The clinical application of ex vivo gene edited cell therapies first began a decade ago with zinc finger nuclease editing of autologous CD4+ T-cells. Editing aimed to disrupt expression of the human immunodeficiency virus co-receptor gene CCR5, with the goal of yielding cells resistant to viral entry, prior to re-infusion into the patient. Since then the field has substantially evolved with the arrival of the new editing technologies transcription activator-like effector nucleases (TALENs) and clustered regularly interspaced short palindromic repeats (CRISPR), and the potential benefits of gene editing in the arenas of immuno-oncology and blood disorders were quickly recognised. As the breadth of cell therapies available clinically continues to rise there is growing interest in allogeneic and off-the-shelf approaches and multiplex editing strategies are increasingly employed. We review here the latest clinical trials utilising these editing technologies and consider the applications on the horizon.
Cell therapy is defined as the administration of live cells to a patient with the aim of repairing or replacing damaged cells or tissues. It relies on a predefined cell population, which can either be from the same patient (autologous) or from a different donor (allogeneic). The type of therapeutic cell varies widely with clinical trials currently dominated by haematopoietic cells, mesenchymal signalling cells  and lymphocytes, but also, at a lower frequency, dendritic cells, hepatocytes, epithelial cells and various others are being investigated [2, 3]. From a disease perspective, oncology is responsible for over half of all cell therapy trials . Notably, the emerging arena of cell therapies has been boosted by several approvals in recent years . Unlike other treatments, cell therapies are live cell products and, via genetic engineering, can be enhanced to achieve better efficacy or tailored to individual patients. Importantly, they require extensive characterisation to demonstrate safety and compatibility. In this context it is noteworthy that their in vivo distribution, survival and efficacy at target, but also off-target tissues are critical parameters. For example, off-target activities led to severe adverse effects, with other life-threatening side effects and fatalities during clinical trials also reported. This together with the fact that most clinical cell therapy trials are still performed without knowledge about the in vivo distribution and fate of the administered therapeutic cells resulted in suggestions to routinely implement in vivo cell tracking (by imaging) [5,6,7] and suicide genes . As better efficacy and tailoring to patients is increasingly achieved through genetic engineering, the latter safety-related aspects can be piggy-backed into therapeutic cells at this stage . Traditionally, genetic engineering has been achieved through the use of viral vectors (e.g. γ-retroviruses, lentiviruses), which more or less randomly integrate the transgenes into the genome . This approach is often also classified as ‘gene therapy’ and has been applied for cell therapies in diverse aetiologies, for example, ranging from cancer immunotherapies to regulation of immune tolerance in autoimmune diseases . A specific form of genetic engineering is gene editing, which offers a much more specific way of integrating a desired genetic payload at a distinct location into the genome of target cells . As the breadth of cell therapies available clinically continues to rise and gene editing approaches provide potentially game-changing opportunities, we review here the latest clinical trials employing this new technology.
The narrow-winding road to genetically engineered cell therapies
Whilst genetic engineering strategies have generally advanced cell therapies to great patient benefit, the journey has not been smooth. The first report of successful cell therapy engineering was in X-linked severe combined immunodeficiency (SCID-X1) patients and involved collecting patient CD34+ hSCs, transducing them ex vivo with a replication-deficient γC Moloney retrovirus containing the γC cytokine receptor common subunit gene, an X-chromosome linked gene that is inactivated in SCID-X1 patients rendering them devoid of mature T and Natural Killer (NK) cells [13, 14]. The goal of the approach was to restore patient capacity to form mature T and NK cells. The engineered hSCs were reinfused into patients and within 10 months positive results were seen, with patient T and NK compartments filled by γC transgene-expressing cells. Unfortunately, nearly 3 years post-infusion two patients developed leukaemia as a result of clonal expansion of engineered T-cells. Both patients had proviral insertions which led to activation of the proto-oncogene LMO2 causing exponential proliferation of these cells . Viral vectors had allowed both robust transgene expression and high engineering efficiency, but also caused the downstream disease and thereby rendered it clear that an improved understanding of the long-term risks of genetic engineering was required. In the years that followed this study scores of new vectors were designed to reduce the potential for insertional mutagenesis and improve safety , but some in the field were already looking at a more precise strategy of introducing transgenes at defined locations in the genome.
Development of site-specific genetic engineering methods
Following the discovery that DNA double-strand breaks (DSB) could induce repair, scientists looked to exploit the repair process in order to manipulate cells with single base pair precision. Distinct nucleases with the capacity to recognise specific DNA sequences of interest (recognition sites) in endogenous mammalian genes were engineered, which could also cleave the DNA at these sites. Researchers were following the principles of homing endonucleases first discovered in budding yeast to do so , and laid the foundations of what became known as ‘gene editing’. These targeted editing approaches are now widely exploited in both preclinical and clinical research.
Zinc-finger nucleases (ZFNs) were the first designer nucleases, produced from a naturally occurring transcription factor family known as zinc finger proteins, fused to FokI endonuclease. The zinc finger proteins work as DNA-binding domains recognising trinucleotide DNA sequences, with proteins linked in series to enable recognition of longer DNA sequences, thereby generating sequence recognition specificity. The fused FokI functions as a dimer , so ZFNs are engineered in pairs to recognise nucleotide sequences in close proximity (Fig. 1a). This ensures DSBs are only produced when two ZFNs simultaneously bind to opposite strands of the DNA, whereby the sequence recognition specificity is determined by the length of aligned DNA-binding domains. This limits off-target effects, but with the downside that arrays of zinc finger motifs influence neighbouring zinc finger specificity, making their design and selection challenging [18,19,20]. Early studies relied on delivery of the ZFN expression cassette to cells via DNA fragments derived from viral vectors. Studies later progressed to using mRNA delivery via electroporation to enable entry into target cells. This approach offers transient but high levels of the expression cassette within cells, presenting a lower risk of insertion/mutagenesis at off-target sites as a result of the shorter mRNA half-life compared to DNA . This improved safety profile is paired with the benefit of highly efficient transfection (with levels > 90% reported) and excellent cell viability (up to 80%) [21,22,23].
Transcription activator-like effector nucleases (TALENs) were the next development following ZFNs. They also employ endonucleases such as FokI to initiate the DNA break, requiring paired binding, but the DNA targeting specificity comes from the fused bacterial TALE proteins [24, 25]. As with ZFNs, modular TALE arrays are linked to recognize flanking DNA sequences, but each TALE recognises only a single nucleotide and has no impact on the binding specificity of its neighbour, offering an improvement over ZFNs and a straightforward design process (Fig. 1b). As with ZFNs, for ex vivo cell therapy gene editing most TALEN-mediated approaches rely on mRNA as the delivery vector, with cell entry facilitated via electroporation.
The most recent system to be developed for gene editing is the clustered regularly interspaced short palindromic repeats (CRISPR) system. CRISPR originates from bacteria and uses a guide RNA (gRNA) which binds to the DNA target site. Subsequently, a nuclease, such as the CRISPR associated protein 9 (Cas9), induces conformational changes before cleaving the DNA (Fig. 1c). Targeting is accomplished through the gRNA molecule, which can be designed to optimise hybridisation with the sequence of interest. This can be done by standard Watson–Crick base pairing but must be followed by a DNA motif called a protospacer adjacent motif (PAM) to enable Cas binding. Like ZFNs and TALENs CRISPR–Cas9 gene editing can be achieved utilising electroporation of the Cas9 mRNA and gRNA but nuclease editing efficiency via this mode of delivery is limited due to instability of the unmodified sgRNA [26, 27]. Chemical stabilisation of the gRNA can limit its degradation, allowing time for the Cas9 protein to be translated following electroporation, and this improves editing efficiency . Alternatively, a ribonucleoprotein (RNP) complex formed as a result of in vitro transcribed guide RNA incubation with Cas9 protein can be used for delivery. RNP complexes offer increased stability, higher editing efficiency and reduced cytotoxicity [26, 27]. They also benefit from accelerated nuclease kinetic activity, potentially reducing the activity window of the nuclease and thus opportunities for off-target effects [27,28,29]. Whilst some report that CRISPR can lead to increased DNA cleavage at off-target sites compared to the paired binding approaches of ZFNs and TALENs, strategies to reduce off-target activity are underway . These include the quantification of imperfect Cas9-induced DSB repair products through primer-extension-mediated sequencing (PEM-seq) to improve determination of editing specificity and efficiency; as well as the use of high-fidelity Cas9 variants. Though there are distinct advantages and disadvantages for employing each of these gene editing strategies (comprehensively reviewed in ), the result is the precise introduction of a DSB.
Following DSB repair is required. The predominant DNA-repair pathway for DSBs in mammalian cells is nonhomologous end-joining (NHEJ) . NHEJ involves direct ligation of the DSB ends with negligible homology and thus is a highly error-prone process. It frequently leads to insertion or deletion of nucleotides (indels) in the DSB region, which can produce truncated proteins (Fig. 2a). This error-prone repair process is exploited in gene editing strategies to enable selective inactivation of genes (termed gene disruption) either to render pathogenic proteins non-functional or preferentially knock-out genes. NHEJ has already been exploited to aid cell therapy development. For example, gene-editing strategies capitalising on NHEJ-induced indels have been adopted to reactivate expression of foetal haemoglobin to compensate for faulty adult haemoglobin in distinct blood disorders .
DSBs can also undergo homology directed repair (HDR), a process primarily active during the S/G2 phase of the cell cycle, when homologous DNA is present in the nucleus. HDR can be utilised to selectively repair a deleterious mutation (targeted gene repair) or incorporate transgenes of interest within desired loci (gene addition) but it requires donor DNA to be co-delivered with the editing agent initiating the DSB, and for this DNA to remain available until cells reach S/G2, to enable incorporation during the repair process (Fig. 2b). HDR-mediated targeted repair is not a common approach in cell therapy, as mutations yielding pathogenic phenotypes can vary significantly between patients, necessitating a range of repair approaches. HDR is more commonly considered for targeted addition of transgenes, offering limited chromosomal positional effects and uniform transgene expression compared to virally mediated genetic engineering strategies. The resultant phenotype is predictable with limited risk of insertional mutagenesis making it an ideal choice for compensatory gene expression. For example, an in vivo gene editing strategy in a phase I clinical gene therapy trial for haemophilia B patients involves intravenous delivery of a ZFN that targets the albumin locus in hepatocytes (NCT02695160) . The goal is to insert a healthy copy of the Factor IX gene, aberrant in these patients, into this locus to enable lifelong therapeutic production of the Factor IX clotting factor. Such in vivo gene therapies exploiting gene-editing strategies remain rare with only a handful approved globally (NCT02695160 for haemophilia B using ZFN by Sangamo; NCT02702115/mucopolysaccharidosis type I/ZFN/Sangamo; NCT03041324/mucopolysaccharidosis type II/ZFN/Sangamo). As the latter approaches are technically not considered cell therapies (cf. definition above) further discussion of these approaches is beyond the scope of this review. However, targeted gene addition in the context of cell therapies will be discussed below.
Clinical trials using zinc finger nucleases
The first clinical use of gene edited cell therapies began roughly a decade ago. The first-in-human application of a targeted gene editing cell therapy involved disruption of the HIV co-receptor gene CCR5 using zinc finger nucleases (ZFNs) in autologous CD4+ T-cells of HIV patients (NCT00842634) . CCR5 is a transmembrane chemokine receptor expressed on the surface of activated T-cells, and is the major co-receptor for HIV-1 entry . Following discovery of a homozygous 32-nucleotide deletion (Δ32) in a CCR5 allele which yielded a truncated protein not expressed on the cell surface in individuals with natural resistance to HIV-1 infection [37,38,39], early clinical trials investigated the potential for inhibiting HIV entry through CCR5 by blocking the HIV-CCR5 interaction using small molecule approaches . Whilst these strategies showed some promise they would eventually result in viral selection for resistant mutants which were able to maintain CCR5 use for viral entry . Given these strategies selected for resistance, a CCR5 knockout approach, analogous to the Δ32 genotype in endogenously resistant individuals, was considered optimal. CD4+ T-cells play a critical role in immune protection, and low counts in HIV-1 patients were strongly associated with progression to acquired immune deficiency syndrome (AIDS), which made this disease an ideal target for attempting treatment using a gene edited cell therapy . Preclinical studies had identified a ZFN pair capable of producing a DSB within a transmembrane domain upstream of the naturally occurring Δ32 mutation in primary human CD4+ T cells. This ZFN pair resulted in a broad range of indels, but a specific five nucleotide addition (duplication of the sequence between ZFN binding sites) accounted for 30% of all sequence modifications, introducing two in-frame stop codons that prevented expression . Following these promising pre-clinical results, in 2009 Sangamo Therapeutics initiated the first clinical trial to evaluate therapeutic safety (NCT00842634). Using an adenoviral vector delivery system, they reinfused autologous CD4+ T-cells edited ex vivo using their ZFN, named SB-728, into 12 patients. Results showed that the edited T-cells were safe in patients, with only one serious adverse event, attributed to a transfusion reaction, recorded. Additionally, some partial acquired resistance was reported where detectable HIV DNA levels decreased in most patients  pointing towards efficacy in this clinical trial. The use of an adenoviral approach allows high delivery efficiency but only transient ZFN expression, avoiding the complications of insertional mutagenesis experienced from earlier retroviral or lentiviral approaches.
The demonstration of clinical safety using this ZFN approach paved the way for future trials, with disruption of CCR5 in cells from HIV patients currently being the most advanced clinical genome editing system. There are eight ongoing or completed clinical trials to date (Table 1). Subsequent clinical trials involved variations of parameters aimed at improving efficacy and homing in on patient populations most likely to benefit from different treatment regimens. Variations included modifying the input cell dose (NCT01044654), infusing multiple doses of edited cells (NCT02225665) and patient lymphodepletion by cyclophosphamide treatment prior to infusion of ZFN-edited T-cells, with the goal of enabling transient reduction of unedited T cell numbers to improve infused T-cell engraftment (NCT01543152). Scientists also moved to an mRNA electroporation method for ZFN delivery into T-cells (NCT02388594), as this strategy offered several safety advantages over DNA fragments derived from viral vectors, and a lower risk of insertion/mutagenesis at off-target sites as a result of shorter mRNA half-life compared to DNA . These CCR5 disruption approaches offer the potential for a ‘functional cure’ for patients if sufficiently high engraftment levels are achieved.
An alternative strategy using ZFN-edited haematopoietic stem/progenitor cells (HSPCs) has also been trialled, which was inspired by the results of the so-called “Berlin patient”. This HIV-1 infected patient, who now has an undetectable viral load [44, 45], underwent allogeneic CD34+ HSPC transplantation for acute myeloid leukaemia (AML) with HLA-matched cells from a donor homozygous for the Δ32 CCR5 allele . Following this approach, preclinical studies established that ZFNs could be used to disrupt CCR5 expression in CD34+ HSPCs, which would also yield CCR5-negative differentiated progeny . A further study established editing by ZFN mRNA electroporation offered less cytotoxicity compared to adenoviral vectors and was better scalable to levels required for clinical translation . A follow-up trial implementing these aspects (NCT02500849) aimed to assess safety and feasibility of transplanting autologous CD34+ CCR5-negative HPSCs in patients who already have undetectable HIV viral loads from combination anti-retroviral therapy but suboptimal CD4+ cell levels. The goal was to provide patients with a HIV-resistant immune system without the need for an allogeneic donor, as progeny of the transplanted CCR5-negative HPSCs would also inherit the resistance. Here, the use of autologous cells was a huge advantage as one of the major risks for the strategy adopted in the Berlin patient was the possibility of graft-versus-host disease (GvHD). The pre-conditioning approach in this trial also differed to the total body irradiation approach of the Berlin patient, with trial patients receiving only the chemotherapeutic busulfan prior to edited HSPC infusions. This was a similar strategy as previously used in the second reported patient, the so-called “London patient”, which had an undetectable HIV viral load as a result of receiving an allogeneic CD34+ Δ32 homozygous HSPC transplant for blood cancer (Hodgkin’s lymphoma) [49, 50]. The London patient received a reduced intensity conditioning regimen exclusively of chemotherapy agents with known activity against lymphoma indicating potential success for this gene edited cell therapy approach. Peer-reviewed results from this follow-up clinical trial are still outstanding and whilst no longer recruiting, the trial is still active as follow-up assessments were scheduled for up to 5 years with completion expected in 2022. Results will be followed with interest by both the HIV and cell therapy communities.
For almost a decade Sangamo’s SB-728 ZFN for HIV patients was the only ZFN gene edited cell therapy entering clinical trials. However, when rival TALEN and CRISPR technologies emerged in clinical trials, Sangamo made the lateral move into blood disorders and pursued the potential for ZFN therapies for haemoglobinopathies, in collaboration with Bioverativ Therapeutics . Haemoglobinopathy patients typically have mutations in the β-globin gene and thus produce malformed haemoglobin, such as in transfusion-dependent β-thalassemia (TDT) or sickle cell disease (SCD). Sangamo has developed ZFNs targeting the BCL11A gene, which is ordinarily involved in repressing production of foetal haemoglobin (Hbf) in adults [52, 53]. Hbf expression allows foetal haemoglobin to compensate for the malformed adult haemoglobin. By using a gene disruption approach, as seen with their CCR5 platform, the goal was to introduce indels that abrogate expression of the erythroid-specific enhancer of BCL11A in autologous CD34+ HSPCs [33, 54]. Following reinfusion and engraftment into patients this will enable mature adult blood cell progeny of the gene edited HSPCs to express high levels of endogenous HbF. The overall aim is to elevate HbF levels to the point where transfusion requirements for blood disorders such as TDT and SCD are alleviated. Whilst the first trials for TDT with the ZFN product ST-400 (NCT03432364) and SCD with BIV003 (NCT03653247) are still in the early stages of phase I, Sangamo has announced early results from the first patient treated in the TDT trial . This patient has β0/β0 TDT, considered the most severe form , and neutrophil and platelet recovery at 2- and 4-weeks post gene edited HSPC infusion was demonstrated, respectively; this indicated successful reconstitution of haematopoiesis in this patient. By 7 weeks, HbF levels have risen from 1% of total haemoglobin to 31% suggesting successful gene editing by ST-400, supported by indels detected in peripheral blood. This patient previously received packed red blood cell transfusions every other week for the past 2 years and following ST-400 infusion continued to receive them for approximately 2 weeks, but subsequently they were no longer required (for at least another 5 weeks at the time of writing the corresponding publication ). Data from additional patients is expected toward the end of 2019, but these early results are encouraging and indicate that ZFNs still have a role to play in the growing cell therapy field.
The early clinical applications of ZFN cell therapy were focussed on HIV patients with many phase I/II trials now completed (Table 1). Despite the completed studies, but perhaps unsurprisingly given the cost and time required to collect, edit and expand sufficient numbers of T-cells/HSPCs for each patient, there is currently little activity to progress ZFN-based therapies toward phase III whilst long-term follow-up data continues to be gathered.
Clinical trials with TALEN technology
Meanwhile, the first TALEN-edited cell therapies entering clinical trials have looked to overcome some of the challenges associated with ZFNs by adopting an ‘off-the-shelf’ approach (Table 2). CD19 is a transmembrane protein expressed on B-cells and B-cell precursors but not on bone marrow stem cells or other tissues. In blood cancers, it can be activated without extracellular stimulation required to transduce a signal, resulting in chronic B-cell activation. A number of promising genetic engineering strategies for autologous T-cell immunotherapy have been aimed at producing anti-CD19 CAR-Ts across a range of cancers to enable targeted treatment of these malignancies [57,58,59]; this includes commercially available CAR-T therapeutics such as tisagenlecleucel (Kymriah™) and axicabtagene ciloleucel (Yescarta™) which obtained approval in several countries [60, 61]. However, the number of patients able to benefit from the latter therapies are limited by the availability of high numbers of functional, expandable T-cells available from each individual patient. Moreover, the source T-cells could also be affected by the patients’ pre-treatment regimes. Notably, recent estimates suggest autologous CAR-T therapies cost around $95 k per dose to manufacture, with their allogeneic equivalents costing only around $4.5 k .
Cellectis SA has developed an allogeneic approach termed Universal Chimeric Antigen Receptor (CAR) T-cells targeting CD19 (UCART19). It is intended to overcome limitations of the autologous approach and aims to offer a standardised therapeutic, with greater consistency, improved quality control and immediate availability to patients. The immunotherapy approach for tumour associated antigen (TAA) targeting follows a similar genetic engineering approach to autologous strategies already in development. Through lentiviral transduction, expression of a single chain variable fragment (scFv) targeting CD19 and linked to CD137 (4-1BB) and CD3ζ co-stimulatory/signalling domains is achieved in GMP grade. Importantly, the starting material are healthy donor peripheral blood mononuclear cells (PBMCs) [63, 64]. Additionally, UCART19 offers an enhanced safety profile over earlier therapies as the anti-CD19 scFv-41BB-CD3ζ is linked to an epitope marker/suicide gene (RQR8) that encodes target epitopes from CD34 and CD20, thereby allowing purification of the engineered population via CliniMACS® CD34 selection. RQR8 is also a suicide gene, offering the option for binding of engineered CAR-Ts to the therapeutic monoclonal antibody rituximab which, in the event of unacceptable levels of toxicity in vivo, would allow selective destruction of transplanted cells . The genetic engineering strategy to enable CD19 TAA targeting is coupled with a multiplexed gene editing approach to prevent GvHD and allow administration of UCART19 in non-HLA matched patients. Therefore, T-cells are electroporated with two pairs of TALEN mRNA targeting the TCRα constant gene (TRAC) and the CD52 gene locus. TRAC knockout yields TCR-negative cells as TCRαβ expression is dependent on formation of an αβ heterodimer, this mitigates the potential of alloreactivity with host cells, and any remaining TCR expressing cells can be depleted using CliniMACS® TCRαβ after ex vivo expansion. CD52 knockout enables UCART19s to survive administration of the anti-CD52 mAb alemtuzumab, which is widely used as a lymphodepleting agent to prevent rejection of transplanted HLA mismatched cells  and as a conditioning therapy before therapeutic stem cell transplantation (SCT). In their first clinical application this multiplex strategy yielded a T-cell product with < 1% TCR expression with 85% of those cells expressing the CAR and 64% CD52-negative .
The preliminary results reported for the phase I paediatric acute B-cell lymphoblastic leukaemia (ALL) trial (PALL;NCT02808442) are promising for this difficult to treat patient group, with 5/5 patients achieving complete remission by day 28–42 after UCART19 infusion, and proceeding to conditioned allo-SCT 7 to 9 weeks later . The corresponding dose escalation trial in adult patients (CALM; NCT02746952) reported 4/6 patients with complete remission (with incomplete blood count recovery, CRi) with no signs of minimal residual disease 28 days post-infusion (as determined by a tumour burden < 0.01% of cells assessed by flow cytometry and/or qPCR) . Further pooled results for the CALM and PALL trials were reported in 2018, these suggest a manageable safety profile for UCART19 in the patients enrolled so far . Whilst showing promising complete remission or CRi rates of 88%, the pooled results have also raised questions on how clinical status, tumour burden and pre-conditioning lymphodepletion impacts UCART19 expansion. These preliminary results suggest anti-leukaemic activity is connected to CAR expansion, as 2/16 patients evaluable for anti-leukaemic activity showed no UCART19 expansion and had refractory disease. Identical to UCART19 in molecular design, another Cellectis approach, ALLO-501, utilises a different manufacturing process with a different contract manufacturing organisation (CMO). Following the promising preliminary results of UCART19 Cellectis have licenced the rights of ALLO-501 to Allogene; and the first ALLO-501 clinical trial, in patients with large B-Cell or follicular non-hodgkin’s lymphoma opened for recruitment in the USA in May 2019 (NCT03939026). This selected target patient population has previously shown response to other anti-CD19 therapies .
Cellectis’ UCART123 was the second TALEN-edited cell therapy to enter clinical trials in 2017. UCART123 targets CD123 (interleukin (IL)-3 receptor α-chain), the primary low-affinity subunit of the IL-3 receptor, which is highly overexpressed in some haematological cancers. Here, Cellectis demonstrated TAA targeting by engineering expression of an anti-CD123 scFv linked to 4-1BB and CD3ζ domains, with the RQR8 epitope marker/suicide gene also incorporated. The same patented TALEN technology as in UCART19 was used to knockout TRAC to enable therapeutic use allogeneically [71, 72]. The phase I UCART123 trial currently underway for AML (NCT03190278) was approved in July 2019, with the first patient dosed in January 2020. This trial utilises a new UCART123 targeting construct and an optimised production process compared to the original investigational new drug (IND) status approved by the FDA . This trial replaces Cellectis’ first AML UCART123 clinical trial which was put on hold by the FDA following adverse events in the first patients dosed due to cytokine release syndrome (CRS) . Following an amendment lowering UCART123 maximum dosing, the trial resumed and an increased dosing regime was subsequently re-approved to accelerate development [75, 76], but no results were reported. Cellectis had previously registered two other UCART123 trials under their earlier UCART123 IND, another to treat AML patients in the UK (NCT04106076, acting as a sister trial to the previous USA AML trial) which was terminated in December 2019, as well as a trial for blastic plasmacytoid dendritic cell neoplasm (BPDCN) patients (NCT03203369) which was terminated at the end of July 2019. Study cessation in both instances was reported as a result of a sponsor decision, not a consequence of safety concerns. There was speculation this was due to low recruitment numbers (with zero and one participant recruited for each trial respectively at time of trial termination) or because of competition with Stemline Therapeutics Inc’s tagraxofusp, but Cellectis did not comment publicly on these decisions. Tagraxofusp (Elzonris™, SL-401), is a CD123-directed cytotoxin therapy and was the first drug and first CD123-targeted therapy approved for patients with BPDCN, demonstrating the potential for success of other CD123-targeted immune cell therapies such as UCART123.
Several other TALEN-edited allogeneic UCART products for haematological cancers have also recently entered phase I clinical trials (Table 2). In December 2019 the first B-ALL patient received the CD22-targeted UCART22 product (NCT04150497) . CD22 is expressed in > 90% B-lineage cells in ALL and has a similar expression pattern to CD19 [78, 79], making anti-CD22 therapies suitable for use in event of resistance developing in patients receiving anti-CD19 therapies or for use as a combination therapy. Similar to the structure UCART19, UCART22 consists of scFv targeting the CD22 antigen, linked to 4-1BB and CD3ζ domains with TALEN-mediated TRAC and CD52 knock-out . Two other TALEN edited UCART products targeting multiple myeloma (MM) antigens have also begun phase I trials—Cellectis’ UCARTCS1 product, targeting the CS1 antigen (NCT04142619) and the B-cell maturation antigen (BCMA)-targeted ALLO-715 product, licensed by Cellectis to Allogene Therapeutics (NCT04093596). As with Cellectis’ earlier UCART products UCARTCS1 and ALLO-751 also utilise multiplex engineering approaches, with mRNA delivered TALENs to knockout TRAC, minimising GvHD and expression of the CAR TAA targeting cassettes following lentiviral transduction incorporating the RQR8 suicide gene . UCARTCS1 further utilises TALEN editing to knock-out CS1 from T-cells prior to CAR-cassette expression, to prevent cross-reactivity with UCART endogenous CS1 expression, as has been demonstrated in other T-cells engineered for CS1-targeting [82,83,84]. Both BCMA and CS1 (also known as SLAMF7/CD319) are highly expressed in MMs, with BCMA expressed in all MM cells in virtually all patients  whilst CS1 is expressed in > 95% of MMs . Antibody immunotherapy trials targeting both these MM antigens (GSK2857916 and elotuzumab respectively) have shown good safety and tolerability [87,88,89], with elotuzumab remission rates of around 80% when administered in combination with lenalidomide and dexamethasone [90, 91], suggesting these new UCART products have promise.
Overall, like ZFNs, TALEN therapies are still in early clinical development, but confidence in design and manufacturing has developed rapidly, leading to four products entering phase I trials in the last quarter of 2019 (Table 2). Cellectis and their licenced partners so far have a monopoly on this editing modality and have focused exclusively on immuno-oncology using well-established target antigens that have shown promise in autologous and antibody-mediated immunotherapies. Combined with the fact that the most established of these studies are already operating in centres across multiple countries it would not be surprising to quickly see TALEN-edited cell therapies surpass the milestones of their ZFN predecessor.
Clinical trials using CRISPR technology
Whilst the CRISPR gene editing system was discovered about 2 years after TALENs, it followed the first TALEN cell therapy into clinical trial just a year later. As with the TALEN therapy UCART19 the gene edited cells used in the first CRISPR trial were also T-cells, but in this instance they were used to treat a patient with advanced non-small cell lung cancer, as part of a phase I trial (NCT02793856) . Like many subsequently registered CRISPR cell therapy trials the focus was on the use of autologous T-cells, edited using CRISPR–Cas9 to knock out the immune checkpoint inhibitor programmed cell death-1 (PD1) prior to reinfusion back into the patient. PD-1 is an inhibitory TCR transiently up-regulated during early activation of T-cells and ordinarily involved in the regulation of immune tolerance, acting to decrease autoimmune reactions, however this inhibitory action also enables cancers to evade immune mediated elimination. Additionally, PD-1 has been recognised as a marker of T-cell exhaustion, as a consequence of perpetual T-cell stimulation, often resulting in tumour re-emergence . Neutralising antibodies for PD-1 or its ligand programmed cell death ligand 1 (PD-L1) have already shown promise as an immunotherapy for a range of cancers, including non-small cell lung cancer [94,95,96,97,98,99], heralding its potential as a target for gene-knockout. Yet, it still remains to be seen if knockout engineered T-cells offer significant enough clinical benefits over PD-1 or PD-L1 antibodies, when considering the laborious and costly process of genetic modification and T-cell propagation. This first-in man phase I study has already preliminarily reported on nine patients and is no longer actively recruiting participants [100, 101]. Split into three cohorts, participants received either 1 × 107/kg, 2 × 107/kg or 4 × 107/kg edited T-cells with the later cohorts receiving the escalated doses. The study reported no serious adverse events at any of the doses, with two patients experiencing 17.6- and 22.0-weeks stable disease, with median progression-free survival of 7.6 weeks. The study concluded that the therapy was safe and larger studies are required to explore effective doses. The indicated safety is promising for other CRISPR trials underway, as several more are in the early stages for a range of different cancers (Table 3).
China is currently leading the way in CRISPR cancer cell therapy trial numbers, with their first competition in the form of the University of Pennsylvania-sponsored ‘NY-ESO-1-redirected CRISPR (TCRendo and PD1) Edited T Cells (NYCE T Cells)’ trial (NCT03399448) . As with the TALEN trials a multiplex genome editing approach is used, combining lentiviral transduction to enable expression of a TCR specific for NY-ESO-1 with triple gene editing using Cas9-complexed guide RNAs targeted to disrupt expression of endogenous TCRα, TCRβ and PD-1. NY-ESO-1 is a highly immunogenic cancer/testis antigen expressed in a range of malignancies, but not ordinarily expressed in normal tissues, besides the placenta and testis [103, 104]. Spontaneous antibody and T-cell reactions are often reported in patients with advanced tumours expressing NY-ESO-1, and in advanced myelomas NY-ESO-1 expression is correlated with tumour proliferation [103,104,105]. Unsurprisingly, given its restricted re-expression profile, many immunotherapy trials targeting NY-ESO-1 are already underway, as comprehensively covered by Thomas et al. . The NYCE multimodal trial, whilst one of the first CRISPR clinical trials, followed on from a phase I/II trial previously published that indicated use of transgenic T-cells with NY-ESO-1 targeting is safe, with cells capable of long-term engraftment (engineered cells detected in 9/10 patients who reached 2-year follow up) and homing to tumour sites, as well as retaining cytotoxic potential over time (for up to a year after infusion) . By combining the previous strategy with endogenous TCR knockout the aim of incorporating the gene editing approaching with NY-ESO-1 targeting is to minimise TCR mispairing and competition of the transduced NY-ESO-1 TCR with endogenous TCRs and potential neo-reactivity or autoimmunity [108, 109], whilst PD-1 knockout is intended to preserve activity of T-cells by preventing exhaustion .
Besides genome editing approaches targeting PD-1 for knockout in immuno-oncology there is significant interest in the potential of CRISPR-edited cell therapies for the treatment of blood disorders. CTX001 is the first in this class to reach the clinical trial stage and was developed in partnership by CRISPR Therapeutics Inc. and Vertex Pharmaceuticals Inc. It is the first industry-sponsored CRISPR therapeutic and competes for the same patient populations as Sangamo’s ZFN products ST-400 and BIV003. It also uses a similar strategy, aiming to abrogate BCL11A expression in autologous CD34+ HSPCs, albeit using CRISPR–Cas9, prior to expansion of edited cells and infusion into the patient. Use of CTX001 in TDT patients was its first application (NCT03655678) about 6 months after the ST-400 trial began, with treatment of SCD patients (NCT03745287) following roughly 2.5 months after the BIV003 trial (see above). Preliminary safety and efficacy data is expected towards the end of 2019, but reports of the first patient treated in the TDT trial are encouraging given they remain transfusion-independent for longer than 4 months post engraftment .
CRISPR therapeutics have recently entered the crowded market of CD19-targeted CAR-Ts with the launch of their first CTX110 clinical trial (previously known as CTX101, NCT04035434). Utilising a multiplex genome editing approach in allogeneic T-cells they have inserted a CD19-targeted CAR into the TRAC locus, simultaneously eliminating TCR expression and yielding consistent CAR expression. Additionally, they have knocked out the β2-microglobulin (B2M) gene to eliminate MHC class I expression, with the aim of improving CAR-T durability. CTX110 represents the first gene-edited cell therapy with a targeted insertion to be reported entering the clinic, although it was originally intended to begin clinical trial in 2018. Despite the relative technical difficulty of high-efficiency gene insertion approaches CRISPR Therapeutics report consistent results of 54–66% cells yielding all three desired edits (B2M and TRAC knockouts and CAR expression from the TRAC locus) across five different donors, indicating such a strategy holds promise for their future pipeline .
Finally, in a throwback to the first gene-edited cell therapy clinical trial, there is also interest in CRISPR-editing of CCR5 in HIV patients, with results of the first patient to receive a bone marrow transplant of CCR5-KO CD34+ HPSCs recently published . Interestingly this report is one of the few CRISPR platforms so far to detail the method of delivery for the editing agent, in this case a ribonucleoprotein complex comprising Cas9 protein and their previously designed gRNAs targeting CCR5 , while most other platforms use proprietary delivery methods. The results demonstrated an acceptable safety profile, with no immunogenicity and no detected off-target effects following analysis of whole-genome sequencing data for translocations or long-range deletions. Whilst this data would suggest that gene editing technologies have now gone full circle, potentially preparing to eliminate the need for ZFNs, these results are limited to a single case report for an individual patient and demonstrate relatively low HPSC editing efficiency (17.8% of cells) compared to their predecessor (54–67% ) demonstrating there is some way to go before this strategy can compete with more established methods.
Off-target effects and preclinical developments in gene editing strategies
One factor that remains a fundamental concern with any gene edited cell therapy and becomes increasingly so as multiplex approaches are progressively adopted, is the potential for off-target effects as a result of nuclease activity at unintended homologous sites; and any downstream consequences arising from such off-target activity. As the range of cell therapies available to treat patients advances over time, so too will the range of targets for editing. Consequently, the ability to accurately identify potential off-target sites becomes increasingly important. Currently, a growing range of strategies to address off-target activity by assessing secondary target sites exist, including SELEX, Digenome-seq, GUIDE-seq, CIRCLE-seq and DISCOVER-seq [115,116,117,118,119]. Mutagenesis levels within cells at the identified sites are preferentially examined by these deep sequencing and targeted PCR approaches, as opposed to whole genome sequencing (WGS) which lacks adequate sequencing depth to detect low frequency mutations in bulk populations of cells. This was demonstrated in the early SCID-X1 retroviral-mediated gene therapy trials where LMO2 proto-oncogene activation in hSCs was estimated to be present in between only 1 and 10 of the ≥ 1 × 106 transduced cells transplanted to the patients who subsequently went on to develop leukaemia . That said, WGS approaches are suitable in instances examining single cell-derived clones such as human induced pluripotent stem cells (hiPSCs), which can be used for clonal expansion prior to therapy, as is the case for upcoming iCART or iPSC-derived NK cells [120, 121] (for details see “Future perspectives of gene edited cell therapies in the clinic” section).
It is important to note that off-target concerns will vary depending on the cell therapy, with risks restricted to only a subset of the genome relevant to the cell type . For example, in the discussed therapies for treating haemoglobinopathies concerns would be related to off-target effects that would impact cells of the haematopoietic lineage, so identifying possible secondary binding sites and assessing their potential impact in those cell types would provide the necessary reassurance of therapeutic safety. This would require screening for and rejecting strategies that present a risk of tumour suppressor gene mutations for instance, as this could result in leukaemia downstream. However off-target effects in a muscle-specific gene, such as dystrophin, which to our knowledge is neither expressed nor necessary in hematopoietic lineage cells may be considered tolerable. Conversely, mutations found in the β-globin gene may be considered tolerable in a muscular dystrophy cell therapy . This is akin to the accepted risk–benefit analysis of side effects in the clinic, where drugs such as small-molecules and antibodies can interact with off-target, structurally similar proteins but the on-target efficacy is sufficiently beneficial for these risks to be deemed acceptable. Here, use of a cell therapy approach is beneficial, because gene editing is restricted only to known populations of ex vivo cultured cells, which can be easily screened, rather than the requirement to ensure successful delivery of the editing agent to specific tissues and more invasive procedures for downstream screening such as biopsies, as with in vivo gene editing .
Finally, improved in silico approaches to predict genome wide off-target activity are set to continue alongside the development of machine-learning methods which are benefitting from the increasing availability of large-scale genome-editing activity datasets [124,125,126,127]. Together with these advances in predicting potential off-target effects researchers are continually pursuing approaches to improve genomic targeting precision. For ZFNs this has included improving cleavage activity by reducing undesired homodimerization of the ZFN pairs through modification of FokI domains . TALEN technologies have focused on virtually eliminating low frequency off-site effects by replacing naturally occurring repeat-variable di-residues (RVDs) within modular TALE arrays (which are responsible for specifying the target nucleotide for binding), using unconventional TALEs not present within the natural TALE repertoire [129,130,131]. These have significantly improved targeting specificity and offer a more simplified means to facilitate multiplex editing strategies for therapeutic use. In the CRISPR field a range of strategies have been tested to improve specificity, including decreasing the gRNA length with truncated gRNAs  and engineered Cas9 variants with reduced non-specific protein–DNA interactions such as structure-guided engineered Cas9s [133, 134]. Other strategies have sought to build on the success of the paired approaches used by their ZFN and TALEN predecessors by using Cas9-nickases (Cas9-n). These modified Cas9 enzymes have been mutated at the nuclease active site to yield single rather than DSBs and can be paired to generate composite DSBs offering double the genome editing specificity of traditional Cas9 approaches [135, 136]. A new approach building on Cas9-ns called ‘prime editing’ may in the future be of particular interest for multiplex strategies or targeted insertion/repair approaches. Prime editing utilises a reverse transcriptase enzyme fused to both an RNA-programmable Cas9-n and a prime editing guide RNA (pegRNA) . This enables genetic information to be directly copied from the extending pegRNA into the target genomic locus without relying on DNA repair or exogenous donor templates, with the higher efficiency of this approach demonstrated by the 270-fold higher ratio of editing:indels seen when prime editing was evaluated relative to a comparable Cas9-initiated HDR strategy in 293T cells . Prime editing is unlikely to be used to make the large insertions or deletions current gene editing/CRISPR approaches are implementing because the long RNA strands required would likely be enzymatically degraded within cells before editing could be achieved. The versatility of prime editing holds significant promise for a range of genetic diseases caused by targetable multi-base mutations such as sickle cell anaemia, Duchenne muscular dystrophy, cystic fibrosis and Tay–Sachs disease and further development of this technique will be followed with interest by the cell therapy community.
Future perspectives of gene edited cell therapies in the clinic
Whilst gene editing in the context of cell therapies has mostly concentrated on immunooncology or blood disorders, recent advances of human induced pluripotent stem cell (hiPSC)-derived therapies to first-in-man studies indicate an increased breadth in application is forthcoming. hiPSCs, like embryonic stem cells (ESCs), have unlimited self-renewal potential and can differentiate into all adult cell types, but as they are derived from somatic cells, they can be generated from donors whose genetic characteristics and health records are well-established, without the ethical implications of ESCs. Several first-in-man studies using hiPSC-derived cells are already underway to treat patients with a variety of aetiologies including dopaminergic neurons for Parkinson’s disease [138,139,140,141], retinal pigment epithelial (RPE) cells and corneal cells for eye diseases [142,143,144,145,146], cardiac progenitors for heart failure ([147, 148] and NCT03763136) and mesenchymal stem cells for steroid resistant GvHD (NCT02923375 ). Many of these therapies have reached the clinic sooner than would have been anticipated as a result of recent legislative changes in Japan, which allowed stem cell treatments fast track approval to clinical use on the basis of safety and efficacy tests using only small patient numbers [150,151,152]. Nevertheless, wider clinical use of hiPSC-therapies could have been limited by the prohibitive costs and time associated with the development of autologous hiPSC lines. An autologous strategy was used for the first patient treated with a hiPSC-derived cell therapy, in this case RPE cells for macular degeneration , and this cost around $1 million, and took over 10 months to produce the cells for transplant . Fortunately, all subsequent clinical use has relied on allogeneic hiPSCs, with the first allogeneic hiPSC-derived cell therapy also using RPE cells, following the same procedure as its autologous predecessor, but with time to surgery reduced to a month and the cost reduced to $200 k per patient [146, 153].
The majority of allogeneic hiPSC lines used have come from the Center for iPS Cell Research and Application at Kyoto University (CiRA). CiRA has been focused on setting up allogeneic hiPSC stocks by selecting rare donors that are homozygous at the three major HLA gene loci, to generate a pool of safe clinical grade hiPSC clones . This would lead to reduced risk of immune rejection following transplantation of differentiated cells if the recipient HLA haplotypes are matched. Once completed the bank is estimated to offer coverage for up to 90% of the Japanese population, but at the cost of comprehensive safety and characterisation testing of as many as 140 lines, following screening of > 150,000 donors. Japan has a less genetically diverse population than the rest of the world, so whilst other banks including the UK based Cell & Gene Therapy Catapult and Cellular Dynamics Inc in the U.S. are also generating hiPSCs from HLA homozygous donors a large number of lines would need to be generated to approach the same level of coverage globally [154, 155].
A competing approach that shows great promise and may herald the next wave of gene-edited cell therapies could involve utilising hiPSC lines that have undergone gene editing to modify the HLA genes. HLA pseudo-homozygous hiPSC lines were recently generated through CRISPR–Cas9 editing of heterozygous HLA class I donor derived lines . Using a precise allele-specific multiplex approach biallelic deletion of HLA-A and HLA-B genes, but retention of a single HLA-C allele was achieved. This approach offers a solution to hurdles in other HLA editing approaches which aimed to create ‘hypoimmunogenic’ hiPSCs by knock-out of the B2M gene . Whilst hypoimmunogenic strategies would prevent immune rejection by depleting all HLA loci, it also precludes natural immune destruction of oncogenically transformed or infected cells post-transplant, as well as exposing these cells to potential destruction by natural killers cells as a result of their HLA-C deficiency [157, 158]. It is predicted that just 12 of these alternative ‘pseudo-homozygous HLA-C retained’ hiPSC lines would be immunologically compatible with > 90% of the global population, which would greatly enhance hiPSC-derived cell therapy applications. Given that CTX110, which involves B2M knockout by CRISPR–Cas9, has already entered phase I trials in the USA and Australia it seems possible regulators could accept additional HLA-edited cell therapies in the clinic in future.
While the debate on the best means to enable globally compatible immune coverage continues, new ‘off-the-shelf’ hiPSC cell therapies suitable for mass production are already starting to emerge in the immunooncology arena. US-based Fate Therapeutics’ (FT) first “Off-the-shelf” iPSC-derived NK cell products FT500 and FT516 are already in phase I clinical trials (NCT03841110, NCT04023071) and their first iPSC-derived CAR-T cell product FT819 looks set to be the first gene-edited hiPSC cell therapy to enter the clinic. It follows a similar strategy to autologous CD19 CAR-Ts and CTX110 in particular. FT819 is differentiated from a hiPSC clonal master line that has undergone CRISPR-mediated disruption of TCR expression by insertion of a novel 1XX CAR signalling domain into the TRAC locus in a similar 2-in-1 TCR-knockout/CAR-knock-in strategy, simultaneously mitigating GvHD risk whilst providing potent targeting [159, 160]. FT819 will compete with Takeda Pharmaceutical Company Ltd, who are in a 10-year partnership with CiRA to develop iPSCs clinically, to be the first hiPSC-derived CAR-T (iCART), as Takeda plan to start clinical trials with their first iCART products in 2021, a CD19-targeted CAR amongst those reported . The real promise of gene edited hiPSC-derived cell therapies has yet to be fulfilled, but editing prior to differentiation into a wide range of cell therapies may ultimately make universal therapies more economically viable in the future, though there is clearly some work to be done to bring down the costs of differentiation protocols before this field matches pace with their edited primary cell counterparts.
Thus far editing strategies entering clinical trial have predominantly focused on gene disruption, either to enable deletion of protein expression for therapeutic gain (e.g. PD-1, CCR5) or for targeted correction of disease phenotypes by compensatory gene reactivation (BCL11A) with many of the therapies on the horizon taking similar approaches. Whilst increasingly sophisticated multiplex approaches are also beginning to emerge, with CTX110 the first targeted gene insertion to enter trial, much more research is likely to be needed before more sophisticated safety features such as reporter genes or suicide cassettes become common place. UCART19 and UCART123 have likely already paved the way for regulatory bodies to accept strategies incorporating suicide genes, with their epitope marker/suicide gene RQR8 already employed as part of their multiplex engineering approach. Moreover, as reporter genes and in vivo imaging become increasingly employed to track cell fate in autologous cell therapy approaches [5, 9, 162,163,164,165,166,167], it is likely that future allogeneic and off-the-shelf gene edited therapies, particularly those derived from iPSCs, will consider incorporating these strategies to offer regulators reassuring safety data by longitudinal therapy tracking.
Availability of data and materials
Caplan AI (2017) Mesenchymal stem cells: time to change the name! Stem Cells Transl Med 6:1445–1451. https://doi.org/10.1002/sctm.17-0051
Heathman TR, Nienow AW, McCall MJ et al (2015) The translation of cell-based therapies: clinical landscape and manufacturing challenges. Regen Med 10:49–64. https://doi.org/10.2217/rme.14.73
Bioinformant cell therapy industry database. https://bioinformant.com/product/cell-therapy-industry-database/. Accessed 3 Oct 2019
Cuende N, Rasko JEJ, Koh MBC et al (2018) Cell, tissue and gene products with marketing authorization in 2018 worldwide. Cytotherapy 20:1401–1413. https://doi.org/10.1016/j.jcyt.2018.09.010
Krekorian M, Fruhwirth GO, Srinivas M et al (2019) Imaging of T-cells and their responses during anti-cancer immunotherapy. Theranostics. https://doi.org/10.7150/thno.37924
Fruhwirth GO, Kneilling M, de Vries IJM et al (2018) The potential of in vivo imaging for optimization of molecular and cellular anti-cancer immunotherapies. Mol Imaging Biol. https://doi.org/10.1007/s11307-018-1254-3
Volpe A, Kurtys E, Fruhwirth GO (2018) Cousins at work: how combining medical with optical imaging enhances in vivo cell tracking. Int J Biochem Cell Biol 102:40–50. https://doi.org/10.1016/j.biocel.2018.06.008
Jones BS, Lamb LS, Goldman F, Di Stasi A (2014) Improving the safety of cell therapy products by suicide gene transfer. Front Pharmacol 5:254. https://doi.org/10.3389/fphar.2014.00254
Keu KV, Witney TH, Yaghoubi S et al (2017) Reporter gene imaging of targeted T cell immunotherapy in recurrent glioma. Sci Transl Med. https://doi.org/10.1126/scitranslmed.aag2196
Goswami R, Subramanian G, Silayeva L et al (2019) Gene therapy leaves a vicious cycle. Front Oncol 9:297. https://doi.org/10.3389/fonc.2019.00297
Saudemont A, Jespers L, Clay T (2018) Current status of gene engineering cell therapeutics. Front Immunol 9:153. https://doi.org/10.3389/fimmu.2018.00153
Maggio I, Gonçalves MAFV (2015) Genome editing at the crossroads of delivery, specificity, and fidelity. Trends Biotechnol 33:280–291. https://doi.org/10.1016/J.TIBTECH.2015.02.011
Cavazzana-calvo AM, Hacein-bey S, Saint Basile GD et al (2000) Gene therapy of human severe combined immunodeficiency (SCID)-X1 disease. Science (80-) 288:669–672
Leonard MDWJ (1996) The molecular basis of X-linked severe combined immunodeficiency: defective cytokine receptor signaling. Annu Rev Med 47:229–239. https://doi.org/10.1146/annurev.med.47.1.229
Hacein-Bey-Abina S, Von Kalle C, Schmidt S et al (2003) LMO2-associated clonal T cell proliferation in two patients after gene therapy for SCID-X1. Science (80-) 302:415–419
Choulika A, Perrin A, Dujon B, Nicolas JF (1995) Induction of homologous recombination in mammalian chromosomes by using the I-SceI system of Saccharomyces cerevisiae. Mol Cell Biol 15:1968–1973. https://doi.org/10.1128/mcb.15.4.1968
Bitinaite J, Wah DA, Aggarwal AK, Schildkraut I (1998) FokI dimerization is required for DNA cleavage. Proc Natl Acad Sci 95:10570–10575
Segal DJ, Dreier B, Beerli RR, Barbas CF (1999) Toward controlling gene expression at will: selection and design of zinc finger domains recognizing each of the 5′-GNN-3′ DNA target sequences. Proc Natl Acad Sci USA 96:2758–2763. https://doi.org/10.1073/pnas.96.6.2758
Beerli RR, Barbas CF (2002) Engineering polydactyl zinc-finger transcription factors. Nat Biotechnol 20:135–141. https://doi.org/10.1038/nbt0202-135
Gonzalez B, Schwimmer LJ, Fuller RP et al (2010) Modular system for the construction of zinc-finger libraries and proteins. Nat Protoc 5:791–810. https://doi.org/10.1038/nprot.2010.34
Genovese P, Schiroli G, Escobar G et al (2014) Targeted genome editing in human repopulating haematopoietic stem cells. Nature 510:235–240. https://doi.org/10.1038/nature13420
Poirot L, Philip B, Schiffer-Mannioui C et al (2015) Multiplex genome-edited T-cell manufacturing platform for “Off-the-Shelf” adoptive T-cell immunotherapies. Cancer Res 75:3853–3864. https://doi.org/10.1158/0008-5472.CAN-14-3321
Mock U, Machowicz R, Hauber I et al (2015) mRNA transfection of a novel TAL effector nuclease (TALEN) facilitates efficient knockout of HIV co-receptor CCR5. Nucleic Acids Res 43:5560–5571. https://doi.org/10.1093/nar/gkv469
Moscou MJ, Bogdanove AJ (2009) A simple cipher governs DNA recognition by TAL effectors. Science (80-) 326:1501. https://doi.org/10.1126/science.1178817
Boch J, Scholze H, Schornack S et al (2009) Breaking the code of DNA binding specificity of TAL-type III effectors. Science (80-) 326:1509–1512. https://doi.org/10.1126/science.1178811
Schumann K, Lin S, Boyer E et al (2015) Generation of knock-in primary human T cells using Cas9 ribonucleoproteins. Proc Natl Acad Sci USA 112:10437–10442. https://doi.org/10.1073/pnas.1512503112
Kim S, Kim D, Cho SW et al (2014) Highly efficient RNA-guided genome editing in human cells via delivery of purified Cas9 ribonucleoproteins. Genome Res 24:1012–1019. https://doi.org/10.1101/gr.171322.113
Hendel A, Bak RO, Clark JT et al (2015) Chemically modified guide RNAs enhance CRISPR-Cas genome editing in human primary cells. Nat Biotechnol 33:985–989. https://doi.org/10.1038/nbt.3290
Hu JH, Davis KM, Liu DR (2016) Chemical biology approaches to genome editing: understanding, controlling, and delivering programmable nucleases. Cell Chem Biol 23:57–73. https://doi.org/10.1016/J.CHEMBIOL.2015.12.009
Yin J, Liu M, Liu Y et al (2019) Optimizing genome editing strategy by primer-extension-mediated sequencing. Cell Discov 5:18. https://doi.org/10.1038/s41421-019-0088-8
Gupta RM, Musunuru K (2014) Expanding the genetic editing tool kit: ZFNs, TALENs, and CRISPR–Cas9. J Clin Invest 124:4154–4161. https://doi.org/10.1172/JCI72992
Kass EM, Jasin M (2010) Collaboration and competition between DNA double-strand break repair pathways. FEBS Lett 584:3703–3708. https://doi.org/10.1016/J.FEBSLET.2010.07.057
Holmes MC, Reik A, Rebar EJ et al (2017) A potential therapy for beta-thalassemia (ST-400) and sickle cell disease (BIVV003). Blood 130:2066
Wechsler T, Meyer KE, Spratt SK et al (2015) ZFN-mediated gene targeting at the albumin locus in liver results in therapeutic levels of human FIX in mice and non-human primates. Blood 126:200
Tebas P, Stein D, Tang WW et al (2014) Gene editing of CCR5 in autologous CD4 T Cells of persons infected with HIV. N Engl J Med 370:901–910. https://doi.org/10.1056/NEJMoa1300662
Loetscher P, Uguccioni M, Bordoli L et al (1998) CCR5 is characteristic of Th1 lymphocytes. Nature 391:344–345. https://doi.org/10.1038/34814
Huang Y, Paxton WA, Wolinsky SM et al (1996) The role of a mutant CCR5 allele in HIV-1 transmission and disease progression. Nat Med 2:1240–1243. https://doi.org/10.1038/nm1196-1240
Liu R, Paxton WA, Choe S et al (1996) Homozygous defect in HIV-1 coreceptor accounts for resistance of some multiply-exposed individuals to HIV-1 infection. Cell 86:367–377. https://doi.org/10.1016/S0092-8674(00)80110-5
Samson M, Libert F, Doranz BJ et al (1996) Resistance to HIV-1 infection in Caucasian individuals bearing mutant alleles of the CCR-5 chemokine receptor gene. Nature 382:722–725. https://doi.org/10.1038/382722a0
Fätkenheuer G, Pozniak AL, Johnson MA et al (2005) Efficacy of short-term monotherapy with maraviroc, a new CCR5 antagonist, in patients infected with HIV-1. Nat Med 11:1170–1172. https://doi.org/10.1038/nm1319
Berro R, Klasse PJ, Moore JP, Sanders RW (2012) V3 determinants of HIV-1 escape from the CCR5 inhibitors Maraviroc and Vicriviroc. Virology 427:158–165. https://doi.org/10.1016/J.VIROL.2012.02.006
Egger M, May M, Chêne G et al (2002) Prognosis of HIV-1-infected patients starting highly active antiretroviral therapy: a collaborative analysis of prospective studies. Lancet 360:119–129. https://doi.org/10.1016/S0140-6736(02)09411-4
Perez EE, Wang J, Miller JC et al (2008) Establishment of HIV-1 resistance in CD4+ T cells by genome editing using zinc-finger nucleases. Nat Biotechnol 26:808–816. https://doi.org/10.1038/nbt1410
Yukl SA, Boritz E, Busch M et al (2013) Challenges in detecting HIV persistence during potentially curative interventions: a study of the berlin patient. PLoS Pathog 9:e1003347. https://doi.org/10.1371/journal.ppat.1003347
Mandavilli A (2019) H.I.V. is reported cured in a second patient, a milestone in the Global AIDS Epidemic. New York Times
Hütter G, Nowak D, Mossner M et al (2009) Long-term control of HIV by CCR5 Delta32/Delta32 stem-cell transplantation. N Engl J Med 360:692–698. https://doi.org/10.1056/NEJMoa0802905
Li L, Krymskaya L, Wang J et al (2013) Genomic editing of the HIV-1 coreceptor CCR5 in adult hematopoietic stem and progenitor cells using zinc finger nucleases. Mol Ther 21:1259–1269. https://doi.org/10.1038/mt.2013.65
DiGiusto DL, Cannon PM, Holmes MC et al (2016) Preclinical development and qualification of ZFN-mediated CCR5 disruption in human hematopoietic stem/progenitor cells. Mol Ther Methods Clin Dev 3:16067. https://doi.org/10.1038/MTM.2016.67
Gupta RK, Abdul-Jawad S, McCoy LE et al (2019) HIV-1 remission following CCR5Δ32/Δ32 haematopoietic stem-cell transplantation. Nature 568:244–248. https://doi.org/10.1038/s41586-019-1027-4
The Lancet HIV (2019) Like London buses, two putative cure cases arrive at once. Lancet HIV 6:e205. https://doi.org/10.1016/S2352-3018(19)30086-4
Sangamo’s genome editing program for hemoglobinopathies to transfer to Biogen’s Spin-Off Bioverativ | Sangamo Therapeutics, Inc. https://investor.sangamo.com/news-releases/news-release-details/sangamos-genome-editing-program-hemoglobinopathies-transfer. Accessed 3 Oct 2019
Liu N, Hargreaves VV, Hong J et al (2017) Fetal hemoglobin (HbF) silencer BCL11A Acts through a novel DNA-motif in the gamma-globin promoters, simplifying the model for hemoglobin switching. Blood 130:283
Xu J, Bauer DE, Peng C, Smith EC, Orkin SH (2013) Identification of BCL11A structure-function domains for fetal hemoglobin silencing. Blood. https://doi.org/10.1182/blood.V122.21.435.435
Moran K, Ling H, Lessard S et al (2018) Ex vivo gene-edited cell therapy for sickle cell disease: disruption of the BCL11A erythroid enhancer with zinc finger nucleases increases fetal hemoglobin in plerixafor mobilized human CD34+ cells. Blood 132:2190. https://doi.org/10.1182/BLOOD-2018-99-116998
Sangamo provides clinical development update including early phase 1/2 beta thalassemia gene-edited cell therapy data | Sangamo Therapeutics, Inc. https://investor.sangamo.com/news-releases/news-release-details/sangamo-provides-clinical-development-update-including-early. Accessed 4 Aug 2019
Thein SL (2013) The molecular basis of β-thalassemia. Cold Spring Harb Perspect Med 3:a011700. https://doi.org/10.1101/cshperspect.a011700
Hirayama AV, Gauthier J, Hay KA et al (2018) Factors impacting progression-free survival after CD19-specific CAR-T cell therapy for relapsed/refractory aggressive B-cell non-Hodgkin lymphoma. Blood 132:1681. https://doi.org/10.1182/BLOOD-2018-99-115126
Gill SI, Vides V, Frey NV et al (2018) Prospective clinical trial of anti-CD19 CAR T cells in combination with ibrutinib for the treatment of chronic lymphocytic leukemia shows a high response rate. Blood 132:298. https://doi.org/10.1182/BLOOD-2018-99-115418
Grupp SA, Frey NV, Aplenc R et al (2013) T cells engineered with a chimeric antigen receptor (CAR) targeting CD19 (CTL019) produce significant in vivo proliferation, complete responses and long-term persistence without Gvhd in children and adults with relapsed, refractory ALL. Blood 122:67
Schuster SJ, Bishop MR, Tam CS et al (2019) Tisagenlecleucel in adult relapsed or refractory diffuse large B-cell lymphoma. N Engl J Med 380:45–56. https://doi.org/10.1056/NEJMoa1804980
Neelapu SS, Locke FL, Bartlett NL et al (2017) Axicabtagene ciloleucel CAR T-cell therapy in refractory large B-cell lymphoma. N Engl J Med 377:2531–2544. https://doi.org/10.1056/NEJMoa1707447
Harrison RP, Zylberberg E, Ellison S, Levine BL (2019) Chimeric antigen receptor-T cell therapy manufacturing: modelling the effect of offshore production on aggregate cost of goods. Cytotherapy 21:224–233. https://doi.org/10.1016/j.jcyt.2019.01.003
Derniame S, Zhan H, Poirot L et al (2014) Multiplex genome editing as a platform for “Off-the-Shelf” adoptive CAR T-cell immunotherapies. Blood 124:1111
Qasim W, Amrolia PJ, Samarasinghe S et al (2015) First clinical application of Talen engineered universal CAR19 T cells in B-ALL. Blood 126:2046
Philip B, Kokalaki E, Mekkaoui L et al (2014) A highly compact epitope-based marker/suicide gene for easier and safer T-cell therapy. Blood 124:1277–1287. https://doi.org/10.1182/blood-2014-01-545020
Zhao Y, Su H, Shen X et al (2017) The immunological function of CD52 and its targeting in organ transplantation. Inflamm Res 66:571–578. https://doi.org/10.1007/s00011-017-1032-8
Qasim W, Ciocarlie O, Adams S et al (2017) Preliminary results of UCART19, an allogeneic anti-CD19 CAR T-cell product in a first-in-human trial (PALL) in pediatric patients with CD19+ relapsed/refractory B-cell acute lymphoblastic leukemia. Blood 130:1271
Graham C, Yallop D, Jozwik A et al (2017) Preliminary results of UCART19, an allogeneic anti-CD19 CAR T-cell product, in a first-in-human trial (CALM) in adult patients with CD19+ relapsed/refractory B-cell acute lymphoblastic leukemia. Blood 130:887
Benjamin R, Graham C, Yallop D et al (2018) Preliminary data on safety, cellular kinetics and anti-leukemic activity of UCART19, an allogeneic anti-CD19 CAR T-cell product, in a pool of adult and pediatric patients with high-risk CD19+ relapsed/refractory B-cell acute lymphoblastic leukemia. Blood 132:896. https://doi.org/10.1182/BLOOD-2018-99-111356
Chavez JC, Bachmeier C, Kharfan-Dabaja MA (2019) CAR T-cell therapy for B-cell lymphomas: clinical trial results of available products. Ther Adv Hematol 10:2040620719841581. https://doi.org/10.1177/2040620719841581
Cai T, Galetto R, Gouble A et al (2016) Pre-clinical studies of anti-CD123 CAR-T cells for the treatment of blastic plasmacytoid dendritic cell neoplasm (BPDCN). Blood 128:4039
Guzman ML, Sugita M, Zong H et al (2016) Allogeneic Tcrα/β deficient CAR T-cells targeting CD123 prolong overall survival of AML patient-derived xenografts. Blood 128:765
(2020) First patient dosed with Cellectis’ new allogeneic UCART123 product candidate for relapsed/refractory acute myeloid leukemia | Cellectis. In: Press Release. https://www.cellectis.com/en/press/first-patient-dosed-with-cellectis-new-allogeneic-ucart123-product-candidate-for-relapsed-refractory-acute-myeloid-leukemia/. Accessed 22 Jan 2020
(2017) Cellectis reports clinical hold of UCART123 studies | Cellectis. http://www.cellectis.com/en/press/cellectis-reports-clinical-hold-of-ucart123-studies/. Accessed 1 June 2019
(2017) FDA lifts clinical hold on cellectis phase 1 clinical trials with UCART123 in AML and BPDCN | Cellectis. http://www.cellectis.com/en/press/fda-lifts-clinical-hold-on-cellectis-phase-1-clinical-trials-with-ucart123-in-aml-and-bpdcn. Accessed 1 June 2019
(2018) Approval of UCART123 amendment in AML to accelerate clinical development | Cellectis. https://www.cellectis.com/en/press/approval-of-ucart123-amendment-in-aml-to-accelerate-clinical-development/. Accessed 1 June 2019
(2019) 1st patient dosed with Cellectis’ allogeneic UCART22 in relapsed/refractory B-cell acute lymphoblastic leukemia | Cellectis. In: Press Release. https://www.cellectis.com/en/press/1st-patient-dosed-with-cellectis-allogeneic-ucart22-in-relapsed-refractory-b-cell-acute-lymphoblastic-leukemia/. Accessed 22 Jan 2020
Raponi S, Stefania De Propris M, Intoppa S et al (2011) Flow cytometric study of potential target antigens (CD19, CD20, CD22, CD33) for antibody-based immunotherapy in acute lymphoblastic leukemia: analysis of 552 cases. Leuk Lymphoma 52:1098–1107. https://doi.org/10.3109/10428194.2011.559668
Shah NN, Stevenson MS, Yuan CM et al (2015) Characterization of CD22 expression in acute lymphoblastic leukemia. Pediatr Blood Cancer 62:964–969. https://doi.org/10.1002/pbc.25410
Wells J, Cai T, Schiffer-Manniou, Cécile Filipe S et al (2017) Pre-clinical activity of allogeneic anti-CD22 CAR-T cells for the treatment of B-cell acute lymphoblastic leukemia. In: American Society of Hematology 59th Annual Meeting
Sommer C, Boldajipour B, Kuo TC et al (2019) Preclinical evaluation of allogeneic CAR T cells targeting BCMA for the treatment of multiple myeloma. Mol Ther 27:1126–1138. https://doi.org/10.1016/j.ymthe.2019.04.001
Mathur R, Zhang Z, He J, et al (2017) Universal SLAMF7-specific CAR T-cells as treatment for multiple myeloma. In: American Society of Hematology 59th Annual Meeting. p Abstract 502
Patel KK (2019) Universal SLAMF7-specific CAR T-cells (UCARTCS1) for multiple myeloma. In: 1st international workshop on CAR-T (iwCAR-T). p Session VII: CAR-T in Multiple Myeloma
Gogishvili T, Danhof S, Prommersberger S et al (2017) SLAMF7-CAR T cells eliminate myeloma and confer selective fratricide of SLAMF7 + normal lymphocytes. Blood 130:2838–2847. https://doi.org/10.1182/blood-2017-04-778423
Tai Y-T, Li X-F, Breitkreutz I et al (2006) Role of B-cell-activating factor in adhesion and growth of human multiple myeloma cells in the bone marrow microenvironment. Cancer Res 66:6675–6682. https://doi.org/10.1158/0008-5472.CAN-06-0190
Hsi ED, Steinle R, Balasa B et al (2008) CS1, a potential new therapeutic antibody target for the treatment of multiple myeloma. Clin Cancer Res 14:2775–2784. https://doi.org/10.1158/1078-0432.CCR-07-4246
Trudel S, Lendvai N, Popat R et al (2019) Antibody-drug conjugate, GSK2857916, in relapsed/refractory multiple myeloma: an update on safety and efficacy from dose expansion phase I study. Blood Cancer J 9:37. https://doi.org/10.1038/s41408-019-0196-6
Trudel S, Lendvai N, Popat R et al (2018) Targeting B-cell maturation antigen with GSK2857916 antibody-drug conjugate in relapsed or refractory multiple myeloma (BMA117159): a dose escalation and expansion phase 1 trial. Lancet Oncol 19:1641–1653. https://doi.org/10.1016/S1470-2045(18)30576-X
Zonder JA, Mohrbacher AF, Singhal S et al (2012) A phase 1, multicenter, open-label, dose escalation study of elotuzumab in patients with advanced multiple myeloma. Blood 120:552–559. https://doi.org/10.1182/blood-2011-06-360552
Lonial S, Dimopoulos M, Palumbo A et al (2015) Elotuzumab therapy for relapsed or refractory multiple myeloma. N Engl J Med 373:621–631. https://doi.org/10.1056/NEJMoa1505654
Lonial S, Vij R, Harousseau J-L et al (2012) Elotuzumab in combination with lenalidomide and low-dose dexamethasone in relapsed or refractory multiple myeloma. J Clin Oncol 30:1953–1959. https://doi.org/10.1200/JCO.2011.37.2649
Cyranoski David (2016) CRISPR gene editing tested in a person. Nature 539:479
Wherry EJ, Kurachi M (2015) Molecular and cellular insights into T cell exhaustion. Nat Rev Immunol 15:486–499. https://doi.org/10.1038/nri3862
Hamid O, Robert C, Daud A et al (2013) Safety and tumor responses with lambrolizumab (anti-PD-1) in melanoma. N Engl J Med 369:134–144. https://doi.org/10.1056/NEJMoa1305133
Brahmer JR, Tykodi SS, Chow LQM et al (2012) Safety and activity of anti-PD-L1 antibody in patients with advanced cancer. N Engl J Med 366:2455–2465. https://doi.org/10.1056/NEJMoa1200694
Brahmer JR, Drake CG, Wollner I et al (2010) Phase I study of single-agent anti-programmed death-1 (MDX-1106) in refractory solid tumors: safety, clinical activity, pharmacodynamics, and immunologic correlates. J Clin Oncol 28:3167–3175. https://doi.org/10.1200/JCO.2009.26.7609
Topalian SL, Hodi FS, Brahmer JR et al (2012) Safety, activity, and immune correlates of anti-PD-1 antibody in cancer. N Engl J Med 366:2443–2454. https://doi.org/10.1056/NEJMoa1200690
Taube JM, Klein A, Brahmer JR et al (2014) Association of PD-1, PD-1 ligands, and other features of the tumor immune microenvironment with response to anti-PD-1 therapy. Clin Cancer Res 20:5064–5074. https://doi.org/10.1158/1078-0432.CCR-13-3271
Reck M, Rodríguez-Abreu D, Robinson AG et al (2016) Pembrolizumab versus chemotherapy for PD-L1-positive non-small-cell lung cancer. N Engl J Med 375:1823–1833. https://doi.org/10.1056/NEJMoa1606774
Lu Y, Xue J, Deng T et al (2018) A phase I trial of PD-1 deficient engineered T cells with CRISPR/Cas9 in patients with advanced non-small cell lung cancer. J Clin Oncol 36:3050. https://doi.org/10.1200/JCO.2018.36.15_suppl.3050
Lu Y, Huang M, Deng T et al (2018) Abstract CT133: a phase I trial of PD-1 deficient engineered T cells with CRISPR/Cas9 in patients with advanced non-small cell lung cancer with PD-L1 expression. In: Clinical Trials. American Association for Cancer Research, p CT133
Reardon S (2016) First CRISPR clinical trial gets green light from US panel. Nat News. https://doi.org/10.1038/nature.2016.20137
Gnjatic S, Nishikawa H, Jungbluth AA et al (2006) NY-ESO-1: review of an immunogenic tumor antigen. Adv Cancer Res 95:1–30. https://doi.org/10.1016/S0065-230X(06)95001-5
Simpson AJG, Caballero OL, Jungbluth A et al (2005) Cancer/testis antigens, gametogenesis and cancer. Nat Rev Cancer 5:615–625. https://doi.org/10.1038/nrc1669
Van Rhee F, Szmania SM, Zhan F et al (2005) NY-ESO-1 is highly expressed in poor-prognosis multiple myeloma and induces spontaneous humoral and cellular immune responses. Blood 105:3939–3944. https://doi.org/10.1182/blood-2004-09-3707
Thomas R, Al-Khadairi G, Roelands J et al (2018) NY-ESO-1 based immunotherapy of cancer: current perspectives. Front Immunol 9:947. https://doi.org/10.3389/fimmu.2018.00947
Rapoport AP, Stadtmauer EA, Binder-Scholl GK et al (2015) NY-ESO-1-specific TCR-engineered T cells mediate sustained antigen-specific antitumor effects in myeloma. Nat Med 21:914–921. https://doi.org/10.1038/nm.3910
van Loenen MM, de Boer R, Amir AL et al (2010) Mixed T cell receptor dimers harbor potentially harmful neoreactivity. Proc Natl Acad Sci USA 107:10972–10977. https://doi.org/10.1073/pnas.1005802107
Legut M, Dolton G, Mian AA et al (2018) CRISPR-mediated TCR replacement generates superior anticancer transgenic T cells. Blood 131:311–322. https://doi.org/10.1182/blood-2017-05-787598
Baylis F, McLeod M (2017) First-in-human phase 1 CRISPR gene editing cancer trials: are we ready? Curr Gene Ther 17:309–319. https://doi.org/10.2174/1566523217666171121165935
CRISPR therapeutics provides business update and reports second quarter 2019 financial results | CRISPR Therapeutics. In: Cris. Ther. Press Release. http://ir.crisprtx.com/news-releases/news-release-details/crispr-therapeutics-provides-business-update-and-reports-1. Accessed 19 Sept 2019
CRISPR Therapeutics I (2019) Creating transformative gene-based medicines for serious diseases: corporate overview
Xu L, Wang J, Liu Y et al (2019) CRISPR-edited stem cells in a patient with HIV and acute lymphocytic leukemia. N Engl J Med. https://doi.org/10.1056/NEJMoa1817426
Xu L, Yang H, Gao Y et al (2017) CRISPR/Cas9-mediated CCR5 ablation in human hematopoietic stem/progenitor cells confers HIV-1 resistance in vivo. Mol Ther 25:1782–1789. https://doi.org/10.1016/j.ymthe.2017.04.027
Cheng Y, Tsai SQ (2018) Illuminating the genome-wide activity of genome editors for safe and effective therapeutics. Genome Biol 19:226. https://doi.org/10.1186/s13059-018-1610-2
Wienert B, Wyman SK, Richardson CD et al (2019) Unbiased detection of CRISPR off-targets in vivo using DISCOVER-Seq. Science 364:286–289. https://doi.org/10.1126/science.aav9023
Hockemeyer D, Soldner F, Beard C et al (2009) Efficient targeting of expressed and silent genes in human ESCs and iPSCs using zinc-finger nucleases. Nat Biotechnol 27:851–857. https://doi.org/10.1038/nbt.1562
Hockemeyer D, Wang H, Kiani S et al (2011) Genetic engineering of human pluripotent cells using TALE nucleases. Nat Biotechnol 29:731–734. https://doi.org/10.1038/nbt.1927
Tsai SQ, Nguyen NT, Malagon-Lopez J et al (2017) CIRCLE-seq: a highly sensitive in vitro screen for genome-wide CRISPR–Cas9 nuclease off-targets. Nat Methods 14:607–614. https://doi.org/10.1038/nmeth.4278
Smith C, Gore A, Yan W et al (2014) Whole-genome sequencing analysis reveals high specificity of CRISPR/Cas9 and TALEN-based genome editing in human iPSCs. Cell Stem Cell 15:12–13. https://doi.org/10.1016/J.STEM.2014.06.011
Veres A, Gosis BS, Ding Q et al (2014) Low incidence of off-target mutations in individual CRISPR–Cas9 and TALEN targeted human stem cell clones detected by whole-genome sequencing. Cell Stem Cell 15:27–30. https://doi.org/10.1016/j.stem.2014.04.020
Carroll D (2019) Collateral damage: benchmarking off-target effects in genome editing. Genome Biol 20:114. https://doi.org/10.1186/s13059-019-1725-0
Sangamo announces interim results of phase 1/2 CHAMPIONS study showing preliminary evidence of in vivo genome editing in patients with MPS II treated with SB-913 | Sangamo Therapeutics, Inc. https://investor.sangamo.com/news-releases/news-release-details/sangamo-announces-interim-results-phase-12-champions-study. Accessed 22 Jan 2020
Fine EJ, Cradick TJ, Zhao CL et al (2014) An online bioinformatics tool predicts zinc finger and TALE nuclease off-target cleavage. Nucleic Acids Res 42:e42. https://doi.org/10.1093/nar/gkt1326
Chuai G, Ma H, Yan J et al (2018) DeepCRISPR: optimized CRISPR guide RNA design by deep learning. Genome Biol 19:80. https://doi.org/10.1186/s13059-018-1459-4
Kim HK, Min S, Song M et al (2018) Deep learning improves prediction of CRISPR–Cpf1 guide RNA activity. Nat Biotechnol 36:239–241. https://doi.org/10.1038/nbt.4061
Abadi S, Yan WX, Amar D, Mayrose I (2017) A machine learning approach for predicting CRISPR–Cas9 cleavage efficiencies and patterns underlying its mechanism of action. PLoS Comput Biol 13:e1005807. https://doi.org/10.1371/journal.pcbi.1005807
Doyon Y, Vo TD, Mendel MC et al (2011) Enhancing zinc-finger-nuclease activity with improved obligate heterodimeric architectures. Nat Methods 8:74–79. https://doi.org/10.1038/nmeth.1539
Gautron A-S, Juillerat A, Guyot V et al (2017) Fine and predictable tuning of TALEN gene editing targeting for improved t cell adoptive immunotherapy. Mol Ther Nucleic Acids 9:312–321. https://doi.org/10.1016/j.omtn.2017.10.005
Miller JC, Zhang L, Xia DF et al (2015) Improved specificity of TALE-based genome editing using an expanded RVD repertoire. Nat Methods 12:465–471. https://doi.org/10.1038/nmeth.3330
Juillerat A, Pessereau C, Dubois G et al (2015) Optimized tuning of TALEN specificity using non-conventional RVDs. Sci Rep 5:8150. https://doi.org/10.1038/srep08150
Fu Y, Sander JD, Reyon D et al (2014) Improving CRISPR-Cas nuclease specificity using truncated guide RNAs. Nat Biotechnol 32:279–284. https://doi.org/10.1038/nbt.2808
Slaymaker IM, Gao L, Zetsche B et al (2016) Rationally engineered Cas9 nucleases with improved specificity. Science 351:84–88. https://doi.org/10.1126/science.aad5227
Kleinstiver BP, Pattanayak V, Prew MS et al (2016) High-fidelity CRISPR–Cas9 nucleases with no detectable genome-wide off-target effects. Nature 529:490–495. https://doi.org/10.1038/nature16526
Ran FA, Hsu PD, Lin C-Y et al (2013) Double nicking by RNA-guided CRISPR Cas9 for enhanced genome editing specificity. Cell 154:1380–1389. https://doi.org/10.1016/J.CELL.2013.08.021
Mali P, Aach J, Stranges PB et al (2013) CAS9 transcriptional activators for target specificity screening and paired nickases for cooperative genome engineering. Nat Biotechnol 31:833–838. https://doi.org/10.1038/nbt.2675
Anzalone AV, Randolph PB, Davis JR et al (2019) Search-and-replace genome editing without double-strand breaks or donor DNA. Nature 576:149–175. https://doi.org/10.1038/s41586-019-1711-4
Doi D, Samata B, Katsukawa M et al (2014) Isolation of human induced pluripotent stem cell-derived dopaminergic progenitors by cell sorting for successful transplantation. Stem Cell Rep 2:337–350. https://doi.org/10.1016/j.stemcr.2014.01.013
(2018) Kyoto trial to evaluate the safety and efficacy of iPSC-derived dopaminergic progenitors in the treatment of Parkinson’s disease (UMIN000033564). In: UMIN Clin. Trials Regist. https://upload.umin.ac.jp/cgi-open-bin/ctr_e/ctr_view.cgi?recptno=R000038278. Accessed 13 Sept 2019
(2018) Announcement of physician-initiated clinical trials for Parkinson’s diseas. In: News Events, Cent. iPS Cell Res. Appl. Kyoto Univ. https://www.cira.kyoto-u.ac.jp/e/pressrelease/news/180730-170000.html. Accessed 13 Sept 2019
Cyranoski D (2018) ‘Reprogrammed’ stem cells implanted into patient with Parkinson’s disease. Nature. https://doi.org/10.1038/d41586-018-07407-9
Cyranoski D (2019) Woman is first to receive cornea made from ‘reprogrammed’ stem cells. Nature. https://doi.org/10.1038/d41586-019-02597-2
Hayashi R, Ishikawa Y, Sasamoto Y et al (2016) Co-ordinated ocular development from human iPS cells and recovery of corneal function. Nature 531:376–380. https://doi.org/10.1038/nature17000
Mandai M, Watanabe A, Kurimoto Y et al (2017) Autologous induced stem-cell-derived retinal cells for macular degeneration. N Engl J Med 376:1038–1046. https://doi.org/10.1056/NEJMoa1608368
Cyranoski D (2014) Japanese woman is first recipient of next-generation stem cells. Nature. https://doi.org/10.1038/nature.2014.15915
Cyranoski D (2017) Japanese man is first to receive “reprogrammed” stem cells from another person. Nature. https://doi.org/10.1038/nature.2017.21730
Cyranoski D (2018) ‘Reprogrammed’ stem cells approved to mend human hearts for the first time. Nat 2019:5577707
Ishigami M, Masumoto H, Ikuno T et al (2018) Human iPS cell-derived cardiac tissue sheets for functional restoration of infarcted porcine hearts. PLoS ONE 13:e0201650. https://doi.org/10.1371/journal.pone.0201650
Bloor A, Patel A, Griffin JE et al (2018) A phase I trial of iPSC-derived MSCs (CYP-001) in steroid-resistant acute GvHD. Blood 132:4562. https://doi.org/10.1182/BLOOD-2018-99-110432
Azuma K, Yamanaka S (2016) Recent policies that support clinical application of induced pluripotent stem cell-based regenerative therapies. Regen Ther 4:36–47. https://doi.org/10.1016/j.reth.2016.01.009
Cyranoski D (2013) Japan to offer fast-track approval path for stem cell therapies. Nat Med 19:510. https://doi.org/10.1038/nm0513-510
Konomi K, Tobita M, Kimura K, Sato D (2015) New Japanese initiatives on stem cell therapies. Cell Stem Cell 16:350–352. https://doi.org/10.1016/j.stem.2015.03.012
Umekage M, Sato Y, Takasu N (2019) Overview: an iPS cell stock at CiRA. Inflamm Regen 39:17. https://doi.org/10.1186/s41232-019-0106-0
Pappas DJ, Gourraud P-A, Le Gall C et al (2015) Proceedings: human leukocyte antigen haplo-homozygous induced pluripotent stem cell haplobank modeled after the california population: evaluating matching in a multiethnic and admixed population. Stem Cells Transl Med 4:413–418. https://doi.org/10.5966/sctm.2015-0052
Huang C-Y, Liu C-L, Ting C-Y et al (2019) Human iPSC banking: barriers and opportunities. J Biomed Sci 26:87. https://doi.org/10.1186/s12929-019-0578-x
Xu H, Wang B, Ono M et al (2019) Targeted disruption of HLA genes via CRISPR–Cas9 generates iPSCs with enhanced immune compatibility. Cell Stem Cell 24:566–578.e7. https://doi.org/10.1016/j.stem.2019.02.005
Deuse T, Hu X, Gravina A et al (2019) Hypoimmunogenic derivatives of induced pluripotent stem cells evade immune rejection in fully immunocompetent allogeneic recipients. Nat Biotechnol 37:252–258. https://doi.org/10.1038/s41587-019-0016-3
Ichise H, Nagano S, Maeda T et al (2017) NK cell alloreactivity against KIR-ligand-mismatched HLA-haploidentical tissue derived from HLA haplotype-homozygous iPSCs. Stem Cell Reports 9:853–867. https://doi.org/10.1016/J.STEMCR.2017.07.020
Eyquem J, Mansilla-Soto J, Giavridis T et al (2017) Targeting a CAR to the TRAC locus with CRISPR/Cas9 enhances tumour rejection. Nature 543:113–117. https://doi.org/10.1038/nature21405
Feucht J, Sun J, Eyquem J et al (2019) Calibration of CAR activation potential directs alternative T cell fates and therapeutic potency. Nat Med 25:82–88. https://doi.org/10.1038/s41591-018-0290-5
(2019) First iPSC-derived CAR T-cell therapy created by Kyoto University CiRA and Takeda Collaboration enters process development toward clinical testing. In: Tak. News Releases. https://www.takeda.com/newsroom/newsreleases/2019/first-ipsc-derived-car-t-cell-therapy-created-by-kyoto-university-cira-and–takeda-collaboration-enters-process-development-toward-clinical-testing/. Accessed 19 Sept 2019
Schächinger V, Aicher A, Döbert N et al (2008) Pilot trial on determinants of progenitor cell recruitment to the infarcted human myocardium. Circulation 118:1425–1432. https://doi.org/10.1161/CIRCULATIONAHA.108.777102
De Vries IJM, Lesterhuis WJ, Barentsz JO et al (2005) Magnetic resonance tracking of dendritic cells in melanoma patients for monitoring of cellular therapy. Nat Biotechnol 23:1407–1413. https://doi.org/10.1038/nbt1154
Zhu J, Zhou L, XingWu FG (2006) Tracking neural stem cells in patients with brain trauma. N Engl J Med 355:2376–2378. https://doi.org/10.1056/NEJMc055304
Won JK, Kang HJ, Kim HS et al (2006) Tissue distribution of 18F-FDG-labeled peripheral hematopoietic stem cells after intracoronary administration in patients with myocardial infarction. J Nucl Med 47:1295–1301
Vrtovec B, Poglajen G, Lezaic L et al (2013) Comparison of transendocardial and intracoronary CD34+ cell transplantation in patients with nonischemic dilated cardiomyopathy. Circulation 128:S42–S49. https://doi.org/10.1161/CIRCULATIONAHA.112.000230
Yaghoubi SS, Jensen MC, Satyamurthy N et al (2009) Noninvasive detection of therapeutic cytolytic T cells with 18F-FHBG PET in a patient with glioma. Nat Clin Pract Oncol 6:53–58. https://doi.org/10.1038/ncponc1278
The authors received support from Guy’s & St. Thomas’ Charity (CAH) and Cancer Research UK [MDPA C48390/A21153 to GOF]. They were also supported by the Wellcome/EPSRC Centre for Medical Engineering at KCL [WT 203148/Z/16/Z]. The views expressed are those of the authors.
Ethics approval and consent to participate
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Ashmore-Harris, C., Fruhwirth, G.O. The clinical potential of gene editing as a tool to engineer cell-based therapeutics. Clin Trans Med 9, 15 (2020). https://doi.org/10.1186/s40169-020-0268-z
- Cell therapy
- Clinical trial
- Zinc finger nuclease