunity that may reduce transduction efficacy. Seroepidemiological and molecular studies indicate that AAV1, AAV2, AAV3, AAV5, AAV6, AAV7, AAV8 and AAV9 are endemic to humans63,71,72,73,74,75. Therefore, isolation of capsids from non-human sources may overcome pre-existing immunity. Capsids isolated from NHPs have thus far shown substantial promise, and NHP-derived AAVrh.8, AAVrh.10 and AAVrh.43 (clade E capsids; AAV8 is also a member) have been shown to transduce a range of tissues. However, the prevalence of anti-AAV8 neutralizing antibodies (NAbs) in the human population ranges from 10% to 40% depending on geographical sampling73. Other clade E capsids may therefore exhibit reactivity despite their promise.
Alternatively, many studies have now focused on the promise of AAV capsids that are isolated from other vertebrate species76,77,78,79,80,81,82,83. Although these capsids have the lowest theoretical chance of eliciting a pre-existing immune response in patients, they may also exhibit lower transduction profiles in humans. Notably, porcine-derived rAAVs were reported to transduce mouse organs with efficiencies contending with gold-standard AAVs84. Most promising of all, porcine AAVs were shown to not be neutralized by pooled human immunoglobulin G (IgG) and have the capacity to transduce the adult mouse brain, suggesting that these vectors can bypass the BBB.
With advances in high-throughput sequencing methodologies, the discovery of natural capsid diversity has become simplified. Long-read sequencing technologies such as single molecule, real-time (SMRT) sequencing allows for the sequencing of full-length proviral genomes without the need for sequence reconstruction85. Because multiple AAV serotypes have been observed in tissue biopsy samples from individual patients, this technology provides the ability to observe variants as a consequence of natural recombination between several AAV genomes86.
Among the first approaches to improve vector capsids was engineering by rational design. Such strategies began with simple grafting of peptide sequences that bind to cell-type-specific receptors87. Introduction of integrin-binding peptide sequences onto the surface of the capsid resulted in the re-targeting of AAV2 to cells resistant to infection88. Other methods employed the fusion of peptide sequences onto the amino terminus of VP2 (ref.89), such as the single-chain variable fragments (scFvs)90 and designed ankyrin repeat proteins (DARPins)91, to confer antibody-like recognition to cell surface markers. Alternatively, it is widely regarded that the 3-fold protrusions play important roles in shaping the tropism profile and immunogenicity of the capsid, therefore making the exposed position of the 3-fold protrusion an ideal position for peptide insertion to augment receptor binding. Such approaches not only can retarget capsids but also have the capacity to deter immunological recognition. For example, the engineered AAV2i8 capsid not only detargets from the liver for increased skeletal and cardiac muscle transduction but also has the added benefit of an altered antigenic profile92. Notably, the first engineered vectorized capsid used in a clinical trial, AAV2.5, was designed rationally93. This capsid, which exhibited improved muscle transduction, was developed by transferring five amino acids from AAV1 onto the AAV2 capsid scaffold.
Although rational modification to capsid structure may improve tropism, it may also negatively impact other characteristics of the capsid, such as its stability. The introduction of codon expansion and click chemistry allows modification of capsids after virion assembly. By taking advantage of the pliability of the 3-fold protrusion, click chemistry amino acid modifications show exemplary ability to alter capsid function without impacting assembly and packaging94,95,96,97.
Another means of improving vector transduction through rational design is to disrupt cellular degradation of capsids. Site-directed mutagenesis of surface-exposed tyrosine residues was shown to increase murine hepatocyte transduction by nearly 30-fold via the inhibition of proteasomal degradation and facilitation of intracellular trafficking98.
Despite the introduction of high-throughput screening methods (discussed below), rational design will always have a place in the engineering of novel vectors. For example, the recently reported AAV2 true-type (AAV-TT) capsid was designed by combining conserved residues identified among natural AAV2 variants from children who were seropositive for AAV2 (ref.99). AAV-TT was found to exhibit increased thermal stability compared with AAV2 and, importantly, to have favourable CNS transduction in mice99. Notably, AAV-TT also lacks the heparan sulfate proteoglycan (HSPG) binding motif, which serves as the binding site for AAV2 and presumably is a result of the adaptive selection of AAV2 in cultured cells. High expression levels of HSPG in the extracellular matrix lead to reduced spread and sequestration of AAV2 in off-target tissues, limiting the therapeutic efficacy of AAV2 when delivered systemically. Although AAV-TT lacks the ability to cross the BBB, it represents a rationally designed capsid that may have usefulness for treatments requiring intraparenchymal vector administration.
Elucidation of the structure–function relationships among several AAV capsids provides important clues for rational engineering. Guided by this structural information, a natural AAV9 capsid variant was isolated from chimpanzee tissues that differs from prototypical AAV9 by four residues, two of which reside at the 3-fold protrusion. When these two residues are mutated on AAV9, the engineered capsid, called AAV9.HR, greatly detargets from peripheral tissues but retains the capacity of AAV9 to cross the BBB following intravascular injection in neonatal mice100. In another study, several capsid antigenic motifs (CAMs) clustered at the 3-fold symmetry axis were identified by analysing the cryo-reconstruction data of AAV1–NAb complexes101. The authors evolved the residues within these motifs and obtained a synthetic capsid named CAM130, which demonstrated reduced NAb recognition compared with the parental AAV1 capsid. Despite the promise of these rationally designed capsids revealed by mouse models, further comparative analyses for these and any newly engineered capsids are required in large animal models before moving to clinical testing.
A major limitation to rational design approaches is related to insufficient knowledge pertaining to AAV cell surface binding, internalization, trafficking, uncoating and gene expression. Therefore, de novo approaches to discovery, namely, directed evolution strategies, are favourable in many instances102,103,104,105,106,107,108. The basis of directed evolution is rooted in the simulation of natural evolution, whereby capsids are under selective pressure to yield genetic variants with specific biological properties and advantageous characteristics (for example, tissue-specific targeting, immunological evasion and transgene expression). Therefore, directed evolution of capsid libraries does not require prior understanding of the molecular mechanisms involved in the selection criteria. For example, iterative rounds of in vitro selection with a library of peptide sequences embedded at the 3-fold protrusion has yielded capsids with remarkable redirected tropisms109,110. Alternatively, error-prone PCR at discrete regions or throughout the entire cap gene is also a viable means of generating capsid libraries for screening103. Many recent studies have also utilized the randomized generation of chimeric capsids (capsid shuffling) from the primary sequences of pre-existing serotypes106,107,108,111. In combination with error-prone PCR, capsid shuffling can achieve a higher diversity of capsid libraries by surveying a wider palette of pre-existing capsids with inherently different tropism profiles112,113. Notably, rAAVs that preferentially target HIV-1-infected H9 T cells have recently been evolved114.
A notable directed evolution method is Cre recombination-based AAV targeted evolution (CREATE)110. This methodology, which also employs the insertion of a randomized peptide fragment into the 3-fold protrusion, relies on Cre recombination to repair an inverted polyadenylation sequence designed into the vector genome. Because Cre recombination requires a double-stranded DNA target, only capsids that can mediate efficient intracellular trafficking and conversion of the single-stranded viral genome to the double-stranded form within the nucleus can be processed by Cre recombinase in Cre-expressing cells. This method led to the identification of AAV-PHP.B and other capsid variants that can cross the BBB to transduce the CNS110,115.
With the advent of next-generation sequencing approaches, directed evolution has become an even more powerful technique for the discovery of novel vector capsids. The ability to screen several thousand barcoded transgenes allows for the iterative enrichment of candidates that can transduce cell or tissue types. The only true limitation for these techniques is that the evolution of capsids needs to be performed in a model that best mimics the intended target tissue. For instance, in vitro-directed evolution of AAV does not simulate crossing blood–organ barriers after vascular administration. Therefore, in vivo screening of capsid libraries is highly preferred. Unfortunately, not all in vivo models are created equal. Preclinical rAAV discovery and validation, on the whole, have been performed in animal models that recapitulate neither AAV tropism in humans nor the vector potency required for therapeutic efficacy. For example, AAV-PHP.B was shown to not outperform AAV9 in the CNS of large animal models116,117,118. These outcomes may be rooted in the model system that was used for its discovery. Because evolving capsids in humans is not feasible, humanized mouse models are the best surrogates for these investigations. For example, using AdV5-mediated viral selection in Fah−/−Rag2−/−Il2rg−/− (FRG) mice that are partially repopulated with primary human hepatocytes can effectively achieve the identification of capsid vectors that are specific to human liver cells102.
In silico bioinformatic approaches
Structural constraints imposed by secondary, tertiary and quaternary interactions within and between monomers add to the layer of complexity when evaluating mutagenesis outcomes within understudied capsid domains. The use of computational tools has greatly improved vector design approaches without the need for complete understanding of AAV capsid biology. For example, in conjunction with high-throughput sequencing, bioinformatic tools can be employed for the design of capsid variant libraries to identify high-variability regions that tolerate manipulation119. Indeed, in silico methods for novel capsid engineering have gained recent attention. For example, by using in silico phylogenetic and statistical modelling of known capsid sequences to infer evolutionary intermediates, ancestral capsid sequences have been predicted120. This work resulted in the discovery of Anc80, which shows promising efficacy in mouse liver, skeletal muscle, retina and cochlea120,121. Similarly, in silico sequence analysis of germline endogenous viral elements (EVEs) among several marsupial species revealed fossilized viral integration events within host DNA122. These EVEs were characterized and reconstructed as novel ancestral capsids with potentially desirable vector properties.
rAAV genome design and engineering
The typical rAAV genome design carries a gene expression cassette, which includes a promoter, a transgene and a transcription termination signal. Together, these components serve the main function of expressing therapeutic levels of gene product once the vector is delivered to the target cell nucleus. Design of the gene expression cassette is tailored to suit the specific requirements of the therapy (for example, transgene expression level, tissue-type and cell-type specificity and packaging size limitations). In addition, DNA-based regulatory elements are being developed to address potential undesired effects such as loss of vector in proliferating cells. This section discusses basic rAAV genome design and engineering. It should be noted that when designing efficacious rAAV vectors, the synergy between the capsid and the genome must also be considered. A combinatorial design approach that marries capsid and vector genome features and characteristics is ultimately needed to develop successful rAAV platforms to treat human disease.
Controlling transgene expression level and specificity
In many cases, rAAV gene therapy platforms utilize a strong and ubiquitous promoter to achieve high transgene expression. Such promoters include the cytomegalovirus (CMV) promoter and the chicken β-actin promoter fused with the CMV enhancer. Other regulatory elements can also enhance gene expression, such as an intron123,124 and the woodchuck hepatitis post-transcriptional regulatory element (WPRE)125,126. Although the WPRE was shown to promote tumorigenesis127, a modified version shows a much safer profile128. For gene expression in human cells, even wild-type human-derived gene sequences are not necessarily optimized to yield robust protein expression. This is in part because a natural sequence may not fully utilize the most preferred codon for an amino acid residue. In addition, elements of the transgene sequence itself, such as GC content, cryptic splice sites, transcription termination signals, motifs that affect RNA stability and nucleic acid secondary structures, can impact on expression. Therefore, codon optimization is widely used in rAAV gene therapy aiming to enhance gene expression129,130,131,132. At the translational level, inclusion of a Kozak sequence can further increase protein expression130. To drive the expression of small RNA molecules such as short hairpin RNAs (shRNAs) and single-guide RNAs (sgRNAs), the human or murine U6 small nuclear RNA promoter and human H1 promoter are commonly used133.
It is important to note that high transgene expression levels are not always preferred. Supra-physiological expression of a protein or RNA molecule may be toxic. This has proved to be a critical consideration for delivering the genes encoding MECP2134,135 and hexosaminidase136 for treating Rett syndrome and GM2 gangliosidosis, respectively. Similarly, shRNA expression that is driven by the strong U6 promoter is associated with toxicity owing to saturation of the endogenous microRNA (miRNA) biogenesis pathway137, which can be ameliorated by using a weaker H1 promoter. Alternatively, new platforms based on the expression of artificial microRNAs (amiRs) by Pol II promoters provide a more versatile solution for RNA interference (RNAi)138,139,140,141,142.
Expression specificity is another important aspect of gene therapy. Gene expression in off-target tissues or cell types may lead to toxicity or trigger an unwanted immune response (see below). From the rAAV genome design perspective, prominent strategies that better confine gene expression in desired compartments include using tissue or cell type-specific promoters130,143 and incorporating miRNA binding sites in the 3ʹ-untranslated region (UTR) to detarget expression from cells that are enriched for the miRNA144,145,146,147. One notable application of such a detargeting strategy concerns professional antigen-presenting cells (APCs) that harbour a high level of miR-142-3p. The inclusion of miR-142-3p binding sites in vector cassettes was shown to efficiently diminish transgene expression in APCs and greatly reduce immunity against the transgene product148,149.
Accommodating large transgenes
One limitation of AAV vectors is their small packaging size (~5.0 kb, including ITRs) compared with other viral vectors. However, several strategies have been investigated to enable delivery of a large therapeutic gene. A seemingly straightforward workaround is to design a shortened version of the gene that encodes a truncated but functional protein. One example involves the development of a micro-dystrophin gene replacement therapy for Duchenne muscular dystrophy (DMD)150. The entire coding sequence of the human dystrophin gene is 11.5 kb, well exceeding the packaging limit of rAAV. A landmark study demonstrated that a half-sized protein is partially functional and associated with an attenuated muscular dystrophy phenotype151. Further studies on the structure and function of dystrophin led to the generation of several smaller forms that can be packaged within AAV vectors150. Development of a micro-gene that is amenable to rAAV delivery likely requires a deep understanding of the structure–function relationship of the protein and is therefore gene-specific. Nevertheless, micro-gene therapy is under extensive clinical evaluation for DMD150 and preclinical testing for dysferlinopathy152 and CEP290-associated Leber congenital amaurosis (LCA)153.
A potentially promising approach for delivering oversized transgenes in rAAVs is to coadminister two AAV vectors that carry separate halves of a gene154,155,156,157,158. The two vector genomes can undergo inter-molecular recombination once co-delivered into the same cell, allowing for the reconstitution of the full-length gene. The ITR or an optimized recombinogenic sequence can serve as the overlapping sequence between the two vector genomes to promote recombination154,159,160,161. A key feature of such a dual-vector design is the utilization of splicing signals flanking the overlapping sequence, which ensures the precise removal of the recombinogenic sequence from the pre-mRNA during splicing. Analogous to mRNA splicing, intein-mediated protein trans-splicing (PTS) precisely fuses two peptides carrying a split intein162. Reconstitution of a full-length protein by PTS has been demonstrated for dystrophin163 and Cas9 (refs164,165), a programmable endonuclease widely used for gene editing. While the micro-gene strategy has progressed into clinical testing and shows promising early results150, the dual-vector and PTS approaches remain under preclinical development. The reconstitution efficiency is one bottleneck that limits broader application. Optimizing the overlapping sequence to promote efficient recombination and engineering split inteins to allow for efficient PTS will greatly facilitate their translational use.
Although rAAVs are a favourable vector for gene therapy, they persist as non-replicating episomes. Transduced vector genomes are therefore gradually lost in mitotic cells. Strategies for retaining transgene expression in replicating cells have been sought. The most straightforward approach to achieving prolonged transgene expression in replicative cell types is the promotion of rAAV genome integration. As discussed in Box 2, rAAV genomes are found to integrate at low frequencies. Such rare and unsupervised integration events usually result in partial genome integration and are therefore not ideal for therapeutic purposes.
Gene editing provides a promising solution to enhance persistence through targeted genomic integration. Once a programmable nuclease introduces DNA breaks in the target genomic locus, the homology-directed repair (HDR) pathway of the host cell can use the rAAV genome as a donor template, resulting in the precise and heritable insertion of a therapeutic gene cassette into the host genome166. If the nuclease is also directed to cleave the rAAV genome, the liberated double-stranded linear DNA fragment carrying the therapeutic gene cassette can be inserted into the targeted genomic locus by homology-independent targeted insertion167,168. In addition, nuclease-free homologous recombination-directed integration has recently gained attention as an alternative approach for gene editing69,169,170. This phenomenon works by inserting flanking segments of sequence that are homologous to genomic target sites into vector genomes171. In this way, stable integration of sequences can be achieved without the need to introduce DNA breaks via a nuclease.
Alternatively, strategies to allow vector persistence via insertion of scaffold/matrix attachment region (S/MAR) sequences into constructs so that episomal forms can undergo replication in transduced cells have been explored172. The use of S/MARs in plasmid constructs has been utilized for long-term gene expression over hundreds of cell doublings173.
As of 13 November 2018, there were 145 interventional clinical trials involving rAAV registered at ClinicalTrials.gov (Fig. 4). To date, there are two vectorized AAV serotypes that have gained regulatory approval for commercial use in patients: AAV1 (Glybera; uniQure) and AAV2 (Luxturna; Spark Therapeutics). There are less than a dozen capsid serotypes that are currently used as vectors in clinical trials, the most numerous being AAV2-based platforms. However, newer and more efficient capsids, such as AAV8, AAV9 and AAVrh.10 are increasingly being utilized in trials. In most cases, the therapeutic strategy involves the targeting of a monogenic recessive disease by gene replacement (Table 1). Phase I/II trials are commonly carried out to expedite the product development for rare genetic diseases with fewer patients. A selection of ongoing interventional clinical trials can be found in Table 1. Some exemplary translational applications and successes are discussed below in the context of target tissues and therapeutic strategies.
Target tissues amenable to rAAV gene delivery
Considering the natural tropism of AAV and unmet medical needs, most rAAV gene therapy programmes focus on the liver, striated muscles and the CNS. Almost all natural AAV capsids can transduce liver efficiently following systemic administration. Thus, rAAVs provide a robust liver-targeting platform to treat a variety of diseases such as haemophilia A and haemophilia B, familial hypercholesterolaemia, ornithine transcarbamylase deficiency and Crigler–Najjar syndrome174. Capsids such as AAV8 and AAV9 can target multiple muscle types throughout the body, enabling rAAV gene therapies to be developed for multiple muscle diseases175, especially those afflicting muscles of the entire body, such as DMD. Notably, transduced muscle can serve as a bio-factory to produce secreted therapeutic proteins for the treatment of non-muscle diseases. Although most heart diseases are polygenic and influenced by environmental factors, several genes involved in signalling and metabolism have been tested to treat heart failure176.
A large percentage of rAAV gene therapy under clinical development is focused on the CNS, including the brain177,178 and eye179,180,181. The eye is a somewhat confined and compartmentalized organ that is amenable to direct ocular rAAV gene delivery. Notably, the first rAAV gene therapy drug approved by the US Food and Drug Administration (FDA), Luxturna, treats patients with an inherited form of vision loss caused by RPE65 gene mutations182. By contrast, the brain is much more complex and larger. Direct intraparenchymal rAAV injections result in localized distribution of rAAV and are ideal for the treatment of CNS diseases that afflict a defined region of the brain, such as the putamen in Parkinson disease. Delivery to the cerebrospinal fluid space by intrathecal injection, on the other hand, can achieve broader CNS distribution. Unfortunately, these routes of administration can be invasive and pose substantial risks. Alternatively, intravenous delivery of certain serotype vectors, such as AAV9 and AAVrh.10, has allowed the vectors to cross the BBB to transduce neurons and glia183,184,185,186. This landmark discovery led to a number of studies demonstrating the therapeutic efficacy of systemic rAAV administration to target diseases that afflict widespread regions of the CNS, including spinal muscular atrophy (SMA)187, amyotrophic lateral sclerosis140,188,189, Canavan disease130,190, GM1 gangliosidosis191 and mucopolysaccharidosis type III192. Multiple clinical trials that utilize this powerful rAAV platform are currently underway193.
rAAV gene therapy strategies
This strategy aims to deliver a gene product to compensate for loss-of-function mutations. Gene replacement is suitable for treating recessive monogenic diseases and has enjoyed the most clinical success, as demonstrated by Glybera and Luxturna. Glybera is a rAAV1-based platform that delivers a hyperactive form of the gene encoding lipoprotein lipase (LPL) to treat LPL deficiency194. The benefit of using a hyperactive variant is that vector potency is increased, enabling a reduction in the vector dose. This not only eases manufacturing burdens but also reduces capsid immunity, as discussed below. Luxturna is an AAV2-based platform that delivers an RPE65 gene cassette to treat retinal dystrophy caused by biallelic mutations in RPE65 (ref.182). Both Glybera and Luxturna are administered locally to the muscle and eye, respectively. AAV vectors derived from AAV1 and AAV2 are still being pursued in some clinical studies aiming to deliver transgenes locally to the muscle, eye or brain (Table 1). However, both capsids have limited capacity to achieve widespread gene delivery following systemic injection.
In the early 2000s, the discovery of a novel family of naturally occurring primate AAV serotypes and variants greatly expanded the toolbox of capsids to achieve much more widespread transgene delivery following intravascular injection63,64. Several ongoing gene replacement clinical trials take advantage of these newer capsids and have demonstrated promising therapeutic outcomes, including trials for haemophilia A and haemophilia B (targeting liver), DMD (targeting whole body muscle) and SMA (targeting the broad CNS, including the spinal cord) (Table 1). Restoration of protein production at a fraction of normal physiological levels can in many cases alleviate the disease. In many disorders, the delivery of functional transgenes to only a subset of cells within an affected tissue is sufficient.
In contrast to gene replacement, gene silencing mainly tackles monogenic diseases caused by gain-of-toxicity mutations, such as Huntington disease. Owing to their potency for inhibiting gene expression, RNAi strategies currently dominate rAAV-based gene silencing platforms. However, compared with the rapidly advancing synthetic RNAi therapeutics, rAAV-based RNAi therapies mostly remain under preclinical development195. Gene silencing often has to occur with high tissue penetrance to achieve meaningful therapeutic outcomes, a challenge for AAV vectors with certain target organs, such as the human brain. In addition, high levels of Pol III-driven shRNAs may overwhelm the endogenous miRNA biogenesis pathway, leading to toxicity137. Off-target silencing by RNAi is another safety concern. Although embedding shRNAs in an amiR scaffold that is transcribed by a Pol II promoter can significantly reduce off-target silencing, as well as generate tolerable amounts of small interfering RNA (siRNA) molecules138,139,140,141,142, RNAi efficacy may be reduced. Regardless of how the shRNA is constructed and expressed, the short hairpin DNA structure that encodes the shRNA was recently shown to cause truncated rAAV genomes during vector production and can compromise vector genome homogeneity196. Interestingly, engineering pri-miR-33 to express siRNAs not only improves rAAV genome integrity but also reduces toxicities associated with off-target silencing and/or saturation of endogenous RNAi machinery197. Importantly, amiRs derived from the pri-miR-33 scaffold have RNAi efficacies that are comparable to Pol III-driven shRNAs197.
In addition to RNAi, the recently reported Cas13 family of proteins provides another means to silence gene expression at the mRNA level198,199. These proteins possess potent RNA-guided ribonuclease activity and appear to be more specific than RNAi. At the transcriptional level, gene expression can be silenced by a CRISPR–Cas9 repressor delivered by dual AAV vectors200. However, the translational uses of CRISPR–Cas will face several obstacles including rAAV packaging size limitations and immune responses against the bacteria-derived foreign protein165,201,202.
Beyond monogenic diseases, rAAV-mediated gene therapy has the potential to tackle complex genetic diseases and acquired diseases by gene addition. Human diseases, such as heart failure and infectious diseases, represent some of the most urgent unmet medical needs. Gene addition can modulate these diseases in multiple ways, such as supplying neurotrophic factors for neurological diseases177 and tuning signalling pathways for heart failure203 and cancer204. A notable gene addition strategy employs rAAV delivery of genes encoding recombinant antibodies that can neutralize deadly viral infections205,206,207,208,209,210. These platforms utilize intramuscular delivery and transform the transduced muscle cells into a bio-factory to produce therapeutic antibodies that are secreted into the bloodstream. This strategy is currently being tested clinically for HIV infection (Table 1). One challenge is the mounting of immunity against the vectored antibodies, as they can be recognized as foreign proteins. This anti-antibody response can suppress the circulating antibody concentration below the targeted threshold, limiting efficacy. rAAV-related immune responses are further discussed below.
The rapidly evolving gene-editing technologies provide a versatile toolbox to directly repair mutations underlying human diseases. Therapeutic gene editing typically occurs in two steps: generation of targeted DNA breaks in the genome and DNA repair that eventually leads to a desired DNA alteration.
A series of programmable nucleases has been developed to generate DNA breaks, such as engineered meganucleases, zinc-finger nucleases (ZFNs), transcription activator-like effector nucleases and CRISPR-associated (Cas) proteins. ZFNs are tolerable because they are derived from human proteins, and their small transgene sizes are amenable to rAAV packaging. In contrast to ZFNs, the Cas proteins are derived from bacteria, such that their immunogenicity is a potential roadblock for rAAV gene delivery. In addition, their large cDNA sizes make rAAV delivery less flexible. Nevertheless, the Cas proteins are a robust gene-editing system that can be easily programmed to target a specific genomic DNA locus and remain the most extensively studied programmable nucleases for both research and therapeutic applications.
The main cellular DNA repair pathways leading to therapeutic gene-editing outcomes include non-homologous end joining (NHEJ) and HDR, and they are usually exploited to introduce gene disruptions and precise corrections, respectively. In addition to delivering the nuclease transgene, the single-stranded rAAV genome can also serve as a donor template to enable HDR. The synergistic effects of sequence-specific nucleases and DNA repair mechanisms can yield many therapeutic gene-editing approaches beyond disrupting a gene by NHEJ211,212,213 and directly repairing a mutation by HDR166,214,215,216,217. For example, the first in vivo rAAV gene-editing clinical trials for lysosomal storage disorders are underway. This strategy utilizes the ZFN platform and HDR pathway to precisely insert a therapeutic gene into the albumin locus to hijack the strong albumin promoter to drive transgene expression in hepatocytes218,219,220. Other notable therapeutic gene-editing approaches include exon deletion to remove a mutation without disrupting the open reading frame221,222,223, splicing modulation to reframe protein-coding sequences224 and allelic exchange to repair recessive compound heterozygous mutations225.
Notably, base editing has emerged as a powerful therapeutic gene-editing approach that directly converts one base pair into another without generating double-stranded DNA breaks. The DNA base editors comprise an RNA-guided, catalytically inactive form of Cas for sequence recognition and a fused effector to achieve base conversion. Refinement of the DNA base editor design has now greatly improved editing efficiency, accuracy and flexibility226.
Large-scale vector manufacturing and cost
A main barrier for AAV-based gene therapy may be the affordability of the drug product. For example, priced at 1 million euros (US$1.2 million) per patient at the time of this Review, Glybera still holds the title for the most expensive drug in the world. Luxturna, which was launched in 2017 at US$425,000 per eye treatment, has a similarly high price tag. Unfortunately, the price is primarily attributed to the high cost of manufacturing. A great deal of resources and expertise with current production systems is required to generate enough vector to treat a target organ, be it the CNS, the liver or muscle, or to systemically target multiple organs.
Triple transfection of plasmid DNA into adherent eukaryotic cells is common for the production of both research-grade and clinical-grade vectors227,228 (Box 1). Unfortunately, scaling this system is costly, as large-scale production requires increasing the surface area needed to grow packaging cell lines. HEK293 cells have been adapted to grow in suspension in bioreactors to yield over 1 × 1014 vector genomes per litre229. Despite these advancements, the three-plasmid transfection system remains somewhat inefficient, as not all cells receive optimal ratios of the plasmids required for efficient packaging. Plasmid imbalance may also contribute to the variation in empty-to-full capsid ratios between vector batches. Multiple feasible approaches for generating stable eukaryotic cell lines to circumvent the need for plasmid transfection have been described230, but these have yet to be adapted to a suitable clinical production pipeline or are hampered by concerns regarding the use of replicating AdV. Recombinant baculovirus platforms have been widely employed for large-scale production of rAAV in Sf9 cells owing to their ease of suspension culturing at high cell densities (Box 1). Glybera is in fact produced utilizing this method. However, these methods are still sufficient for only a limited number of patients, as the doses necessary to be effective can be very high.
Although treating monogenic disease by rAAV vectors has now become more feasible than ever, the high risk and high cost of developing rAAV-based investigational new drugs (INDs) discourage many investigators from transitioning preclinical studies to clinical trials. Typical FDA-approval for IND trials requires extensive preclinical studies to measure toxicology, safety, dose and bio-distribution227. Difficulties with purification of rAAV particles from cellular and viral impurities and removal of AAV empty capsids, lack of standardization (many times owing to differences in vector capsid variant) and inherent batch-to-batch variation of vector potency all impact production costs.
Vector quality control and assay standardization
Empty capsids can range from 20% to over 98% in vector preparations when produced by standard transient transfection production pipelines231. Common semi-quantitative methods of surveying empty or partially empty particles employ electron microscopy, where empty capsids are easily differentiated after negative staining. Absolute quantification of empty versus full capsids used for assaying clinical-grade vectors can be obtained by optical density measurements or sedimentation velocity analytical ultracentrifugation231,232. More sophisticated methods employing charge detection mass spectrometry not only are capable of quantifying the distribution of empty-to-full capsids but also can reveal the distribution of partial and/or truncated genomes that are packaged into virions233.
Robust potency assays for rAAVs should measure the effectiveness of gene transfer. Additionally, these tests should also gauge any biological effects of the transferred gene, which can include toxicity, immunogenicity or transgene clearance. Accurate assessment of rAAV potencies is limited by multiple factors: the animal model it is tested in, the sex of the test subject, the expected effective dose and therapeutic window, the capacity of the vector to evade the immune response, its on-target and off-target infection profile, proper cytosolic trafficking through cellular compartments, mechanisms of capsid escape and transcription of the transgene. In order to provide a robust potency assay for rAAVs, surrogate models, such as mice, serve as the standard in vivo test system for the transduction of the liver234. Unfortunately, in vivo models suffer from poor reproducibility. Furthermore, inter-species variation in AAV tropism and transgene expression can result in misrepresented potencies. In vitro proxy assays would be favourable in light of in vivo variability. Thus, potency assays have been developed with fairly high reproducibility235,236. Recent reports of ex vivo potency assays for retinal rAAV gene therapy using human retinal explants represent robust potency assays that do not rely on animal models237,238.
Owing to the increasing interest in using rAAVs as clinical vectors, quality control standards for rAAV production are becoming more important than ever. Vector preparation impurities that are carried through from the production workflow can pose substantial risk. Safety profiling assays to screen for adventitious agents are now standard for clinical AAV vectors. The most direct solution to these issues is to employ single-use equipment during production, starting from DNA preparation steps and ending with the validation of DNA purity by high-throughput sequencing approaches239.
There has yet to be a standard for assessing the DNA content packaged into AAV particles. For example, in current rAAV production pipelines, nucleic acid contaminants can originate from cellular, viral and plasmid sources. The FDA recommends that the level of residual cell substrate DNA should be below 10 ng per dose and that the median DNA size should be 200 bp or lower. Platforms such as SSV-seq that are based on short-read high-throughput sequencing technologies, can unbiasedly detect host genome contaminants beyond what is feasible for quantitative PCR-based methods240. A long-read sequencing method named AAV-GPseq has achieved full single-genome resolution from ITR to ITR and can now determine the distribution of truncated forms196, as well as chimeric genomes arising from recombination events that result in the generation of heterologous DNAs that can harbour ITRs241. The identification and quantification of these species are critical, as these species can theoretically persist once they are transduced into cells after undergoing episome formation via ITR-mediated recombination. These species pose a substantial hazard because they may express proteins or regulatory RNAs. Functionally inert genomes, on the other hand, are counter-productive to efficient gene therapy and may require increased doses to compensate for poor batch potencies. This in turn may cause increased capsid immunological burden and/or possible integration-mediated genotoxicity in patients. Notably, the current platform for AAV-GPseq can also profile single-stranded AAV viral genomes242.
With the development of engineered novel capsids, especially those carrying modifications of VP2 or that are generated from systems that may yield heterogeneity in VP1:VP2:VP3 ratios, methods for the accurate assessment of capsid stability are in high demand. Additionally, the use of mixed serotype (mosaic) capsids that can outperform single serotype capsids243 necessitates methods that can quantify the extent of mosaicism. Importantly, what remains under-investigated is whether different production platforms may result in heterogenous capsid characteristics. As alluded to in Box 1, early versions of baculovirus Sf9 production schemes yielded poor packaging efficiencies for certain serotypes and variable performances in vivo. Classical methods to quantify capsid protein abundance such as silver stain gels are inadequate for assessing capsid heterogeneity. To meet this need, assays based on differential scanning fluorimetry have been developed to detect the differential unfolding of capsids in response to a temperature gradient244,245,246.
Immunological barriers to rAAV gene delivery
The rAAV protein capsid, its DNA genome and the protein product of the transgene can interact with host immune systems at multiple layers, posing substantial barriers to effective gene delivery and persistent gene expression247,248 (Fig. 5). The first barrier concerns the NAbs against the rAAV capsids that are identical or similar to the capsids of wtAAVs. NAbs in the blood circulation are found in a large portion of the human population owing to natural wtAAV infection and can effectively block rAAV gene delivery, especially following intravenous injection249,250. The immune-privileged brain can tolerate a somewhat high NAb titre following a direct CNS delivery but is not completely shielded from circulating NAbs251,252. Several strategies have been developed to overcome this barrier, such as plasmapheresis253,254 and using empty capsids as decoys255, but they are not effective in tackling high-titre NAbs. Another approach is to engineer rAAV capsid by eliminating NAb-interacting epitopes101. The effectiveness of these strategies under clinical settings remains to be tested. Currently, NAb screening and excluding seropositive subjects from enrolment remain necessary steps in many clinical studies256,257.
Following rAAV administration, the vector capsid triggers a robust humoral immune response to generate NAbs, preventing re-administration in most cases258. For applications likely requiring repeated dosing, transient B cell depletion upon the first injection259 and induction of immune tolerance by rapamycin260,261,262 may be considered. In addition, the capsid can trigger a cytotoxic T lymphocyte (CTL)-mediated cytotoxicity, which may lead to the clearance of transduced cells and therefore loss of transgene expression249,263. This phenomenon appears prominent in humans and is not readily modelled in animals. It should be noted that the CTL response mounted against the rAAV capsid is much weaker than those mounted against other viral vectors such as adenoviral vectors. CTL response caused by rAAV administration may compromise therapeutic efficacy over time but generally does not pose a major safety concern118,264. Some muscle-targeting clinical studies suggest that regulatory T (Treg) cells may play a role in restraining the effect of CD8+ CTLs265. Pharmacological suppression of CD8+ T cells with steroids is effective in managing liver CTL response following systemic rAAV delivery and ensuring long-term transgene expression256,257. Inspired by the induction of endogenous Treg cells in muscle-directed rAAV gene therapy and their potential role in limiting CTL response, administering autologous Treg cells as an adjuvant to in vivo gene transfer may provide a powerful approach for modulating rAAV immunity266.
The transgene may encode a protein that is foreign to the host, as is the case for gene replacement therapies in patients with a null genotype or gene addition therapies with vectored antibody-like molecules. The transgene product may therefore trigger both B cell-mediated and T cell-mediated adaptive responses to generate transgene product-specific antibodies and CTLs. Circulating antibodies may prevent lasting therapeutic efficacy. Likewise, anti-antibody responses are currently a major barrier for developing AAV vectored antibodies for infectious diseases. The transgene product-specific CTL response was reported in muscle-targeted clinical trials267 but not in liver-directed haemophilia trials256,257. Establishing the necessary enrolment criteria could have helped to mitigate such a risk. Importantly, the tolerogenic ability of the liver also impacts rAAV gene transfer268,269,270. The transgene product-specific immune tolerance induced by liver-directed rAAV gene delivery is dose-dependent and likely involves Treg cells. This endogenous immune modulation phenomenon can be harnessed to achieve stable transgene expression and therapeutic efficacy271,272.
In addition to eliciting adaptive responses, the rAAV capsid and vector genome are also sensed shortly after delivery by the innate immunity through Toll-like receptor 2 (TLR2) and TLR9, respectively. This response leads to the production of pro-inflammatory cytokines and promotes the adaptive response273. Self-complementary rAAV genomes274 or vector genomes with high GC content275 were shown to further enhance the innate immune response. Therefore, preventing TLR signalling by depleting CpG dinucleotides in the rAAV genome has the potential to enhance rAAV-mediated gene expression275. Another promising strategy is to incorporate a TLR9-inhibitory DNA sequence, such as multiple copies of TTAGGG derived from human telomeres, into the rAAV genome to evade innate immune surveillance276. This approach was reported to reduce the immune responses associated with rAAV delivery in mice.
Conclusions, perspectives and future directions
In conclusion, we have provided an AAV-centric view of current trends, challenges and milestones in the field of gene therapy. This Review has covered only a small part of an ever-expanding field. The range of technology platforms that constitute gene therapy is quite diverse, and substantial innovations have been made in the areas of cell therapy, gene editing, nanoparticle engineering and other gene delivery platforms. As technology continues to advance, the gene therapy field may become so diverse and accelerate so quickly that some of these technologies may fall out of favour before reaching the clinic. This is certainly possible for some rAAV-based strategies. Nevertheless, the current exponential growth of clinical trials using AAV vectors suggests that we are only at the beginnings of what is achievable for an inconsequential virus that has now become a programmable vector to improve human health.
Although the study of AAV is necessarily a discipline of virology, to adapt AAV into a gene therapy vector required a multidisciplinary approach. It has become abundantly clear that such advances would not have been possible were it not for contributions from the fields of molecular biology, bioinformatics, epidemiology, structural biology, immunology, genomics and all other disciplines that fall under the umbrella of biomedical research. Our hope is that as the AAV field continues to expand, a multidisciplinary approach to gene therapy drug development will continue to be fostered. In many ways, this goal is self-fulfilling, as gene therapy represents one of the final frontiers for curing human ailments. The human genome projects have achieved near complete annotation of the genome. Additionally, genome-wide association study projects and big data studies that explore the epigenome have provided the blueprints for linking genetic differences with disease. These achievements have put us in the middle of the very exciting genomics and gene therapeutics age. Harnessing the genetic code to develop innovative medicines will require contributions from all areas of scientific expertise to fully tap into the promise of rAAV gene therapy and to overcome current challenges.
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The authors thank H. Ma for figure concepts and illustration and L. Ren for compiling data for the table of adeno-associated virus (AAV) gene therapy clinical trials. The authors thank all members of the Gao laboratory and their numerous colleagues for productive collaborations and stimulating discussions on AAV and gene therapy. They also thank The American Society of Gene and Cell Therapy and all members of the gene therapy field for their invaluable contributions. The authors apologize for not being able to be more comprehensive in reviewing all the work of their colleagues owing to space limitations. Research in the Gao laboratory is supported by grants from the National Institutes of Health (NIH), the CHDI Foundation, the Grace Science Foundation and the authors’ industry partners.
G.G. is a scientific co-founder of Aspa Therapeutics and Voyager Therapeutics and holds equity in the companies. G.G. is an inventor of patents related to adeno-associated virus (AAV) gene therapy with potential royalties licensed to Aspa Therapeutics, Voyager Therapeutics and other biopharmaceutical companies.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
A field of study based on the bioengineering of delivery vehicles for biomolecules such as DNA and RNA.
The biological process of producing fully assembled vector particles, such as recombinant adeno-associated viruses (rAAVs) consisting of the DNA genome within the capsid.
A classification system for capsids or viral strains established by surface antigens.
- Episomal DNA
DNA that is autonomous from the host chromosomal DNA; the term is used for circularized, double-stranded adeno-associated virus (AAV) vector genome species that persist within the transduced cell nucleus.
- Blood–brain barrier
(BBB). A semipermeable physiological barrier that separates the circulating blood from the central nervous system and comprises endothelial cells, astrocytes and pericytes.
Pertaining to the epidemiological study of blood serum antibodies or antigens in populations.
- Codon expansion
A synthetic biology technique that reprogrammes a codon to encode an amino acid that is not naturally encoded.
Within the bulk of the tissue or organ.
- Artificial microRNAs
(amiRs). Molecular tools that are based on natural microRNA sequences and structures that house a small interfering RNA (siRNA) cassette designed to target a desired sequence.
- Homology-directed repair
(HDR). A DNA repair mechanism in the presence of a homologous DNA piece as the repair template.
- Multiplicity of infection
The ratio of infectious agents (for example, recombinant adeno-associated virus (rAAV)) to infection targets (for example, cells).
- Non-homologous end joining
(NHEJ). A DNA repair mechanism that directly ligates two broken DNA ends without a homologous DNA template.
- Adventitious agents
Any potentially harmful and unintentionally introduced agent (viruses, bacteria, mycoplasma, fungi, protozoa, parasites, transmissible spongiform encephalopathies, etc.) that may be found in manufactured drug products.
Damaging effect on the genome, whereby deleterious mutations are created.
The combined chromatin state (for example, DNA and histone modifications and non-coding RNA associations) throughout the genome of an organism that imparts heritable influence over gene expression.
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Wang, D., Tai, P.W.L. & Gao, G. Adeno-associated virus vector as a platform for gene therapy delivery. Nat Rev Drug Discov 18, 358–378 (2019). https://doi.org/10.1038/s41573-019-0012-9
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