Steven Lin

RNA-programmed genome editing in human cells

Type II CRISPR immune systems in bacteria use a dual RNA-guided DNA endonuclease, Cas9, to cleave foreign DNA at specific sites. We show here that Cas9 assembles with hybrid guide RNAs in human cells and can induce the formation of double-strand DNA breaks (DSBs) at a site complementary to the guide RNA sequence in genomic DNA. This cleavage activity requires both Cas9 and the complementary binding of the guide RNA. Experiments using extracts from transfected cells show that RNA expression and/or assembly into Cas9 is the limiting factor for Cas9-mediated DNA cleavage. In addition, we find that extension of the RNA sequence at the 3′ end enhances DNA targeting activity in vivo. These results show that RNA-programmed genome editing is a facile strategy for introducing site-specific genetic changes in human cells. DOI: http://dx.doi.org/10.7554/eLife.00471.001

High-throughput profiling of off-target DNA cleavage reveals RNA-programmed Cas9 nuclease specificity

The RNA-programmable Cas9 endonuclease cleaves double-stranded DNA at sites complementary to a 20-base-pair guide RNA. The Cas9 system has been used to modify genomes in multiple cells and organisms, demonstrating its potential as a facile genome-engineering tool. We used in vitro selection and high-throughput sequencing to determine the propensity of eight guide-RNA:Cas9 complexes to cleave each of 1012 potential off-target DNA sequences. The selection results predicted five off-target sites in the human genome that were confirmed to undergo genome cleavage in HEK293T cells upon expression of one of two guide-RNA:Cas9 complexes. In contrast to previous models, our results show that guide-RNA:Cas9 specificity extends past a 7- to 12-base-pair seed sequence. Our results also suggest a tradeoff between activity and specificity both in vitro and in cells as a shorter, less-active guide RNA is more specific than a longer, more-active guide RNA. High concentrations of guide-RNA:Cas9 complexes can cleave off-target sites containing mutations near or within the PAM that are not cleaved when enzyme concentrations are limiting.

Structures of Cas9 Endonucleases Reveal RNA-Mediated Conformational Activation.

Introduction Bacteria and archaea defend themselves against invasive DNA using adaptive immune systems comprising CRISPR (clustered regularly interspaced short palindromic repeats) loci and CRISPR-associated (Cas) genes. In association with Cas proteins, small CRISPR RNAs (crRNAs) guide the detection and cleavage of complementary DNA sequences. Type II CRISPR systems employ the RNA-guided endonuclease Cas9 to recognize and cleave double-stranded DNA (dsDNA) targets using conserved RuvC and HNH nuclease domains. Cas9-mediated cleavage is strictly dependent on the presence of a protospacer adjacent motif (PAM) in the target DNA. Recently, the biochemical properties of Cas9–guide RNA complexes have been harnessed for various genetic engineering applications and RNA-guided transcriptional control. Despite these ongoing successes, the structural basis for guide RNA recognition and DNA targeting by Cas9 is still unknown. Structures of Cas9 endonucleases reveal RNA-mediated conformational activation. (A) Crystal structures of S. pyogenes (SpyCas9) and A. naeslundii (AnaCas9) Cas9 proteins. (B) Left: Negative-stain EM reconstructions of apo-SpyCas9 (top) and SpyCas9-RNA-target DNA complex (bottom) show that nucleic acid binding causes a reorientation of the nuclease (blue) and α-helical (gray) lobes in SpyCas9. Right: Cartoon representations of the structures. tracrRNA, trans-activating crRNA. Rationale To compare the architectures and domain organization of diverse Cas9 proteins, the atomic structures of Cas9 from Streptococcus pyogenes (SpyCas) and Actinomyces naeslundii (AnaCas9) were determined by x-ray crystallography. Crosslinking of target DNA containing 5-bromodeoxyuridines was conducted to identify PAM-interacting regions in SpyCas9. To test functional interactions with nucleic acid ligands, structure-based mutant SpyCas9 proteins were assayed for endonuclease activity with radiolabeled oligonucleotide dsDNA targets, and target DNA binding was monitored by electrophoretic mobility shift assays. To compare conformations of Cas9 in different states of nucleic acid binding, three-dimensional reconstructions of apo-SpyCas9, SpyCas9:RNA, and SpyCas9:RNA:DNA were obtained by negative-stain single-particle electron microscopy. Guide RNA and target DNA positions were determined with streptavidin labeling. Exonuclease protection assays were carried out to determine the extent of Cas9–target DNA interactions. Results The 2.6 Å–resolution structure of apo-SpyCas9 reveals a bilobed architecture comprising a nuclease domain lobe and an α-helical lobe. Both lobes contain conserved clefts that may function in nucleic acid binding. Photocrosslinking experiments show that the PAM in target DNA is engaged by two tryptophan-containing flexible loops, and mutations of both loops impair target DNA binding and cleavage. The 2.2 Å–resolution crystal structure of AnaCas9 reveals the conserved structural core shared by all Cas9 enzyme subtypes, and both SpyCas9 and AnaCas9 adopt autoinhibited conformations in their apo forms. The electron microscopic (EM) reconstructions of SpyCas9:RNA and SpyCas9:RNA:DNA complexes reveal that guide RNA binding results in a conformational rearrangement and formation of a central channel for target DNA binding. Site-specific labeling of guide RNA and target DNA define the orientations of nucleic acids in the target-bound complex. Conclusion The SpyCas9 and AnaCas9 structures define the molecular architecture of the Cas9 enzyme family in which a conserved structural core encompasses the two nuclease domains responsible for DNA cleavage, while structurally divergent regions, including the PAM recognition loops, are likely responsible for distinct guide RNA and PAM specificities. Cas9 enzymes adopt a catalytically inactive conformation in the apo state, necessitating structural activation for DNA recognition and cleavage. Our EM analysis shows that by triggering a conformational rearrangement in Cas9, the guide RNA acts as a critical determinant of target DNA binding. Cas9 Solved Clustered regularly interspaced short palindromic repeats (CRISPR)–associated (Cas) loci allow prokaryotes to identify and destroy invading DNA. Not only important to bacteria, the universal value of Cas endonuclease specificity has also resulted in Cas9 being exploited as a tool for genome editing. Jinek et al. (10.1126/science.1247997, published online 6 February) determined the 2.6 and 2.2 angstrom resolution crystal structures of two Cas9 enzymes to reveal a common structural core with distinct peripheral elaborations. The enzymes are autoinhibited, undergo large conformational changes on binding RNA, and have channels lined with basic residues that are candidates for an RNA-DNA binding groove. Based on these and other insights from the structures, this work provides important revelations both for the CRISPR mechanism and for genome editing. Binding of a guide RNA triggers structural changes in a set of DNA-cleaving enzymes. Type II CRISPR (clustered regularly interspaced short palindromic repeats)–Cas (CRISPR-associated) systems use an RNA-guided DNA endonuclease, Cas9, to generate double-strand breaks in invasive DNA during an adaptive bacterial immune response. Cas9 has been harnessed as a powerful tool for genome editing and gene regulation in many eukaryotic organisms. We report 2.6 and 2.2 angstrom resolution crystal structures of two major Cas9 enzyme subtypes, revealing the structural core shared by all Cas9 family members. The architectures of Cas9 enzymes define nucleic acid binding clefts, and single-particle electron microscopy reconstructions show that the two structural lobes harboring these clefts undergo guide RNA–induced reorientation to form a central channel where DNA substrates are bound. The observation that extensive structural rearrangements occur before target DNA duplex binding implicates guide RNA loading as a key step in Cas9 activation.

Enhanced homology-directed human genome engineering by controlled timing of CRISPR/Cas9 delivery.

The CRISPR/Cas9 system is a robust genome editing technology that works in human cells, animals and plants based on the RNA-programmed DNA cleaving activity of the Cas9 enzyme. Building on previous work (Jinek et al., 2013), we show here that new genetic information can be introduced site-specifically and with high efficiency by homology-directed repair (HDR) of Cas9-induced site-specific double-strand DNA breaks using timed delivery of Cas9-guide RNA ribonucleoprotein (RNP) complexes. Cas9 RNP-mediated HDR in HEK293T, human primary neonatal fibroblast and human embryonic stem cells was increased dramatically relative to experiments in unsynchronized cells, with rates of HDR up to 38% observed in HEK293T cells. Sequencing of on- and potential off-target sites showed that editing occurred with high fidelity, while cell mortality was minimized. This approach provides a simple and highly effective strategy for enhancing site-specific genome engineering in both transformed and primary human cells. DOI: http://dx.doi.org/10.7554/eLife.04766.001

Generation of knock-in primary human T cells using Cas9 ribonucleoproteins

Significance T-cell genome engineering holds great promise for cancer immunotherapies and cell-based therapies for HIV, primary immune deficiencies, and autoimmune diseases, but genetic manipulation of human T cells has been inefficient. We achieved efficient genome editing by delivering Cas9 protein pre-assembled with guide RNAs. These active Cas9 ribonucleoproteins (RNPs) enabled successful Cas9-mediated homology-directed repair in primary human T cells. Cas9 RNPs provide a programmable tool to replace specific nucleotide sequences in the genome of mature immune cells—a longstanding goal in the field. These studies establish Cas9 RNP technology for diverse experimental and therapeutic genome engineering applications in primary human T cells. T-cell genome engineering holds great promise for cell-based therapies for cancer, HIV, primary immune deficiencies, and autoimmune diseases, but genetic manipulation of human T cells has been challenging. Improved tools are needed to efficiently “knock out” genes and “knock in” targeted genome modifications to modulate T-cell function and correct disease-associated mutations. CRISPR/Cas9 technology is facilitating genome engineering in many cell types, but in human T cells its efficiency has been limited and it has not yet proven useful for targeted nucleotide replacements. Here we report efficient genome engineering in human CD4+ T cells using Cas9:single-guide RNA ribonucleoproteins (Cas9 RNPs). Cas9 RNPs allowed ablation of CXCR4, a coreceptor for HIV entry. Cas9 RNP electroporation caused up to ∼40% of cells to lose high-level cell-surface expression of CXCR4, and edited cells could be enriched by sorting based on low CXCR4 expression. Importantly, Cas9 RNPs paired with homology-directed repair template oligonucleotides generated a high frequency of targeted genome modifications in primary T cells. Targeted nucleotide replacement was achieved in CXCR4 and PD-1 (PDCD1), a regulator of T-cell exhaustion that is a validated target for tumor immunotherapy. Deep sequencing of a target site confirmed that Cas9 RNPs generated knock-in genome modifications with up to ∼20% efficiency, which accounted for up to approximately one-third of total editing events. These results establish Cas9 RNP technology for diverse experimental and therapeutic genome engineering applications in primary human T cells.

Biotin synthesis begins by hijacking the fatty acid synthetic pathway

Although biotin is an essential enzyme cofactor found in all three domains of life, our knowledge of its biosynthesis remains fragmentary. Most of the carbon atoms of biotin are derived from pimelic acid, a seven carbon dicarboxylic acid, but the mechanism whereby Escherichia coli assembles this intermediate remains unknown. Genetic analysis identified only two genes of unknown function required for pimelate synthesis, bioC and bioH. We report in vivo and in vitro evidence that the pimeloyl moiety is synthesized by a modified fatty acid synthetic pathway in which the ω-carboxyl group of a malonyl-thioester is methylated by BioC which allows recognition of this atypical substrate by the fatty acid synthetic enzymes. The malonyl-thioester methyl ester enters fatty acid synthesis as the primer and undergoes two reiterations of the fatty acid elongation cycle to give pimeloyl-acyl carrier protein (ACP) methyl ester which is hydrolyzed to pimeloyl-ACP and methanol by BioH.

Precise and Heritable Genome Editing in Evolutionarily Diverse Nematodes Using TALENs and CRISPR/Cas9 to Engineer Insertions and Deletions

Exploitation of custom-designed nucleases to induce DNA double-strand breaks (DSBs) at genomic locations of choice has transformed our ability to edit genomes, regardless of their complexity. DSBs can trigger either error-prone repair pathways that induce random mutations at the break sites or precise homology-directed repair pathways that generate specific insertions or deletions guided by exogenously supplied DNA. Prior editing strategies using site-specific nucleases to modify the Caenorhabditis elegans genome achieved only the heritable disruption of endogenous loci through random mutagenesis by error-prone repair. Here we report highly effective strategies using TALE nucleases and RNA-guided CRISPR/Cas9 nucleases to induce error-prone repair and homology-directed repair to create heritable, precise insertion, deletion, or substitution of specific DNA sequences at targeted endogenous loci. Our robust strategies are effective across nematode species diverged by 300 million years, including necromenic nematodes (Pristionchus pacificus), male/female species (Caenorhabditis species 9), and hermaphroditic species (C. elegans). Thus, genome-editing tools now exist to transform nonmodel nematode species into genetically tractable model organisms. We demonstrate the utility of our broadly applicable genome-editing strategies by creating reagents generally useful to the nematode community and reagents specifically designed to explore the mechanism and evolution of X chromosome dosage compensation. By developing an efficient pipeline involving germline injection of nuclease mRNAs and single-stranded DNA templates, we engineered precise, heritable nucleotide changes both close to and far from DSBs to gain or lose genetic function, to tag proteins made from endogenous genes, and to excise entire loci through targeted FLP-FRT recombination.

Mechanisms of Spectral Tuning in Blue Cone Visual Pigments VISIBLE AND RAMAN SPECTROSCOPY OF BLUE-SHIFTED RHODOPSIN MUTANTS

Spectral tuning by visual pigments involves the modulation of the physical properties of the chromophore (11-cis-retinal) by amino acid side chains that compose the chromophore-binding pocket. We identified 12 amino acid residues in the human blue cone pigment that might induce the required green-to-blue opsin shift. The simultaneous substitution of nine of these sites in rhodopsin (M86L, G90S, A117G, E122L, A124T, W265Y, A292S, A295S, and A299C) shifted the absorption maximum from 500 to 438 nm, accounting for 2,830 cm−1, or 80%, of the opsin shift between rhodopsin and the blue cone pigment. Raman spectroscopy of mutant pigments shows that the dielectric character and architecture of the chromophore-binding pocket are specifically altered. An increase in the number of dipolar side chains near the protonated Schiff base of retinal increases the ground-excited state energy gap via long range dipole-dipole Coulomb interaction. In addition, the W265Y substitution causes a decrease in solvent polarizability near the chromophore ring structure. Finally, two substitutions on transmembrane helix 3 (A117G and E122L) act in combination with the other substitutions to alter the binding-pocket structure, resulting in stronger interaction of the protonated Schiff base group with the surrounding dipolar groups and the counterion. Taken together, these results identify the amino acid side chains and the underlying physical mechanisms responsible for a majority of the opsin shift in blue visual pigments.

Closing in on complete pathways of biotin biosynthesis

Biotin is an enzyme cofactor indispensable to metabolic fixation of carbon dioxide in all three domains of life. Although the catalytic and physiological roles of biotin have been well characterized, the biosynthesis of biotin remains to be fully elucidated. Studies in microbes suggest a two-stage biosynthetic pathway in which a pimelate moiety is synthesized and used to begin assembly of the biotin bicyclic ring structure. The enzymes involved in the bicyclic ring assembly have been studied extensively. In contrast the synthesis of pimelate, a seven carbon α,ω-dicarboxylate, has long been an enigma. Support for two different routes of pimelate synthesis has recently been obtained in Escherichia coli and Bacillus subtilis. The E. coli BioC-BioH pathway employs a methylation and demethylation strategy to allow elongation of a temporarily disguised malonate moiety to a pimelate moiety by the fatty acid synthetic enzymes whereas the B. subtilis BioI-BioW pathway utilizes oxidative cleavage of fatty acyl chains. Both pathways produce the pimelate thioester precursor essential for the first step in assembly of the fused rings of biotin. The enzymatic mechanisms and biochemical strategies of these pimelate synthesis models will be discussed in this review.

Orientation of the protonated retinal Schiff base group in bacteriorhodopsin from absorption linear dichroism.

Linear dichroism experiments are performed on light-adapted bacteriorhodopsin (BR568) films containing native retinal (A1) and its 3,4-dehydroretinal (A2) analogue to measure the angle between the chromophore transition dipole moment and the membrane normal. QCFF/pi calculations show that the angle between the transition moment and the long axis of the polyene is changed by 3.4 degrees when the C3-C4 bond is unsaturated. The difference vector between the two transition moments points in the same direction as the Schiff base (N----H) bond for the all-trans BR568 chromophore. Because the plane of the chromophore is perpendicular to the membrane plane, a comparison of the transition moment orientations in the A1- and A2-pigments enables us to determine the orientation of the N----H bond with respect to the absolute chromophore (N----C5 vector) orientation. The angles of the transition moments are 70.3 degrees +/- 0.4 degrees and 67.8 degrees +/- 0.4 degrees for the A1- and A2-pigments, respectively. The fact that the change in the transition moment angle (2.5 degrees) is close to the predicted 3.4 degrees supports the idea that the chromophore plane is nearly perpendicular to the membrane plane. The decreased transition moment angle in the A2-analogue requires that the N----H bond and the N----C5 vector point toward the same membrane surface. Available results indicate that the N----C5 vector points toward the exterior in BR568. With this assignment, we conclude that the N----H bond points toward the exterior surface and its most likely counterion Asp-212. This information makes possible the construction of a computer graphics model for the active site in BR568.