Click here to load reader
Upload
jin-ming
View
214
Download
0
Embed Size (px)
Citation preview
Targeted isolation and analysis of single tumor cells with aptamer-encodedmicrowell array on microfluidic device{
Qiushui Chen, Jing Wu, Yandong Zhang, Zhen Lin and Jin-Ming Lin*
Received 27th July 2012, Accepted 24th September 2012
DOI: 10.1039/c2lc40858a
Microfluidic-based single cells analysis has been of great interest in recent years, promising disease
diagnosis and personalized medicine. Current technologies are challenging in bioselectively isolating
specific single cells from complex matrices. Herein, a novel microfluidic platform integrated with cell-
recognizable aptamer-encoded microwells was specifically developed to isolate single tumor cells with
satisfied single-cell occupancy and unique bioselectivity. In this work, the designed microwell-
structures enable us to encourage strong 3D local topographic interactions of the target cell surface
with biomolecules and regulate the single-cell resolution. Under the optimized size of microwells, the
single-cell occupancy was significantly enhanced from 0.5% to 88.2% through the introduction of the
aptamer. Analysis of the target cells was directly performed in short time periods (,5.0 min) with
small volumes (4.5 mL). Importantly, such an aptamer-enabled microfluidic device shows an excellent
selectivity for target single cells isolation compared with three control cells. Subsequently, targeted
isolation and analysis of single tumor cells were demonstrated by using artificial complex cell samples
at simulated conditions, and various cellular carboxylesterases were studied by time-course
measurements of cellular fluorescence kinetics at individual-cell level. Thus, our technique will open
up a new opportunity in single-cell level-based disease diagnosis and personalize medicine screening.
Introduction
New diagnostic technologies at single-cell level have now
changed the understanding and clinical practice of oncology.1,2
The studies of cellular heterogeneity in proteomics and gene
expression will enable early diagnosis and personalized medi-
cine.3 Currently, single-cell analysis is emerging as a powerful
tool to reveal the cellular heterogeneity in cell populations at the
individual-cell level for understanding various single cells
signaling.4–6 Nowadays, flow cytometry is a traditional approach
to examine the cellular components of single cells with high-
throughput using fluorescence labeling.7,8 Alternatively, capil-
lary electrophoresis (CE) combined with laser-induced fluores-
cence (LIF),9 electrochemistry10 and chemiluminescence11 are
also widely utilized for single cells separation and analysis.
Despite such achievements, however, those analytical technolo-
gies make it difficult to provide information on both temporal
and spatial cellular responses.
Over the last decade, microfluidic technologies increasingly
play an important role in biological research, promising high-
throughput assays, fast analysis and low reagent require-
ments.12–16 Of particular interest is microfluidic single-cell
analysis that enables single-cell manipulations,17 long-time
culture,18 drug-related treatments19 and high-efficiency screen-
ing20 on temporal and spatial micro-scales. Microfluidic-based
single cells analysis, such as polymerase chain reaction,21,22 drug-
induced apoptosis19 and enzyme kinetics,23,24 shows great
potential for application in medical diagnosis and clinical
treatment. A number of approaches have been explored in the
isolation and operation for single cells, including physical
barriers,18,23,25 fluid mechanics,17,26–28 or gravity mechan-
isms.24,29,30 Although these strategies represent important
advances, much improvement is still needed. For example, the
approaches of micro-fabricated structures, such as microwell-
based docking,26,29,30 microdam-based locating23,31 and micro-
cavity-based trapping,32,33 which rely on the degree of physical
structure capture, are technically challenging in bioselectively
isolating single cells. Besides, the encapsulation of single cells and
reagents in independent aqueous microdroplets provided excel-
lent cellular microenvironments and increased throughputs,20,27
but showed limited capability to deal with complex cell samples
(e.g. cell suspensions and whole blood samples). Thus, targeted
isolation of single cells presents a tremendous interest. Given
these technical challenges, bio-recognizable microfabricated
physical structures will be a powerful strategy and open up
unique opportunities for isolating single specific cells.
It has been well-demonstrated that aptamers, a kind of nucleic
molecule (RNA or DNA), can bind to target tumor cells with
high specificity and affinity.34,35 Herein, we report a novel
Beijing Key Laboratory of Microanalytical Method and Instrumentation,Department of Chemistry, Tsinghua University, Beijing, 100084, China.E-mail: [email protected]; Fax: (+86) 10 62792343{ Electronic Supplementary Information (ESI) available: See DOI:10.1039/c2lc40858a
Lab on a Chip Dynamic Article Links
Cite this: Lab Chip, 2012, 12, 5180–5185
www.rsc.org/loc PAPER
5180 | Lab Chip, 2012, 12, 5180–5185 This journal is � The Royal Society of Chemistry 2012
Dow
nloa
ded
by Q
ueen
s U
nive
rsity
- K
ings
ton
on 0
1/05
/201
3 03
:28:
21.
Publ
ishe
d on
24
Sept
embe
r 20
12 o
n ht
tp://
pubs
.rsc
.org
| do
i:10.
1039
/C2L
C40
858A
View Article Online / Journal Homepage / Table of Contents for this issue
microfluidic platform for the targeted isolation of single tumor
cells with aptamer-coated microwells based on the single-cell-
containable micro-chambers and their bio-specific interactions.
The specifically designed microwell-structures enable us to
encourage strong 3D local topographic interactions of the target
cell surface with biomolecules and regulate the single-cell
resolution (Fig. 1A and C). Such an aptamer-enabled micro-
fluidic device obtained unique bioselectivity and significantly
enhanced single-cell occupancy ranging from 0.5% to 88.2%
(Fig. 1A and B). Subsequently, targeted isolation and analysis of
single tumor cells were demonstrated by using artificial complex
cell samples at simulated conditions, and various cellular
carboxylesterases were temporally and spatially studied by
measuring cellular fluorescence kinetics at an individual-cell
level. Consequently, the development of the bio-selective single
cells isolation microchip platform serves two purposes. First, it
will permit us to separate specific tumor cells from complex
clinical samples, such as cell suspensions and whole blood
samples, allowing direct single-cell level-based disease diagnosis.
Second, it will enable a high-throughput assay of cellular enzyme
kinetics in individual tumor cells, promising personalized
medicine. We believe this aptamer-encoded microwell-based
microchip will represent a novel platform for single-cell analysis
and offer new opportunities in clinical application.
Experimental
Materials and chemicals
Dulbecco’s modified Eagle’s minimal essential medium (DMEM,
Gibco, Grand Island, NY), RPMI medium 1640 (Gibco, Grand
Island, NY), trypsin EDTA (Gibco, Grand Island, NY), sodium
pyruvate (100 mM) and calcein AM were purchased from
Invitrogen (CA, USA). Chromium layer patterned glass sub-
strate was fabricated by Qingyi Precision Maskmaking Co., Ltd.
(Shenzhen, China). Silicon wafers were purchased from Xilika
Crystal Polishing Material Co., Ltd. (Tianjin, China). Negative
photoresist (SU-8 2050) and developer were purchased from
Microchem Corp. (Newton, MA). Poly-dimethylsiloxane
(PDMS) and the curing agent were obtained from Dow
Corning (Sylgard 184, Midland, MI, USA). Avidin and
Phosphate Buffered Saline (PBS, pH = 7.4) were purchased
from Sigma-Aldrich Company. The aptamer was synthesized by
Sangon Biotech Co., Ltd. TD05: 59-AAC ACC GGG AGG
ATA GTT CGG TGG ATG TTC AGG GTC TCC TCC CGG
TGT TTT TTT TTT-39-Biotin. All other reagents were of
analytical reagent grade and used without further purification.
Cell culture and preparation
All cancer cell lines (Ramos cells, CCRF-CEM cells, MCF-7
cells and HepG2 cells) were obtained from the Cancer Institute &
Hospital, Chinese Academy of Medical Science. Ramos and
CCRF-CEM cells were cultured in RPMI medium 1640
supplemented with 10% FBS and 100 IU mL21 penicillin–
streptomycin. HepG2 and MCF-7 cells were cultured in DMEM
media with 10% FBS and 100 IU mL21 penicillin–streptomycin.
Specially, 0.11 g L21 sodium pyruvate was added to RPMI
medium 1640 for CCRF-CEM cells culture. Both cell lines were
cultured in a 5% CO2-humidified air atmosphere at 37 uC and
maintained by passaging twice weekly. The MCF-7 and HepG2
cells were dissociated from the culture dish with 0.25% Trypsin
EDTA in exponential growth phase. In the experiments, the cells
were centrifugated 5.0 min at 1000 rpm after being rinsed with
PBS buffer, and a cell concentration of 5.0 6 107 cells mL21 was
used for single-cell capture.
Fabrication of the microwell-structured array on a microfluidic
device
The microfluidic chip was fabricated using standard soft
lithography and replica molding techniques (see the details in
the Supporting Information{).36 The fabrication of the micro-
well array on the glass substrate was carried out by using the
chromium layer as its photomask. The glass substrate was then
cut to pieces of 2.5 cm 6 2.5 cm. The chromium image was
designed using AutoCAD software with 18 000 (120 6 150)
Fig. 1 A schematic illustration of the microfluidic platform used for single target cells isolation. (A) The microfluidic device consists of a PDMS layer
with microchannels and a glass substrate with microwells. (B) The three-dimensional topography of the microwell array was characterized by a
scanning electron microscope (SEM). (C) Two steps for glass surface functionalization were conducted by the deposition of avidin and immobilization
of biotin–aptamer.
This journal is � The Royal Society of Chemistry 2012 Lab Chip, 2012, 12, 5180–5185 | 5181
Dow
nloa
ded
by Q
ueen
s U
nive
rsity
- K
ings
ton
on 0
1/05
/201
3 03
:28:
21.
Publ
ishe
d on
24
Sept
embe
r 20
12 o
n ht
tp://
pubs
.rsc
.org
| do
i:10.
1039
/C2L
C40
858A
View Article Online
adjacent spot (total space: 2.1 mm 6 2.4 mm). The microwell
array on the glass substrate was etched by hydrofluoric acid/
ammonium fluoride (HF/NH4F, 5.0 M/5.0 M) solution for about
2.0 min. Four different sizes of microwell structure with
diameter/depth were fabricated at 18 mm/5.0 mm, 20 mm/5.0
mm, 22 mm/5.0 mm and 20 mm/8.0 mm, respectively. The microwell
sizes can be easily controlled by the etching time with the help of
an optical microscope. After washing with deionized water, the
glass substrate was soaked in chromium etchant for 5.0 min to
remove the patterned chromium layer. The prepared microwell
array on glass substrate was then cleaned by piranha solution
(H2SO4:30% H2O2 = 3 : 1, v/v). The microwell structure was
characterized by a scanning electron microscope (SEM). Non-
covalent bonding between the PDMS layer and the glass slide
was conducted using two clamps for recycling the glass slide with
the microwell array (see Fig. S1){.
Aptamer-encoded microwell array
A key experimental detail was to keep the microwell array on
the glass substrate hydrophilic to reduce nonspecific adhesion
of cells. This was achieved by cleaning the microwell array using
piranha solution (H2SO4:30% H2O2 = 3 : 1, v/v) in 100 uC to
form a hydrophilic interface each time. After rinsing with
deionized water three times, the glass slide was dried under
nitrogen gas at room temperature, but not at a high
temperature. Then, the microwell array was covered with a
PDMS layer with two microchannels, and bubbles in the
microchannel were removed by sampling 50 mL PBS buffer
(10 mM, pH = 7.4). Avidin (1.0 mg ml21, 5.0 mL) in PBS buffer
was first incubated in the microwells for 5.0 min and rinsed with
5.0 mL PBS buffer three times. Finally, biotin–aptamer (5.0 mL,
100 mM) in tris-EDTA (TE) buffer was incubated for 5.0 min
and rinsed with 5.0 mL PBS buffer three times. The prepared
microdevice was kept at 4 uC. Tapping mode atomic force
microscopy (AFM) was conducted to characterize the immobi-
lization of avidin and aptamer on the glass substrate (see
Fig. S2){.
Isolation of single cells and optimizing conditions
In the experiments, a cell concentration of 5.0 6 107 cells mL21
was rinsed with PBS buffer. To study the effect of aptamer
concentrations on single cells occupancy, a series of concentra-
tions (0, 25, 50, 75, 100 mM) was prepared to be immobilized on
the microwells. To study the effect of microwell size on
single cells occupancy, single cells isolation was conducted on
four different sizes of microwells. In all of these experiments, 4.5
mL Ramos cells were used as the target cells by a transfer
pipette. To study the selectivity of single cells occupancy,
Ramos cells (lymphoma cancer, target cells), CCRF-CEM cells
(leukemic lymphoblasts, control), MCF-7 cells (breast cancer,
control) and HepG2 cells (liver cancer, control) in PBS buffer
were introduced to microchannels under static conditions. After
1.0 min of cells capture, the microchannel was washed three
times with PBS buffer and observed under a fluorescence
microscope. The captured single cells can be easily counted
by image analysis software (Image-Pro plus 6.0, Media
Cybernetics, USA).
Analysis of single-cell enzyme kinetics
An artificial mixture of cells (Ramos cells and CEM cells, 1 : 1)
was used as complex biological samples. A cell concentration of
5.0 6 107 cells mL21 was rinsed with PBS buffer and then
introduced to the microchannel for selective single cells isolation.
10 mL PBS buffer was used to rinse the microchannel after 1.0
min. The single cells in the microfluidic device were stored in a
humidified 5% CO2 environment at 37 uC. To perform time-
course enzyme kinetics analysis, this microdevice was placed on
the platform of a fluorescence microscope. 4.5 mL of 4.0 mM
calcein AM in PBS solution was introduced into the micro-
channel. The intracellular fluorescence was monitored by a
fluorescence microscope at the wavelength of 488 nm for 10 min.
This fluorescence microscope was equipped with a cooled CCD
camera (DFX 3000) and software of Leica Application Suite,
LAS V2.7. A series of images (1 s exposure) were acquired at 10 s
intervals.
Results and discussion
Design and operation of the aptamer-immobilized microwell-
structured microdevice
The designed microdevice consists of two components: an
overlaid polydimethysiloxane (PDMS) layer with two micro-
fluidic channels and a glass substrate with aptamer patterned
microwell array (Fig. 2A and B and Fig. S1a{). Previous reports
have confirmed that the low height of the microchannels (60 mm
in this case) will encourage cell-substrate contact frequency,
which increases cell capture efficiency.35,37,38 The designed
microchannels were crucial to controlling the cell microenviron-
ment, low reagent consumption and repeatable high-throughput
assay. The microwell-structured substrate was fabricated by
using a lithographic method and chemical etching process. A
diameter of 18–22 mm and depth of approximately 5.0 mm and
8.0 mm were chemically etched onto the chromium-patterned
glass substrate, yielding a feature of density of 3500 wells per
mm2 (Fig. 2C). According to previous methods,34 an avidin
coating (4.5 mL, 1.0 mg ml21) was introduced onto microwell-
structured glass substrates for 5.0 min (Fig. 2D). Prior to the
Fig. 2 A schematic illustration of the microfluidic platform used for
single target cells isolation. (A), (B) The microfluidic device consists of a
PDMS layer with microchannel and a glass substrate with microwells.
(C) The three-dimensional topography of the microwell array was
characterized by a scanning electron microscope (SEM). (D) Two steps
for glass surface functionalization were conducted by the deposition of
avidin and the immobilization of biotin–aptamer.
5182 | Lab Chip, 2012, 12, 5180–5185 This journal is � The Royal Society of Chemistry 2012
Dow
nloa
ded
by Q
ueen
s U
nive
rsity
- K
ings
ton
on 0
1/05
/201
3 03
:28:
21.
Publ
ishe
d on
24
Sept
embe
r 20
12 o
n ht
tp://
pubs
.rsc
.org
| do
i:10.
1039
/C2L
C40
858A
View Article Online
single cells capture experiments, 4.5 mL of biotinylated aptamer
was conducted onto the avidin-coated substrates in each
microchannel. Accordingly, single target cells will be selectively
captured by the aptamer coated microwells from the complex cell
samples, which is attributed to the fitted 3D local topographic
interactions between the cell surface and aptamer on microwells
(Fig. 1A). On the contrary, the microwell array without an
aptamer coating will lose the ability of isolating single cells owing
to a lack of bio-specific interactions with target cells (Fig. 1B).
Typically, the microwell structure is crucial to regulate the single-
cell resolution (Fig. 1C). The whole microfluidic system
integrated with an aptamer-coated microwell array, therefore,
can be designed for selectively isolating single target cells and
high-throughput single cell assays.
Single cells capture with aptamer-encoded microwell-structured
micro-platform
The performance of single-cell analysis in this integrated
microdevice was first demonstrated by isolating leukemia cells
(Ramos cells) that functioned as target cancer cells. An optimal
cell concentration (5 6 107 cells per mL) was determined
according to the resulting single-cell occupancy at static cell-
capture conditions. As shown in Fig. 3A, the aptamer-
immobilized microwell enables high single-cell occupancy
(percentage of microwells containing single cells). As a control,
microwell-structured substrates without any surface modifica-
tion and only modified with avidin were also examined in
parallel. The single cells capture yield was only 1.4% and 0.5% on
microwell-structured substrates and avidin-modified substrates,
as opposed to 88.2% on aptamer-immobilized microwell-
structured substrates. This result suggests that aptamer-enabled
microwells are possibly responsible for the high single cells
occupancy (Fig. 3B). This is reasonable because the 3D-
structured microwells exhibited obvious morphology differences
in the target cells capture: i) the microwells substrates with 3D-
structure is more matched with the spherical cells and thereby
creates more recognition sites between the surface antigen of the
cell membrane and the aptamer immobilized on the microwells,
which yields strong 3D local topographic interactions for single
cells capture;37 ii) the structure of microwells is playing an
important role in regulating the single-cell resolution.
Consequently, these evidences indicated that the integrated
aptamer-encoded microwell-structured substrate in the micro-
device was a novel single-cell-capture platform for biological
application.
Effect of aptamer concentration and microwell-size on single cells
occupancy
Since the aptamer shows excellent capability in target cells
capture, the concentration of aptamer was reported to directly
relate to its capture efficiency.35 To investigate this effect,
different concentrations of aptamer were immobilized onto the
microwell-structured glass substrate. As shown in Fig. 4A, the
single cells occupancy was obviously increasing with the
increased concentrations of aptamer, ranging from 0 to 100
mM. In our experiments, the single cells occupancy was as high as
88.2%, compared with the control (no aptamer immobilization)
of 0.5%. Therefore, the results also demonstrated that the
immobilization of aptamer plays an important role in the
performance of single cells capture.
To capture and analyze single cells with high-efficiency, the
optimal geometry of microwells was conducted with the
diameters of 18, 20 and 22 mm at the depth of 5.0 mm and 8.0
mm (Fig. 4B). When the microwells were 18 mm in diameter, most
of the microwells were filled with target cells at single-cell
resolution (occupancy 88.2%). However, the single cells occu-
pancy was decreasing with increased diameter of the microwells
at 20 and 22 mm with the deposition of two cells. When the
microwells were at the diameter of 20 mm, the single cells
occupancy was achieved in different depths at 5.0 mm and 8.0
mm. It shows that the single cell occupancy of 5.0 mm depth will
be a little higher than that of 8.0 mm depth; these results are
reasonable, because the larger volume will lead to a high
probability of double cells per microwell. Thus, the microwells
with 5.0 mm depth and 18 mm diameter were finally selected for
further experiments. All of the single-cell occupancies under
Fig. 3 The performance of single Ramos cells onto the microwell array.
(A) Bright field images of single cells captured onto the aptamer-coated
microwells and the non-modified microwell array as a control. (B)
Quantitative evaluations of single-cell occupancy were performed under
control, avidin-coated microwell array and avidin/biotin–aptamer-coated
microwell array, respectively. Avidin: 1.0 mg ml21, Biotin–aptamer: 100
mM.
Fig. 4 The effect of aptamer concentrations and microwell sizes on
single-cell occupancy. (A) The single Ramos cells occupancy was raised
with increasing aptamer concentrations immobilized in the microwell
array. The concentrations were studied in 0, 25, 50, 75, 100 mM. (B)
Ramos cells occupancy was conducted under different sizes (diameter
and depth) of aptamer-encoded microwells. Concentration of aptamer:
100 mM. Error bars show standard deviations (n = 6).
This journal is � The Royal Society of Chemistry 2012 Lab Chip, 2012, 12, 5180–5185 | 5183
Dow
nloa
ded
by Q
ueen
s U
nive
rsity
- K
ings
ton
on 0
1/05
/201
3 03
:28:
21.
Publ
ishe
d on
24
Sept
embe
r 20
12 o
n ht
tp://
pubs
.rsc
.org
| do
i:10.
1039
/C2L
C40
858A
View Article Online
different sizes of microwells are listed in Table 1. In brief, the
diameter of the microwell was an important factor for high
single-cell occupancy, and the designed microwell array was
responsible for regulating the single-cell resolution.
Selectivity of single cells isolation from multiple-types of cancer
cells
Although a number of approaches have been developed to
isolate single cells for biological studies, they are always lacking
the ability to capture specific target cells for single-cell analysis.
Here, the selectivity of single-cell capture on the aptamer-
immobilized microwell-structured substrates was clearly demon-
strated by the target cells and three kinds of control cells. An
average of 88.2% single-cell occupancy was achieved by using the
Ramos cells as target cells. For comparison, other cancer-cell
lines (i.e., CEM, MCF-7 & HepG2 cancer cell lines, representing
both suspension and adherent cell types, respectively) were
employed as controls. Fig. 5 shows the low single-cell occupancy
of these three cancer-cell lines, that is, the aptamer-encoded
microwell-structured substrates are only capturing specific single
Ramos cells (target cancer-cell line). Our approach significantly
improved selectivity in target single cells capture that is distinct
from traditional physical methods.17,18,20,23–33 Thereby, this
fabricated microfluidic platform shows excellent performance
in selectively isolating single cells that will be potentially applied
in complex biological samples, which is promising for disease
diagnosis and drug assay at the single-cell level.
Enzyme kinetic analysis at single-cell level
Targeted isolation of single cells will enable its application in
complex biological samples and is thus promising for monitoring
drug-related intracellular responses at individual-cell level before
pharmacological treatment. For example, various carboxyles-
terases between individual cells hold essential biochemical
functions of aster and amide hydrolysis that are crucial to
activate antidrugs and inactivate other pharmaceuticals.39 To
establish this concept, artificial complex biological samples were
prepared by spiking lymphoma cells (target tumor cells: Ramos
cells) with an aliquot of CEM cells in media solutions. Our
approach resulted in isolating single Ramos cells with excellent
selectivity, providing the possibility of high-throughput single
cells analysis. Further, calcein AM was used as a substrate for
carboxylesterase that generates intracellular green fluorescence,
and the study of enzyme kinetic activity at individual-cell level
was achieved by time-course fluorescence analysis in further
experiments. As shown in Fig. 6A, the fluorescence intensities of
each single-cell increased as a function of time. The kinetic
curves for each single-cell present the different amounts of
intracellular carboxylesterase, revealing the diversity of condi-
tions or viability in target single cells that are associated with
cancers (Fig. 6B). This phenomenon is reasonable because of the
variations in cellular carboxylesterase expression levels between
individual cells.23,39 Based on this strategy, drug dosages and
combinations of therapies could be patient-defined to treat
individual disease in a clinical setting, thus providing the
possibility of developing personalized medicine.
Table 1 Single-cell occupancies under different sizes of microwells
Diameter (D) /depth (H) D = 18 mm/H = 5 mm D = 20 mm/H = 5 mm D = 22 mm/H = 5 mm D = 20 mm/H = 8 mm
Single-cell per microwell (%) 88.2 62.8 46.4 52.6SD (%) ¡3.4 ¡4.4 ¡7.3 ¡8.7Two cells per microwell (%) 7.5 10.7 21.7 14.1SD (%) ¡1.7 ¡2.5 ¡2.1 ¡2.0
Fig. 5 Investigation of single-cell capture selectivity on aptamer-
encoded microwells using Ramos cells (target cells), HepG2 cells
(control), CEM cells (control) and MCF-7 cells (control). Aptamer
concentration: 100 mM. Cell concentration: 5 6 107 cells mL21.
Fig. 6 Time-course measurements of carboxylesterase dynamic
responses to 10 mM calcein-AM at individual cells by a fluorescence
microscope. (A) The fluorescence images were recorded using a cooled
CCD camera at a 406 objective. (B) Relative fluorescence intensities of
single cells are increased as a function of time.
5184 | Lab Chip, 2012, 12, 5180–5185 This journal is � The Royal Society of Chemistry 2012
Dow
nloa
ded
by Q
ueen
s U
nive
rsity
- K
ings
ton
on 0
1/05
/201
3 03
:28:
21.
Publ
ishe
d on
24
Sept
embe
r 20
12 o
n ht
tp://
pubs
.rsc
.org
| do
i:10.
1039
/C2L
C40
858A
View Article Online
Conclusion
In summary, a novel single-cell capture platform based on an
aptamer-encoded microwell-structured microdevice, described
here, was demonstrated to exhibit excellent selectivity. Our results
indicated that the highly-efficient single-cell occupancy was
obviously dependent on the concentrations of aptamers and the
size of the microwells. The 3D-structured microwell can also
encourage the interactions of the target cell surface with the DNA-
aptamer, resulting in a satisfactory single-cell occupancy
(y88.2%). The performance of single cells isolation with bio-
selectivity is distinct from existing technologies. Finally, the
isolation of single cells from the artificial complex of biological
samples was further applied to enzyme kinetic analysis on an
individual-cell level. We believe that the aptamer-enabled
selectivity of single cells isolation technology will open up
opportunities for the isolation of single tumor cells and for
personalized medicine based on a single-cell level, which is
promising for biological and medical application.
Acknowledgements
This work was supported by the National Natural Science
Foundation of China (Nos. 20935002).
References
1 J. Sun, M. D. Masterman-Smith, N. A. Graham, J. Jiao, J.Mottahedeh, D. R. Laks, M. Ohashi, J. DeJesus, K. Kamei, K. B.Lee, H. Wang, Z. T. F. Yu, Y. T. Lu, S. A. Hou, K. Y. Li, M. Liu, N.G. Zhang, S. T. Wang, B. Angenieux, E. Panosyan, E. R. Samuels, J.Park, D. Williams, V. Konkankit, D. Nathanson, R. M. van Dam,M. E. Phelps, H. Wu, L. M. Liau, P. S. Mischel, J. A. Lazareff, H. I.Kornblum, W. H. Yong, T. G. Graeber and H. R. Tseng, CancerRes., 2010, 70, 6128–6138.
2 N. Papadopoulos, K. W. Kinzler and B. Vogelstein, Nat. Biotechnol.,2006, 24, 985–995.
3 K. K. Jain, Expert Opin. Pharmacother., 2005, 6, 1463–1476.4 S. S. Rubakhin, E. V. Romanova, P. Nemes and J. V. Sweedler, Nat.
Methods, 2011, 8, 20–29.5 D. G. Spiller, C. D. Wood, D. A. Rand and M. R. H. White, Nature,
2010, 465, 736–745.6 Y. Lin, R. Trouillon, G. Safina and A. G. Ewing, Anal. Chem., 2011,
83, 4369–4392.7 P. O. Krutzik, J. M. Crane, M. R. Clutter and G. P. Nolan, Nat.
Chem. Biol., 2008, 4, 132–142.8 S. Helaine, J. A. Thompson, K. G. Watson, M. Liu, C. Boyle and D.
W. Holden, Proc. Natl. Acad. Sci. U. S. A., 2010, 107, 3746–3751.9 W. Xie, A. Xu and E. S. Yeung, Anal. Chem., 2009, 81, 1280–1284.
10 X. Sun, Y. Niu, S. Bi and S. Zhang, J. Chromatogr., B: Anal. Technol.Biomed. Life Sci., 2008, 870, 46–50.
11 S. Zhao, X. Li and Y. -M. Liu, Anal. Chem., 2009, 81, 3873–3878.12 D. Huh, B. D. Matthews, A. Mammoto, M. Montoya-Zavala, H. Y.
Hsin and D. E. Ingber, Science, 2010, 328, 1662–1668.
13 A. Khademhosseini, R. Langer, J. Borenstein and J. P. Vacanti, Proc.Natl. Acad. Sci. U. S. A., 2006, 103, 2480–2487.
14 V. Lecault, M. VanInsberghe, S. Sekulovic, D. J. H. F. Knapp, S.Wohrer, W. Bowden, F. Viel, T. McLaughlin, A. Jarandehei, M.Miller, D. Falconnet, A. K. White, D. G. Kent, M. R. Copley, F.Taghipour, C. J. Eaves, R. K. Humphries, J. M. Piret and C. L.Hansen, Nat. Methods, 2011, 8, 581–593.
15 H. Lee, E. Sun, D. Ham and R. Weissleder, Nat. Med., 2008, 14,869–874.
16 W. Shi, J. Qin, N. Ye and B. Lin, Lab Chip, 2008, 8, 1432–1435.17 G. T. Roman, Y. Chen, P. Viberg, A. H. Culbertson and C. T.
Culbertson, Anal. Bioanal. Chem., 2007, 387, 9–12.18 D. Di Carlo, L. Y. Wu and L. P. Lee, Lab Chip, 2006, 6, 1445–1449.19 D. Wlodkowic, S. Faley, M. Zagnoni, J. P. Wikswo and J. M.
Cooper, Anal. Chem., 2009, 81, 5517–5523.20 E. Brouzes, M. Medkova, N. Savenelli, D. Marran, M. Twardowski,
J. B. Hutchison, J. M. Rothberg, D. R. Link, N. Perrimon and M. L.Samuels, Proc. Natl. Acad. Sci. U. S. A., 2009, 106, 14195–14200.
21 V. Sanchez-Freire, A. D. Ebert, T. Kalisky, S. R. Quake and J. C.Wu, Nat. Protoc., 2012, 7, 829–838.
22 H. Zhang, G. Jenkins, Y. Zou, Z. Zhu and C. J. Yang, Anal. Chem.,2012, 84, 3599–3606.
23 D. Di Carlo, N. Aghdam and L. P. Lee, Anal. Chem., 2006, 78, 4925–4930.24 C. Liu, J. Liu, D. Gao, M. Ding and J. -M. Lin, Anal. Chem., 2010,
82, 9418–9424.25 A. R.Wheeler, W. R. Throndset, R. J. Whelan, A. M. Leach, R. N.
Zare, Y. H. Liao, K. Farrell, I. D. Manger and A. Daridon, Anal.Chem., 2003, 75, 3581–3586.
26 K. Chung, C. A. Rivet, M. L. Kemp and H. Lu, Anal. Chem., 2011,83, 7044–7052.
27 S.-Q. Gu, Y.-X. Zhang, Y. Zhu, W.-B. Du, B. Yao and Q. Fang,Anal. Chem., 2011, 83, 7570–7576.
28 M. C. Park, J. Y. Hur, H. S. Cho, S.-H. Park and K. Y. Suh, LabChip, 2011, 11, 79–86.
29 M. Deutsch, A. Deutsch, O. Shirihai, I. Hurevich, E. Afrimzon, Y.Shafran and N. Zurgil, Lab Chip, 2006, 6, 995–1000.
30 J. R. Rettig and A. Folch, Anal. Chem., 2005, 77, 5628–5634.31 A. M. Skelley, O. Kirak, H. Suh, R. Jaenisch and J. Voldman, Nat.
Methods, 2009, 6, 147–152.32 M. Hosokawa, A. Arakaki, M. Takahashi, T. Mori, H. Takeyama
and T. Matsunaga, Anal. Chem., 2009, 81, 5308–5313.33 M. Hosokawa, T. Hayashi, T. Mori, T. Yoshino, S. Nakasono and T.
Matsunaga, Anal. Chem., 2011, 83, 3648–3654.34 W. Liu, H. Wei, Z. Lin, S. Mao and J.-M. Lin, Biosens. Bioelectron.,
2011, 28, 438–442.35 J. A. Phillips, Y. Xu, Z. Xia, Z. H. Fan and W. Tan, Anal. Chem.,
2009, 81, 1033–1039.36 Q. Chen, J. Wu, Y. D. Zhang and J.-M. Lin, Anal. Chem., 2012, 84,
1695–1701.37 S. Wang, K. Liu, J. Liu, Z. T.-F. Yu, X. Xu, L. Zhao, T. Lee, E. K.
Lee, J. Reiss, Y.-K. Lee, L. W. K. Chung, J. Huang, M. Rettig, D.Seligson, K. N. Duraiswamy, C. K.-F. Shen and H.-R. Tseng, Angew.Chem., Int. Ed., 2011, 50, 3084–3088.
38 S. L. Stott, C. H. Hsu, D. I. Tsukrov, M. Yu, D. T. Miyamoto, B. A.Waltman, S. M. Rothenberg, A. M. Shah, M. E. Smas, G. K. Korir,F. P. Floyd, A. J. Gilman, J. B. Lord, D. Winokur, S. Springer, D.Irimia, S. Nagrath, L. V. Sequist, R. J. Lee, K. J. Isselbacher, S.Maheswaran, D. A. Haber and M. Toner, Proc. Natl. Acad. Sci. U. S.A., 2010, 107, 18392–18397.
39 M. Essodaigui, H. J. Broxterman and A. Garnier-Suillerot,Biochemistry, 1998, 37, 2243–2250.
This journal is � The Royal Society of Chemistry 2012 Lab Chip, 2012, 12, 5180–5185 | 5185
Dow
nloa
ded
by Q
ueen
s U
nive
rsity
- K
ings
ton
on 0
1/05
/201
3 03
:28:
21.
Publ
ishe
d on
24
Sept
embe
r 20
12 o
n ht
tp://
pubs
.rsc
.org
| do
i:10.
1039
/C2L
C40
858A
View Article Online