Technical Reports
An extracorporeal blood-cleansing device for
sepsis therapy
npg
© 2014 Nature America, Inc. All rights reserved.
Joo H Kang1–3,7, Michael Super1,7, Chong Wing Yung1,2, Ryan M Cooper1,2,4, Karel Domansky1,
Amanda R Graveline1, Tadanori Mammoto2, Julia B Berthet1, Heather Tobin2, Mark J Cartwright1,
Alexander L Watters1, Martin Rottman1,6, Anna Waterhouse1, Akiko Mammoto2, Nazita Gamini1,
Melissa J Rodas1, Anxhela Kole1, Amanda Jiang2, Thomas M Valentin1, Alexander Diaz1, Kazue Takahashi5 &
Donald E Ingber1–3
Here we describe a blood-cleansing device for sepsis therapy
inspired by the spleen, which can continuously remove
pathogens and toxins from blood without first identifying the
infectious agent. Blood flowing from an infected individual is
mixed with magnetic nanobeads coated with an engineered
human opsonin—mannose-binding lectin (MBL)—that
captures a broad range of pathogens and toxins without
activating complement factors or coagulation. Magnets pull
the opsonin-bound pathogens and toxins from the blood; the
cleansed blood is then returned back to the individual. The
biospleen efficiently removes multiple Gram-negative and
Gram-positive bacteria, fungi and endotoxins from whole
human blood flowing through a single biospleen unit at up to
1.25 liters per h in vitro. In rats infected with Staphylococcus
aureus or Escherichia coli, the biospleen cleared >90% of
bacteria from blood, reduced pathogen and immune cell
infiltration in multiple organs and decreased inflammatory
cytokine levels. In a model of endotoxemic shock, the
biospleen increased survival rates after a 5-h treatment.
The presence of microbial pathogens in the bloodstream triggers systemic inflammation and can lead to sepsis, which often overcomes
the most powerful antibiotic therapies and causes multiorgan systems
failure, septic shock and death1–4. Sepsis afflicts 18 million people
worldwide every year5, with a 30–50% mortality rate even in state-ofthe-art hospital intensive care units3–8, and its incidence is increasing
because of the emergence of antibiotic-resistant microorganisms6.
Sepsis treatment usually involves the use of empiric, broad-spectrum
antibiotic therapy because it takes days to identify the source of the
infection and blood cultures are often negative. But these broadspectrum agents are not as effective as therapeutics targeted against
specific microbes, and they can produce severe side effects7; as a
result, mortality rates increase as much as 9% for every hour before
the correct antibiotic therapy is administered8. This situation is even
more devastating in patients with antibiotic-resistant pathogens
because of the lack of effective drugs, and in immunosuppressed
patients and neonates with fungal infections because of the high
toxicity of antifungal agents6,9. Other methods used to treat sepsis
(for example, administration of fluids, anti-thrombosis therapy,
hemofiltration of inflammatory mediators and extracorporeal
organ support10) do not address the root of the problem, which is
the persistence of both live and dead pathogens that release
toxins into the bloodstream2. With the 2011 withdrawal of the
Eli Lilly drug Xigris (drotrecogin alpha), the recombinant form of
activated protein C, there are now no drugs specifically approved
to treat sepsis11.
We initiated our project based on the observations that blood
pathogen load is known to be a major contributor to both disease
severity and mortality in patients with sepsis12, and that many patients
respond to appropriately targeted antibiotic therapies that work exclusively by lowering the number of live pathogens. Thus, we set out to
develop an extracorporeal blood-cleansing therapy that can rapidly
remove microorganisms and endotoxins from blood without the need
to first identify the source of the infection and without altering blood
contents. Although combined micromagnetic-microfluidic techniques have been used for many applications13–15, including pathogen isolation16,17, this approach has not been used to cleanse whole
blood. Here we describe an improved extracorporeal microfluidic
device that incorporates a flow channel design inspired by the microarchitecture of the spleen, which can be used to cleanse pathogens
from the flowing blood of patients with sepsis when combined with
broad-spectrum magnetic opsonins. These capture agents are composed of magnetic nanobeads coated with a genetically engineered
version of human MBL that binds to a wide variety of pathogens and
is easily manufactured but lacks key functional domains that could
complicate therapy.
1Wyss Institute for Biologically Inspired Engineering, Boston, Massachusetts, USA. 2Vascular Biology Program, Boston Children’s Hospital and Harvard Medical
School, Boston, Massachusetts, USA. 3Harvard School of Engineering and Applied Sciences, Cambridge, Massachusetts, USA. 4Harvard-MIT Health Sciences and
Technology Graduate Program, Cambridge, Massachusetts, USA. 5Massachusetts General Hospital and Harvard Medical School, Boston, Massachusetts, USA.
6Current address: Université de Versailles St-Quentin en Yvelines, Versailles, France and Service de Microbiologie, Hôpitaux Universitaires Île de France Ouest,
AP-HP, Garches, France. 7These authors contributed equally to this work. Correspondence should be addressed to D.E.I. (don.ingber@wyss.harvard.edu).
Received 30 December 2013; accepted 25 April 2014; published online 14 September 2014; doi:10.1038/nm.3640
nature medicine
VOLUME 20 | NUMBER 10 | OCTOBER 2014
1211
npg
© 2014 Nature America, Inc. All rights reserved.
Technical Reports
RESULTS
Engineering a human opsonin for blood cleansing
To develop a broad-spectrum opsonin that can be used without complication to cleanse whole blood flowing through an extracorporeal
fluidic circuit, we genetically engineered the large (650 kDa) native
MBL protein by deleting its collagen-helix domain that contains the
molecule’s natural complement-fixation and blood coagulation–
promoting activities as well as its ability to bind to receptors on macrophages18,19 (Fig. 1a). The remaining carbohydrate-recognition
domain and neck domains of the human MBL were fused to human
IgG1 Fc, enabling high expression and secretion as well as efficient,
rapid and low-cost purification of the smaller (90 kDa), recombinant
protein20. The Fc-containing MBL (FcMBL) was biotinylated at its
N terminus by addition of the tripeptide sequence alanine-lysinethreonine. Site-specific biotinylation of the terminal tripeptide
sequence enabled us to uniformly orient FcMBL at high density on
the surface of streptavidin-coated superparamagnetic nanobeads
(128-nm diameter) to create multivalent magnetic opsonins (Fig. 1a).
Notably, the engineered FcMBL retained the same potent pathogenand endotoxin-binding capabilities as reported for wild-type MBL21–23
when we tested the magnetic opsonins in standard in vitro binding
assays against Candida albicans, Saccharomyces cerevisiae, E. coli and
S. aureus (Fig. 1b and Supplementary Fig. 1a), a broad range of other
Gram-negative and Gram-positive bacteria and fungi (Supplementary
Table 1 and Supplementary Fig. 1a), and lipopolysaccharide (LPS)
endotoxin from Gram-negative bacteria (Supplementary Fig. 1b).
The FcMBL also bound to multiple antibiotic-resistant organisms,
including methicillin-resistant S. aureus, Staphylococcus epidermidis,
Klebsiella pneumoniae and E. coli (Supplementary Table 1)24–26. The
FcMBL also displayed greatly decreased coagulation-promoting,
complement-activation and DNA-binding activities compared with
MBL (Supplementary Fig. 1c,d and Online Methods).
Bioinspired fluidic device design
To efficiently remove magnetically opsonized pathogens and endotoxins from septic blood flowing at liters per hour without loss or
dilution of blood, we developed a fluidic device design inspired by the
microarchitecture of the living spleen (Fig. 1c and Supplementary
Fig. 2a–c). The biospleen unit consists of two adjacent, rectangular
fluidic channels. One acts like a vascular channel (2 mm × 0.6 mm ×
27 mm; width × height × length) that contains flowing blood (up to
1.25 liter h−1), and the other one (2 mm × 0.34 mm × 27 mm) contains
saline under intermittent or slow flow (0–0.1 liter h−1; 5 min on and
60 min off), much like in the spleen’s venous sinusoids. In the living
spleen, opsonized pathogens are cleared from the blood by resident
macrophages as the blood is filtered through slits between adjacent
endothelial cells when flow slows down and trickles from the marginal
zone and red-pulp cords into the venous sinuses27. Similarly, the bio
spleen contains a series of open rectangular slits (2 mm × 0.34 mm ×
0.34 mm, spaced every 0.43 mm) that provide direct access between
the blood channel and the saline-filled sinusoid channel (Fig. 1c);
we based the channel and slit dimensions on our previous device
design15. To increase isolation efficiency at higher flow rates, the
single inflow channel into the device branches 4 times before entering
a
Figure 1 Magnetic opsonin and biospleen device. (a) Design scheme
MBL
CRD
for genetic engineering of native mannose-binding lectin (MBL) to
produce the generic opsonin FcMBL and coat it on magnetic nanobeads
MBL
Magnetic
neck
(128 nm) to produce magnetic opsonins, as shown at the right. FcMBL
nanobead
Collagen
IgG1
was produced by engineering the protein to retain MBL’s carbohydratehelix
Fc
recognition domain (CRD) while removing its collagen-helix regions.
FcMBL (90 kDa)
MBL (650 kDa)
These regions contain domains that support binding of MBL-associated
serine proteases that mediate cleavage of complement and fibrinogen—
Magnetic
bead
responsible for MBL’s complement-fixation and coagulation-promoting
E. coli
activities36, respectively—as well as domains that are responsible for
MBL’s binding to complement and collectin receptors on the surfaces of
macrophages18,19. These regions were then replaced with the Fc region
of IgG1 to ensure stability and facilitate protein purification, and a
S. aureus
terminal biotinylation site (not shown) was used to consistently orient
Discard out
the FcMBL at high density on the surface of the streptavidin-coated
Saline in
Venous system
Magnets
nanobeads with the CRD facing outward. (b) Pseudocolored scanning
electron micrographs showing multiple opsonin-coated magnetic beads
Venous
(128 nm) bound to the bacteria S. aureus (orange/brown; left) and
Arterial
Sinusoid
Sinusoid
red-pulp
slits
E. coli (blue; right). Scale bars, 1 µm; arrows indicate pathogen with bound
cord
Arterial
beads. (c) Schematics of a venous sinus in the red pulp of the spleen (left)
and a longitudinal view of the biospleen (right), with a photograph of an
Magnetic
Endothelial
opsonin in
engineered device (top right). The blood-cleansing biospleen mimics the
cells
Septic
Cleansed
Stress fiber
architecture and function of the human spleen by incorporating a highblood in
blood out
flow vascular arterial channel perfused with contaminated whole blood
Peristaltic pump
and interconnected by open slits to a parallel low- or intermittent-flow
Magnetic
venous sinusoid channel perfused with isotonic sterile saline; this mimics
opsonins
Anesthesia
the arterial red-pulp cord and venous system separated by sinusoid slits
between neighboring endothelial cells. Magnetic opsonins are added
Jugular
to the flowing septic (contaminated) blood and passed through an
Static mixer
catheters
in-line spiral mixer and incubation loop that promote nanobead-pathogen
binding (shown in d) before entering the arterial channel of the biospleen.
Stationary magnets positioned directly above the sinusoid channel pull
Incubation
loop
the magnetic opsonins and bound pathogens through the open slits, into
the saline-filled channel and into a discard collection vial (Supplementary
Magnets
Magnetic separator unit
Video 1). A micromachined aluminum magnetic separator unit of the
biospleen is shown at the right above the diagram (scale bar, 50 mm); the inset shows a higher-magnification view of the slit regions of the same device
(scale bar, 20 mm). (d) Photograph of the experimental animal setup for extracorporeal blood cleansing, with components labeled.
b
c
∆B
∆B
∆B
d
1212
VOLUME 20 | NUMBER 10 | OCTOBER 2014
nature medicine
Technical Reports
npg
© 2014 Nature America, Inc. All rights reserved.
Removal of pathogens and endotoxin from blood in vitro
When we tested the efficiency of the biospleen at removing pathogens prebound to magnetic opsonins and spiked into saline or blood
in vitro, we confirmed removal efficiencies of 99% and 90% for
S. aureus in saline and blood, respectively, at a flow rate of 535 ml h−1
(Supplementary Fig. 3d), as predicted by our theoretical model
(Supplementary Fig. 3c). Moreover, we still could clear ~85% and
~60% of these pathogens when the flow was raised to 1 liter h −1
(Supplementary Fig. 3d). However, many patients with sepsis are
infected with multiple microbes simultaneously (for example, because
of an intestinal injury). To model this condition, the cecal contents
of meat-fed rats (Online Methods) were spiked into banked whole
human blood (3.5 × 104 anaerobe CFU and 1.5 × 104 aerobe CFU in
10 ml) in an anaerobic environment, which mimics intra-abdominal
sepsis. We determined pathogen-removal efficiencies for clearance
of this complex mixture of anaerobic and aerobic bacteria using the
continuous-flow biospleen device at a flow rate of 10 ml h−1 with the
magnetic opsonins (0.5 mg ml−1) injected at 7.1 µl min−1. These studies
revealed that >98% and >80% of anaerobic and aerobic bacteria were
removed from blood, respectively, after only a single pass through the
blood-cleansing device; it also successfully removed other pathogens,
including C. albicans, S. aureus and E. coli (all at ~104 CFU ml−1), from
blood with efficiencies consistently above 90% (Fig. 2a).
Using fresh, whole human blood that we anticoagulated with
heparin (16 units ml−1) and experimentally contaminated with
S. aureus (104 CFU ml−1), we removed about 60% of the bacterial load
with each pass through the device at a flow rate of 10 ml h−1. Notably,
more than 90% of these Gram-positive pathogens were removed
from the fresh, flowing blood after five sequential passes through
nature medicine
VOLUME 20 | NUMBER 10 | OCTOBER 2014
Isolation efficiency (%)
50
50
co
li
ro
ce bic
c
Ae al
r
ce obic
ca
l
0
Experimental
Kinetic analysis
0
2
4
Time (h)
ae
Untreated
Biospleen + FcMBL beads
4
2
0
0
100
An
re
u
au
lb
ic
a
S.
C
.a
c
E.
s
0
ns
Isolation efficiency (%)
b
100
d
LPS levels (OD450)
a total of 16 magnetic separator channels, which then merge into a
single outlet channel (Fig. 1c).
To carry out blood cleansing, we continuously injected the
nanomagnetic opsonins into flowing whole blood and thoroughly
mixed them with pathogens by flowing them through a Kenics
inline mixer28 followed by an incubation loop composed of helically
coiled tubing to enhance transverse convective flux29 for 5–10 min
before they entered the magnetic separator (Fig. 1d, Supplementary
Fig. 2d and Online Methods). This design was based on a theoretical
analysis that predicted >99% bead capture at a maximum flow rate of
~560 ml h−1 (Supplementary Fig. 3c and Online Methods), assuming the magnetic flux density gradient is >1.0 T2 m−1 with a blood
channel height of ~600 µm. This analysis assumed that a single spherical pathogen (~1-µm diameter) will be bound by about 40 magnetic
opsonins (128-nm diameter) on average based on our electron micros
copy imaging results (Fig. 1b) and our past findings16.
a
E. coli levels (log CFU ml–1)
Figure 2 Magnetic capture efficiency of the biospleen device in vitro.
(a) Pathogen-isolation efficiency for various types of pathogens, including
C. albicans fungi, Gram-positive S. aureus bacteria, Gram-negative E. coli
bacteria and mixed populations of anaerobic or aerobic cecal microbial
flora, when spiked into human blood and flowed through the bloodcleansing device at 10 ml h−1 while FcMBL-coated magnetic beads
(0.5 mg ml−1) were added continuously into the device (7.1 µl min−1)
(n = 3). (b) Pathogen-removal efficiencies calculated using a kinetic
analysis model (dashed line) and results obtained experimentally (solid
line) with the biospleen device using whole blood spiked with S. aureus
(104 CFU ml−1) in vitro (n = 3). (c) Depletion of E. coli in blood by
continuous cleansing in vitro using the biospleen device at a flow rate of
10 ml h−1 (n = 3; P < 0.03). (d) Depletion of LPS when LPS endotoxin
spiked into fresh human whole blood (10 µg ml−1) was flowed through
the biospleen device at 10 ml h−1 (n = 3). Error bars, s.e.m.
2
Time (h)
4
Biospleen + no FcMBL beads
Biospleen + FcMBL beads
Background
1.0
0.5
0
0
2
Time (h)
4
the biospleen device over 5 h, which correlates closely with a theoretical model based on Monod kinetics (Fig. 2b and Online Methods).
Moreover, we also were able to significantly (P < 0.03) deplete Gramnegative pathogen levels when we continuously infused E. coli into
human blood at a dose and rate (5 × 108 CFU ml−1 h−1) previously
used in an animal model of sepsis30 and then flowed it through the
biospleen device with magnetic opsonins for 5 h in vitro (Fig. 2c).
Finally, as bacterial toxin levels in blood are a crucial contributing
factor in sepsis31, we also assessed how efficiently the blood-cleansing
device can remove LPS endotoxin from flowing blood. When we
spiked heparinized, fresh, whole human blood (10 ml) with LPS
(10 µg ml−1) and continuously flowed it through the blood-cleansing
device with magnetic opsonins at 10 ml h−1 for 5 h in vitro, endotoxin
levels decreased by a factor of more than 4, almost to background
levels (Fig. 2d). In contrast, endotoxin levels remained consistently
high when we used the biospleen device with uncoated magnetic
beads (Fig. 2d), hence demonstrating the critical requirement for
FcMBL in this blood-cleansing therapy.
Although we efficiently removed pathogens or endotoxin
bound to multiple magnetic opsonins, we removed only ~80% of
unbound, single nanomagnetic beads because they have extremely
small magnetic moments due to their small size (128 nm). To more
effectively remove all magnetic opsonins (and prevent potential
complications of the beads entering a patient’s circulation in the
future), we administered larger (1-µm diameter), uncoated superparamagnetic beads along with the 128-nm, FcMBL-coated beads;
these larger beads act as local magnetic field gradient concentrators that magnetize and attract the smaller beads when exposed
to an external magnetic field (i.e., only when passing through the
magnetic separator) (Online Methods). Experimental studies confirmed that addition of these larger beads increased magnetic capture of the smaller magnetic opsonins from ~80% to 99.6 ± 0.6%
when the beads were flowed through the biospleen at 10 ml h −1
(Supplementary Fig. 4c).
Extracorporeal blood cleansing in living animals
To test the blood-cleansing capability of the biospleen in vivo, we
linked the device (containing the static mixer, incubation loop,
magnetic separator unit and a syringe pump injecting the magnetic
opsonin beads) to the jugular veins of living, anesthetized rats using
1213
b
Untreated
Biospleen alone
Biospleen + FcMBL beads
E. coli in blood
(log CFU ml–1)
S. aureus in blood
(log CFU ml–1)
a
2
1
0 10
c
Biospleen + uncoated beads
Biospleen + FcMBL beads
3
2
1
0
0
12
Time (h)
–
–
+
–
14
–
–
+
+
2
Time (h)
0
+
–
+
+
–
–
4
+
–
+
+
+
CD45 S. aureus
S. aureus
Biospleen
e
-6
IL
G
M
α
0
-4
Kidney
IL
Spleen
-C
Lung
-γ
0
50
-1
1
100
N
2
Untreated
Biospleen + FcMBL beads
IL
Cytokine levels
(pg ml–1)
Untreated
Biospleen + FcMBL beads
Kidney
SF
d
Spleen
IF
Lung
S. aureus intensity
(a.u.)
Figure 3 In vivo blood cleansing using the biospleen blood-cleansing
device in a rat bacteremia model. (a) Depletion of pathogen levels in
the blood of rats injected intraperitoneally with S. aureus (5 × 108 CFU)
by biospleen treatment 10 h later with (n = 6) or without (n = 3)
opsonin-coated magnetic nanobeads as compared to untreated controls
(n = 5). (b) Depletion of pathogen levels in the blood of rats continuously
infused with E. coli (5 × 108 CFU h−1) by immediate biospleen treatment
using FcMBL-coated nanobeads (solid line) or the same beads without the
coating (dashed line) (biospleen with FcMBL beads, n = 3; biospleen
with uncoated beads, n = 3). (c) Immunofluorescence micrographs of
lung, spleen and kidney removed from normal rats (left) or rats injected
intraperitoneally with S. aureus that were either untreated (middle) or
treated (right) for 5 h with the biospleen device, showing reduced levels
of S. aureus in each organ. Top images were stained with antibodies that
recognize S. aureus (green); bottom images identify CD45+ immune
cells (green); nuclei were stained with DAPI (blue) in both sets of images.
Scale bar, 50 µm. (d) Quantitative analysis of the images obtained
from six random fields (untreated, n = 3; biospleen with FcMBL beads,
n = 3) shows that biospleen treatment significantly lowered S. aureus
levels (a.u., arbitrary units) in each organ (P < 0.05). (e) Blood levels
of five types of proinflammatory cytokines—granulocyte-macrophage
colony–stimulating factor (GM-CSF), interferon-γ (IFN-γ), interleukin-1α
(IL-1α), IL-4 and IL-6—in the circulation of rats infected with S. aureus
with (black bars) or without (white bars) subsequent treatment with the
biospleen device (biospleen with FcMBL beads, n = 3; untreated, n = 3).
Error bars, s.e.m.
medical-grade tubing and catheters (Fig. 1d and Supplementary
Fig. 2d). We first tested the biocompatibility of the system (Online
Methods) and found that flowing the animal’s blood continuously
through the biospleen for 5 h had no detectable effect on the animal’s
physiology (temperature and breathing rates), nor did it induce blood
coagulation as measured by thrombin–antithrombin complex formation (Supplementary Fig. 4e).
Much as we observed in our in vitro studies, the device removed
~90% of live S. aureus (Fig. 3a) and E. coli (Fig. 3b) pathogens from
the septic rat’s blood within 1 h using FcMBL-coated nanomagnetic
opsonins combined with the larger magnetic concentrator beads
(Online Methods). Use of the biospleen device with magnetic FcMBLcoated beads also maintained significantly (P < 0.01 for S. aureus;
a
LPS intensity (a.u.)
Survival (%)
b
Biospleen
Untreated
100
50
0
0
1
c
2
3
Time (h)
+
–
4
+
+
0.6
0.4
0
Lung
+
–
+
+
Spleen
–
–
Kidney
+
–
+
+
CD45+
Lung
Spleen
80
60
40
20
0
0
1214
1
2
3
Time (h)
Kidney
e
Temperature (°C)
d
4
5
P < 0.004 for E. coli) lower levels of pathogens in the septic rat’s circulation for the entire 5-h treatment period than those in infected
animals that did not experience blood cleansing or rats treated with
the biospleen either in the absence of added magnetic opsonin beads
(S. aureus) or using beads that lacked the FcMBL coating (E. coli).
Control biospleen studies clearly showed that the blood must be
treated with magnetic FcMBL opsonins to produce effective blood
cleansing as passage of blood through the magnetic separator without
beads or with uncoated beads had no effect on pathogen clearance
(Fig. 3a,b). Notably, histological analysis revealed that reduction of
blood pathogen levels using the biospleen device with the FcMBL
magnetic opsonins also resulted in a major decrease in both pathogen load and the level of inflammatory cell (CD45+) infiltrate and
interstitial edema in the lung, spleen and kidney (Fig. 3c,d). This
likely explains why the treated animals did not exhibit detectable symptoms of clinical distress (such as labored breathing and
lower body temperature) that we observed in untreated animals.
Treating the bacteremic rats with the biospleen using magnetic
0.2
5
–
–
Untreated
Biospleen
0.8
LPS
LPS –
Biospleen –
Respiratory rate
(min–1)
npg
© 2014 Nature America, Inc. All rights reserved.
Technical Reports
38
36
34
32
0
0
1
2
3
Time (h)
4
5
Figure 4 In vivo blood cleansing using the biospleen device in a rat acute
endotoxic shock model. (a) Kaplan-Meier plot showing increased survival
in rats treated with the biospleen after intravenous injection with a lethal
dose of LPS endotoxin (13.6 × 106 endotoxin units per ml) (biospleen
with FcMBL beads (solid line), n = 9; untreated (dashed line), n = 7).
(b) Quantitative analysis of immunostained histological sections of lung,
spleen and kidney (untreated, n = 3; biospleen, n = 3) (c) obtained
from six random fields (n = 3). (c) Immunofluorescence micrographs of
lung, spleen and kidney harvested from normal rats (left) or rats injected
intravenously with LPS endotoxin only (middle) or with subsequent
treatment for 5 h with the biospleen device (right) (scale bar, 50 µm).
Top images were stained with antibodies that recognize LPS endotoxin
(green); bottom images identify CD45 + immune cells (green); nuclei were
stained with DAPI (blue) in both sets of images. (d,e) Respiratory rates (d)
and body temperature (e) (untreated, n = 7; biospleen, n = 9) measured
in control rats with endotoxemia (untreated, dashed line) produced by
intravenous LPS injection versus similar endotoxemic animals treated with
the biospleen device (solid line). Error bars, s.e.m.
VOLUME 20 | NUMBER 10 | OCTOBER 2014
nature medicine
npg
© 2014 Nature America, Inc. All rights reserved.
Technical Reports
opsonins for 5 h also significantly (P < 0.05) lowered levels of multiple proinflammatory cytokines, including granulocyte-macrophage
colony–stimulating factor, interferon-γ, interleukin-1α, interleukin-4
and interleukin-6 (Fig. 3e), all of which play an important role in the
sepsis cascade32. This extended blood-cleansing treatment significantly (P < 0.05) decreased levels of cell-free hemoglobin in plasma
as well (Supplementary Fig. 4d), which is important because this
is a well-known complication of sepsis caused by the release of
toxic hemoglobin from large numbers of damaged erythrocytes33.
The 5-h biospleen treatment by itself only reduced the hematocrit
from 40% to 30% in control animals, which was likely due to the fluidresuscitation therapy required in this animal protocol. Hence, the
reduced free hemoglobin levels we measured with the blood-cleansing
therapy are likely due to the lower pathogen levels, which resulted in
reduced hemolysis.
Finally, when we injected rats with a lethal dose of LPS endotoxin
to model acute endotoxemic shock and treated them with the bio
spleen device, we found that we could significantly (P < 0.02) improve
animal survival (Fig. 4a). Treatment with the blood-cleansing device
also resulted in a significant decrease in the amount of LPS endotoxin and leukocytes (P < 0.05) that infiltrated the lungs and other
organs of these animals (Fig. 4b,c). Because of the potential toxicities
of long-term inhalational anesthesia, all rats had to be killed at 5 h
to minimize pain and distress. However, these studies revealed that
although 86% of untreated rats died after intravenous injection of
LPS, 89% of animals treated with the blood-cleansing device survived
for the entire 5-h experiment. Also, it should be noted that endotoxemic rats treated with the biospleen device exhibited significant
(P < 0.01) improvement in various physiological responses, including respiratory rate (Fig. 4d), temperature (Fig. 4e) and restoration
of normal leukocyte levels (which drop rapidly to ~1.2 × 109 l−1 after
LPS injection and return to 3.0 × 109 l−1 within 5 h in biospleentreated animals).
DISCUSSION
Despite extensive efforts at eradicating sepsis over the past century,
treating patients with sepsis remains a daunting task. Our biologically
inspired, extracorporeal blood-cleansing system addresses the root
cause of sepsis by removing pathogens and endotoxins simultaneously.
The biospleen also allows researchers and clinicians to overcome two
major practical barriers that have not been previously addressed in
the field. First, use of the broad-spectrum FcMBL opsonin makes
it possible to rapidly treat systemic blood infections and prevent
sepsis progression without having to first identify the pathogen. This
is a crucial advantage because many patients with sepsis have negative blood cultures, and thus it is not possible to select an optimal
antibiotic therapy. Second, the whole blood volume of a patient can
be quickly processed, and multiple rounds of blood cleansing can
be carried out, without producing detectable blood coagulation or
significantly altering blood composition.
Sepsis progresses rapidly, eventually resulting in extremely high
mortality rates due to progressive development of multiorgan failure
and septic shock34. Many patients with severe sepsis are already in
intensive care units on extracorporeal circuits; thus, upon observing disease progression (for example, decreased kidney or lung
function), a clinician could add a biospleen module like the one
we describe into the existing extracorporeal circuit. Initial human
clinical trials likely would be carried out with patients in this setting. In contrast, in patients with earlier-stage disease, physicians
would likely require confirmation of septicemia before they could
nature medicine
VOLUME 20 | NUMBER 10 | OCTOBER 2014
initiate this type of extracorporeal therapy. Blood culture is not
sufficient because most patients with fulminant sepsis are bloodculture negative; however, the results shown here suggest that it
might in future be possible to use FcMBL magnetic opsonins to
detect the presence of live and dead pathogens, as well as released
toxins, within blood samples. It is also notable that sepsis caused by
antibiotic-resistant bacteria is one of the most critical public health
issues we face today, even in well-resourced countries35. As FcMBL
binds to multiple clinical isolates of antibiotic-resistant organisms
(for example, methicillin-resistant S. aureus and K. pneumonia)
(Supplementary Table 1), the biospleen also could offer an effective therapeutic strategy for these patients who are not helped by
existing drug therapies.
Our dialysis-like blood-cleansing system allows the entire blood
volume to be processed multiple times through the device during
a single treatment. Hence, even if only a portion of pathogens are
removed in a single pass, the pathogen load in the bloodstream can
be significantly lowered by circulating the blood several times over a
24-h period. Although this therapy will not remove pathogens present
within organs or abscesses, our results suggest that it will significantly
reduce the spread of infectious agents to distal sites and lower levels
of circulating endotoxin, toxic free hemoglobin and inflammatory
cytokines. All of these factors are key contributors to disease progression, and thus, this treatment could critically extend the time available to identify the nidus of infection and initiate optimal antibiotic
therapy. In fact, wide-spectrum or targeted antibiotic therapy can be
coadministered with this blood-cleansing therapy because the magnetic FcMBL opsonins bind to both dead and live pathogens. The
ability of the biospleen device to efficiently capture pathogens also
provides a potential way to rapidly collect large numbers of living
infectious agents; therefore, this device could greatly accelerate pathogen identification and antibiotic susceptibility determination. Finally,
this blood-cleansing device is a platform technology in that it could
be used to remove proteins (such as cytokines or autoantibodies) as
well as other types of cells (such as circulating cancer cells, stem cells,
fetal cells in maternal circulation, etc.) from the whole blood volume
of patients simply by coating the magnetic beads with appropriate
cell- or protein-specific ligands.
Methods
Methods and any associated references are available in the online
version of the paper.
Accession codes. KJ710775
Note: Any Supplementary Information and Source Data files are available in the
online version of the paper.
Acknowledgments
This work was supported by Defense Advanced Research Projects Agency grant
N66001-11-1-4180 and contract HR0011-13-C-0025, Department of Defense/
Center for Integration of Medicine and Innovative Technology and the Wyss
Institute for Biologically Inspired Engineering at Harvard University. We thank
M. Montoya-Zavala and D. Breslau for micromachining of the blood-cleansing
microdevice and technical support; P. Snell and J. Tomolonis for microbiology
assistance; A. Schulte for assistance in biospleen experiments; J. Weaver for help with
scanning electron microscopy; R. Betensky for statistical analysis assistance; and
A. Onderdonk, M. Puder, A. Nedder and their teams for assistance in developing the
rat cecal contents sepsis model. We thank J. Fiering and his team for helpful discussions
during the early phase of this project. J.H.K. is a recipient of a Wyss Technology
Development Fellowship from the Wyss Institute and a professional development
postdoctoral award from Harvard University. Scanning electron microscopy images
were obtained at the Center for Nanoscale Systems at Harvard University, supported
by the National Science Foundation under award no. ECS-0335765.
1215
Technical Reports
AUTHOR CONTRIBUTIONS
J.H.K. designed and performed blood-cleansing experiments with assistance from
R.M.C., J.B.B., N.G., A.R.G., A.D. and A.W., and analyzed the data and prepared
the manuscript. K.D. contributed to the design and integration of the biospleen
device. J.H.K., C.W.Y., A.R.G. and H.T. established the rat sepsis models, and J.H.K.
and A.R.G. conducted animal studies with help from T.M., A.M. and A.J.; C.W.Y.
designed the prototype biospleen device and obtained preliminary data. M.S. and
A.L.W. designed, engineered and produced FcMBL with assistance from M.J.R.,
J.B.B. and A.K.; M.S., M.J.C. and M.R. performed blood analysis for quantitating
LPS levels with help from N.G. and helped establish an endotoxemia model in rats.
T.M.V. fabricated devices, performed scanning electron microscopy and assisted
with conducting studies. K.T. performed experiments to characterize FcMBL
versus native MBL. D.E.I. led efforts to design the device and the opsonin, assisted
in data analysis and helped write the manuscript.
COMPETING FINANCIAL INTERESTS
The authors declare no competing financial interests.
npg
© 2014 Nature America, Inc. All rights reserved.
Reprints and permissions information is available online at http://www.nature.com/
reprints/index.html.
1. Bone, R.C. The pathogenesis of sepsis. Ann. Intern. Med. 115, 457–469
(1991).
2. Cohen, J. The immunopathogenesis of sepsis. Nature 420, 885–891 (2002).
3. Hotchkiss, R.S. & Karl, I.E. The pathophysiology and treatment of sepsis.
N. Engl. J. Med. 348, 138–150 (2003).
4. Kumar, A. Optimizing antimicrobial therapy in sepsis and septic shock.
Crit. Care Clin. 25, 733–751 (2009).
5. Anonymous. Focus on sepsis. Nat. Med. 18, 997 (2012).
6. O’Brien, T.F. Global surveillance of antibiotic resistance. N. Engl. J. Med. 326,
339–340 (1992).
7. Lineaweaver, W. et al. Topical antimicrobial toxicity. Arch. Surg. 120, 267–270
(1985).
8. Garnacho-Montero, J. et al. Timing of adequate antibiotic therapy is a greater
determinant of outcome than are TNF and IL-10 polymorphisms in patients with
sepsis. Crit. Care 10, R111 (2006).
9. Stoll, B.J. et al. Late-onset sepsis in very low birth weight neonates: the experience
of the NICHD Neonatal Research Network. Pediatrics 110, 285–291 (2002).
10. Neff, L.P. et al. Extracorporeal organ support following trauma: the dawn of a new
era in combat casualty critical care. J. Trauma Acute Care Surg. 75, S120–S129
(2013).
11. Angus, D.C. Drotrecogin alfa (activated). a sad final fizzle to a roller-coaster party.
Crit. Care 16, 107 (2012).
12. Chuang, Y.-C., Chang, S.-C. & Wang, W.-K. High and increasing Oxa-51 DNA load
predict mortality in Acinetobacter baumannii bacteremia: implication for
pathogenesis and evaluation of therapy. PLoS ONE 5, e14133 (2010).
13. Gijs, M.A.M. Magnetic bead handling on-chip: new opportunities for analytical
applications. Microfluid. Nanofluidics 1, 22–40 (2004).
14. Kang, J.H., Choi, S., Lee, W. & Park, J.-K. Isomagnetophoresis to discriminate
subtle difference in magnetic susceptibility. J. Am. Chem. Soc. 130, 396–397
(2008).
15. Kang, J.H. et al. A combined micromagnetic-microfluidic device for rapid capture
and culture of rare circulating tumor cells. Lab Chip 12, 2175 (2012).
1216
16. Xia, N. et al. Combined microfluidic-micromagnetic separation of living cells in
continuous flow. Biomed. Microdevices 8, 299–308 (2006).
17. Yung, C.W., Fiering, J., Mueller, A.J. & Ingber, D.E. Micromagnetic-microfluidic
blood cleansing device. Lab Chip 9, 1171 (2009).
18. Dommett, R.M., Klein, N. & Turner, M.W. Mannose-binding lectin in innate
immunity: past, present and future. Tissue Antigens 68, 193–209 (2006).
19. Sheriff, S., Chang, C.Y. & Ezekowitz, R.A.B. Human mannose-binding protein
carbohydrate recognition domain trimerizes through a triple alpha-helical coiled-coil.
Nat. Struct. Biol. 1, 789–794 (1994).
20. Lo, K.M. et al. High level expression and secretion of Fc-X fusion proteins in
mammalian cells. Protein Eng. 11, 495–500 (1998).
21. Neth, O. et al. Mannose-binding lectin binds to a range of clinically relevant
microorganisms and promotes complement deposition. Infect. Immun. 68,
688–693 (2000).
22. Townsend, R., Read, R.C., Turner, M.W., Klein, N.J. & Jack, D.L. Differential
recognition of obligate anaerobic bacteria by human mannose-binding lectin.
Clin. Exp. Immunol. 124, 223–228 (2001).
23. Takahashi, K., Ip, W.E., Michelow, I.C. & Ezekowitz, R.A.B. The mannose-binding
lectin: a prototypic pattern recognition molecule. Curr. Opin. Immunol. 18, 16–23
(2006).
24. Orsini, J. et al. Microbiological profile of organisms causing bloodstream infection
in critically ill patients. J. Clin. Med. Res. 4, 371–377 (2012).
25. Castanheira, M., Farrell, S.E., Krause, K.M., Jones, R.N. & Sader, H.S. Contemporary
diversity of β-lactamases among Enterobacteriaceae in the nine U.S. census regions
and ceftazidime-avibactam activity tested against isolates producing the most
prevalent β-lactamase groups. Antimicrob. Agents Chemother. 58, 833–838
(2014).
26. Morrow, B.J. et al. Activities of carbapenem and comparator agents against
contemporary US Pseudomonas aeruginosa isolates from the CAPITAL surveillance
program. Diagn. Microbiol. Infect. Dis. 75, 412–416 (2013).
27. Mebius, R.E. & Kraal, G. Structure and function of the spleen. Nat. Rev. Immunol.
5, 606–616 (2005).
28. Meijer, H.E.H., Singh, M.K. & Anderson, P.D. On the performance of static mixers:
a quantitative comparison. Prog. Polym. Sci. 37, 1333–1349 (2012).
29. Jayakumar, J.S., Mahajani, S.M., Mandal, J.C., Iyer, K.N. & Vijayan, P.K. CFD
analysis of single-phase flows inside helically coiled tubes. Comput. Chem. Eng.
34, 430–446 (2010).
30. Pass, L.J., Schloerb, P.R., Pearce, F.J. & Drucker, W.R. Cardiopulmonary response
of the rat to Gram-negative bacteremia. Am. J. Physiol. 246, H344–H350
(1984).
31. Wiesel, P. et al. Endotoxin-induced mortality is related to increased oxidative stress
and end-organ dysfunction, not refractory hypotension, in heme oxygenase-1–
deficient mice. Circulation 102, 3015–3022 (2000).
32. Netea, M.G. Proinflammatory cytokines and sepsis syndrome: not enough, or too
much of a good thing? Trends Immunol. 24, 254–258 (2003).
33. Janz, D.R. et al. Association between cell-free hemoglobin, acetaminophen, and
mortality in patients with sepsis: an observational study. Crit. Care Med. 41,
784–790 (2013).
34. Rello, J. Severity of pneumococcal pneumonia associated with genomic bacterial
load. Chest 136, 832 (2009).
35. Levy, S.B. & Marshall, B. Antibacterial resistance worldwide: causes, challenges
and responses. Nat. Med. 10, S122–S129 (2004).
36. Takahashi, K. et al. Mannose-binding lectin and its associated proteases (MASPs)
mediate coagulation and its deficiency is a risk factor in developing complications
from infection, including disseminated intravascular coagulation. Immunobiology
216, 96–102 (2011).
VOLUME 20 | NUMBER 10 | OCTOBER 2014
nature medicine
ONLINE METHODS
npg
© 2014 Nature America, Inc. All rights reserved.
Biomimicry of human blood opsonins. To develop a viable clinical therapy
using this blood-cleansing approach, we studied how the living spleen naturally
works in combination with the innate immune system to remove pathogens
from blood with high efficiency (for example, virtually all fungal pathogens are
captured by the spleen within one minute after intravenous injection in rabbits;
Supplementary Fig. 5). In the human body, pathogen capture is mediated by
natural blood opsonins, such as mannose-binding lectin (MBL). MBL is a
soluble, circulating, calcium-dependent (C-type) lectin that binds to terminal
mannose and fucose residues on branched oligosaccharides that are expressed
on the surface of over 90 different pathogen species (including Gram-negative
and Gram-positive bacteria, fungi, protozoa and viruses) as well as endotoxin
but not on mammalian cells37–39. The MBL-opsonized pathogens are then
bound and phagocytosed by macrophages in the spleen as flow slows and the
blood trickles from the arterial circulation through the marginal zones and
red-pulp cords and into venous sinuses.
Fabrication of magnetic opsonins. Native human MBL was genetically engineered to create the Fc-fusion opsonin protein FcMBL, which consists of the
tripeptide alanine-lysine-threonine (AKT) followed by the hinge, CH2 and
CH3 domains of human IgG1 Fc (residues E216–G446 with two point mutants,
C220S and N297D), followed by a single alanine linker fused to the neck and
carbohydrate-recognition domain (CRD) region of human MBL2 (residues
81–228 of the mature protein). cDNA for this construct (GenBank accession code: KJ710775) was cloned downstream of the Ig κ–light chain leader
sequence in an HTLV-driven expression plasmid for transient transfection in
HEK293F Freestyle cells (Invitrogen) and into an HTLV expression plasmid
with DHFR under the control of an IRES for stable transfection into CHODG44 cells (Invitrogen), following the manufacturer’s suggested protocols.
FcMBL was purified from conditioned medium using protein A Sepharose
(GE Healthcare Life Sciences) on an AKTA-Avant system (GE Healthcare
Life Sciences). Using expression of the FcMBL from CHO cell lines and a
single-step, Fc-based purification technique, we were able to produce large
amounts (0.112 g liter−1) of single band–quality FcMBL that were efficiently
immobilized on the magnetic nanobeads. Purity was confirmed to >95% by
SDS-PAGE electrophoresis, and functionality was confirmed by the ability to
bind to mannan-coated plates. By fusing the tripeptide AKT into the N terminus for site-specific biotinylation, we are able to orient coupling of the FcMBL
to streptavidin-coated superparamagnetic beads (Ademtech AS) so that the
N-terminal Fc hinge attached to the bead surface and the CRD faced outward.
The N-terminal amine of FcMBL was modified to an aldehyde using pyridoxal5-phosphate monohydrate treatment as previously described 40,41; the AKT
tripeptide at the N-terminus has been identified as an optimal sequence for
this reaction42. Briefly, FcMBL protein at 4 mg ml−1 was incubated overnight
at room temperature in 7.5 mM PLP (Alfa Aesar) in 50 mM sodium phosphate
buffer, pH 6.4. The PLP-treated protein was dialyzed 3 times against 50 mM
sodium phosphate, pH 6.4, and then incubated overnight in the presence of
25 µg of aminooxy biotin (Biotum) per 1 mg of FcMBL. Biotinylated FcMBL
was coupled to 128-nm streptavidin-coated magnetic beads (Ademtech AS)
at a ratio of 25 µg of protein mg−1 of beads for 30 min at room temperature.
To create the magnetic opsonin beads, streptavidin-coated superparamagnetic
nanobeads (128 nm; Ademtech Inc.) were incubated with biotinylated FcMBL
(25 µg protein mg−1 beads) for 30 min at room temperature, and remaining
unbound streptavidin sites on the beads were blocked with polyethylene glycol
(PEG)-biotin (1 kDa PEG; Nanocs Inc.). The beads (5 mg beads ml−1) were
resuspended in 1% BSA in PBS and stored at 4 °C until use. The PEG was used
to minimize nonspecific binding of serum proteins and blood components
to the magnetic beads as it has been shown to effectively prevent nonspecific
binding of molecules in vitro43 and in vivo44,45, in addition to already being
used for this purpose in multiple FDA-approved blood-compatible clinical products. In addition, we confirmed that the FcMBL magnetic beads do
not deplete blood cells nonspecifically (Supplementary Fig. 4b) when we
treated human blood with the biospleen devices using the same conditions
as in the rat study, and then carried out complete blood counts using a commercial CBC machine. In addition, we confirmed that FcMBL failed to induce
significant coagulation or complement activation in blood versus native
doi:10.1038/nm.3640
recombinant human MBL (rhMBL) (Supplementary Fig. 1c,d, using previ
ously described methods46–48 to quantitate the thrombin-like activity and
complement-binding activity of MBL, respectively (rhMBL manufactured by
Enzon Pharmaceuticals Inc. was provided by K. Takahashi (Massachusetts
General Hospital)49). Moreover, when FcMBL-coated beads were incubated with
50 µg of DNA isolated from salmon sperm, they did not exhibit any detectable
binding. This is in stark contrast to wild-type MBL, which has been shown to
bind to DNA50. Generic ligands for pathogen binding have been developed in
the past. For example, the synthetic organic molecule zinc(II)-dipicolylamine
binds to enriched anionic phospholipids of bacterial cell walls by forming
coordination complexes51,52. However, their binding capacity is limited: they
do not bind to as wide a range of pathogens, toxins and viruses, and their
binding strength is much weaker than that exhibited by MBL for its microbial
cell-surface ligands53. The major advantage of the FcMBL opsonin is that the
clinical development path should be much more straightforward as it is an
engineered version of a human blood protein. FcMBL also can be produced in
large quantities at low cost using protein A purification, and the Fc moiety has
been previously used in multiple US Food and Drug Administration–approved
protein therapeutics54.
Biospleen device design and fabrication. The microdevice developed in our
past studies had insurmountable limitations that prohibited its clinical application for sepsis therapy55,56. First, as the identity of the infectious agent is not
known when a patient first presents with symptoms of systemic infection, it is
not possible to select appropriate microbe-specific antibodies, and the cost of
using numerous antibodies directed against virtually all potential pathogens
would be prohibitive. Second, endotoxins that are released by many microbes
when killed by endogenous immune responses or antibiotic therapies are a
major trigger for the inflammatory cascade that leads to sepsis57, yet these toxins were not cleared with the initial method. Third, the microfluidic channel
design used in the original device could not support the high flow rates (liters
per hour) necessary for clinical use without causing blood loss or dilution.
The dimensions of the channels and slits were initially based on our previous device design58, which enabled high (>99%) magnetic bead capture efficiencies but only at very low flow rates (<0.0012 liter h−1). To further optimize
system function, magnetic flux density gradients across the blood channel were
estimated using computational simulations59 (Supplementary Fig. 3b), and
the distance the magnetic bead–bound pathogens would travel perpendicular
to the blood channel while flowing through the device was calculated as a
function of the magnetic flux density gradient and flow rate (Supplementary
Fig. 3c). We then redesigned the channels to obtain a removal efficiency
of >99% using these results. The channel width (2 mm) and overall device
dimensions were determined by the size of the permanent magnets (50 mm
in length) and capacity of the micro-milling machine. We calculated the magnetic force acting on a pathogen bound with magnetic opsonin beads and how
fast they are pulled by the magnetic flux density gradient of the permanent
magnets (Nd2Fe14B, BY042SH; magnetization, M = 106 A m−1) (KJ Magnetics,
Jamison, PA, USA). The magnetic drag velocity of a pathogen bound with
nanomagnetic opsonin beads was determined by the equation59
Vmag (x ) =
2R2 ∆ c B(x)
9 m0h
(1)
where Vmag(x) is the magnetic drag velocity, R is a radius of a magnetic
bead, ∆χ is difference in magnetic susceptibility between magnetic beads
and solution, µ0 is the vacuum permeability, η is the dynamic viscosity and
B(x) is the magnetic flux density gradient. Then, Dt can be calculated by
equations (2) and (3)
Dt = Vmag (x ) × tres
tres =
whL
Q
(2)
(3)
where tres is the residence time of the magnetic beads in the channel while they
are flowing through the device; w, h and L are width, height and length of the
channel; and Q is the flow rate (ml h−1). The saline channel of the magnetic
nature medicine
© 2014 Nature America, Inc. All rights reserved.
npg
separator unit of the blood-cleansing microdevice is 340 µm in height, whereas
the blood channel is 600-µm high; thus, the magnetic force acting on the
nanomagnetic opsonin and magnetically labeled pathogens is much enhanced,
resulting in further increased pathogen removal efficiency. Both the blood
and saline channels are 2 mm wide. To enhance flow throughput, the single
inflow channel into the device was designed so that it undergoes 4 branches
before entering a total of 16 magnetic separator channels, which then join in a
symmetrical quadruple branching pattern to merge into a single outlet channel
(Fig. 1c (top) and Supplementary Fig. 2a). Sheets (1.58 mm) of aluminum
(Fig. 1c), medical-grade polysulfone (Supplementary Fig. 2b) or PMMA
(Supplementary Fig. 2c) were micromachined using a Microlution 5100-S
(Microlution Inc.) machine, and the upper and lower surfaces of the device
containing the fluidic channels were covered with thin layers of transparent
PMMA adhesive tape (76-µm thickness, McMaster-Carr); similar isolation
efficiencies were obtained with all devices from three types of materials. As
shown in Supplementary Figure 2a, two upper and two lower connector
blocks were then aligned with the ends of the taped device using dowel pins,
and assembled into a single integrated device that was held together by socket
head cap screws (McMaster-Carr, 92290A117). Four O-rings also were located
between through-holes on the connector blocks and the device to prevent
leakage, and luer lock connectors were inserted into each port to create a bio
spleen device that can connect to fluid sources (Supplementary Fig. 2a,c) and
capture magnetic opsonins flowing through its slits when stationary magnetics
are placed on its top surface (Supplementary Fig. 2a). Similar results were
obtained with the aluminum (Fig. 1c) and polymeric devices (Supplementary
Fig. 2b,c) in our in vitro studies, and we used the aluminum biospleen device
for treating septic rats. The assembled blood-cleansing magnetic separator
unit and attached tubing and connectors were sterilized using ethylene oxide
before use in animal studies.
One of the key challenges of the blood-cleansing microdevice is that we
need to continuously mix blood with nanomagnetic opsonins and then incub
ate them without damaging blood in laminar flow. We incorporated a Kenics
static inline mixer60 into the blood-cleansing microdevice system (Fig. 1d,
Supplementary Figs. 2d and 3a) to ensure that the continuously injected
nanomagnetic opsonins were thoroughly mixed with blood so that pathogens
in blood could bind to the FcMBL nanomagnetic beads. After passing through
the inline mixer, pathogens and nanomagnetic opsonins need to be mixed in
the flowing blood before it reaches the magnetic separator unit of the bloodcleansing microdevice. To accomplish this, we inserted an incubation loop
composed of helically coiled tubing (internal diameter, 1.58 mm; 100 cm long)
between the mixer and the separator unit (Fig. 1d and Supplementary Fig. 2d)
to enhance transverse convective flux along the tubing61. This flux is determined by the Dean number (De = Re (r Rc−1)0.5, De = 0.17) in a curved duct,
where Re is the Reynolds number, r is an inner radius of the tubing (1.59 mm)
and Rc is a coil radius (6.3 mm). We confirmed that incorporation of the mixer
with this loop design increased binding and removal efficiencies for S. aureus
bacteria from ~40% to 99% when they were spiked (104 CFU ml−1) into banked
whole blood or buffer flowing at 10 ml h−1 (Supplementary Fig. 3a).
Fluidic resistance measurements. It is critical to control the fluidic resistance of the extracorporeal system because changes in resistance may affect
blood pressure of patients and cause blood coagulation due to fluidic
resistance–driven shear stress62. We measured the fluidic resistance across
the blood-cleansing microdevice system, including tubing and an inline
Kenics mixer (FMX8214; Omega Engineering Inc.), at a high flow rate up to
1.6 liter h−1 of saline in a single device and determined this to be 15.5 mm Hg,
which is compatible with the pressure drops of other extracorporeal devices63
(Supplementary Fig. 3e). Our final design also ensured that shear stresses
within the blood channel were low (<3 dyne cm−2; Supplementary Fig. 4a)
and well within the physiological range (<15 dyne cm−2)64. We also demonstrated high throughput by circulating 200 ml of human blood (CPDA-1 anticoagulated blood-bank blood) through a single blood-cleansing microdevice
system at a flow rate of 1.25 liter h−1 for over 25 h without any evidence of
blood clotting or coagulation. After 25 h of circulation through the device,
the blood was passed through a 40-µm cell strainer (Cat. No.: 352340, BD
Falcon, BD Biosciences), and no blood clots were seen. Units of human blood
nature medicine
were obtained from Brigham and Women’s Specimen Bank (protocol number
M20403-101). Analysis of system function also confirmed that blood loss and
dilution were minimal using this design because the flow through the saline
channel was static during the cleansing step, and its total volume (<1 ml)
was significantly smaller than the volume of blood that flowed continuously
through the blood channel (Supplementary Fig. 3f).
Blood-cleansing device operation. Because we planned to carry out proof-ofconcept studies in rat sepsis models, we carried out pathogen-clearance studies
in vitro and in vivo using 10 mL of blood flowing at 10 ml h−1 based on the
known volume and flow rate of blood in a rat65,66. In the in vitro studies, bacteria (104 CFU ml−1) were spiked into 10 ml of human whole blood and flowed
through the device. Magnetic opsonins (0.5 mg ml−1 in saline) were introduced
continuously (7.1 µl min−1) into the blood path through a three-way connector
(Supplementary Fig. 2d), and then the blood was passed through the spiral
mixer and coiled tubing to ensure complete pathogen binding before entering
the magnetic separator of biospleen device (Fig. 1d). After passing through
the device, the cleansed blood that exits the outlet then returns back to the
inlet, producing a closed, extracorporeal blood-circulation loop. Quantitation
of pathogen depletion from blood was determined by collecting small (100 µl)
blood samples over time and carrying out quantitative blood culture assays
to determine pathogen colony-forming units. Controls included running
the contaminated blood sample through the device without the magnets or
with magnets but without adding the magnetic opsonin beads, and neither
produced significant pathogen removal.
The capture efficiency was lower in blood than in buffer likely because of
the high numbers of blood cells (~109 red blood cells ml−1, ~108 platelets ml−1
and 106 white blood cells ml−1) and higher fluid viscosity that decrease the
efficiency of magnetic capture. But in studies with various samples of human
blood that had differences in hematocrit over the normal range (40–55%), we
did not observe significant differences in capture efficiency. This isolation
efficiency can be further improved by increasing magnetic flux density gradients65,67 and modifying the channel geometry to utilize the stronger magnetic
forces. Moreover, as flow through this device scales linearly, the biospleen can
be adapted for use at rates as high as 10 or more liters per hour, if required for
large animal or human studies, simply by connecting multiple (>8) separator
units in parallel.
Taken together, these studies show that the biospleen device can efficiently
cleanse flowing whole blood of various types of pathogens, as well as endotoxins, without significantly altering blood composition or inducing coagulation
in vitro. Notably, we were able to obtain near-complete removal of pathogens
and endotoxins that were magnetically opsonized because multiple nanobeads
bind to each pathogen or endotoxin-containing pathogen fragment. However,
we only removed about 80% of unbound, single nanomagnetic beads because
they have extremely small magnetic moments due to their small size (128 nm).
In future therapeutic applications, it would be advantageous to minimize release
of unbound magnetic nanobeads into the individual’s circulation; therefore, we
added larger (1-µm diameter), uncoated superparamagnetic beads to the blood
(50 µl in 10 ml of blood) along with the 128-nm, FcMBL-coated beads. These
larger beads act as local magnetic field gradient concentrators that magnetize and
attract the smaller, 128-nm FcMBL beads flowing in the liquid when exposed to
an external magnetic field (i.e., only when passing through the magnetic separator). This results in the formation of larger bead aggregates, which increases
their effective magnetic radius and, thus, their ability to be magnetically cleared
from the blood channel in the biospleen device68. To quantitate removal efficiency of unbound, single nanomagnetic beads (128 nm), we labeled the beads
with fluorescein isothiocyanate (FITC) and flowed them through the device in
saline with larger (1 µm, Dynabeads MyOne; Invitrogen), uncoated magnetic
flux concentrator beads at a flow rate of 10 ml h−1 and then measured the fluorescent signal of the sample collected from the outlet (Supplementary Fig. 4c).
Experimental studies confirmed that addition of these larger beads increased
magnetic capture of the smaller magnetic opsonins from ~80% to 99.6 ± 0.6%
when flowed through the biospleen at 10 ml h−1 (Supplementary Fig. 4c).
If additional bead capture is required in the future, a component capable of continuously removing magnetic nanobeads67 could be incorporated downstream
in the circuit before blood is returned to the individual.
doi:10.1038/nm.3640
npg
© 2014 Nature America, Inc. All rights reserved.
Microbial cell culture. To model sepsis induced by intestinal injury, we fed
Wistar rats a diet of raw ground beef and collected their cecal contents, which
contain a complex mixture of aerobic and anaerobic bacteria, including E. coli
and B. fragilis. Aerobic bacterial cultures (i.e., Staphylococcus aureus, Bacillus
subtilis, Pseudomonas aeruginosa, Klebsiella pneumoniae and Escherichia coli)
and aerobic microbes isolated from rat cecal contents as described 69 were
grown in LB medium at 37 °C, shaking at 200 rpm. Anaerobic bacteria isolated from rat cecal contents69 were cultured on LB agar plates at 37 °C in an
anaerobic chamber (Coy Laboratories). Fungal cultures (i.e., Candida albicans, Pichia pastoris, Candida parapsilosis and Saccharomyces cerevisiae) were
grown in YPD medium at 30 °C, shaking at 200 rpm. Cell concentrations were
measured with OD600 spectrometry (M5 SpectraMax, Molecular Devices); cell
concentrations below 104 cells ml−1 (OD600 ~10−4) were quantified by culture
on blood agar plates. Stock aliquots containing a defined number of cells per
tube were obtained by FACS (BD FACS Aria, BD Biosciences) and used in various depletion and separation assays to enhance experimental consistency.
Cell-binding and capture assays. Initial testing of the pathogen-capturing
efficiency of the magnetic opsonins was carried out by spiking 104 CFU
S. aureus into 10 ml of heparinized, whole human blood and then adding
50 µl of the FcMBL beads (5 mg ml−1). Human blood was obtained from
healthy donors with informed consent in accordance with the Harvard
University Faculty of Medicine Committee on Human Studies and the Defense
Advanced Research Projects Agency (protocol number M20403-101). After
mixing in an inverting mixer (Invitrogen) for 20 min, the blood samples
were flowed through the biospleen magnetic separator unit at 10 ml h−1, and
samples of the collected blood (100 µl) were plated on blood agar plates for
quantitating pathogen-capture efficiency. In subsequent studies, aliquots of
C. albicans, S. cerevisiae, S. aureus, E. coli and cecal contents with a known
pathogen concentrations stored at −80 °C were thawed and diluted to 104 CFU
ml−1 and used to test magnetic opsonin binding and capture. Characterization
of bead binding to different pathogens was carried out using 500-µl samples
of each pathogen strain diluted in 0.1 M Tris buffered saline, pH 7.4, with
0.05% Tween 20 (TBST) (Boston BioProducts) buffer with 5mM CaCl2 or
diluted in human blood with 5 mM CaCl2 and incubated for 20 min with
FcMBL-coated nanobeads (5 mg ml−1) in a tube with agitation on an inverting mixer (Invitrogen); a positive control for each strain was taken before the
beads were added. The solution containing the beads and pathogens was then
flowed through the biospleen device at 10 ml h−1 to determine the efficiency
of removal of magnetic opsonin-bound pathogens. This flow rate and the
volume (3.5 ml) used to prime the system with saline were determined based
on the previous reports using rats of similar weight to those we eventually used
for our in vivo studies65,66. Aliquots of the fluid remaining in each tube after
magnetic removal of the bound pathogens were plated out onto blood agar
plates to determine the number of microbes that eluded binding and capture.
Fungi were plated out onto dextrose agar plates and cultured at 30 °C; bacteria
were cultured on LB agar (or blood agar) plates at 37 °C. Colonies were counted
24 h later to determine the pathogen concentration in the positive control and
depleted samples. Binding efficiencies were determined by measuring the ratio
of bound to unbound pathogens in each experiment.
Endotoxin-binding assay. Lipopolysaccharide (LPS) endotoxin extracted
from E. coli was spiked into TBST buffer with 5 mM CaCl2 at concentrations
of 20, 2, 0.2 and 0 µg ml−1, and the capture capacity of the magnetic beads
coated with FcMBL opsonins was assessed by a sandwich immunoassay using
the FcMBL magnetic beads and the horseradish peroxidase (HRP)-labeled
FcMBL protein diluted in 0.1 M TBST. The colorimetric reaction was detected
with the Pierce 1-Step TMB Substrate (Thermo Scientific) according to the
manufacturer’s protocol, and results were read at 450 nm. For measuring
LPS levels in blood, we collected blood samples (100 µl) from the biospleen
circuit and performed the sandwich immunoassay as described above. The
background signal of heparinized, fresh human whole blood is around 0.15
arbitrary units at 450 nm (Fig. 2d).
Rat sepsis models. All animal protocols were reviewed and approved by the
Institutional Animal Care and Use Committee (IACUC) of Boston Children’s
doi:10.1038/nm.3640
Hospital and Harvard Medical School, and the Animal Care and Use Review
Office of the US Army Medical Research and Material Command Office and
Department of Defense. Rats (Wistar 12-week-old male, 350 g) used in this
study were obtained with double catheters placed in their jugular veins from
Charles River Laboratories. Before initiating experiments with infected animals, we tested the biocompatibility of the biospleen device by connecting it
to jugular vein catheters of a living rat we randomly selected and circulated the
animal’s blood through the extracorporeal circuit and the biospleen device for
5 h. Healthy catheterized rats (n = 3) were anesthetized with isoflurane using a
nose cone and two 23-gauge needles were inserted into the catheters and then
connected to male luer-barb fitting connectors (EW-45504-00, Cole-Parmer)
at each end of the biospleen tubing loop (Tygon 1/16” ID, PVC) (Fig. 1d and
Supplementary Fig. 2d). We continuously injected saline (90 ml kg−1 day−1)
containing heparin (50 unit kg−1 h−1) as required by IACUC protocols to prevent dehydration of the rats and coagulation of blood while circulating blood
through the biospleen circuit. Heparin administration is also standard medical
practice in humans receiving extracorporeal hemodialysis or extracorporeal
membrane oxygenation.
To study the utility of the blood-cleansing device in an animal with a systemic bacterial infection, we used the previously described sepsis model using
Wistar rats70 we randomly selected in which 1 ml of PBS containing S. aureus
(ATCC No.: 12598, 5 × 108 CFU ml−1) was injected into the peritoneal cavity.
In this model, pathogen levels in blood increased 3–4 h after injection and
peaked around 10 h (ref. 70). At 10 h, we anesthetized the rats, connected their
jugular catheters to the tubing of the biospleen device and initiated peristaltic
pumping at a flow rate of 10 ml h−1; the syringe pump was used to inject saline
containing heparin (50 unit kg−1 h−1), the magnetic opsonins (0.5 mg ml−1)
and larger magnetic flux concentrator beads (0.5 mg ml−1) at a flow rate of
7.1 µl min−1. Every hour, we collected small blood samples (300 µl) through a
3-way valve in the circuit, which were used to measure cytokines (Bio-Plex Pro
kit, Bio-Rad) and plasma hemoglobin (using a colorimetric assay) and to carry
out blood-culture analysis in a blinded fashion (n = 3 for biospleen treatment;
n = 3 for the untreated group). The control rats randomly selected were either
untreated or treated with biospleen without adding magnetic opsonins while
receiving saline and heparin as described above.
In a separate study, we used the E. coli Gram-negative bacteremia
model that was reported previously71,72 by injecting a bolus of saline containing 5 × 108 CFU ml−1 of E. coli followed by continuously infusing 5 × 108
CFU ml−1 of E. coli (ATCC No. 8739) for 5 h while treating the rats with the
biospleen device (n = 3). In a control experiment (n = 3), we treated the rats
with the same experimental biospleen setup except that the magnetic beads
were not coated with FcMBL (i.e., they were only coated with PEG).
In the bacteremia animal models, the experimental and control animals
received the same continuously infused volume of saline and heparin for continuous fluid resuscitation. The only difference was that the experimental
animals received FcMBL beads, whereas the controls either received no beads
or beads without FcMBL attached. Thus, the fluid due to bead administration
(~250 µl of the bead stock solution for 5 h) was minimal compared to the
large volume of saline (90 ml kg−1 day−1 into rats of 350-g weight; 6.6 ml total
volume in 5 h) that we have to infuse into the animals over time during the
extracorporeal treatment to keep them hydrated.
To determine the ability of the biospleen to treat animals with endotoxemia, we injected LPS endotoxin (13.5 × 106 endotoxin units ml−1) extracted
from E. coli (0111:B4)73 into the jugular catheters of the rats (n = 7 for the
untreated group; n = 9 for biospleen treatment) and then immediately connected the rats to the blood-cleansing system. We continuously infused saline
with heparin at the same flow rate in the untreated animals as we did for the
biospleen treatment group to keep them hydrated, so the only difference was
that blood was circulated through the biospleen device in the experimental
group. Blood sample collection and analysis were similar to that described
above. Rats also were observed continuously to monitor symptoms of morbidity, as measured by body temperature, respiratory rates, mucous membrane
color, perfusion quality and labored breathing. After 5 h of blood cleansing,
the rats were humanely euthanized according to the protocol and the major
organs were harvested, fixed in 10% formalin, cryosectioned and processed
for immunohistochemistry and HE staining in a blinded fashion as previously
nature medicine
© 2014 Nature America, Inc. All rights reserved.
described74. The levels of S. aureus present in the organs were quantified using
computerized microfluorimetry to measure fluorescence intensity (green) in
six random fields out of samples from three rats from each group.
These results strongly support our hypothesis that removing pathogens and
endotoxins from septic blood should be able to significantly attenuate sepsis
progression that leads to organ dysfunction and mortality and, thus, potentially save the lives of septic patients. It is important to note, however, that we
were not able to test the long-term efficacy of the biospleen device because
our rat studies were limited to 5-h duration by our animal protocol (after
which surviving animals had to be euthanized) due to the use of isoflurane
anesthesia, which can produce significant respiratory suppression in rats. In
future large-animal and human studies, this blood-cleansing device would
likely be used continuously in combination with broad-spectrum antibiotics
until clinical response is observed.
Hematology. To determine whether treatment with the biospleen significantly
changes blood chemistry, blood samples (300 µl) were collected from rats after
being connected to the extracorporeal circuit containing the blood-cleansing
device for 5 h. The blood samples were centrifuged (×500 g) for 15 min and the
supernatant-containing, platelet-depleted plasma was collected. Thrombin–
anti-thrombin complexes (TAT) were measured using a sandwich ELISA kit
according to the manufacturer’s instructions (Wuhan EIAAB Science). Red
blood cell lysis also was analyzed to determine release of free hemoglobin in
plasma. Plasma hemoglobin was measured by a hemoglobin colorimetric assay
(Cayman Chemical, Item #700540). Plasma was diluted 1:10 in hemoglobin
detector and incubated at room temperature for 15 min. Absorbance at 575 nm
was subsequently measured and concentrations were calculated by reference to
an eight-point hemoglobin standard curve (Cayman Chemical, Item# 700453).
Plasma cytokine levels were measured using the Bio-Plex Pro Rat Cytokine
24-plex assay (Bio-Rad) according to the kit directions. Briefly, plasma samples
were diluted 1:4 before mixing with coupled beads for cytokine measurement.
All plate washes were performed with a Bio-Plex Pro magnetic wash station
(Bio-Rad). Samples were measured using the Bio-Plex 3D Suspension array
system (Bio-Rad) and the accompanying Bio-Plex Manager software was used
for all data acquisition and analysis.
Kinetic model for estimating pathogen clearance. The systemic pathogen
clearance efficiency from septic blood can be calculated by the simplified
mathematical model of Monod kinetics56
npg
dC p
dt
Fj
= C p m −
V
(4)
where Cp is the concentration of pathogen in blood, t is time, µ is the growth
rate of the pathogen (for example, S. aureus: 0.13 h−1)75, F is the flow rate (ml
h−1), ϕ is the pathogen-removal efficiency in a single-round pass and V is the
blood volume. The pathogen-removal efficiency was plotted in Figure 2b.
Scanning electron microscopy. All scanning electron microscopy images were
collected using a Zeiss FESEM Supra at the Center for Nanoscale Systems
at Harvard University. Samples were fixed in 2.5% glutaraldehyde in 0.1 M
sodium cacodylate and dehydrated through an ethanol gradient followed by
hexamethyldisilazane drying. Specimens were captured on a porous membrane
for visualization.
Statistical analysis. All measured values are reported as an average of at least
triplicate samples ± s.e.m., as indicated by error bars in all graphs. Significant
differences in survival rates in the endotoxemia rat model were determined
using the Mantel-Cox test and the Gehan-Breslow-Wilcoxon test (P < 0.05).
Other significant differences were determined by the ANOVA t-test, as defined
by P values <0.05.
37. Neth, O. et al. Mannose-binding lectin binds to a range of clinically relevant
microorganisms and promotes complement deposition. Infect. Immun. 68,
688–693 (2000).
nature medicine
38. Townsend, R., Read, R.C., Turner, M.W., Klein, N.J. & Jack, D.L. Differential
recognition of obligate anaerobic bacteria by human mannose-binding lectin.
Clin. Exp. Immunol. 124, 223–228 (2001).
39. Takahashi, K., Ip, W.E., Michelow, I.C. & Ezekowitz, R.A.B. The mannose-binding
lectin: a prototypic pattern recognition molecule. Curr. Opin. Immunol. 18, 16–23
(2006).
40. Gilmore, J.M., Scheck, R.A., Esser-Kahn, A.P., Joshi, N.S. & Francis, M.B.
N-terminal protein modification through a biomimetic transamination reaction.
Angew. Chem. Int. Ed. Engl. 45, 5307–5311 (2006).
41. Scheck, R.A. & Francis, M.B. Regioselective labeling of antibodies through
N-terminal transamination. ACS Chem. Biol. 2, 247–251 (2007).
42. Witus, L.S. et al. Identification of highly reactive sequences for PLP-mediated
bioconjugation using a combinatorial peptide library. J. Am. Chem. Soc. 132,
16812–16817 (2010).
43. Shim, M., Shi Kam, N.W., Chen, R.J., Li, Y. & Dai, H. Functionalization of
carbon nanotubes for biocompatibility and biomolecular recognition. Nano Lett. 2,
285–288 (2002).
44. Åkerman, M.E., Chan, W.C.W., Laakkonen, P., Bhatia, S.N. & Ruoslahti, E.
Nanocrystal targeting in vivo. Proc. Natl. Acad. Sci. USA 99, 12617–12621
(2002).
45. Korin, N. et al. Shear-activated nanotherapeutics for drug targeting to obstructed
blood vessels. Science 337, 738–742 (2012).
46. Takahashi, K. et al. Mannose-binding lectin and its associated proteases (MASPs)
mediate coagulation and its deficiency is a risk factor in developing complications
from infection, including disseminated intravascular coagulation. Immunobiology
216, 96–102 (2011).
47. Petersen, S.V., Thiel, S., Jensen, L., Steffensen, R. & Jensenius, J.C. An assay for
the mannan-binding lectin pathway of complement activation. J. Immunol. Methods
257, 107–116 (2001).
48. Vorup-Jensen, T. et al. Recombinant expression of human mannan-binding lectin.
Int. Immunopharmacol. 1, 677–687 (2001).
49. Michelow, I.C. et al. A novel l-ficolin/mannose-binding lectin chimeric molecule
with enhanced activity against Ebola virus. J. Biol. Chem. 285, 24729–24739
(2010).
50. Palaniyar, N. et al. Nucleic acid is a novel ligand for innate, immune pattern
recognition collectins surfactant proteins A and D and mannose-binding lectin.
J. Biol. Chem. 279, 32728–32736 (2004).
51. Lakshmi, C., Hanshaw, R.G. & Smith, B.D. Fluorophore-linked zinc(ii)dipicolylamine
coordination complexes as sensors for phosphatidylserine-containing membranes.
Tetrahedron 60, 11307–11315 (2004).
52. Lee, J.-J. et al. Synthetic ligand-coated magnetic nanoparticles for microfluidic
bacterial separation from blood. Nano Lett. 14, 1–5 (2014).
53. Ji, X., Gewurz, H. & Spear, G.T. Mannose binding lectin (MBL) and HIV.
Mol. Immunol. 42, 145–152 (2005).
54. Beck, A. & Reichert, J.M. Therapeutic Fc-fusion proteins and peptides as successful
alternatives to antibodies. MAbs 3, 415–416 (2011).
55. Xia, N. et al. Combined microfluidic-micromagnetic separation of living cells in
continuous flow. Biomed. Microdevices 8, 299–308 (2006).
56. Yung, C.W., Fiering, J., Mueller, A.J. & Ingber, D.E. Micromagnetic–microfluidic
blood cleansing device. Lab Chip 9, 1171 (2009).
57. Wiesel, P. et al. Endotoxin-induced mortality is related to increased oxidative stress
and end-organ dysfunction, not refractory hypotension, in heme oxygenase-1–
deficient mice. Circulation 102, 3015–3022 (2000).
58. Kang, J.H. et al. A combined micromagnetic-microfluidic device for rapid capture
and culture of rare circulating tumor cells. Lab Chip 12, 2175 (2012).
59. Kang, J.H., Choi, S., Lee, W. & Park, J.-K. Isomagnetophoresis to discriminate
subtle difference in magnetic susceptibility. J. Am. Chem. Soc. 130, 396–397
(2008).
60. Ling, F. & Zhang, X. A numerical study on mixing in the Kenics static mixer. Chem.
Eng. Commun. 136, 119–141 (1995).
61. Jayakumar, J.S., Mahajani, S.M., Mandal, J.C., Iyer, K.N. & Vijayan, P.K. CFD
analysis of single-phase flows inside helically coiled tubes. Comput. Chem. Eng.
34, 430–446 (2010).
62. Ofsthun, N.J., Jensen, J.C. & Kray, M. Effect of high hematocrit and high blood
flow rates on transmembrane pressure and ultrafiltration rate in hemodialysis.
Blood Purif. 9, 169–176 (1991).
63. Krisper, P. & Stauber, R.E. Technology insight: artificial extracorporeal liver
support—how does Prometheus compare with MARS? Nat. Clin. Pract. Nephrol. 3,
267–276 (2007).
64. Huh, D. et al. Reconstituting organ-level lung functions on a chip. Science 328,
1662–1668 (2010).
65. Ordodi, V.L. et al. Artificial device for extracorporeal blood oxygenation in rats.
Artif. Organs 32, 66–70 (2008).
66. Lee, H.B. & Blaufox, M.D. Blood volume in the rat. J. Nucl. Med. 26, 72–76
(1985).
67. Kang, J.H. & Park, J.-K. Magnetophoretic continuous purification of single-walled
carbon nanotubes from catalytic impurities in a microfluidic device. Small 3,
1784–1791 (2007).
68. Cooper, R.M. A Generic Pathogen Capture Technology for Sepsis Diagnosis (MIT
Press, 2013).
69. Onderdonk, A.B., Weinstein, W.M., Sullivan, N.M., Bartlett, J.G. & Gorbach, S.L.
Experimental intra-abdominal abscesses in rats: quantitative bacteriology of infected
animals. Infect. Immun. 10, 1256–1259 (1974).
doi:10.1038/nm.3640
73. Remick, D.G., Newcomb, D.E., Bolgos, G.L. & Call, D.R. Comparison of the mortality
and inflammatory response of two models of sepsis: lipopolysaccharide vs. cecal
ligation and puncture. Shock 13, 110–116 (2000).
74. Mammoto, A. et al. Control of lung vascular permeability and endotoxin-induced
pulmonary oedema by changes in extracellular matrix mechanics. Nat. Commun.
4, 1759 (2013).
75. Lindqvist, R. Estimation of Staphylococcus aureus growth parameters from turbidity
data: characterization of strain variation and comparison of methods. Appl. Environ.
Microbiol. 72, 4862–4870 (2006).
npg
© 2014 Nature America, Inc. All rights reserved.
70. Liang, J. et al. Enhanced clearance of a multiple antibiotic resistant Staphylococcus
aureus in rats treated with PGG-glucan is associated with increased leukocyte counts
and increased neutrophil oxidative burst activity. Int. J. Immunopharmacol. 20,
595–614 (1998).
71. Parker, S.J. & Watkins, P.E. Experimental models of Gram-negative sepsis. Br. J.
Surg. 88, 22–30 (2001).
72. Pass, L.J., Schloerb, P.R., Pearce, F.J. & Drucker, W.R. Cardiopulmonary response
of the rat to Gram-negative bacteremia. Am. J. Physiol. 246, H344–H350
(1984).
doi:10.1038/nm.3640
nature medicine
Copyright of Nature Medicine is the property of Nature Publishing Group and its content may
not be copied or emailed to multiple sites or posted to a listserv without the copyright holder's
express written permission. However, users may print, download, or email articles for
individual use.