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Journal of Medical and Biological Engineering, 31(2): 121-127
121
Microfluidic Trapping of Antibody-secreting Cells
Sean F. Romanuik1,* Samantha M. Grist1 Moeed Haq1 Bonnie L. Gray1
Naveed Gulzar2 Jamie K. Scott2,3 Donna Hohertz4 Karen L. Kavanagh4
Rajinder Nirwan5 Christy Hui5 Alexandre G. Brolo5 Reuven Gordon6
1Microinstrumentation Laboratory, School of Engineering Science, Simon Fraser University, Burnaby, B.C. V5A 1S6, Canada 2Department of Molecular Biology and Biochemistry, Simon Fraser University, Burnaby, B.C. V5A 1S6, Canada
3Faculty of Health Sciences, Simon Fraser University, Burnaby, B.C. V5A 1S6, Canada 4Department of Physics, Simon Fraser University, Burnaby, B.C. V5A 1S6, Canada 5Department of Chemistry, University of Victoria, Victoria, B.C. V8W 2Y2, Canada
6Department of Electrical and Computer Engineering, University of Victoria, Victoria, B.C. V8W 2Y2, Canada
Received 4 Sep 2010; Accepted 14 Dec 2010; doi: 10.5405/jmbe.841
Abstract
The development of antibody-based drugs typically begins with the isolation and screening of thousands of
antibody-secreting cells, often requiring 4-6 weeks to identify only 1-10 cell lines of interest. We are developing a
novel immunobiosensing device to afford direct and rapid assessment of the antibody production of each of thousands
of living cells captured on a single slide. Each cell shall be trapped near a designated surface plasmon-resonant
nanohole array immunobiosensor to detect the binding of the cell’s secreted antibodies to an immobilized target antigen.
This paper presents arrays of single-cell traps consisting of concave hydrodynamic structures and inset microwells.
Each design is fabricated using either SU-8 photoresist or poly(dimethyl siloxane) (PDMS) and then tested using
polystyrene microspheres and 17/9 mouse B cell hybridoma cells. Although we find that PDMS adheres more strongly
to our substrates than SU-8, we also find that channels fabricated in PDMS are wider than expected and thus fail to
limit cellular passage. The hydrodynamic tests agree with the predictions of finite element modeling using COMSOL®
Multiphysics. We find that the hydrodynamic designs featuring concave traps inset into spirals and serpentine bends
capture cells more efficiently than our other hydrodynamic designs. Testing also verifies the functionality of our
microwell traps, with 5-20 cells/well trapped following a 10 min settling time. Moreover, untrapped cells beyond the
microwells are removed via peristaltic pumping, with minimal trapped cell displacement. Furthermore, 4-24 hr
trapped-cell incubations verify the biocompatibility of each of our fabricated designs, provided that a Cr-free substrate
is used.
Keywords: Single-cell trap, Hydrodynamic cell trap, Microwell, Immunobiosensor, Therapeutic antibody
1. Introduction
There is a growing interest in the therapeutic use of human
and humanized monoclonal (M) antibodies (Abs) that bind to
antigens (Ags) related to human diseases. MAb development
typically begins with the labour-intensive isolation and
screening of thousands of antibody-secreting cells (ASCs),
often requiring 4-6 weeks to identify only 1-10 cell lines
producing the desired antibodies. There are currently no
automated large-scale methods for the identification, isolation
and cloning of such ASCs. We are developing a novel
immunobiosensing device affording rapid and simultaneous
* Corresponding author: Sean F. Romanuik
Tel: +1-778-7826966; Fax: +1-778-7824951
E-mail: [email protected]
direct assessment of the Ab production, dynamics and
characteristics of each of thousands of living ASCs. Each ASC
shall be microfluidically trapped near a designated
immunobiosensor, to detect the binding of the ASC’s secreted
Abs to an immobilized target Ag. This paper expands upon
previous conference papers [1,2] that presented our single-cell
trap array designs, utilizing both hydrodynamic concave
structures and inset microwells. Our hydrodynamic designs are
first evaluated using COMSOL® [3] simulations. Our
hydrodynamic and microwell trap arrays are then fabricated
using SU-8 photoresist (PR) [4] and poly(dimethyl siloxane)
(PDMS) [5]. Our fabricated traps are tested using
fluid-suspended polystyrene microspheres (PSS) [6] and 17/9
mouse B cell hybridoma cells. Our immunobiosensing system
should shorten the time required to identify the ASCs secreting
J. Med. Biol. Eng., Vol. 31 No. 2 2011
122
the Abs of interest and provide a platform affording the
isolation and cloning of Ab-genes from the individual ASCs.
2. Motivation
In response to pathogenic infection or immunization, a
subset of the human body’s lymphocytes, B cells, differentiate
into ASCs that produce and secrete Abs. Abs bind to a protein
or a site on the invading pathogen, referred to as an Ag,
neutralizing and/or flagging the pathogen for destruction. Over
time, the in vivo secretion of Abs in the absence of persistent
Ag develops an individual’s immunological memory,
providing protective immunity against pathogens bearing this
Ag. Immunological memory also serves as a biological
indicator of the individual’s past pathogenic exposure [7,8].
There is growing interest in the therapeutic use of human
and humanized MAbs that bind to human disease-related Ags.
Such MAbs have shown promise during the treatment of
cancer, autoimmune diseases and infectious diseases [9-12].
The production of therapeutic MAbs commonly begins with
the isolation and screening of a large ASC population isolated
from humans or transgenic mice. Hybridoma cell lines are
usually produced via the fusion of human or murine B cells
with myeloma cells [13,14]. Supernatants from these cultured
cell lines are then collected and tested for the presence of the
desired Ab(s). Using cloned expressed Ab-encoding genes,
cultured cells are then transformed into clonal ASC lines that
produce the desired MAb(s) in large quantities [12,15]. As
only a fraction of the B cells used to create the hybridoma cell
lines produce the desired Ab(s), thousands of ASCs must be
screened in a labour-intensive limiting step typically requiring
4-6 weeks to yield only 1-10 cell lines of interest.
Other groups have developed devices to isolate and
identify individual ASCs, secreting the desired Ab(s), within a
population of thousands [16,17]. However, these systems
neither detect this Ab-Ag binding in real time nor quantify its
affinity. We are developing a device ultimately intended to
monitor the Ab production by individually trapped ASCs at
this scale. This device shall measure, and quantify the affinity
of, the binding of secreted Abs to an immobilized target Ag in
real time. We envision a two-component system, consisting of:
an array of immunobiosensors, coated with immobilized target
Ag; and a polymeric microfluidic system that traps individual
ASCs near designated immunobiosensors [18,19].
Each immunobiosensor consists of an array of nanoholes
milled, via a focused Ga+ beam, through a gold film adhered to
a glass substrate [18,19]. Such metal-dielectric interfaces can
sustain coherent collective electronic oscillations called
surface plasmons (SPs) [20]. Optical excitation of SPs
generates quasi-particles called SP polaritons (SPPs). Many of
these SPPs decay into photons, resulting in an optical
transmission through the array of subwavelength nanoholes
exceeding classical aperture theory, a phenomenon termed
extraordinary optical transmission (EOT) [21]. EOT spectra
peak at resonant wavelengths, λSPR, dependent upon the
permittivities of the metallic and dielectric layers [22]. This
dependence has been widely exploited to monitor various
surface binding events [20,23]. The binding of Abs to Ag
immobilized onto the milled gold surface alters the
permittivity of the dielectric media contacting a nanohole array,
shifting λSPR by ∆λSPR. The affinity of this Ab-Ag binding can
be deduced by monitoring the rates of Ab binding and release
from the immobilized Ag via the time response of the
corresponding ∆λSPR shifts.
Before conducting ∆λSPR measurements on the desired
scale, we must first develop a system that individually captures
large ASC populations within arrays of single-cell traps.
Single-cell manipulation has been a major focus in
microfluidics research [24]. Di Carlo et al. [25] report u-shaped
concave structures facing an oncoming fluid flow,
hydrodynamically trapping suspended cells via perfusion.
Ogunniyi et al. [17] and Tokimitsu et al. [16] demonstrated
trapping fluid-suspended ASCs, settling under gravity, into
microwells inset into a planar surface. This paper presents our
initial work developing similar single-cell trap arrays.
3. Design and simulation of single-cell trap arrays
3.1 Design of hydrodynamic cell trap arrays
Figure 1 presents our first hydrodynamic cell trap design.
Fluid flow carries suspended cells into the concave openings
of heart-, c-, or v-shaped structures. The 10-µm-wide channel
bisecting each structure is too narrow to afford further cellular
passage, hydrodynamically trapping the captured cell against
the fluid flow via perfusion.
Figure 1. Fluid flow carries a cell into the concave opening of a heart-,
c-, or v-shaped cell trap bisected by a narrow channel,
hydrodynamically trapping the said cell via perfusion.
Figure 2 depicts our second hydrodynamic cell trap
design, which adds two 50-µm-by-50-µm chambers, referred
to as nanohole array shelters, connected to each bisecting
channel via 10-µm-wide channels. Each nanohole array shall
be positioned within a designated shelter, to be exposed to Abs
secreted by the nearby trapped ASC and partially shielded
from the Abs secreted by all other ASCs.
Figures 3-5 portray hydrodynamic cell trap designs with
concave cell traps and nanohole array shelters inset into curved
microfluidic channel walls. Centrifugal force Fc pushes cells
denser than the fluid out to the walls, where the fluid flow then
carries them into the concave cell traps.
Microfluidic Trapping of Antibody-secreting Cells
123
Figure 2. Hydrodynamic cell traps with two 50-µm-by-50-µm nanohole
array shelters connected via additional 10-µm-wide channels.
Figure 3. Hydrodynamic cell traps and nanohole array shelters inset into
a serpentine channel’s bends.
Figure 4. Hydrodynamic cell traps and nanohole array shelters inset
between a ramped channel’s bends.
Figure 5. Hydrodynamic cell traps and nanohole array shelters inset into
a spiraled channel.
Figure 3 presents concave cell traps and nanohole array
shelters inset into the walls of serpentine bends. This design is
inspired by the serpentine channels commonly utilized as
microfluidic mixers [26], capitalizing on the back and forth
motion of the normally laminar fluid flow as induced by Fc.
Notably, the wall to which Fc pushes a given cell changes after
a bend. Regardless, the commonness of the serpentine channel
lends itself as a logical starting point in the development of
curved channel designs.
Figure 4 depicts concave cell traps and nanohole array
shelters inset into ramps. As with the serpentine channel, the
wall to which Fc pushes cells changes following a bend. The
placement of the cell traps between the bends, rather than on
the bends themselves, makes this design a logical perturbation
of the serpentine channel.
Figure 5 portrays concave cell traps and nanohole array
shelters inset into a spiral. Unlike the designs of Figs. 3 and 4,
Fc always pushes cells towards the same wall. The spiraled
design is thus expected to trap cells more efficiently than the
serpentine and ramp designs.
Fluid shall be pumped through these designs during the
cell trapping stage only. After a sufficient number of cells have
been trapped, this fluid flow shall cease. As such, the dispersal
of the trapped ASCs’ supernatant shall be entirely diffusive.
Moreover, the distance separating the nanohole arrays is such
that any cross-talk induced by the supernatant of remote ASCs
is expected to be negligible compared to the signal induced by
the supernatant of the nearby trapped ASC.
3.2 Simulation of hydrodynamic cell trap arrays
The designs of Section 3.1 were modeled using
COMSOL® [3] Multiphysics 2D Incompressible Navier-Stokes
Module [27], to compute the respective fluid velocities ννννs by
solving the incompressible Navier-Stokes equation,
ρ (∂ννννs / ∂t) - ∇•{-P � + µ [∇ννννs + (∇ννννs)T]} + ρ ννννs •∇ννννs =Fv (1)
where ρ ≈ 1000 kg m-3 is fluid density, P is fluid pressure,
µ ≈ 0.001 kg s-1 m-1 is dynamic viscosity, Fv are the volumetric
body forces acting on the fluid and � is the identity matrix [27].
Simple 2D models erroneously estimate ννννs in channels
with a depth d much less than their length L, as they exclude
the effect of the un-modeled boundaries upon the flow [27].
The shallow channel approximation compensates via an
additional Fv term, Fv = -12 µ ννννs d-2. Our simulations use a
d = 100 µm shallow channel approximation. No additional Fv
terms beyond the shallow channel approximation were used.
Eq. (1) is constrained by: (i) the mass flow continuity
equation, ∇•ννννs = 0 [27]; (ii) no-slip channel wall boundary
conditions (BCs), ννννs = 0; and (iii) normal stress BCs along the
fluid ports’ edges,
{-P � + µ [ ∇ννννs + (∇ννννs)T ] } n = -F0 n (2)
where n is the outward unit vector normal to the edges and F0
is the stress vector magnitude along n [27]. In our simulations,
Eq. (2) implicitly constrains P such that P ≈ F0 [27]. F0 was
specified as: (i) zero along the outlets; and (ii) non-zero and
constant along the inlets.
J. Med. Biol. Eng., Vol. 31 No. 2 2011
124
COMSOL® solved Eq. (1) using the Generalized Minimal
Residual Method (GMRES) solver, an incomplete LU
preconditioner, 0.0001 drop tolerance and automatic matrix
symmetry. The solver was stepped in time from t = 0-30 s in
0.1 s steps, with 0.01 and 0.001 relative and absolute
tolerances, respectively. Sufficient mesh density was assured
in each case.
To conserve memory, the designs of Section 3.1 were not
modeled in their entirety. For example, neither the nanohole
array shelters nor their channels were included within the
models. However, since ννννs is expected to be negligible in these
regions, the errors in the computed ννννs due to their absence are
also expected to be insignificant.
To verify the accuracy of the computed ννννs, we compared
the mean |ννννs| within the main 100-µm-wide channels to their
analytical values, |ννννa|, as predicted using well-known fluid
resistance theory [28]. To obtain the |ννννa| values, we first
compute each channel’s effective hydraulic diameter Deff,
Deff = 256 A / ( k P ) (3)
where A is the channel’s cross-sectional area, P is the
channel’s wetted perimeter and k ≈ 56.91 is a geometric factor
corresponding to the channel’s square cross-section. For our
channels, Deff ≈ 112 µm. We then compute the fluidic
resistance R of our simulated channels as
R = 128 µ L / ( π Deff4 ) (4)
We then compute the mean |ννννa| within the simulated
100 µm wide channels as
|ννννa| = ∆P / ( A R ) (5)
Table 1 presents the ∆P normal stress BCs used to
initialize each simulation (inlet P ≈ F0 relative to outlet
P ≈ F0 = 0), each channel’s L and R and the mean |ννννs| and |ννννa|
within the 100-µm-wide channels at t = 30 s. Table 1 verifies
the accuracy of the computed ννννs within each simulation.
Table 1. Predicted and computed mean |ννννs| and |ννννa| within the
100-µm-wide channels of each simulation at t = 30 s.
Design ∆P [Pa]
L
[mm]
R
[kg s-1 m-4] |ννννa|
[mm s-1] |ννννs|
[mm s-1]
♥-trap 20 9 2.29 × 1012 0.9 1.0
C-trap 20 9 2.29 × 1012 0.9 0.9
V-trap 20 9 2.29 × 1012 0.9 1.0
Traps with shelters
20 9 2.29 × 1012 0.9 0.9
Serpentine 15 10 2.54 × 1012 0.6 0.7
Ramped 20 11 2.80 × 1012 0.7 0.8
Spiralled 20 9.5 2.42 × 1012 0.8 0.9
The cellular trajectories within these ννννs profiles were
estimated via ννννs streamlines. The accuracy of these estimations
was later confirmed via particle tracing simulations.
Table 2 presents, for each entry in Table 1, the total
number of: cell traps, streamlines and cell traps bisected by a
streamline. The bisecting of a cell trap by a streamline
suggests that cells would likely be trapped within that
structure.
Table 2. Number of cell traps bisected by a ννννs streamline, for each
simulation, at t = 30 s.
Design ∆P [Pa]
No. ννννs streamlines
No. cups No. cups
bisected
♥-traps 20 20 12 5
C-traps 20 20 9 5
V-traps 20 20 10 7
Traps with shelters 20 30 6 0
Serpentine 15 12 12 12
Ramped 20 8 16 3
Spiralled 20 20 28 14
Table 2 suggests that, for a given ∆P, the designs of
Figs. 1, 3 and 5 should trap cells more efficiently than those of
Figs. 2 and 4. Moreover, |ννννs| is low within each simulated cell
trap, implying that the trapped cells would experience minimal
fluid drag and supernatant dispersal in the presence of the fluid
flow.
Figure 6 presents |ννννs| within the simulated spiral. The top
inset shows a streamline bisecting a cell trap, whilst the bottom
inset portrays a cell trap that is not bisected by a streamline.
|ννννs| as computed within the other designs of Section 3.1 are
presented elsewhere [2].
Figure 6. The |ννννs| field (color) and ννννs streamlines (white) within the
design of Figure 5 (at t = 30 s), simulated using COMSOL®
Multiphysics with ∆P = 20 Pa and 20 streamlines.
3.3 Design of microwell cell trap arrays
We have developed 7 × 7 arrays of microwells
(30-200 µm diameters, 60-80 µm depths and 3.77 mm
periodicity) inset into polymer films (400-700 µm thick).
Following the trapping of cells into these microwells and the
subsequent removal of untrapped cells, an immunobiosensing
nanohole array is to be aligned atop each microwell. The
distance separating the microwells is such that any cross-talk
induced by the supernatant of remote ASCs is expected to be
negligible compared to the signal induced by the supernatant
of the nearby trapped ASC.
Microfluidic Trapping of Antibody-secreting Cells
125
4. Polymeric fabrication of single-cell trap arrays
4.1 Fabrication of hydrodynamic cell trap arrays
Our hydrodynamic cell traps were fabricated on
RCA-cleaned, soda-lime glass slides (1” × 1.5” × 1 mm,
1” × 3” × 1 mm and 3” × 3” × 1 mm) with and without
sputtered Ti or Cr adhesion layers (5 nm thick) or Pyrex wafers
(4” diameter and 500 µm thick). SU-8 2035 PR [4] films
(30-120 µm thick) were spun onto these substrates and
soft-baked on a 65°C hot-plate. Each SU-8 film was then
photolithographically patterned using a Mylar contact mask
featuring all of the designs of Figs. 1-5. The SU-8 films were
then post-exposure baked on a 95°C hot-plate before being
developed using MicroChem’s SU-8 developer. Utilized spin
speeds and exposure and baking times were set by the desired
film thicknesses as based upon the SU-8 2025-2075 datasheet
[4], as subsequently optimized for our equipment.
Some SU-8 films were instead patterned with the said
mask’s negative, creating soft-lithographic molds to fabricate
the designs of Figs. 1-5 using Dow Corning’s Sylgard®
184 PDMS [5] (as per [29]). In addition to the aforementioned
substrates, RCA-cleaned Si wafers (4” diameter and 525 µm
thick) were also used during the fabrication of these molds.
10-15 µm wide SU-8 structures suffered from poor
adhesion (Fig. 7(b)), whereas similar PDMS structures did not
suffer from this poor adhesion. However, PDMS shrinkage
and/or poor SU-8 mold definition resulted in widened channels
that failed to prevent cellular passage (Fig. 8(b)). We were thus
unable to fabricate the hydrodynamic cell trap arrays presented
in Fig. 1.
Figure 7. (a) Hydrodynamic cell traps and nanohole array shelters inset
into a SU-8 based spiral. (b) Partial cell trap delamination,
due to poor SU-8 adhesion.
4.2 Fabrication of microwell cell trap arrays
Our 7 × 7 arrays of microwells (30-200 µm diameters,
60-80 µm depths and 3.77 mm periodicities) were fabricated in
SU-8 [4] and PDMS [5] (400-700 µm thick), as per
Section 4.1.
Figure 8. (a) PSS trapped in a cell trap inset into a PDMS-based spiral.
(b) 17/9 hybridoma cells densely populated along a PDMS
serpentine bend. Cells were able to enter the nanohole array
shelters.
5. Experimental testing of fabricated single-cell trap
arrays: results and discussion
5.1 Testing of fabricated hydrodynamic cell trap arrays
Our fabricated hydrodynamic cell trap arrays were
sonicated in phosphate-buffered saline (PBS, pH 7.4) and then
tested using: PSS (20 µm diameter) [6], suspended in
deionized water (DI H2O); and 17/9 mouse B cell hybridoma
cells (10-20 µm diameter) [7], re-suspended in cell culture
media (Dulbecco’s modified Eagle’s medium; DMEM).
Concentrations and flow rates on the order of 105/mL and tens
of µL/min, respectively, were used throughout these tests.
Optical microscopy showed that most cells flowed around
the SU-8 traps, with few becoming trapped. This is likely due
to the reduced flow through these cell traps as a consequence
of poor SU-8 adhesion.
Optical microscopy also demonstrated that the serpentine
and spiraled designs trapped cells most efficiently, as predicted
in Section 3.2. Moreover, cell trapping occurred along the
complete length of the serpentine and spiraled channels.
Figure 8 presents: (a) a PSS trapped in a cell trap inset
into a PDMS spiral; and (b) cells densely populated along a
PDMS serpentine bend, alongside cells that passed through
widened shelter channels. This cellular buildup suggests an
affinity between the cells and the PDMS, which may be
reduced by treating the PDMS with O2 plasma or bovine serum
albumin (BSA). Reducing the number of traps containing
multiple cells could be achieved via reducing the concentration
of the suspended cells, at the cost of a greater number of traps
containing no cells. To prevent cells from entering the
nanohole array shelters, the connecting channel width defined
within the photolithographic masks could be reduced to
compensate for the widening observed during fabrication, so
as to achieve the desired channel width that is too narrow to
afford cellular passage.
The removal of untrapped cells beyond the traps is
difficult using our current hydrodynamic cell trap designs.
Surface treatments and/or pressure bursting methods may
afford their removal. In addition, we intend to explore various
hydrodynamic flow steering and/or cell sorting methods for the
removal of specific trapped ASCs.
J. Med. Biol. Eng., Vol. 31 No. 2 2011
126
Optical microscopy confirms the viability of trapped cells
following a 4 hr incubation at 37°C in a 5% CO2 environment.
Cells in traps featuring Cr adhesion layers did not survive, but
remained viable in all other traps. Fortunately, we have also
shown that SU-8 adheres more strongly to Ti than Cr [30].
5.2 Testing of fabricated microwell cell trap arrays
The fabricated microwell arrays were tested with
17/9 mouse B cell hybridoma cells (10-20 µm diameter) [7]
re-suspended in DMEM, using a procedure adapted from
Ogunniyi et al. [17]. A PDMS film (670 µm thick) with a
7 × 7 array of inset microwells (200 µm diameter and
70-80 µm deep) was incubated in PBS with fetal bovine serum
(FBS, 25% v/v) for 24 hr at 4°C, to block nonspecific binding
sites, and then sonicated in PBS. Figure 9 presents optical
microscopy images of one microwell prior to-, and 10 min
after-, the deposition of 17/9 hybridoma cells (100 µL,
4x105 cells/mL). During this period, each microwell filled with
5-20 cells. Peristaltic pumping then removed untrapped cells
with minimal trapped cell displacement. Cells remained viable
in the microwells during 24 hrs of incubation at 37°C in a 5%
CO2 environment, as assessed via optical microscopy.
(a) After PBS sonication (b) After 10 min of settling
(c) After peristaltic pumping
(d) After 24 hr incubation
Figure 9. A microwell (200 µm diameter and 70-80 µm deep) inset
into PDMS (670 µm thick): (a) after sonication in PBS; (b)
10 min after depositing DMEM-suspended 17/9 hybridoma
cells (100 µL, 4 × 105 cells/mL); (c) after using a peristaltic
pump to remove untrapped cells; and (d) after 24 hrs of
incubation.
In contrast to our success trapping cells into PDMS-based
microwells, we had difficulty trapping cells into SU-8 based
microwells, likely due to SU-8’s surface charge or
hydrophobicity.
Although we are encouraged by our preliminary
microwell tests, further refinements are necessary to yield
arrays capable of individually trapping large numbers of ASCs
on a single slide. These refinements most likely include
reducing the size of the microwell traps and/or reducing the
concentration of the deposited cellular suspension. However,
even this experimentally observed trapping density is a
significant achievement as it affords examining the Ab
production of individual 5-20 cell subpopulations, narrowing
identification of the ASCs of interest to their associated
subpopulations. The subsequent removal of trapped ASCs
shall most likely be achieved via a micropipetting procedure.
6. Conclusions
We have designed various single-cell trap arrays for
individually capturing large ASC populations. Hydrodynamic
cell trap designs, fabricated using SU-8 [4] and PDMS [5], have
been verified via COMSOL® [3] simulations and experimental
testing using fluid-suspended PSS [6] and 17/9 hybridoma cells.
Although we find that PDMS adheres more strongly to our
substrates than SU-8, we also find that channels fabricated in
PDMS are wider than expected and thus fail to limit cellular
passage. The simulations and tests demonstrate that our
hydrodynamic designs featuring traps inset into serpentine
bends and spirals trap more efficiently than our other
hydrodynamic designs. Our PDMS based microwell traps were
also tested using fluid-suspended 17/9 hybridoma cells,
verifying their functionality. Furthermore, 4-24 hr trapped cell
incubations verify the biocompatibility of each of our fabricated
designs, provided that a Cr-free substrate is used.
Although encouraged by our preliminary results, our cell
trap designs and/or experimental methods must be further
refined to yield single-cell trap arrays capable of trapping large
ASC populations on a single slide. It shall also be necessary to
remove untrapped cells, to isolate each immunobiosensor from
the Abs secreted by ASCs other than the nearby trapped ASC.
In the case of microwell traps, untrapped cells have been
removed via peristaltic pumping, with minimal trapped cell
displacement. It shall also be necessary to remove specific
trapped ASCs.
We consider the results reported in this paper to be good
progress towards a polymeric microfluidic system capable of
individually trapping thousands of ASCs, each in the vicinity of
a designated nanohole array based immunobiosensor. The
successful development of our immunobiosensing device
should streamline the process of isolating and identifying ASCs
secreting desired Ab(s), which is a limiting step in the current
methods of therapeutic Ab-based drug development.
Acknowledgments
We thank Jody D. Berry (Cangene Inc.), Jasbir N. Patel
(Simon Fraser University; SFU) and Ajit Khosla (SFU) for
their assistance. We also acknowledge the finance and
resources provided by the Natural Sciences and Engineering
Research Council of Canada (NSERC), the Canada Foundation
for Innovation (CFI), the British Columbia Knowledge
Development Fund (BCKDF), CMC Microsystems, Cangene
Inc. and the Canada Research Chairs (CRC).
References
[1] S. F. Romanuik, S. M. Grist, M. Haq, B. L. Gray, N. Gulzar and
Microfluidic Trapping of Antibody-secreting Cells
127
J. K. Scott, “The microfluidic trapping of antibody-secreting cells,” Proc. CMBEC33, 1: 1-4, 2010.
[2] S. F. Romanuik, S. M. Grist, M. Haq, B. L. Gray, N. Gulzar and
J. K. Scott, “The microfluidic trapping of antibody-secreting cells,” Proc. FEDSM-ICNMM, 1: 1-10, 2010.
[3] COMSOL®, Inc.: COMSOL® Multiphysics modeling and simulation, 2010, available: http://www.comsol.com
[4] MicroChem Corp.: SU-8 2000 permanent epoxy negative
photoresist – processing guidelines for: SU-8 2025, SU-8 2035, SU-8 2050 and SU-8 2075, 2010, available:
http://www.microchem.com/products/pdf/SU-82000DataSheet2025thru2075Ver4.pdf
[5] Dow Corning Corp.: Sylgard® 184 silicone elastomer kit, 2010,
available: http://www.dowcorning.com//applications/search/ default.aspx?R=131EN
[6] Polysciences, Inc.: Polybead® Microspheres, 2010, available: http://www.polysciences.com/SiteData/docs/TDS%20788/fa3c3
00bf743114f6efc0b6b377e6ec4/TDS%20788.pdf
[7] R. Ahmed and D. Gray, “Immunological memory and protective immunity: understanding their relation,” Science, 272: 54-60,
1996. [8] M. K. Sifka and R. Ahmed, “Long-lived plasma cells: a
mechanism for maintaining persistent antibody production,”
Curr. Opin. Immunol., 10: 252-258, 1998. [9] C. Piggee, “Therapeutic antibodies coming through the
pipeline,” Anal. Chem., 80: 2305-2310, 2008. [10] S. Lawrence, “Pipelines turn to biotech,” Nat. Biotechnol., 25:
1342, 2007.
[11] M. Baker, “Upping the ante on antibodies,” Nat. Biotechnol., 23: 1065-1072, 2005.
[12] S. K. Dessain, S. P. Adekar and J. D. Berry, “Exploring the native human antibody repertoire to create antiviral
therapeutics,” in: S. K. Dessain (Ed.), Human Antibody
Therapeutics for Viral Disease: Current Topics in Microbiology and Immunology, Berlin: Springer-Verlag, 155-183, 2008.
[13] S. K. Dessain, S. P. Adekar, J. B. Stevens, K. A. Carpenter, L. M. Skorski, B. L. Barnoski, R. A. Goldsby and R. A. Weinberg,
“High efficiency creation of human monoclonal
antibody-producing hybridomas,” J. Immunol. Meth., 291: 109-122, 2004.
[14] A. Lanzaecchia, D. Corti and F. Sallusto, “Human monoclonal antibodies by immortalization of memory B cells,” Curr. Opin.
Biotechnol., 18: 523-528, 2007.
[15] J. S. Babcook, K. B. Leslie, O. A. Olsen, R. A. Salmon and J. W. Schrader, “A novel strategy for generating monoclonal
antibodies from single, isolated lymphocytes producing antibodies of defined specificities,” Proc. Natl. Acad. Sci. USA,
93: 7843-7848, 1996.
[16] Y. Tokimitsu, H. Kishi, S. Kondo, R. Honda, K. Tajiri, K. Motoki, T. Ozawa, S. Kadowaki, T. Obata, S. Fujiki, C. Tateno,
H. Takaishi, K. Chayama, K. Yoshizato, E. Tamiya, T. Sugiyama
and A. Muraguchi, “Single lymphocyte analysis with a microwell array chip,” Cytometry A, 71A: 1003-1010, 2007.
[17] A. O. Ogunniyi, C. M. Story, E. Papa, E. Guillen and J. C. Love,
“Screening individual hybridomas by microengraving to discover monoclonal antibodies,” Nat. Protoc., 4: 767-782,
2009. [18] S. F. Romanuik, S. M. Grist, B. L. Gray, N. Gulzar, J. K. Scott,
D. Hohertz, K. L. Kavanagh, R. Nirwan, C. Hui, A. G. Brolo and
R. Gordon, “The detection of antibodies secreted by microfluidically trapped biological cells via extraordinary
optical detection-based nanoscale immunobiosensing arrays,” Proc. µTAS, 1: 289-291, 2010.
[19] S. F. Romanuik, S. M. Grist, B. L. Gray, D. Hohertz, K. L.
Kavanagh, N. Gulzar, J. K. Scott, R. Nirwan, C. Hui, A. G. Brolo and R. Gordon, “Sensing of antibodies secreted by
microfluidically trapped cells via extraordinary optical transmission through nanohole arrays,” Proc. IEEE Sensors, 1:
2105-2108, 2010.
[20] J. Homola, “Surface plasmon resonance sensors for detection of chemical and biological species,” Chem. Rev., 108: 462-493,
2008. [21] T. W. Ebbesen, H. L. Lezec, H. F. Ghaemi, T. Thio and P. A.
Wolff, “Extraordinary optical transmission through
sub-wavelength hole arrays,” Nature, 391: 667-669, 1998. [22] A. Krishnan, T. Thio, T. J. Kim, H. J. Lezec, T. W. Ebbesen, P. A.
Wolff, J. Pendry, L. Martin-Moreno and F. J. Garcia-Vidal, “Evanescently coupled resonance in surface plasmon enhanced
transmission,” Opt. Commun., 200: 1-7, 2001.
[23] M. E. Stewart, C. R. Anderton, L. B. Thompson, J. Maria, S. K. Gray, J. A. Rogers and R. G. Nuzzo, “Nanostructured plasmonic
sensors,” Chem. Rev., 108: 494-521, 2008. [24] H. Andersson and A. van den Berg, “Microfluidic devices for
cellomics: a review,” Sens. Actuators B Chem., 92: 315-325,
2003. [25] D. D. Carlo, L. Y. Wu and L. P. Lee, “Dynamic single cell
culture array,” Lab Chip, 6: 1445-1449, 2006. [26] H. Song, J. D. Tice and R. F. Ismagilov, “A microfluidic system
for controlling reaction networks in time,” Angew. Chem. Int. Ed.
Engl., 42: 767-772, 2003. [27] COMSOL®, Inc. (Ed.), MEMS Module User’s Guide (Version
3.4), Los Angles: COMSOL®, Inc., 2007. [28] F. M. White (Ed.), Fluid Mechanics (7th Ed.), Whitby, Canada:
McGraw-Hill, 2010.
[29] B. D. Gates, Q. Xu, M. Stewart, D. Ryan, C. G. Willson and G. M. Whitesides, “New approaches to nanofabrication: molding,
printing, and other techniques,” Chem. Rev., 105: 1171-1196, 2005.
[30] S. Grist, J. N. Patel, M. Haq, B. L. Gray and B. Kaminska,
“Effect of surface treatments/coatings and soft bake profile on surface uniformity and adhesion of SU-8 on a glass substrate,”
Proc. SPIE, 7593: 1-10, 2010.
J. Med. Biol. Eng., Vol. 31 No. 2 2011
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