Cre-dependent selection yields AAV variants for widespread gene transfer to the adult brain

Cre-dependent selection yields AAV variants for widespread

gene transfer to the adult brain

Benjamin E. Deverman

Piers L. Pravdo

Bryan P. Simpson

Sripriya Ravindra Kumar

Ken Y. Chan

Abhik Banerjee

Wei-Li Wu

Bin Yang

Nina Huber

Sergiu P. Pasca

, and

Viviana Gradinaru

Division of Biology and Biological Engineering, California Institute of Technology Pasadena, CA

Department of Psychiatry and Behavioral Sciences, Stanford University School of Medicine,

Stanford, CA

Abstract

Recombinant adeno-associated viruses (rAAVs) are commonly used vehicles for

in vivo

gene

transfer

. However, the tropism repertoire of naturally occurring AAVs is limited, prompting a

search for novel AAV capsids with desired characteristics

. Here we describe a capsid selection

method, called Cre-recombination-based AAV targeted evolution (CREATE), that enables the

development of AAV capsids that more efficiently transduce defined Cre-expressing cell

populations

in vivo

. We use CREATE to generate AAV variants that efficiently and widely

transduce the adult mouse central nervous system (CNS) after intravenous injection. One variant,

AAV-PHP.B, transfers genes throughout the CNS with an efficiency that is at least 40-fold greater

than that of the current standard, AAV9

, and transduces the majority of astrocytes and neurons

across multiple CNS regions.

In vitro

, it transduces human neurons and astrocytes more efficiently

than does AAV9, demonstrating the potential of CREATE to produce customized AAV vectors for

biomedical applications.

rAAVs are the preferred vehicles for many

in vivo

gene transfer applications to non-dividing

cell populations and are proving safe in clinical trials

. However, therapeutic applications

have been limited by inefficient transduction of target cell populations. A prime example is

gene transfer to the CNS; the transduction efficiency of currently available vectors in the

mouse CNS after intravenous administration is at least an order of magnitude lower than in

Users may view, print, copy, and download text and data-mine the content in such documents, for the purposes of academic research,

subject always to the full Conditions of use:http://www.nature.com/authors/editorial_policies/license.html#terms

To whom correspondence should be addressed: Benjamin E. Deverman, Ph.D., Division of Biology and Biological Engineering,

California Institute of Technology, 1200 East California Blvd. MC 156-29, Pasadena, CA 91125, Phone: (626) 395-2776,

bd@caltech.edu, Viviana Gradinaru, Ph.D., Division of Biology and Biological Engineering, California Institute of Technology, 1200

East California Blvd. MC 156-29, Pasadena, CA 91125, Phone: (626) 395-6813, viviana@caltech.edu.

AUTHOR CONTRIBUTIONS

B.E.D designed and performed experiments, analyzed data, prepared figures and wrote the manuscript. P.L.P., B.P.S., S.K., A.B., and

K.C. performed experiments, virus production and characterization. W.L.W. performed tissue processing and IHC. B.Y. assisted with

tissue clearing and imaging. N.H. and S.P.P. performed the experiments with human cells, analyzed the data, and prepared the

associated figure and text. V.G. helped with study design and data analysis, manuscript and figure preparation and supervised the

project. All authors edited and approved the manuscript.

Competing Financial Interests

B.E.D. is listed as an inventor on a patent application relating to this work.

HHS Public Access

Author manuscript

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Published in final edited form as:

Nat Biotechnol

. 2016 February ; 34(2): 204–209. doi:10.1038/nbt.3440.

Author Manuscript

the liver

. Encouragingly, the transduction efficiency of rAAVs can be enhanced by creating

AAV capsid libraries and selecting for variants with more desirable characteristics

. This

approach, however, has not been successfully applied to the development of more effective

gene delivery vehicles for global CNS transduction. Because the highly selective blood brain

barrier (BBB) and cellular heterogeneity of the CNS present challenges for gene transfer to

the CNS through the vasculature, we reasoned that it would be beneficial to provide selective

pressure for capsids that cross the BBB and functionally transduce specific cell types. To

meet these needs, we devised CREATE—a Cre recombination-dependent approach to

selectively recover capsids that transduce predefined Cre expressing target cell populations

(

Fig. 1a

CREATE uses an rAAV capsid genome (rAAV-Cap-in-cis-lox) that couples a full-length

AAV

Cap

gene, controlled by regulatory elements from the AAV

Rep

gene (

Fig. 1b

and

Methods

), with a Cre-invertible switch (

Fig. 1b

). By building capsid libraries within the

rAAV-Cap-in-cis-lox backbone and delivering the virus libraries to animals with Cre

expression in a defined cell population, the system enables the selective amplification and

recovery of sequences that have transduced the target population (

Fig. 1c

). Because the

rAAV-Cap-in-cis-lox genome lacks a functional

Rep

gene,

Rep

must be provided in trans for

virus production. For this purpose, we modified an AAV2/9 rep-cap plasmid to eliminate

capsid protein expression by inserting in-frame stop codons within the reading frame for

each capsid protein, VP1-3 (

Fig. 1d

). These stop codons do not alter the amino acid

sequence of the assembly-activating protein (AAP), which is expressed from an alternative

reading frame within the

Cap

gene

. This split rAAV-Cap-in-cis-lox genome and Rep-AAP

AAV helper system efficiently generates rAAV (

Fig. 1e

) and is the foundation of the

CREATE selection platform, which enables capsid sequence recovery from genetically

defined Cre-expressing cell populations within heterogeneous tissue samples (see

Supplementary Fig. 1

Within the rAAV-Cap-in-cis-lox acceptor genome we generated a library of AAV variants by

inserting 7 amino acids (AA) of randomized sequence (7-mer) between AA588-589 (VP1

position) of the AAV9 capsid (

Fig. 1f, g

). To select for vectors that crossed the BBB and

transduced cells throughout the CNS, we administered the capsid library intravenously into

adult GFAP-Cre mice, which express Cre in astrocytes

. One week later, we isolated DNA

from brain and spinal cord tissue and recovered capsid sequences by PCR from viral

genomes that had undergone Cre-mediated recombination. We cloned the entire library of

recovered Cap sequences back into the rAAV-Cap-in-cis-lox acceptor genome to generate

the library GFAP1 and randomly chose 13 clones for sequencing. All tested sequences

recovered from the GFAP1 library were unique, and therefore we used the GFAP1 plasmid

library to generate a second virus library and performed an additional round of selection in

GFAP-Cre mice. After the second selection, several variants were enriched (

Supplementary

Table 2

) and showed enhanced CNS transduction (

Supplementary Fig. 2a

). We chose the

most enriched variant, AAV-PHP.B, which represented 25% of recovered library sequences

and encodes the 7-mer sequence TLAVPFK, for further tropism evaluation

in vivo

AAV-PHP.B and AAV9 capsids were used to package a single-stranded (ss) GFP reporter

vector driven by the ubiquitous CAG promoter (ssAAV-CAG-GFP). Both AAV-PHP.B and

Deverman et al.

Page 2

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

AAV9 produced virus with similar efficiencies (

Supplementary Fig. 2b

). We next

administered 1×10

vector genomes (vg) of either vector to six-week-old mice by

intravenous injection and assessed transduction by GFP expression three weeks later. Our

data show that AAV-PHP.B transduced the entire adult CNS with high efficiency as indicated

by imaging GFP immunohistochemistry (IHC) (

Fig. 2a

) or native eGFP fluorescence in

several brain regions (

Fig. 2b

), the spinal cord (

Fig. 2c

) and retina (

Fig. 2d

). Using PARS-

based CLARITY for whole body tissue clearing

, we imaged native eGFP fluorescence

through cleared sections of tissue from the spinal cord (

Fig. 2c

), cortex and striatum (

Fig.

). These 3D renderings (also see

Supplementary Movies 1-3

) further demonstrate the

broad and efficient CNS transduction with the AAV-PHP.B vector. Outside the CNS, the

cellular level tropism of AAV-PHP.B and AAV9 appeared similar in several organs, with the

exception of the pancreas where the efficiency of transduction by AAV-PHP.B was reduced

as compared with AAV9 (

Fig. 2f

To quantify the efficiency of gene transfer to the CNS and peripheral organs by AAV-PHP.B

as compared with AAV9, we measured the number of viral genomes present in several brain

regions and organs 25 days post-injection (

Fig. 2g

). AAV-PHP.B provided significantly

greater gene transfer than AAV9 to each of the CNS regions examined: cortex (40-fold),

striatum (92-fold), thalamus (76-fold), cerebellum (41-fold) and spinal cord (75-fold).

Vector genome biodistribution outside the CNS showed that AAV-PHP.B transferred genes

to the pancreas and adrenal gland less efficiently than AAV9 (

Fig. 2g

). No significant

differences were found between the two vectors in the liver, heart, skeletal muscle and

kidneys. When considered together with the CNS biodistribution data, in all CNS areas

except the cerebellum, the number of viral genomes detected in mice treated with AAV-

PHP.B was similar to that measured in the liver, an organ efficiently transduced by

AAV9

, and greater than that observed in other organs. In contrast, AAV9-mediated gene

transfer to each of the examined CNS regions was at least 120-fold lower than in the liver.

Therefore, although the tropism of AAV-PHP.B is not CNS specific, the enhanced gene

transfer characteristics of this vector are CNS specific.

AAV9 preferentially transduces astrocytes when delivered intravenously to adult mice and

non-human primates, but it also transduces neurons in several regions

. To examine the

cell types transduced by AAV-PHP.B, we analyzed the co-localization of GFP with several

cell-type markers. Owing to the highly efficient transduction, individual GFP expressing

astrocytes were difficult to discern in mice that received 1×10

vg AAV-PHP.B (

Fig. 2a

but could be more easily identified morphologically by their compact, highly ramified

processes in animals that received 10-fold less virus (

Fig. 2a, b

) and by co-localization with

IHC for GFAP (

Fig. 3a

). In addition to astrocytes, AAV-PHP.B transduced CC1

oligodendrocytes (

Fig. 3b

) and all neuronal subtypes examined, including NeuN

throughout the brain (

Fig. 3c

) as well as midbrain tyrosine hydroxylase (TH)

dopaminergic

neurons (

Fig. 3d

), Calbindin

cerebellar Purkinje cells (

Fig. 3e

), and several interneuron

populations (

Supplementary Fig. 3a-d

). AAV-PHP.B also transduced CD31

endothelial

cells (

Supplementary Fig. 3e

) but did not appear to transduce Iba1

microglia

(

Supplementary Fig. 3f,g

). The paucity of GFP

microglia seen after intravenous AAV-

PHP.B delivery is consistent with previous reports of rare or nonexistent AAV-mediated gene

Deverman et al.

Page 3

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

expression in this cell population

. We have observed native GFP expression

throughout the brain over a year after administration of AAV-PHP.B, suggesting that AAV-

PHP.B can provide long-term, CNS-directed transgene expression (

Supplementary Fig. 4

We next quantified the fraction of several cell types transduced by AAV-PHP.B as compared

to AAV9. To facilitate reliable individual cell counting, we constructed a vector expressing a

nuclear-localized GFP (NLS-GFP) under the control of the CAG promoter, ssAAV-CAG-

NLS-GFP. A single injection of 2×10

vg/mouse of ssAAV-PHP.B:CAG-NLS-GFP

transduced the majority of Aldh1L1

astrocytes (

Fig. 3f

and

Supplementary Fig. 5a

) and

NeuN

neurons (

Fig. 3g

and

Supplementary Fig. 5b

), as well as a modest fraction of

Olig2

oligodendrocyte lineage cells (

Fig.3h

and

Supplementary Fig. 5c

) across all brain

regions examined. In all cases, AAV-PHP.B provided significantly enhanced transduction as

compared to the same dose of AAV9. Notably, AAV-PHP.B also transduced over 94% of

Chat

motor neurons throughout the spinal cord (

Fig. 3i

), 91.4±1.6% of TH

midbrain

dopaminergic neurons (

Supplemental Fig. 5d

) and 91.7±5.8% of Calbindin

Purkinje cells

(

=5). In sum, adult intravenous administration of AAV-PHP.B efficiently targets multiple

neuronal and glial cell types in the adult mouse.

The method used to identify AAV-PHP.B only selects for transduction of the target cell

population; it does not necessarily select for specificity. Nevertheless, in a separate trial in

GFAP-Cre mice, we identified (after two rounds of

in vivo

selection) another AAV capsid

variant, AAV-PHP.A, with the 7-mer sequence, YTLSQGW, that exhibits both more efficient

and selective CNS astrocyte transduction (

Fig. 4a-d

), as well as reduced tropism for the liver

(

Fig. 4e, f

) and other peripheral organs (

Fig. 4f

), as compared to AAV9. The increase in

specificity for gene transfer to the CNS over the liver provided by AAV-PHP.A versus AAV9

is 400- to 1200-fold, resulting from a combination of enhanced adult CNS gene transfer

(2.6- to 8-fold more depending on the specific region) and reduced liver gene transfer (152-

fold). Two other variants enriched in this trial (

Supplementary Fig. 2a

) did not show

enhanced GFP expression in CNS neurons or glia as compared with AAV9.

To determine whether AAV-PHP.A and AAV-PHP.B can also transduce human neural cells,

we tested them on cortical neurons and astrocytes derived from human induced pluripotent

stem cells (hiPSCs) using a 3D differentiation method

. HiPSC lines from two individuals

were differentiated into 3D cerebral cortex-like structures (cortical spheroids), and

maintained

in vitro

for up to 200 days. Aged cortical spheroids contain superficial and deep

layer cortical excitatory neurons and up to 20% astrocytes

. In dissociated cortical

spheroids that were exposed to the three viruses in monolayer, AAV-PHP.B more efficiently

transduced both GFAP-expressing astrocytes and MAP2-expresing neurons in comparison

with either AAV9 or AAV-PHP.A (Supplemental Fig. 5; two-way ANOVA p<0.01, n=3). In

addition, all three viruses were capable of transducing intact 3D cortical spheroids

(Supplementary Fig. 5c).

Using CREATE, we have developed new AAV variants that enable efficient widespread gene

transfer to the adult mouse CNS after intravenous administration. An important advantage of

this system is that it introduces selective pressure for capsids that mediate efficient

intracellular trafficking and conversion of the single-stranded viral genome to persistent

Deverman et al.

Page 4

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

double-stranded DNA (dsDNA) forms necessary for long-term transduction (only the

dsDNA genomes should serve as substrates for Cre). This additional selective pressure for

functional capsids may have contributed to the identification of AAV-PHP.A and the AAV-

PHP.B variants in independent trials after only two rounds of

in vivo

selection. In

comparison, many previous

in vivo

and

in vitro

AAV capsid selection methods have applied

3-10 rounds of selection to identify capsid variants with enhanced properties

In principle, CREATE could be applied to discover AAV capsid variants that target defined,

CRE-expressing cell types in any organ. Thus, it could be used not only in transgenic

animals, as shown here, but also to develop AAV variants that target (i) specific Cre

cell

types in spheroid cultures

or organoid cultures, (ii) cells made Cre

in non-transgenic

animals by, for example, viral injections that achieve population-, projection

-, or activity-

based Cre expression

or (iii) Cre

human cells in human/mouse chimeric animals.

Given the reported AAV tropism differences between animal models and humans

selection schemes that use human Cre

cells

in vivo,

cell-specific Cre expression in three-

dimensional hiPSC-derived cellular models, or future Cre transgenic marmosets

may be

desirable for developing improved vectors for clinical applications. In addition, the success

of AAV-based gene therapies, especially those requiring systemic delivery, can be hindered

by the presence of neutralizing AAV capsid antibodies in the human population

. By

using CREATE together with exposure of AAV libraries to pooled human sera, one could

envision simultaneously selecting for capsids with retained or enhanced transduction

characteristics that are also less susceptible to antibody-mediated neutralization.

A limitation of CREATE and other reported capsid selection methods is that it is difficult to

predict, beyond an increase in target cell transduction efficiency, what characteristics the

enriched variants will have before they are tested. In our two trials for astrocyte targeting, we

identified several variants, AAV-PHP.B, B2, and B3 (

Supplementary Fig. 2

) that provide

broad CNS transduction of both neurons and glia, and AAV-PHP.A that provides selectively

more efficient astrocyte transduction. Identification of capsids with distinct properties from

the same selection scheme was expected given that the recovery method we used selected for

astrocyte transduction rather than for any specific intermediate step(s), e.g., brain vascular

association, BBB transcytosis or astrocyte binding/internalization. Therefore, capsid variants

that are more efficient at any of these intermediate steps should be recovered in our selection

process. Indeed, by immunostaining for capsids we found that unlike AAV9, both AAV-PHP

capsids readily localized to the brain vasculature shortly after intravenous administration

(

Supplementary Fig. 7a, b

). In addition, by 24 hours post-administration, significantly

more GFP-expressing cells were observed along the brain vasculature of mice that received

AAV-PHP.B as compared with those that received AAV9 or AAV-PHP.A (

Supplementary

Fig. 7c, d

). Considered together with the transduction characteristics of AAV-PHP.B and

AAV-PHP.A

in vivo

(

Figs. 2-4

) and in human neural cultures (

Supplementary Fig. 6

), these

data suggest that while both AAV-PHP vectors more efficiently associate with the brain

vasculature, they may differ in subsequent cell type-specific entry or transport step(s).

In the future, CREATE could be used with next-generation sequencing to better predict the

characteristics of the recovered sequences prior to testing the variants individually.

Sequencing both the entire pool of variants recovered from the Cre-expressing target cells

Deverman et al.

Page 5

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

along with the unselected virus library should enable quantification of the relative extent of

enrichment of each recovered sequence. Furthermore, sequencing capsids recovered from

multiple Cre-expressing or Cre non-expressing populations could provide a means to

perform both positive and negative selection in multiple cell types in a single experiment.

Such

in vivo-in silico

selection approaches should increase the power of CREATE to

enhance gene transfer to the CNS and other difficult-to-target cell populations.

METHODS

Plasmids

The rAAV-Cap-in-cis-lox genome plasmid contains three main elements flanked by AAV2

ITRs: (i) an mCherry expression cassette, which is comprised of a 398bp fragment of the

human UBC gene upstream of the mCherry cDNA followed by a synthetic polyadenylation

sequence

; (ii) the AAV9 capsid gene and regulatory sequences, which are comprised of the

AAV5 p41 promoter sequence (1680-1974 of GenBank AF085716.1)

and splicing

sequences taken from the AAV2 rep gene; and (iii) a Cre-dependent switch, which is

comprised of the SV40 polyadenylation sequence (pA) flanked by inverted lox71 and lox66

sites

(Fig. 1b). The rAAV-Cap-in-cis-lox genome plasmid was further modified to

introduce two unique restriction sites, XbaI and AgeI, within the capsid sequence. These

sites flank the region (AA450-592) that is replaced by the randomized library fragment. The

introduction of the XbaI site introduces a K449R mutation, which does not have an overt

effect on vector production or transduction. The mutations required to insert the AgeI site

are silent. For the rAAV-ΔCap-in-cis acceptor plasmid used for the capsid library cloning,

the coding region between the XbaI and AgeI sites was removed to prevent virus production

from the acceptor plasmid lacking the library fragment.

As a template for the library fragment, we PCR amplified the region spanning the XbaI and

AgeI sites of the modified AAV9. This sequence was modified to remove a unique EarI

restriction site and insert a unique KpnI site (both silent mutations) to create the xE

fragment. The modified xE fragment was TA cloned into pCRII (Life Technologies) to

generate pCRII-9Cap-xE. Eliminating the EarI site provided a second method that could be

used, if necessary, to selectively digest contaminating (AAV9) capsid sequences recovered

by PCR, but not digest the library-derived sequences. We did not find it necessary to use this

digestion step. Using the rAAV-ΔCap-in-cis acceptor for cloning the libraries and taking

standard PCR precautions (e.g., UV treating reagents and pipettors) was sufficient to prevent

contamination.

The AAV2/9 REP-AAP helper plasmid was constructed by introducing five stop codons into

the coding sequence of the VP reading frame of the AAV9 gene at VP1 AAs: 6, 10, 142, 148

and 216. The stop codon at AA216 was designed not to disrupt the coding sequence of the

AAP protein, which is encoded within an alternative reading frame.

Several rAAV genomes were used in this study. Each is constructed within a single stranded

(ss) rAAV genome with a reporter driven by the ubiquitous CMV-

-Actin-intron-

-Globin

hybrid promoter (CAG). For simplicity, the vector descriptions have been abbreviated in the

text. ssAAV-CAG-GFP refers to ssAAV-CAG-eGFP-2A-Luc-WPRE-SV40 polyA. ssAAV-

Deverman et al.

Page 6

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

CAG-NLS-GFP refers to ssAAV-CAG-NLS-GFP-WPRE-SV40 polyA, which was

constructed by inserting the nuclear localization sequence PKKKRKV at both the N- and C-

termini of GFP. ssAAV-CAG-mNeGreen-f refers to ssAAV-CAG-mNeonGreen-f-WPRE

with a human growth hormone polyA signal. The mNeonGreen

was modified with the

membrane targeting (farnesylation and palmitoylation signals) sequence from c-Ha-Ras

Capsid library generation

The random 7-mer library fragment (inserted between amino acids 588 and 589) was

generated by PCR using Q5 Hot Start High-Fidelity DNA Polymerase (NEB; M0493),

primers XF and 7×MNN and pCRII-9Cap-xE as a template. A schematic showing the

approximate primer binding sites and a table of the primer sequences are given in

Supplementary Figure 1

and

Supplementary Table 1

, respectively. To generate the rAAV-

based library, the PCR products containing the library and the XbaI- and AgeI-digested

rAAV-ΔCap-in-cis acceptor plasmid were assembled using Gibson Assembly (NEB; E2611).

The reaction products were then treated with Plasmid Safe (PS) DNase (Epicentre; E3105K)

to digest any unassembled fragments and purified using a QIAquick PCR Purification Kit

(Qiagen). This reaction typically yielded over 100 ng of assembled plasmid (as defined by

the amount of DNA remaining after the PS DNase digestion step). 100 ng is sufficient to

transfect ten 150mm tissue culture dishes at 10 ng/dish. Note, the libraries can also be

constructed by ligation or Gibson Assembly and then amplified in

E. coli

, but bacterial

transformation reduces the library diversity. By directly transfecting the assembled reaction

products, the library diversity is limited instead by the number of successfully transfected

HEK293 producer cells.

Virus production and purification

Recombinant AAVs were generated by triple transfection of 293T cells (ATCC) using

polyethylenimine (PEI)

. Viral particles were harvested from the media at 72 hrs post

transfection and from the cells and media at 120 hrs. Cell pellets were resuspended in 10mM

Tris with 2mM MgCl

, pH 8, freeze-thawed three times, and treated with 100 U/mL

Benzonase (Epicentre) at 37°C for at least 1 hr. Viral media was concentrated by

precipitation with 8% polyethylene glycol 8000 (Sigma-Aldrich) with 500 mM sodium

chloride

, resuspended in Tris-MgCl

, and then added to the lysates. The combined stocks

were then adjusted to 500 mM NaCl, incubated at 37°C for 30 minutes, and clarified by

centrifugation at 2000 × g. The clarified stocks were then purified over iodixanol (Optiprep,

Sigma; D1556) step gradients (15%, 25%, 40% and 60%)

. Viruses were concentrated and

formulated in phosphate buffered saline (PBS). Virus titers were determined by measuring

the number of DNaseI-resistant vg using qPCR with linearized genome plasmid as a

standard

For capsid library virus generation, two modifications were made to the above virus

production protocol to reduce the production of mosaic capsids that could arise from the

presence of multiple capsid sequences in the same cell. First, only 10 ng of the rAAV-Cap-

in-cis library plasmid was transfected (per 150 mm dish) to increase the likelihood that most

transfected cells only received one capsid variant sequence. Second, the virus was collected

at 48 hrs (media) and 60 hrs (cells and media), rather than at 72 hrs and 120 hrs as described

Deverman et al.

Page 7

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

above, to minimize the secondary transduction of producer cells with rAAV library virus

released into the medium.

Animals

All procedures were approved by the California Institute of Technology Institutional Animal

Care and Use Committee (IACUC). GFAP-Cre mice expressing Cre under the control of the

mouse GFAP promoter (012886)

and C57Bl/6J mice (000664) were purchased from the

Jackson Laboratory (JAX). Intravenous administration of rAAV vectors was performed by

injecting the virus into the retro-orbital sinus. Mice were randomly assigned to groups of

predetermined sample size. No mice were excluded from these analyses. Experimenters

were not blinded to sample groups.

In vivo

selection

For the selections in GFAP-Cre mice, 1×10

vg of the capsid libraries were injected

intravenously into adult Cre

mice of either sex. Seven to eight days post-injection, mice

were euthanized and the brain and spinal cord were collected. Vector DNA was recovered

from one hemisphere of the brain and half of the spinal cord using 4-5 ml of Trizol (Life

Technologies; 15596). To purify viral DNA, the upper aqueous fraction was collected

according to the manufacturer's extraction protocol. We found that the aqueous fraction

contains a significant portion of the viral DNA genomes as well as RNA. RNA was then

digested by treatment with 1 uL of RNase A (Qiagen) at 37 °C overnight. Next, a two-step

PCR amplification strategy was used to selectively recover

Cap

sequences from Cre-

recombined genomes. The first amplification step preferentially amplifies Cre-recombined

rAAV-Cap-in-cis-lox sequences using the primers 9CapF and CDF (see

Supplementary

Fig. 1

). The PCR was performed for 20-26 cycles of 95°C for 20 sec, 60°C for 20 sec and

72°C for 30 sec using Q5 Hot Start High-fidelity DNA Polymerase. The PCR product was

then diluted 1:10 or 1:100 and then used as a template for a second Cre-independent PCR

reaction using primers XF and AR (

Supplementary Fig. 1C

). The second PCR generated

the fragment that was cloned back into the rAAV-ΔCap-in-cis acceptor plasmid as described

above. 1 μL of the Gibson Assembly reactions were then diluted 1:10 and transformed into

SURE2 competent cells (Agilent; 200152) to generate individual clones for sequencing.

Variants that showed evidence of enrichment were cloned into an AAV Rep-Cap plasmid

and transformed into DH5

competent cells (NEB). The novel AAV Rep-Cap variants, or

AAV2/9 Rep-Cap as a control, were then evaluated using one of the reporter genomes

described above.

Vector biodistribution

Six-week-old mice female C57Bl/6 mice were injected intravenously with 1×10

vg of the

ssAAV-CAG-GFP vector packaged into the indicated AAV capsid. Animals were randomly

assigned to groups. 25 days after injection, the mice were euthanized and tissues and

indicated brain regions were collected and frozen at −80°C. DNA was isolated from the

tissue samples using Qiagen DNeasy Blood and Tissue kit. Vector genomes were detected

using PCR primers that bind to the WPRE element and were normalized to mouse genomes

using primers specific to the mouse glucagon gene. Absolute quantification was performed

Deverman et al.

Page 8

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

using serial dilutions of linearized plasmid standards of known concentration

. One

randomly chosen animal injected with AAV-PHP.B was removed from the bio-distribution

study for histological analysis.

Tissue preparation, immunohistochemistry and imaging

Mice were anesthetized with Nembutal and transcardially perfused with 0.1 M phosphate

buffer (PB) at room temperature (RT) at pH 7.4 and then with freshly prepared, ice-cold 4%

paraformaldehyde (PFA) in PB. Brains were post-fixed in 4% PFA overnight and then

sectioned by vibratome or cryoprotected and sectioned by cryostat. IHC was performed on

floating sections with primary and secondary antibodies in PBS containing 10% goat or

donkey serum and 0.5% Triton X-100 (no detergent was used for GAD67 staining). Primary

antibodies used were mouse anti-AAV capsid (1:20; American Research Products,

03-65158, clone B1), rabbit anti-GFP (1:1000; Invitrogen, A11122), chicken anti-GFP

(1:1000; Abcam, ab13970), mouse anti-CC1 (1:200; Calbiochem, OP80), rabbit anti-GFAP

(1:1000; Dako, Z0334), mouse anti-NeuN (1:500; Millipore, MAB377), rabbit anti-IbaI

(1:500; Biocare Medical, CP290), mouse anti-Calbindin D28K (1:200; Sigma, CB-955),

rabbit anti-Calretinin (1:1000; Chemicon, AB5054), mouse anti-GAD67 (1:1000; Millipore,

MAB5406), guinea pig anti–MAP2 (1:1000; Synaptic Systems, 188004), mouse anti-

Parvalbumin (1:1000; Sigma), Tyrosine Hydroxlyase (1:1000, Aves) and rabbit anti-CD31

(1:50; Abcam, ab28364). Primary antibodies incubations were performed for 16-24 hrs at

RT. The sections were then washed and incubated with secondary Alexa-conjugated

antibodies (1:1000; Invitrogen) for 2-16 hrs. For capsid detection with the B1 antibody that

recognizes an internal epitope

, floating sections were treated with 2M HCl for 15 minutes

at 37°C and then washed extensively with PBS prior to incubation with the primary

antibody. For some images, the 16-bit green channel (GFP) gamma was adjusted to enable

visualization (without oversaturation) of both low and high GFP-expressing cells present

within the same field of view. In all cases, changes to gamma or contrast as well as

microscope and laser settings remained consistent across sets of images. Images were taken

with a Zeiss LSM 780 confocal microscope fitted with the following objectives: Fluar 5×/

0.25 M27 Plan-Apochromat 10×/0.45 M27 (working distance 2.0 mm), Plan-Apochromat

25×/0.8 Imm Corr DIC M27 multi-immersion and LD C-Apochromat 40×/1.1 W Korr and

Plan-Apochromat 100×/1.46 Oil DIC objectives. 3D MIP images and Supplementary

Movies were generated with Imaris (Bitplane).

Quantification of cell type-specific transduction

Six-week-old female mice were randomly assigned to groups and injected intravenously

with 2×10

vg of ssAAV-CAG-NLS-GFP packaged into AAV9, AAV-PHP.B or AAV-

PHP.A. Three weeks later, the mice were perfused and the brains were processed and

immunostained for the indicated antigen as described above. The number of animals per

group was pre-established; no animals were excluded from the analysis. Confocal single-

plane images of the cell type-specific immunostaining and native NLS-GFP fluorescence

were taken. To prevent bias, images were taken from the indicated matched regions

identified by viewing only the cell type-specific immunostaining channel, rather than from

GFP expression, prior to image acquisition. Likewise, cell counting was performed by first

counting and marking each cell stained by the cell-specific antigen by viewing the IHC

Deverman et al.

Page 9

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

channel. Next those marked IHC

cells that were positive for native GFP fluorescence were

counted. Due to the stark transduction efficiency differences between capsids, the counting

was not blinded by group.

Tissue clearing

Mice were perfused as above with 60-80 mL of ice-cold 4% PFA in PB at a flow rate of 14

mL per minute. The flow rate was then reduced to 2-3 mL/min and continued for 2 hrs at

RT. The mice were then placed in individual custom-built chambers

and perfused with 200

mL of recycling RT 4% acrylamide in PB at 2-3 mL/min overnight followed by a 2-hr

perfusion flush with PB to remove residual polymers/monomers from the vasculature. The

polymerization process was initiated by placing the chambers in a 42°C water bath and

delivering, by perfusion (2-3 mL/min), of 200 mL of recycling, degassed PB containing

0.25% VA-044 initiator for 2-4 hrs. The mice were then perfused with 8% SDS in PB, pH

7.5 for 7 days. The SDS containing solution was refreshed two times during the 7 days and

then flushed out by perfusion of 2 L of non-recirculating PB overnight. Cleared tissue

samples were mounted in RIMS solution (refractive index of 1.46)

for imaging.

Generation of cortical spheroids from human iPSC

Human cortical spheroids were generated from iPSC as previously described

. Briefly,

iPSC lines derived from two healthy control individuals were grown on inactivated mouse

embryonic fibroblast feeders in the following medium: DMEM/F12, Knockout Serum 20%,

1 mM non-essential amino acids (1:100), GlutaMax (1:200),

-mercaptoethanol (0.1 mM),

penicillin and streptomycin (1:100) (Life Technologies). Cultures were regularly tested and

maintained mycoplasma free. Colonies of iPSCs were detached intact with dispase (0.35

mg/ml, Invitrogen) and transferred into low-attachment plates in iPSC medium

supplemented with dorsomorphin (5 μM, Sigma) and SB-431542 (10 μM, Tocris), and the

medium was changed daily. On day six of

in vitro

differentiation, neural spheroids were

transferred to NPC medium (Neurobasal A, B27 without vitamin A, GlutaMax (1:100),

penicillin and streptomycin; Life Technologies), which was supplemented with EGF (20

ng/ml) and FGF2 (20 ng/ml) until day 24, and then supplemented with BDNF (20 ng/ml)

and NT3 (20 ng/ml) from day 25 to 42. From day 43 onwards, cortical spheroids were

maintained in NPC medium, which was changed every 4 days.

Dissociation and viral infection of cortical spheroids

For enzymatic dissociation and culture in monolayer, cortical spheroids at day 170-200 of

vitro

differentiation (two independent neural differentiations of one iPSC line from one

individual and one differentiation of an iPSC line from another individual) were incubated

with Accutase (Innovative Cell Technologies) for 25 min at 37°C, washed three times with

NPC media and gently triturated with a P-200 pipette. Cells were plated on poly-ornithine

and laminin coated glass coverslip (15 mm) at ~300,000 cells/well and maintained in NPC

media supplemented with BDNF (20 ng/ml) and NT3 (20 ng/ml) for the first 24 hrs, and

then maintained in NPC media without growth factors.

Cultures grown on coverslips were infected with each of the viruses at a titer of 1×10

vg/

well and fixed 5 days later with 4% paraformaldehyde (PFA) for 10 min. For

Deverman et al.

Page 10

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

immunocytochemistry, cells were permeabilized with 0.2% Triton X-100 for 10 min and

blocked with 10% goat serum in PBS for 1 hr. Coverslips were then incubated with

antibodies diluted in blocking solution for 2 hr. Nuclei were visualized with Hoechst 33258

(Life Technologies, 1:10,000).

Cells were imaged with a Zeiss M1 Axioscope using a 40× objective. The proportion of

GFP

cells co-labeled with either GFAP or MAP2 was quantified in images of 10 random

fields per coverslip for each experimental condition. Results presented are the average of

two separate dissociation and infection experiments.

To infect intact 3D cultures with AAVs, single human cortical spheroids at day 197 days of

in vitro

differentiation were transferred overnight into 1.5 ml Eppendorf tubes containing

6×10

vg/400 μl in NPC media, and were fixed 7 days later in 4% PFA overnight. Fixed

spheroids were then transferred into 30% sucrose for 24 hrs, embedded in O.C.T. (Fisher

Scientific) and cut at 14 μm sections. For immunohistochemistry, sections were blocked with

10% goat serum in PBS containing 0.3% Triton-X100 for 1 hr. Images were collected with a

Leica TCS SP8 confocal microscope.

Supplementary Material

Refer to Web version on PubMed Central for supplementary material.

ACKNOWLEDGMENTS

This article and the naming of the novel AAV clones is dedicated to the memory of Paul H. Patterson (PHP) who

passed away during the preparation of this manuscript. We wish to thank Laura Rodriguez and Pat Anguiano for

administrative assistance, Alex Balazs and Stijn Cassenaer and the entire Gradinaru and Patterson laboratories for

helpful discussions and Andrea Choe for helpful comments on the manuscript. We thank the U. Penn vector core

for the AAV2/9 rep-cap plasmid, A. Balazs and David Baltimore for the AAV genome plasmid, and the Biological

Imaging Facility, supported by the Caltech Beckman Institute and the Arnold and Mabel Beckman Foundation, for

use of imaging equipment. This work was supported by the Hereditary Disease foundation and the Caltech-City of

Hope Biomedical Initiative (to PHP), and by grants to VG: NIH Director's New Innovator IDP20D017782-01;

NIH/NIA 1R01AG047664-01; Beckman Institute for CLARITY, Optogenetics and Vector Engineering Research;

Gordon and Betty Moore Foundation through Grant GBMF2809 to the Caltech Programmable Molecular

Technology Initiative. Work in the Gradinaru Laboratory is also funded by the following awards (to VG): NIH

BRAIN 1U01NS090577; NIH/NIMH 1R21MH103824-01; Pew Charitable Trust; Kimmel Foundation; Human

Frontiers in Science Program; Caltech-GIST; Caltech-City of Hope Biomedical Initiative. Work in the Pasca

Laboratory is supported by a US National Institute of Mental Health (NIMH) 1R01MH100900 and

1R01MH100900-02S1, the NIMH BRAINS Award (R01MH107800), MQ Fellow Award and the Donald E. and

Delia B. Baxter Foundation Scholar Award (to S.P.P.).

References

1. Kaplitt MG, et al. Safety and tolerability of gene therapy with an adeno-associated virus (AAV)

borne GAD gene for Parkinson's disease: an open label, phase I trial. Lancet. 2007; 369:2097–2105.

doi:10.1016/S0140-6736(07)60982-9. [PubMed: 17586305]

2. Wu Z, Asokan A, Samulski RJ. Adeno-associated virus serotypes: vector toolkit for human gene

therapy. Molecular therapy : the journal of the American Society of Gene Therapy. 2006; 14:316–

327. doi:10.1016/j.ymthe.2006.05.009. [PubMed: 16824801]

3. High KH, Nathwani A, Spencer T, Lillicrap D. Current status of haemophilia gene therapy.

Haemophilia : the official journal of the World Federation of Hemophilia 20 Suppl. 2014; 4:43–49.

doi:10.1111/hae.12411.

Deverman et al.

Page 11

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

4. Borel F, Kay MA, Mueller C. Recombinant AAV as a platform for translating the therapeutic

potential of RNA interference. Molecular therapy : the journal of the American Society of Gene

Therapy. 2014; 22:692–701. doi:10.1038/mt.2013.285. [PubMed: 24352214]

5. Ojala DS, Amara DP, Schaffer DV. Adeno-associated virus vectors and neurological gene therapy.

Neuroscientist. 2015; 21:84–98. doi:10.1177/1073858414521870. [PubMed: 24557878]

6. Betley JN, Sternson SM. Adeno-associated viral vectors for mapping, monitoring, and manipulating

neural circuits. Hum Gene Ther. 2011; 22:669–677. doi:10.1089/hum.2010.204. [PubMed:

21319997]

7. Bartlett JS, Kleinschmidt J, Boucher RC, Samulski RJ. Targeted adeno-associated virus vector

transduction of nonpermissive cells mediated by a bispecific F(ab'gamma)2 antibody. Nat

Biotechnol. 1999; 17:181–186. doi:10.1038/6185. [PubMed: 10052356]

8. Muller OJ, et al. Random peptide libraries displayed on adeno-associated virus to select for targeted

gene therapy vectors. Nat Biotechnol. 2003; 21:1040–1046. doi:10.1038/nbt856. [PubMed:

12897791]

9. Grimm D, et al. In vitro and in vivo gene therapy vector evolution via multispecies interbreeding and

retargeting of adeno-associated viruses. Journal of virology. 2008; 82:5887–5911. doi:10.1128/JVI.

00254-08. [PubMed: 18400866]

10. Dalkara D, et al. In vivo-directed evolution of a new adeno-associated virus for therapeutic outer

retinal gene delivery from the vitreous. Science translational medicine. 2013; 5:189ra176. doi:

10.1126/scitranslmed.3005708.

11. Lisowski L, et al. Selection and evaluation of clinically relevant AAV variants in a xenograft liver

model. Nature. 2014; 506:382–386. doi:10.1038/nature12875. [PubMed: 24390344]

12. Maheshri N, Koerber JT, Kaspar BK, Schaffer DV. Directed evolution of adeno- associated virus

yields enhanced gene delivery vectors. Nature biotechnology. 2006; 24:198–204. doi:10.1038/

nbt1182.

13. Excoffon KJDA, et al. Directed evolution of adeno-associated virus to an infectious respiratory

virus. Proceedings of the National Academy of Sciences of the United States of America. 2009;

106:3865–3870. doi:10.1073/pnas.0813365106. [PubMed: 19237554]

14. Foust KD, et al. Intravascular AAV9 preferentially targets neonatal neurons and adult astrocytes.

Nature biotechnology. 2009; 27:59–65. doi:10.1038/nbt.1515.

15. Bevan AK, et al. Systemic gene delivery in large species for targeting spinal cord, brain, and

peripheral tissues for pediatric disorders. Molecular therapy : the journal of the American Society

of Gene Therapy. 2011; 19:1971–1980. doi:10.1038/mt.2011.157. [PubMed: 21811247]

16. Maguire CA, Ramirez SH, Merkel SF, Sena-Esteves M, Breakefield XO. Gene therapy for the

nervous system: challenges and new strategies. Neurotherapeutics. 2014; 11:817–839. doi:

10.1007/s13311-014-0299-5. [PubMed: 25159276]

17. Gray SJ, et al. Preclinical Differences of Intravascular AAV9 Delivery to Neurons and Glia: A

Comparative Study of Adult Mice and Nonhuman Primates. Molecular therapy : the journal of the

American Society of Gene Therapy. 2011; 19:1058–1069. doi:10.1038/mt.2011.72. [PubMed:

21487395]

18. Maguire AM, et al. Safety and efficacy of gene transfer for Leber's congenital amaurosis. N Engl J

Med. 2008; 358:2240–2248. doi:10.1056/NEJMoa0802315. [PubMed: 18441370]

19. Nathwani AC, et al. Long-term safety and efficacy following systemic administration of a self-

complementary AAV vector encoding human FIX pseudotyped with serotype 5 and 8 capsid

proteins. Molecular therapy : the journal of the American Society of Gene Therapy. 2011; 19:876–

885. doi:10.1038/mt.2010.274. [PubMed: 21245849]

20. Gaudet D, et al. Review of the clinical development of alipogene tiparvovec gene therapy for

lipoprotein lipase deficiency. Atherosclerosis. Supplements. 2010; 11:55–60. doi:10.1016/

j.atherosclerosissup.2010.03.004. [PubMed: 20427244]

21. Pulicherla N, et al. Engineering Liver-detargeted AAV9 Vectors for Cardiac and Musculoskeletal

Gene Transfer. Molecular therapy : the journal of the American Society of Gene Therapy. 2011;

19:1070–1078. doi:10.1038/mt.2011.22. [PubMed: 21364538]

Deverman et al.

Page 12

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

22. Sonntag F, Schmidt K, Kleinschmidt JA. A viral assembly factor promotes AAV2 capsid formation

in the nucleolus. Proceedings of the National Academy of Sciences of the United States of

America. 2010; 107:10220–10225. doi:10.1073/pnas.1001673107. [PubMed: 20479244]

23. Garcia ADR, Doan NB, Imura T, Bush TG, Sofroniew MV. GFAP-expressing progenitors are the

principal source of constitutive neurogenesis in adult mouse forebrain. Nature neuroscience. 2004;

7:1233–1241. doi:10.1038/nn1340. [PubMed: 15494728]

24. Yang B, et al. Single-Cell Phenotyping within Transparent Intact Tissue through Whole-Body

Clearing. Cell. 2014; 158:945–958. doi:10.1016/j.cell.2014.07.017. [PubMed: 25088144]

25. Xie J, et al. MicroRNA-regulated, Systemically Delivered rAAV9: A Step Closer to CNS-

restricted Transgene Expression. Molecular therapy : the journal of the American Society of Gene

Therapy. 2010; 19:526–535. doi:10.1038/mt.2010.279. [PubMed: 21179009]

26. Samaranch L, et al. Adeno-associated virus serotype 9 transduction in the central nervous system

of nonhuman primates. Hum Gene Ther. 2012; 23:382–389. doi:10.1089/hum.2011.200. [PubMed:

22201473]

27. Dufour BD, Smith CA, Clark RL, Walker TR, McBride JL. Intrajugular vein delivery of AAV9-

RNAi prevents neuropathological changes and weight loss in Huntington's disease mice.

Molecular therapy : the journal of the American Society of Gene Therapy. 2014; 22:797–810. doi:

10.1038/mt.2013.289. [PubMed: 24390280]

28. Bartlett, JS.; Samulski, RJ.; McCown, TJ. Selective and Rapid Uptake of Adeno-Associated Virus

Type 2 in Brain. 1998.

http://dx.doi.org/10.1089/hum.1998.9.8-1181

29. Wang H, et al. Widespread spinal cord transduction by intrathecal injection of rAAV delivers

efficacious RNAi therapy for amyotrophic lateral sclerosis. Hum Mol Genet. 2014; 23:668–681.

doi:10.1093/hmg/ddt454. [PubMed: 24108104]

30. Chakrabarty P, et al. Capsid serotype and timing of injection determines AAV transduction in the

neonatal mice brain. PLoS One. 2013; 8:e67680. doi:10.1371/journal.pone.0067680. [PubMed:

23825679]

31. Pasca AM, et al. Functional cortical neurons and astrocytes from human pluripotent stem cells in

3D culture. Nature methods. 2015; 12:671–678. doi:10.1038/nmeth.3415. [PubMed: 26005811]

32. Ying Y, et al. Heart-targeted adeno-associated viral vectors selected by in vivo biopanning of a

random viral display peptide library. Gene therapy. 2010; 17:980–990. doi:10.1038/gt.2010.44.

[PubMed: 20393510]

33. Wall NR, Wickersham IR, Cetin A, De La Parra M, Callaway EM. Monosynaptic circuit tracing in

vivo through Cre-dependent targeting and complementation of modified rabies virus. Proc Natl

Acad Sci U S A. 2010; 107:21848–21853. doi:10.1073/pnas.1011756107. [PubMed: 21115815]

34. Kawashima T, et al. Functional labeling of neurons and their projections using the synthetic

activity-dependent promoter E-SARE. Nat Methods. 2013; 10:889–895. doi:10.1038/nmeth.2559.

[PubMed: 23852453]

35. Guenthner CJ, Miyamichi K, Yang HH, Heller HC, Luo L. Permanent genetic access to transiently

active neurons via TRAP: targeted recombination in active populations. Neuron. 2013; 78:773–

784. doi:10.1016/j.neuron.2013.03.025. [PubMed: 23764283]

36. Izpisua Belmonte JC, et al. Brains, genes, and primates. Neuron. 2015; 86:617–631. doi:10.1016/

j.neuron.2015.03.021. [PubMed: 25950631]

37. van der Marel S, et al. Neutralizing antibodies against adeno-associated viruses in inflammatory

bowel disease patients: implications for gene therapy. Inflamm Bowel Dis. 2011; 17:2436–2442.

doi:10.1002/ibd.21673. [PubMed: 21370319]

38. Calcedo R, Vandenberghe LH, Gao G, Lin J, Wilson JM. Worldwide epidemiology of neutralizing

antibodies to adeno-associated viruses. J Infect Dis. 2009; 199:381–390. doi:10.1086/595830.

[PubMed: 19133809]

39. Boutin S, et al. Prevalence of serum IgG and neutralizing factors against adeno-associated virus

(AAV) types 1, 2, 5, 6, 8, and 9 in the healthy population: implications for gene therapy using

AAV vectors. Hum Gene Ther. 2010; 21:704–712. doi:10.1089/hum.2009.182. [PubMed:

20095819]

40. Levitt N, Briggs D, Gil A, Proudfoot NJ. Definition of an efficient synthetic poly(A) site. Genes

and Development. 1989; 3:1019–1025. doi:10.1101/gad.3.7.1019. [PubMed: 2570734]

Deverman et al.

Page 13

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

41. Chiorini JA, Kim F, Yang L, Kotin RM. Cloning and characterization of adeno- associated virus

type 5. J Virol. 1999; 73:1309–1319. [PubMed: 9882336]

42. Farris KD, Pintel DJ. Improved Splicing of Adeno-Associated Viral (AAV) Capsid Protein-

Supplying Pre-mRNAs Leads to Increased Recombinant AAV Vector Production. Human gene

therapy. 2008; 19:1421–1427. doi:10.1089/hum.2008.118. [PubMed: 18785816]

43. Albert H, Dale EC, Lee E, Ow DW. Site-specific integration of DNA into wild-type and mutant lox

sites placed in the plant genome. The Plant journal : for cell and molecular biology. 1995; 7:649–

659. [PubMed: 7742860]

44. Shaner NC, et al. A bright monomeric green fluorescent protein derived from Branchiostoma

lanceolatum. Nat Methods. 2013; 10:407–409. [PubMed: 23524392]

45. Hancock JF, Cadwallader K, Paterson H, Marshall CJ. A CAAX or a CAAL motif and a second

signal are sufficient for plasma membrane targeting of ras proteins. EMBO J. 1991; 10:4033–4039.

[PubMed: 1756714]

46. Gray SJ, et al. Production of recombinant adeno-associated viral vectors and use in in vitro and in

vivo administration. Current protocols in neuroscience / editorial board, Jacqueline N. Crawley.

2011 [et al.] Chapter 4, Unit 4 17, doi:10.1002/0471142301.ns0417s57.

47. Ayuso E, et al. High AAV vector purity results in serotype- and tissue-independent enhancement of

transduction efficiency. Gene therapy. 2010; 17:503–510. doi:10.1038/gt.2009.157. [PubMed:

19956269]

48. Zolotukhin S, et al. Recombinant adeno-associated virus purification using novel methods

improves infectious titer and yield. Gene therapy. 1999; 6:973–985. doi:10.1038/sj.gt.3300938.

[PubMed: 10455399]

49. Wobus CE, et al. Monoclonal antibodies against the adeno-associated virus type 2 (AAV-2) capsid:

epitope mapping and identification of capsid domains involved in AAV-2-cell interaction and

neutralization of AAV-2 infection. J Virol. 2000; 74:9281–9293. [PubMed: 10982375]

Deverman et al.

Page 14

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

Figure 1. Cre-dependent recovery of AAV capsid sequences from transduced target cells

(

) An overview of the CREATE selection process. PCR is used to introduce diversity (full

visual spectrum vertical band) into a capsid gene fragment (yellow). The fragment is cloned

into the rAAV genome harboring the remaining capsid gene (gray) and is used to generate a

library of virus variants. The library is injected into Cre transgenic animals and PCR is used

to selectively recover capsid sequences from Cre

cells. (

) The rAAV-Cap-in-cis-lox rAAV

genome. Cre inverts the polyadenylation (pA) sequence flanked by the lox71 and lox66

sites. PCR primers (half arrows) are used to selectively amplify Cre-recombined sequences.

(

) PCR products from Cre recombination-dependent (top) and -independent (bottom)

amplification of capsid library sequences recovered from two Cre

or Cre

−

mice are shown.

Schematics (bottom) show the PCR amplification strategies (see

Supplementary Fig. 1

for

details). (

) Schematic shows the AAV genes within the Rep-AAP AAV helper plasmid and

the proteins encoded by the

cap

gene. Stop codons inserted in the

cap

gene eliminate VP1,

VP2 and VP3 capsid protein expression. (

) DNase-resistant AAV vector genomes (vg)

produced with the split AAV2/9 rep-AAP and rAAV-Cap-in-cis-lox genome (top) as

compared to the vg produced with standard AAV2/9 rep-cap helper and rAAV-UBC-

mCherry genome (middle) or with the AAV2/9 rep-AAP and rAAV-UBC-mCherry genome

(bottom).

=3 independent trials per group; mean ± s.d.; **

<0.01, ***

<0.001; one-way

ANOVA and Tukey multiple comparison test. (

) Cloning the 7-mer capsid library into the

rAAV-ΔCap-in-cis vector. (

) The AAV9 surface model shows the location of the 7-mer

inserted between AA588-589 (magenta). Sites encoded with the PCR-generated library

fragment (AA450-592) are shown in yellow.

Deverman et al.

Page 15

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

Figure 2. AAV-PHP.B mediates efficient gene delivery throughout the CNS after intravenous

injection in adult mice

(

a-f

) ssAAV9:CAG-GFP or ssAAV-PHP.B:CAG-GFP, at 1×10

vg/mouse or 1×10

(

right), was intravenously injected into adult mice. Images show GFP expression 3 weeks

after injection. (

) Representative images of GFP IHC in the brains of mice given AAV9

(left) or AAV-PHP.B (middle and right). (

Native GFP fluorescence in the cortex (left) or

striatum (right) in 50 μm maximum intensity projection (MIP) confocal images. (

GFP

fluorescence in the PARS-cleared

lumbar spinal cord. (

GFP fluorescence in the retina

(left: 20 μm MIP, transverse section; right: whole-mount MIP).

GFP fluorescence in 3D

MIP images of PARS-cleared tissue from AAV-PHP.B transduced cortex and striatum (

)

and indicated organs from mice transduced with AAV9 (top) or AAV-PHP.B (bottom) (

Arrows highlight GFP

nerves. Asterisks in the image of the pancreas highlight GFP

islet

cells. Major tick marks in 3D projections are 100 μm. (

AAV biodistribution in the

Deverman et al.

Page 16

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript

indicated brain regions (top) and organs (bottom) 25 days after intravenous injection of

1×10

vg into adult mice.

=3 for AAV-PHP.B and

=4 for AAV9; mean ± s.d.; **

<0.01,

***

<0.001, unpaired t tests corrected for multiple comparisons by the Holm-Sidak method.

Scale bars: 1 mm (

(left)); 50 μm

(right),

). Major tick marks in 3D projections

are 100 μm.

Deverman et al.

Page 17

Nat Biotechnol

. Author manuscript; available in PMC 2016 October 31.

Author Manuscript