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Experimental Neurology 1
Effects of the perivascular space on convection-enhanced delivery of
liposomes in primate putamen
Michal T. Krauzea, Ryuta Saitoa, Charles Nobleb, John Bringasa, John Forsayetha,
Tracy R. Mcknightc, John Parkb, Krystof S. Bankiewicza,*
aDepartment of Neurological Surgery, Laboratory of Molecular Therapeutics, University of California, 1855 Folsom Street,
Room 226, San Francisco, CA 94103, USAbDivision of Hematology-Oncology, University of California, San Francisco, CA 94103, USA
cDepartment of Radiology, University of California, San Francisco, CA 94103, USA
Received 3 May 2005; revised 11 July 2005; accepted 14 July 2005
Available online 16 August 2005
Abstract
Convection-enhanced delivery has recently entered the clinic and represents a promising new therapeutic option in the field of
neurodegenerative diseases and treatment of brain tumors. Understanding of the principles governing delivery and flow of macromolecules
within the CNS is still poorly understood and requires more investigation of the microanatomy and fluid dynamics of the brain. Our
previously established, reflux-free convection-enhanced delivery (CED) technique and real-time imaging MR method for monitoring CED
delivery of liposomes in primate CNS allowed us to closely monitor infusions of putamen. Our findings indicate that CED in putamen is
associated with perivascular transport of liposomes, throughout CNS arteries. The results may explain side effects seen in current clinical
trials using CED. In addition, they clearly show the necessity for a monitoring technique for future direct delivery of therapeutic agents to the
human central nervous system. Based on these findings, we believe that the physiological concept that the perivascular space serves as a
conduit for distribution of endogenous molecules within the CNS also applies to interstitially infused agents.
D 2005 Elsevier Inc. All rights reserved.
Keywords: Convection-enhanced delivery; MRI; Primate; Liposomes; Perivascular space; Putamen
Introduction
Direct delivery of therapeutic agents to the human central
nervous system (CNS) is one of the most challenging new
approaches for gene and molecular therapy for neurological
diseases. Mechanisms and pathways by which drugs and viral
vectors are distributed in the CNS are still under investigation
and remain an unpredictable factor for clinical studies. A
clearer understanding of how the microanatomy and fluid
dynamics of the brain govern delivery and flow of macro-
molecules within the CNS still requires more investigation.
In the present study, we have investigated the distribution
of liposomes delivered by CED in non-human primate
putamen. We have previously established a reflux-free CED
0014-4886/$ - see front matter D 2005 Elsevier Inc. All rights reserved.
doi:10.1016/j.expneurol.2005.07.009
* Corresponding author. Fax: +1 415 514 2177.
E-mail address: [email protected] (K.S. Bankiewicz).
technique and real-time imaging MR method for monitoring
CED delivery of liposomes in primate CNS (Saito et al.,
submitted for publication). This allowed us to monitor
liposomal distribution in real time in the putamen nucleus.
In addition to observing the robust distribution of liposomes
in the putamen, the most important finding was liposomal
‘‘leakage’’ along primate cerebral arteries, a phenomenon
independent of the cannula placement. This finding suggested
the existence of a transport mechanism further to the pressure
gradient provided by CED.
The concept that the perivascular space serves as a conduit
for the distribution of molecules within the CNS has been
explored for the last 30 years or so (Cserr and Ostrach, 1974;
Rennels et al., 1985, 1990). Perivascular spaces are extensions
of the subarachnoid spaces that accompany vessels that
penetrate the brain down to the level of capillaries. Physio-
logical and anatomical studies in a variety of mammalian
96 (2005) 104 – 111
M.T. Krauze et al. / Experimental Neurology 196 (2005) 104–111 105
species have emphasized the immunological role of perivas-
cular spaces in the brain similar to lymphatic drainage
pathways (Kida et al., 1995; Knopf et al., 1995; Weller et
al., 1992, 1996). Tracers injected into rat gray matter drain
along perivascular spaces which are lined by immunocompe-
tent perivascular cells (Cserr et al., 1992; Kida et al., 1993).
This lymphatic drainage pathway plays a key role in the
immunology of the central nervous system, perhaps explaining
why removal of cervical lymph nodes significantly reduces
immune reactions in the brain mediated by both B and T
lymphocytes (Cserr et al., 1992; Harling-Berg et al., 1989;
Knopf et al., 1995; Phillips et al., 1995, 1997; Weller et al.,
1996). Previous studies of peri-arterial spaces in the human
cerebral cortex have shown that arteries are surrounded by a
layer of leptomeninges that is subtended from the pia mater
(Zhang et al., 1990) and, by this anatomical arrangement, the
perivascular spaces of the intra-cortical arteries are contiguous
with the peri-arterial domains in the sub-arachnoid space. The
lack of similar coating of leptomeningeal cells around veins in
the cerebral cortex suggests that peri-venous spaces are
contiguous with the sub-pial space (Weller, 1995; Zhang et
al., 1990) and probably do not function as lymphatic drainage
pathways in the same way as peri-arterial spaces (Pollock et
al., 1997). Further studies revealed that arteries in the basal
ganglia are surrounded by 2 distinct layers of leptomeninges
separated by a perivascular space contiguous with the peri-
arterial, sub-arachnoid space (Pollock et al., 1997). The
anatomy of the peri-arterial spaces in the basal ganglia differs
significantly from those in the cerebral cortex where there is
only a single peri-arterial layer of leptomeninges. Pollock and
colleagues have suggested that differences seen in the structure
of peri-arterial spaces in different sites in the brain may be
reflected in differing relative efficiencies in the drainage of
interstitial fluid (Pollock et al., 1997). Drainage in perivascular
spaces has been examined with various markers and is clearly
affected by cardiac pulsation of cerebral arteries (Rennels et
al., 1985).
In this study, we tested the hypothesis that perivascular
spaces of lateral striate arteries in the putamen, and in large
sub-arachnoid arteries, are capable of transporting therapeu-
tic agents throughout the CNS. This hypothesis is based
upon previously described physiological and anatomical
properties of perivascular spaces and observations of MR-
monitored liposomal infusions as well as histological
analysis of infused animals. Transport of liposomes in the
peri-arterial space could have implications for gene and
molecular therapy for neurological diseases and might
explain some side effects seen in clinical trials.
Methods
Liposome preparation
Separate liposomes were prepared for detection by MRI
and by histological examination. Liposomes that contained
the MRI contrast agent were composed of 1,2-dioleoyl-sn-
glycero-3-phosphocholine (DOPC)/cholesterol/1,2-dis-
tearoyl-sn-glycero-3-phosphoethanolamine-N-[methoxy(po-
lyethylene glycol)-2000] (PEG-DSPE) with a molar ratio of
3:2:0.3. DOPC and PEG-DSPE were purchased from Avanti
Polar Lipids (Alabaster, AL) and cholesterol was purchased
from Calbiochem (San Diego, CA). The lipids were
dissolved in chloroform/methanol (90:10, vol/vol), and then
the solvent was removed by rotary evaporation, resulting in
a dried lipid foam. The lipid foam was hydrated with a
commercial United States Pharmacopeia solution of 0.5 M
gadoteridol (a gadolinium complex of 10-(2-hydroxy-
propyl)-1,4,7,10-tetraazacyclododecane-1,4,7-triacetic acid,
Prohance; Bracco Diagnostics, Princeton, NJ) by 6 succes-
sive cycles for rapid freezing and thawing. Residual
chloroform was removed from the hydrated lipid by a brief
treatment with rotary evaporation. Unilamellar liposomes
were formed by extrusion (Lipex; Northern Lipids, Vancou-
ver, Canada) with 15 passes through double-stacked
polycarbonate membranes (Whatman Nucleopore, Clifton,
NJ) with a pore size of 100 nm, resulting in a liposome
diameter of 85.1 T 37.5 nm as determined by light scattering
(N4Plus particle size analyzer, Beckman Coulter, Fullerton,
LA). Unencapsulated gadoteridol was removed with a
Sephadex G-75 (Sigma, St. Louis, MO) size-exclusion
column eluted with HEPES-buffered saline (5 mM HEPES,
135 mM NaCl, pH 6.5, adjusted with NaOH).
Liposomes, loaded with sulforhodamine B for histolo-
gical studies, were formulated with the same lipid compo-
sition and preparation method as the gadoteridol-containing
liposomes except that the lipids were hydrated directly with
20 mM sulforhodamine B (Sigma) in HEPES-buffered
saline (pH 6.5) by 6 successive cycles of rapid freezing and
thawing. The sulforhodamine B liposomes had a diameter of
79.0 T 34.3 nm (used for co-infusion with the gadoteridol-
containing liposomes). Both of the final liposomal con-
structs consist of an ionic, water soluble, small molecule
indicator that is contained within the aqueous liposome
interior by the organized hydrophobic membrane bilayer.
Each liposome exterior surface has a slight negative net
charge from the presence of the PEG-DSPE at 10% (mol/
mol) of the phospholipid (6.0% of the total lipid).
Quantification of liposome-entrapped gadoteriodol by
magnetic resonance imaging
The concentration of gadoteriodol entrapped in the lip-
osomes was determined from nuclear MR relaxivity measure-
ments. The relationship between the change in the intrinsic
relaxation rate imposed by a paramagnetic agent (DR), also
known as ‘‘T1 shortening,’’ and the concentration of the agent
is defined by the equation: DR = r1[agent], in which r1 =
relaxivity of the paramagnetic agent and DR = (1/T1observed1/T1intrinsic). As gadoteriodol was encapsulated within the
liposome, we corrected for the change in the observed T1
imposed by the lipid by measurement of the T1 of solubilized
M.T. Krauze et al. / Experimental Neurology 196 (2005) 104–111106
liposomes with and without gadoteriodol by means of an
iterative inversion-recovery MRI sequence on a 2-T Brucker
Omega scanner (Brucker Medical, Karlsruhe, Germany). The
relaxivity of gadoteriodol had been empirically derived
previously on the same system and had a value of 4.07
mM�1 s�1. The concentration of the encapsulated gadoter-
iodol was then calculated with the following equation:
[gadoteriodol] = [(1/T1wGado) � (1/T1w/oGado)]/4.07.
Experimental subjects
The protocol was reviewed and approved by the Institu-
tional Animal Care and Use Committees at the University of
California San Francisco (San Francisco, CA). Adult male
Cynomolgus monkeys (Macaca fasicularis, n = 3, 3–5 kg)
were individually housed in stainless steel cages. Each animal-
room was maintained on a 12-h light/dark cycle and room
temperature ranged between 64-F and 84-F. Purina Primate
Diet was provided daily in amounts appropriate for the size
and age of the animals. This diet was supplemented with fruit
or vegetables daily. Also, small bits of fruit, cereal or other
treats were provided as part of the environmental enrichment
program. Tap water was freely available to each animal
through an automatic watering device or an attached water
bottle. Prior to assignment to the study, all imported animals
underwent at least a 31-day quarantine period as mandated by
the Centers for Disease Control and Prevention (Atlanta, GA).
Liposome infusion procedure
Infusion of gadoteriodol/rhodamine-loaded liposomes
during real-time magnetic resonance imaging monitoring
Primates (n = 3, 3–5 kg) received a baseline MRI scan and
underwent neurosurgical procedures to position MRI-compat-
ible guide-cannulas in the left putamen. Each customized
guide cannula was cut to a specified length and stereotacti-
cally guided to its target through a burr-hole created in the
skull. The guide-cannula was secured to the skull with dental
acrylic, and the tops of the guide-cannula assemblies were
capped with stylet screws for simple access during the
infusion procedure. Animals recovered for at least 2 weeks
before starting liposome infusions. Under isoflurane anes-
thesia, the animal’s head was placed in an MRI-compatible
stereotactic frame and a baseline MRI scan was performed.
Vital signs, such as heart rate and PO2, were monitored
throughout the procedure. Infusions were performed accord-
ing to previously established CED techniques for non-human
primates (Bankiewicz et al., 2000). Briefly, the infusion
system consisted of a fused-silica needle cannula that was
connected to a loading line (containing liposomes) and an oil-
infusion line. A 1-ml syringe (filled with oil), mounted onto a
micro-infusion pump (BeeHive; Bioanalytical Systems, West
Lafayette, IN), regulated the flow of fluid through the system.
Based on MRI coordinates, cannula was mounted onto a
stereotactic holder, and manually guided to the targeted region
of the brain through a guide-cannula previously secured. The
length of each infusion cannula was measured to ensure that
the distal tip extended approximately 3 to 4 mm beyond the
length of the respective guide. This created a stepped design at
the tip of the cannula to maximize fluid distribution during
CED procedures. Following secure placement of the needle
cannula, the animal’s head was repositioned in the MRI gantry
and CED procedures were initiated while MRI data were
continuously acquired. Putamen infusion volume was 99 Al in2 primates and 300 Al for the third primate. An initial infusion
rate of 0.1 Al/min was applied and increased at 10-min
intervals to 0.2, 0.5, 0.8, 1.0 Al/min and 1.5 Al/min in the 99-
Al primates and up to 3 Al/min in the 300-Al primate. Each
animal received a mixture of liposomal Gd and rhodamine
liposomes; the approximate concentration of liposomes
injected corresponded to a formulated concentration of 10
mM phospholipids and 5 mM gadoteriodol. Approximately
15 min after infusion, the cannula was withdrawn from the
brain. Each animal was infused up to 3 times with at least 4-
week intervals between each infusion procedure. Immediately
after the last intracranial CED procedure, the animal was
euthanized with an overdose of pentobarbital. The brain was
then harvested and coronally sectioned into 3 to 6 mm blocks.
Each brain slice was immediately frozen in cooled isopentane/
dry-ice, and processed for histological analysis.
MRI and MRA acquisition
T1-weighted images of primate brains were acquired on a
1.5-T Signa LX scanner (GE Medical Systems, Waukesha,
WI) with a 5-in. surface coil. Prior to insertion of infusion
cannulas, baseline spoiled gradient echo (SPGR) images
were taken: repetition time (TR)/echo time (TE)/flip angle =
28 ms/8 ms/40-, number of excitations (NEX) = 4, matrix =
256 � 192, field of view (FOV) = 16 cm � 12 cm, slice
thickness = 1 mm. These parameters resulted in a 0.391 mm3
voxel volume. Once the cannulas were inserted and infusion
commenced, SPGR scans were taken consecutively
throughout the infusion. The scan-time was dependent on
the number of slices needed to cover the extent of infusion
and ranged from 9.73 min to 11.88 min.
MRA was performed using UCSF Radiology standard
imaging protocol for 2D MR Angiography of CNS.
Signal quantification and three-dimensional reconstruction
from MR images
The Signal of gadoteriodol liposome distribution for each
infused primate putamen was quantified with BrainLabRsoftware (Heimstetten, Germany). MR Images acquired
during the infusion procedure were correlated with volume
of infusion at each series started during an infusion
procedure. BrainLab software reads all data specifications
from MR images. After the pixel threshold value for
liposomal signal is defined, the software calculates the signal
above a defined threshold value, and establishes the volume
of distribution from primate brain. This allows volume of
M.T. Krauze et al. / Experimental Neurology 196 (2005) 104–111 107
distribution to be determined at any given time-point and can
be reconstructed in a three-dimensional image.
Results
MRI monitored leakage out of non-human primate striatum
after liposomal infusion
We established a method to monitor in real time the
infusion of liposomes loaded with a surrogate marker. We then
used this system to infuse various anatomical structures in
non-human primate brain including putamen. CED of up to
300 Al of liposomes was performed in non-human primate
putamen, and subsequent distribution was monitored (Figs. 1
and 2). Placement of cannula in primate putamen was verified
for each animal by MRI prior infusion of liposomes. MRI was
used to monitor CED of liposomes throughout the infusion
procedure and reflux-free delivery was established to ensure
optimal convection parameters. After starting the primate
putamen infusion procedure, signal enhancement was detected
in the perivascular space of the medial cerebral artery (MCA)
(Figs. 1a, c, d, e, f). At the lateral putamen border, lateral
striate arteries (LSA) also showed signal enhancement (Fig.
1b). Volume infused into each animal at which MCA signal
enhancement was first seen on MRI was as follows: A—50 Al(Figs. 1a, b), B—20 Al (Figs. 1c, d) and C—15 Al (Figs. 1e, f).Signal enhancement continued to spread in the perivascular
space along branches of MCA (Figs. 1a, c, f). Increasing
signal enhancement in the Sylvian fissure and insular region
was also visible, while infusion of liposomes into putamen
Fig. 1. Coronal images showing robust distribution of CED delivered liposomes
MCA to finally accumulate in the sylvian fissure and insula cortex area (a– f). Sa
Axial view showing accumulation of liposomes in sylvian fissure after putamen
continued with perivascular MCA signal present (Figs. 1a, e).
No signal in the external capsula bordering on insular cortex
was seen throughout the infusions (Figs. 1a, b, e).
MRA (Magnetic Resonance Angiography) of non-human
primate cerebral vessels
The signal seen in primate cerebral arteries (Figs. 2d–f)
after performing MRA shows the luminal MCA signal in
coronal, axial and sagittal views. This signal location
exactly matched liposomal MRI signal seen after putamen
infusions in same anatomical views (Figs. 2a–c). Results of
this study confirmed the (perivascular) arterial origin and
perivascular transport of the liposomal signal seen during
intra-putaminal infusions. Post-mortem examination con-
firmed localization of LSA with respect to perivascular
transport of liposomes seen during MRI (see Figs. 4 and 5).
Reconstruction in three dimensions of putamen infusion and
leakage pathway
To understand special relationship between localization of
the vessels and the pattern of perivascular transport of
liposomes 3-dimensional (3-D) reconstruction was performed.
3D reconstruction is seen from an anterior superior view, after
delineating the liposomal signal seen after putamen infusion
(Figs. 3a, b). Although MCA leakage was seen first after 50 Alinfusion (Animal A), data for delineation was taken at the
150-Al infusion volume in order to visualize the complete
leakage pathway. This reconstruction enabled us to demon-
strate clearly distribution in the putamen, and leakage of
in primate putamen (a, b). Liposomal signal is visible to drain along LSA,
gittal view of putamen infusion including perivascular signal in MCA (d).
infusion (e).
Fig. 2. Coronal section with liposomal leakage shown on top with the corresponding MRA below (a–f). MRA identifies LSAvessels in the putamen and MCA
in horizontal part (d). Axial view of primate liposomal perivascular MCA enhancement on top (b) compared to axial MRA of MCA vessel below (e). Sagittal
view of liposomal enhanced MCA (c) and the corresponding MCA signal in MRA.
M.T. Krauze et al. / Experimental Neurology 196 (2005) 104–111108
liposomes, in relation to MRI data (Fig. 3a). Digital
subtraction of MR image allowed further detailed analysis
of the leakage pathway in relation to primate brain anatomy
(Fig. 3b). The following landmarks are shown: liposomal
putamen distribution, anterior lateral leakage following
perivascular space of LSA connecting to perivascular space
of medial cerebral artery and termination of signal in the
Sylvian fissure and insular cortex (Fig. 3b). Insula and sylvian
Fig. 3. 3-dimensional re-construction of putamen distribution and leakage. Liposo
distribution components and perivascular transport in relation to anatomical landm
fissure again display accumulation of liposomal signal seen in
MR imaging during the infusion procedure.
Analysis of anatomical structures and fluorescence along
the leakage pathway
In order to correlate data obtained in vivo with post-
mortem examination, MRI data were compared with data
mal distribution overlapped with MR imaging (a). Detailed analysis of all
arks (b).
Fig. 4. Primate putamen hematoxylin and eosin histology section showing
branches of lateral striate arteries along lateral putamen border penetrating
into putamen nucleus.
M.T. Krauze et al. / Experimental Neurology 196 (2005) 104–111 109
from histological analysis of non-human primate brains.
Vessels of the lateral striate arteries with perforating
branches, that are the arterial supply for the putamen, are
seen at the lateral putamen border in a more ventral section
seen from infusion site (Fig. 4).
Co-infusion of gadoteridol- and sulforhodamine B-
loaded liposomes allowed us to perform primate histology
for fluorescent marker (Fig. 5), thus making comparison
between MRI and histological demonstration of perivascular
transport possible. Our previous experience with these
Fig. 5. Fresh frozen coronal primate histology section with putamen, LSA and MC
seen after infusion of 300 Al liposomes in basal areas of primate brain (b, 5� ma
formulations of liposome-loaded surrogate markers has
demonstrated the surrogate to be retained within, and
accurately represent the location of the liposome carrier.
Minimal leakage followed by subsequent dilution and rapid
clearance of the hydrophilic markers diminishes the signal
contribution of extraliposomal gadoteridol and sulforho-
damine B. Structures that were enhanced on MRI were
histologically analyzed for fluorescence to confirm the
perivascular origin of transport. A histological section that
contained putamen, LSA vessels and MCA vessel was
analyzed to demonstrate structures involved in leakage
pathway (Fig. 5a). Clear fluorescent signal can be seen at
the basal areas of brain surrounding the perivascular space
of a MCA vessel (Fig. 5b).
Discussion
In the light of current clinical trials and efforts to design
safe clinical trials in the future, controlled distribution of
therapeutic agents within the CNS is essential for any
approach to gene or molecular therapy. The concept of a
perivascular pump as an integral part of physiological
drainage mechanisms in the CNS has been known for years,
but is still controversial. What role it plays in the movement
of interstitially infused therapeutics is still unclear. Although
the distribution of different molecules depends on their
specific physicochemical properties, such as size, charge
and affinity for cellular receptors, our results indicate that a
distinct perivascular space pathway in the putamen might
apply to every interstitially applied agent. Anatomical
differences in perivascular ultrastructures in putamen and
A (a, 1.5� magnification). Intense MCA and LSA vessel wall fluorescence
gnification).
M.T. Krauze et al. / Experimental Neurology 196 (2005) 104–111110
sub-arachnoid arteries might explain the rather unusual
transport of liposomes out of putamen infusion site. The 2
distinct layers of leptomeninges in the putamen very likely
allow perivascular liposomal transport against the blood
flow in the LSAwhereas further perivascular transport in the
single leptomeningeal-coated MCA clearly shows transport
in direction of blood-flow. Postmortem histological analysis
shows the high vessel density in the ventral putamen and the
strong fluorescent vessel signal seen from MCA to sylvian
fissure. Diffusion of liposomal dye into cerebral cortex of
the insula region also suggests leakage of liposomes into
CSF during perivascular transport.
Liposomes are a good marker to visualize transport
throughout the CNS. However, it is currently not possible to
predict, based on the putamen cannula placement, the
amount of infusate needed to achieve leakage. A large part
of the putamen relies on blood flow that is mainly supplied
by the LSA vessels that arise from the MCA. This anatomy,
together with our histological findings, explains why no
liposomal signal is seen in other sub-arachnoid arteries. As
the diameter of LSA vessels is rather small compared to the
MCA, perivascular liposomes might give less signal on
MRI in LSA vessels, since the MCA signal seems to appear
earlier in the infusion. These MRI findings were not
confirmed by histology as fluorescent liposomal signal
was seen along the entire leakage pathway.
Our liposomal findings suggest that every therapeutic
given into putamen should be closely monitored for
distribution since the possibility of side effects increases
greatly with leakage out of infusion site. It is unclear
whether placement of the cannula in different parts of the
putamen would allow a greater volume of infusion
without corresponding perivascular transport along ves-
sels. Adding our findings to the body of knowledge
regarding the immunological role of perivascular spaces
might explain the antibodies reported in some clinical trial
subjects after GDNF infusion into putamen nucleus (Hood
and Sherer, 2004). The fast transport through the
perivascular space after infusion of up to just 300 Al ofliposomes shown here strongly suggests that infusion of 8
ml of GDNF in PD patients (Gill et al., 2003; Slevin et
al., 2005) most likely followed the same route and ended
up in the regions that are remote form the infusion site,
including CSF. Clearance pathways of liposomes in the
CNS strongly suggest perivascular transport occurs over
the entire CNS if very large volumes are infused. This
also raises the possibility of therapeutics being transported
away from their intended site of action, with concomitant
side effects.
In summary, our study indicates the potential hazards and
challenges for future human gene and molecular therapy.
Furthermore, it advances the importance of monitoring
strategies during delivery of therapeutics to CNS. The
importance of perivascular transport after intracranial
delivery warrants further investigation, as our understanding
of the latter is still poor.
Acknowledgments
Special thanks to BrainLAB for support and help with
iPlanR software.
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