High-sensitivity online detection for microfluidics via cavity ringdownspectroscopy
Dean James,a Bobby Oag,a Cathy M. Rushworth,a Jason W. L. Lee,a Joanna Davies,b Joao T. Cabralb and
Claire Vallance*a
Received 23rd February 2012, Accepted 2nd April 2012
DOI: 10.1039/c2ra20349a
We report the coupling of cavity ringdown spectroscopy (CRDS) with a microfluidic chip fabricated
using a rapid prototyping method, in order to demonstrate high-sensitivity, non-contact online
detection in microfluidics. Conventional UV-vis absorption techniques are largely ineffective for
microfluidic detection due to the small sample volumes and short path lengths. The multipass
absorption achieved in cavity ringdown spectroscopy increases the effective absorption pathlength by
several orders of magnitude, and hence enhances the detection sensitivity. A cavity ringdown
spectrometer, operating at a single wavelength of 532 nm for the purposes of the proof-of-concept
measurements presented here, has been developed for online detection on a polymer/glass microchip
fabricated by frontal photopolymerisation. High sensitivity absorption measurements on liquid
samples with volumes of tens to hundreds of nanolitres and absorption pathlengths ranging from tens
to hundreds of microns are demonstrated. A series of proof-of-concept experiments show that the
technique has the ability to monitor both static and time-varying analyte concentrations. Firstly, the
detection limit of the system is estimated from a three-standard-deviation error analysis of absorption
measurements made on dilute aqueous solutions of potassium permanganate (natural absorption
coefficient (4805 ¡ 10) M21 cm21 at 532 nm). The detection limit was found to be y210 nM for a
466 mm pathlength, corresponding to an absorption of 1.0 6 1023 cm21. Online pH measurements on
a 20 nL sample are performed by monitoring the absorption of phenolphthalein indicator present at
millimolar concentrations. Finally, CRDS has been applied, for the first time, to monitoring chemical
reaction kinetics on a microfluidic chip, tracking the oscillation period of the well-known Belousov–
Zhabotinsky reaction.
1 Introduction
Detection and quantification of the tiny volumes of chemical
species produced in microfluidic systems remains a major
challenge to the full exploitation of microfluidics in biochemical
synthesis and analysis. Numerous authors have identified the
issue of ‘‘efficient extraction and utilisation of the vast amounts
of information produced’’ in microfluidic experiments.1–3
Droplet-based microfluidics have brought a paradigm shift in
high-throughput experimentation. Each droplet represents an
independent ‘‘reactor’’ volume,4,5 and the ability to produce
droplets at up to kHz rates opens up a vast number of
applications in biological, chemical and materials synthesis.
However, such approaches place additional demands on the
detection methods employed, as any detection scheme must be
commensurate with these high droplet production rates. At
present, chemical analysis is often carried out off-chip6 using
conventional laboratory techniques, thus becoming the rate
limiting step in what would otherwise be a high-throughput
microfluidic reactor.
Optical detection provides an appealing approach for online
measurements of microfluidic systems. Several optical and
spectroscopic on-chip detection methods have thus been
integrated with microreactors in recent years to permit the
spatio-temporal mapping of reactions and their optimisation,
and are the subject of several recent reviews.3,7–10 Laser-induced
fluorescence provides a powerful approach for rapid, in situ,
detection due to its high sensitivity and small mass requirements,
which are well suited to droplet analysis.4,5 Advances in
fluorescence lifetime imaging (FLIM) have permitted flow
mapping within droplets with 1 ms temporal resolution.11,12
However, such approaches are restricted in scope since they
require the presence of fluorophores, and the labelling of
reagents is not always possible or is undesirable; for example,
in reaction screening and discovery.
UV-vis spectroscopy;13–15 Fourier transform infrared spectro-
sopy (FT-IR),13,16–18 including multiple-internal reflection
aDepartment of Chemistry, University of Oxford, Chemistry ResearchLaboratory, 12 Mansfield Rd, Oxford, OX1 3TA, UK.E-mail: [email protected] of Chemical Engineering, ACE 311A, Imperial CollegeLondon, London, SW7 2AZ, UK
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(MIR)16 and imaging;18 Raman scattering;13,20–22 microcoil
nuclear magnetic resonance (NMR)19,23,24 or stripline detec-
tion25 with microcoils; and surface plasmon resonance (SPR),
have all been reported as approaches to online detection in
microfluidics. In general, these approaches involve a high degree
of spatial averaging over large detection areas (for example, in
plane optical detection26) or integration over relatively long
times17,22 in order to acquire statistically significant spectro-
scopic data. They are therefore suitable for single phase,
continuous reactions with stationary (time-invariant) composi-
tion profiles, but are not generally applicable to multiphase
flows. Recently, surface-enhanced Resonance Raman spectro-
scopy (SERRS) has been reported to achieve sub-millisecond
time resolution with high sensitivity on droplets containing
magnetic nanoparticles,27 and progress in FT-IR imaging
has enabled the label-free resolution of segmented flows with
y100 ms time resolution.18
Advanced UV-vis absorption techniques are particularly
attractive for microfluidic detection due to their universal nature
and potential for high sensitivity: every analyte absorbs light in
some region of the electromagnetic spectrum, and by selecting a
wavelength range across which the solvent is transparent and
there are no significant overlapping absorption bands from other
species, a sufficiently sensitive absorption measurement can
allow for label-free analyte detection. However, minute detection
volumes (pL–nL) and short path lengths (typically a few hundred
microns or less) severely limit the application of traditional
single-pass absorption spectroscopy in microdevices. Cavity
ringdown spectroscopy (CRDS) is a highly sensitive absorption
technique based on the decay of light within a high finesse
optical cavity.28 Most CRDS measurements, including ours,
employ a simple confocal Fabry–Perot cavity, comprised of two
highly reflective concave mirrors (reflectivity . 99.8%). A pulse
of laser light is directed into the back face of the first mirror and
a small amount couples through the mirror into the cavity. The
light is repeatedly reflected back and forth between the mirrors,
decaying exponentially with time as a constant fraction couples
out from the cavity on each interaction with the mirrors. The
decay time constant, or ‘ringdown time’, t is determined purely
by the geometry of the cavity and the round-trip transmission T:
t0~ncd
c({ ln T)(1)
where d is the cavity length (defined as the centre-to-centre
distance between the front faces of the two cavity mirrors), nc is
the refractive index within the cavity medium, and c is the speed of
light. For a two-mirror cavity, the cavity loss L = 1 2 T is
determined simply by the reflectivity of the mirrors. However,
inserting a microfluidic chip into the cavity introduces increased
scattering and reflection losses at the surface boundaries, which
must also be included in L. When an absorbing sample is
introduced into the cavity, absorption by the sample increases the
cavity losses, reducing the ringdown time, which is now given by:
t~ncd
c0({ ln TzaCl)(2)
where a is the absorption coefficient, C the concentration, and l is
the single-pass path length through the sample. A comparison
between the ringdown times recorded in the absence and presence
of a sample yields a quantitative determination of the sample
absorption.29 The absorption per unit pathlength, k = aC can be
shown to be:
k~aC~ncd
cl(1
t{
1
t0) (3)
CRDS and related techniques are currently amongst the most
sensitive spectroscopic absorption techniques available for both
the gas-phase30 and the liquid-phase,31,32 although they have
been much more widely applied in the gas-phase. The high
sensitivity results firstly from the vast increase in optical path
length relative to single pass techniques, and secondly from the
fact that because the technique relies on a measurement of the
rate of decay of light intensity within the cavity rather than on
the intensity itself, the signal is decoupled from the initial light
intensity and is therefore largely immune to noise arising from
shot-to-shot variations in the light source. While the method is
relatively insensitive to fluctuations in the incident light intensity,
the source intensity is one of the key factors that determine the
signal-to-noise ratio of the ringdown signal, and therefore the
accuracy to which the ringdown time can be determined.
The high sensitivity of CRDS makes it an attractive option for
microfluidics applications, providing a vastly increased optical
pathlength without increasing the sample volume probed. To our
knowledge, most attempts to couple CRDS with microfluidic
systems have so far employed optical fibre loop cavities rather
than Fabry–Perot cavities.33 This approach has the advantage
that optical fibres are well matched in size to the dimensions of
microfluidic channels, with fibre core diameters commonly less
than 500 mm. However, fibre-loop CRDS has relatively high
intrinsic cavity losses,34 resulting in a reduced sensitivity. Here
we describe the application of conventional two-mirror CRDS to
the interrogation of microfluidic liquid samples. CRDS measure-
ments on liquid samples are inherently less sensitive than gas-
phase measurements due to increased scattering and absorption
losses associated with both the sample and its container, but still
represent a considerable improvement on single-pass methods.
While liquid can be introduced to fill the entire space between the
cavity mirrors,35–38 the requirement of probing small liquid
sample volumes in microfluidics usually necessitates the intro-
duction of (typically glass) containers (otherwise known as
absorption cells) into the cavity. Past work on liquid-phase
CRDS has focused on the introduction of cuvettes39,40 or flow
cells41,42 into the cavity, with a particular emphasis on the use of
CRDS for small volume HPLC. The path lengths and detection
sensitivities achieved using these techniques are summarised in
Table 1 of ref. 43. The majority of liquid-phase CRDS have
probed sample volumes . 1 mL, with notable exceptions being
the work of Snyder and coworkers,41 Bechtel and coworkers42
and Alexander.43 The reader is also directed to a recent review of
liquid-phase CRDS techniques.44
We report what we believe to be the first example of CRDS
measurements on a microfluidic chip inserted into a two-mirror
cavity. The chip can be readily fabricated via rapid prototyping
and the non-contact nature of the two-mirror approach should
allow for the spatio-temporal mapping of the chip, avoiding
expensive integrated and less flexible spectroscopic probe
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arrangements. We have characterised the sensitivity of our
microfluidic-CRDS system and also include proof-of-concept
demonstrations of pH measurements and real-time tracking of
an oscillating reaction.
2 Experimental
2.1 Instrumentation
A schematic of the experimental setup used is shown in Fig. 1(a).
The light source is a pulsed Nd/YAG laser: either a Teem
Photonics NP-10620-100 (6 mJ per pulse, 900 ps pulse width,
7.4 kHz repetition rate), which was used for the detection limit
measurements, or a Teem Photonics SNP-08E-100 (8 mJ per
pulse, 900 ps pulse width, 7.4 kHz repetition rate), which was
used for the remaining experiments. In each case, the laser
output is frequency doubled to produce a beam of 532 nm light.
The optical cavity is formed from two concave dielectric mirrors
(CVI Melles Griot, reflectivity . 99.8% at 532 nm) with a
diameter of 25 mm and a radius of curvature of 1 m. For the
majority of experiments presented here, the mirror separation
was 875 mm, except for the detection sensitivity measurements
described in Section 2.2.1, for which the separation was 585 mm.
Light is coupled into the cavity by directing the laser pulse into
the rear of one of these mirrors. An iris is placed in front of the
cavity such that the beam radius in the centre of the cavity is
estimated to be around 300 mm. Light emerging from the cavity
is detected by a photomultiplier tube (PMT, Hamamatsu,
H6780-20), which is either placed directly behind the second
mirror (in which case the PMT is shrouded in blackout material
to reduce background signal caused by ambient light), or
coupled to the cavity output via a 3 mm diameter liquid light-
guide (Edmund Optics, NT53-428). The signal from the PMT is
displayed on a digital oscilloscope (Tektronix, TDS 3044B),
which is interfaced to a personal computer via a GPIB-USB
interface (National Instruments, 778927-01). In all the experi-
ments presented here, the laser pulse duration of 900 ps is less
than the round trip time of the cavity, such that the cavity output
consists of a train of pulses with exponentially decaying
intensities.
Data is acquired and analysed in real time using a home-written
LabVIEW program. The data acquisition time, corresponding to
a full ringdown trace, is typically 1 ms, commensurate with online
droplet analysis. However, the data transfer between the
oscilloscope and the computer is currently limited to four traces
per second. In a typical measurement, the ringdown trace is
averaged 512 times on the oscilloscope, and 50 averaged traces are
recorded and saved. For each trace, signal intensity and time
thresholds are applied if required to limit the data analysis to the
exponentially decaying region of the ringdown pulse train. A
peak-finding algorithm is employed to determine the baseline-
subtracted amplitude S of each peak in the pulse train, and the
ringdown time is determined from a linear fit to a log plot of the
resulting intensity vs. time data, i.e.
ln S~ ln S0{t
t(4)
where S0 is the intensity of the first fitted peak. The fitting
procedure generally returns R2 values of 0.998 or better.
The microfluidic chip is mounted in the centre of the cavity on
a double-rotation (Thorlabs, RP01) and three-axis translation
stage (Newport Corporation, 443), with micrometer resolution
actuators (Newport Corporation, SM-25), allowing individual
microfluidic channels to be precisely located within the laser
beam path. Two different designs of microfluidic chip were
employed in this work, both fabricated by rapid prototyping of a
multifunctional thiol-ene negative resist via frontal photopoly-
merisation,45–48 and yielding organic solvent resistant polymer
matrices sandwiched between two glass faces. The first liquid cell
was manufactured by sealing a 100 mm thick glass cover slip
against a 1 mm glass microscope slide which had been drilled
with inlet and outlet ports. A thiolene-based negative photoresist
(Norland Optical Adhesive, NOA 81) was applied around the
edges of the cover slip, sealing the system and resulting in a single
5 mm wide, 61 mm deep channel; this cell was employed to
make pH measurements, sampling a volume of around 20 nL
(assuming in this case a beam radius of around 320 mm). The
second type of microdevice was fabricated by sandwiching the
thiolene resist between two 141 mm thick glass cover slips,
separated by silicon wafer spacers at a distance of 380 mm. A
photomask printed on an acetate film with a negative of the chip
design (shown in Fig. 1(b)) was then secured over the top layer,
and the system was cured via frontal photopolymerisation using
a collimated UV source. A calibrated UV light dose was
delivered to ensure that the thiolene in the unmasked regions
was completely cured. The uncured photoresist was then pushed
out of the resulting microfluidic channels (at a temperature of
65 uC, to reduce viscosity) using pressurised air, followed by
acetone. The channels were inspected using an inverted micro-
scope (Olympus, IX71) to ensure that no defects or contaminants
were present. Nanoports (Upchurch Scientific) were fitted to
holes pre-drilled through one of the glass cover slips, forming
inlets/outlets capable of connection to a syringe pump. The edge
of the completed microfluidic chip was then mounted on a 1 mm
thick glass microscope slide, such that the microscope slide did
not infringe on the path of the laser, to provide a rigid point at
which the chip could be clamped securely in place inside the
ringdown cavity. Once mounted within the cavity, one or more
syringe pumps (Chemyx Inc, Fusion 400) were used to inject the
samples into the microdevice.
Incorporating a microfluidic chip into the cavity introduces
four additional surfaces at which scattering and reflection can
Fig. 1 (a) Schematic of the experimental setup (see text for details); (b)
design of the microfluidic chip used for the majority of the work
described in this paper. Inlet/outlet ports are labelled A, B, and C.
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occur, as illustrated in Fig. 2(a). In order to minimise scattering
losses, great care was taken to ensure high quality and cleanliness
of all surfaces, including the internal surfaces of the chip.
Reflection losses may be reduced either by ensuring that all
surfaces are normal to the laser beam, which in practice is
extremely difficult to achieve using our current chip fabrication
procedure, or by mounting the chip within the cavity at
approximately Brewster’s angle to the (p-polarised) laser beam.
In our setup, the chip is mounted on a rotation stage, allowing
the angle of the chip to the cavity axis to be adjusted so as to
optimise the ringdown time. Ringdown measurements on an
empty cavity indicate that the intrinsic cavity losses resulting
from transmission through the mirrors are around 0.2%. An
additional loss of typically around 0.5% is incurred by placing a
water-filled thiolene-glass microfluidic chip within the cavity at
an optimised angle of 59u (see discussion of optimisation
procedure below), reducing the measured ringdown time from
952 ns to around 272 ns.
Prior to carrying out any spectroscopic measurements, the
dependence of the ringdown signal on the chip angle within the
cavity was characterised. Fig. 2(b) shows the experimentally
measured ringdown time as a function of the angle between the
chip surface normal and the cavity axis. There is a clear
maximum in ringdown at an angle of 59u, and this chip angle was
used for all further ringdown measurements. We note that at the
optimum angle of 59u the optical pathlength through the sample
is increased significantly from the optical pathlength at normal
incidence.
The dependence of the ringdown time on chip angle may be
explained simply by considering the reflection losses at each
surface within the cavity. Fig. 2(a) shows the various interfaces
encountered by the light beam as it passes through the chip. The
angles of refraction at each interface are defined by Snell’s law:
n1sinh1 = n2sinh2 (5)
where n1 and n2 are the refractive indices of the media on either
side of a boundary, and h1 and h2 are the angles of the light beam
to the surface normals. The reflection loss at each interface can
then be modelled using the Fresnel equations:
Rp~
n1
ffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffi
1{(n1
n2sinh1)2
r
{n2cosh1
n1
ffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffi
1{(n1
n2
sinh1)2
r
zn2cosh1
2
6
6
6
4
3
7
7
7
5
2
(6)
where Rp is the proportion of p-polarised laser light reflected. To
a good approximation, the total cavity loss per pass is the sum of
the reflection losses from the chip surfaces and at the surfaces of
the two cavity mirrors. Once the total loss per pass has been
calculated in this way as a function of chip angle, eqn (1) may be
used to convert the angle-dependent losses into angle-dependent
ringdown times. The result is shown together with the experi-
mental data in Fig. 2(a). The measured and modelled curves are
in good agreement, though the optimum angle of 59u measured
experimentally is slightly higher than the 56u predicted by the
model. The discrepancy is most likely due to slight imperfections
in the chip, for example surfaces that are not precisely parallel to
each other.
2.2 Measurements
2.2.1 Detection limits. The minimum detection limit, kmin, may
be determined from the minimum detectable change Dtmin in the
baseline ringdown time, t0. Assuming tt0 # t02, we have49
kmin~ncd
cl
Dtmin
t20
(7)
In this work, we define Dtmin as three times the standard
deviation (s) in the baseline ringdown time t0. It can be seen
from eqn (7) that improving the sensitivity of a ringdown
measurement relies primarily on minimising the baseline losses to
maximise t0, as well as on increasing the pathlength of light
through the sample (l). Short pathlengths are inherent in
microfluidic systems, and significant cavity losses are unavoid-
able when including a microfluidic chip. While this will limit the
sensitivity of the system, considerable increases in sensitivity over
single pass measurements are still gained by cavity enhancement.
For comparison with the above estimate of our detection
sensitivity, the detection limits of the system were also evaluated
via absorption measurements on a series of low-concentration
aqueous solutions of potassium permanganate, KMnO4, a strongly
absorbing species whose visible absorption maximum lies close to
the wavelength of our laser (532 nm). Concentrations spanning the
range from 1024 to 1027 M were prepared by serial dilution, flowed
through the microfluidic chip mounted within the cavity at a
constant flow rate of 0.2 mL min21, and probed using CRDS as
described above. Between each measurement, the microfluidic chip
was flushed with water flowing at 0.2 mL min21 for five minutes,
and a measurement of the baseline ringdown time (t0) was obtained
Fig. 2 (a) Interfaces experienced by the light beam as it passes through
the microfluidic chip; (b) measured dependence of the ringdown time on
the incidence angle of the laser to the microfluidic chip within the cavity.
The measurements are compared with the results of the simple model
described in the text, which is based on quantifying the reflection losses at
each interface.
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to ensure that the chip was not contaminated with residual KMnO4
solution. The (natural) absorption coefficient, a, for KMnO4 at
532 nm was determined in a conventional single pass absorption
measurement (repeated five times) through a 1 cm cuvette filled
with 6.5 6 1024 M KMnO4 to be (4805 ¡ 10) M21 cm21 (Varian
Cary-100 Bio UV-vis spectrometer). Given that the 380 mm
pathlength across the chip was found to vary by several tens of
microns (measured using a micrometer), as the two chip faces were
not perfectly parallel to each other, rather than using a fit of the
ringdown data to eqn (3) to determine the a value, instead the
pathlength across the chip at the intersection point of the laser beam
was determined using a which was precisely known from the UV-vis
spectrometer data.
2.2.2 pH measurements. As a proof-of-concept, the cavity
ringdown spectrometer was used to measure the pH of a series of
buffer solutions (pH 7.6 to pH 11) through detection of the
change in absorption coefficient of the phenolphthalein indicator
at 532 nm. Phenolphthalein, shown in Fig. 3 (compound A), is
colourless below pH 8.2, but deprotonates between pH 8.2 and
10.0 to form the pink compound B, which absorbs at 532 nm.
Above pH 11, the pink colour begins to fade as compound C is
produced.
The process involved in the colour change may be summarised
as HInd > H+ + Ind2, where HInd and Ind2 are the protonated
and deprotonated forms of the indicator, respectively, with
pKa~{ log½Hz�½Ind{�½HInd� (8)
The concentration of deprotonated phenolphthalein, [Ind2],
may be determined from the results of an absorption measure-
ment, using eqn (3). Rearranging eqn (8) then allows the pH to
be determined, assuming the initial concentration of indicator is
known.
pH~pKaz log½Ind{�
½HInd�0{½Ind{� (9)
For these measurements, a stock solution of 0.015 M
phenolphthalein solution was prepared in a 1 : 1 mixture of
ethanol and water. For each measurement, 0.1 mL of indicator
was added to 5 mL of buffer solution, to give a total indicator
concentration of 2.9 6 1024 M, and the absorption of the
resulting solution was determined following a measurement of
the ringdown time t. Two types of buffer solution were used: a
sodium tetraborate and hydrochloric acid buffer solution was
used for the range of pH 7.6 to 9.4; and a glycine and sodium
hydroxide solution was used for the range from pH 9.0 to 11.0.
The absorption coefficient of phenolphthalein was determined
for each pH used.
As a reference for comparison, the experiment was repeated in a
1 cm cuvette using a commercial UV/vis spectrometer (Unicam,
UV2-100). A concentration of 1.49 6 1023 M phenolphthalein
was used for these measurements, an order of magnitude larger
than that used in the microfluidic experiment. To account for this
difference, the single-pass data was scaled by the ratio of indicator
concentrations.
2.2.3 Oscillations of the Belousov–Zhabotinsky reaction. To
demonstrate that time-resolved measurements are also possible
with our system, the Belousov–Zhabotinsky (BZ) reaction was
performed on a microfluidic chip inside the cavity. The BZ
reaction is an example of an oscillating reaction,50 in which
Ce(IV)/Ce(III) is used to catalyse the oxidation and bromination
of malonic acid by BrO32 in H2SO4. The reaction occurs in a
periodic cycle, with a clear red to blue colour change in the
presence of Ferroin indicator. Under our experimental condi-
tions, the oscillation time was several tens of seconds. When red,
the solution absorbs at our operating wavelength of 532 nm,
which allows the progress of the reaction to be monitored.
For simplicity, the reagents (5 mL of 0.23 M NaBrO3 aqueous
solution, 5 mL of a 0.31 M malonic acid and 0.059 M NaBr
aqueous solution, 5 mL of a 0.019 M Ce(NH4)2(NO3)6 and
2.7 M H2SO4 solution, with 0.1 mL of 0.0125M Ferroin
indicator)51 were mixed in bulk prior to being injected into the
chip. The reaction mixture was injected into the chip at a flow
rate of 0.1 mL min21, but once the continuous liquid flow had
passed the laser beam position, flow was stopped and the
oscillations were recorded under static conditions. Ringdown
traces were averaged 32 times on the oscilloscope, and data was
acquired at a rate of 1 Hz. The oscillations were then followed by
monitoring the change in t over time.
To obtain a reference to compare with, the experiment was
repeated at the same concentration in a 1 cm cuvette and
monitored as a function of time, via a single-pass 532 nm
absorption measurement using the same laser and a silicon
photodiode detector (Thorlabs DET 10A).
2.2.4 Droplet flow measurements. We next consider the
applicability of this approach to droplet microfluidics, with
high-throughput applications in mind.52 As mentioned above,
droplet-based microfluidics present additional challenges, parti-
cularly in the requirement of fast data acquisition rates to resolve
individual travelling droplets. In addition, we expect higher
losses than found in continuous flow because of the presence of
possible lubrication layers between microchannel, carrier fluid
and suspended phases. As a second demonstration of time-
resolved measurements using our experimental system, the two-
mirror cavity was used to monitor droplets of 1 6 1026 M
aqueous rhodamine 6G (R6G) solution. The aqueous sample
was injected into Input B of the thiolene-glass chip (illustrated in
Fig. 1(b)), and a carrier phase of toluene was injected into Input
A, resulting in aqueous plugs compartmentalised by the toluene
carrier phase. Ringdown measurements were performed in which
the flow rates were varied between 0.003 mL min21 and
0.05 mL min21 in order to vary the size of the plugs over theFig. 3 Structural forms of phenolphthalein.
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range from 2 to 10 mm and their travel velocity in the channel
over the range from 130 to 2200 mm s21.
3 Results and discussion
3.1 Detection limits
As described in Section 2.2.1, ringdown times were recorded for
a series of aqueous solutions of KMnO4, with concentrations
ranging from 1024 to 1027 M. Typical ringdown signals are
shown in Fig. 4. When used in combination with the known
absorption coefficient a for KMnO4 of (4806 ¡ 106) M21 cm21
(determined in a separate single-pass measurement using a
solution housed in a commercial cuvette) these measurements
allow us both to determine an accurate value for the pathlength
within the microfluidic chip, and to determine the limit of
detection for KMnO4. The pathlength is determined from the
gradient of a plot of k against concentration (eqn (3)), shown in
Fig. 5, to be 466 ¡ 10 mm.
The measured ringdown time for a chip filled with pure water
was 271 ns, with a standard deviation of 0.6 ns. Determining the
detection limit as described in Section 2.2.1, we have Dt = 3s =
1.8 ns, which when substituted into eqn (7) yields an absorbance
detection limit of kmin = 1.0 6 1023 cm21. This corresponds to a
concentration detection limit for KMnO4 of approximately 214 nM
in an illuminated volume of 132 ¡ 3 nL, which is in qualitative
agreement with the concentration at which a change in ringdown
time can be discerned relative to the reference measurement.
The detection limit can also be estimated from the 3s
uncertainty in the intercept of the plot shown in Fig. 5. The
value of 5.2 6 1023 cm21 obtained in this way is somewhat
higher than that determined above from the baseline noise in our
t0 measurement. This is unsurprising, as the measurement based
on t0 assumes that there are no sources of error other than the
intrinsic noise in the ringdown measurement. In reality, factors
such as a drift in the cavity alignment and uncertainties in the
analyte concentration are likely to contribute to the overall
measurement uncertainty.
While we believe our work marks one of the first applications
of CRDS to measurements on microfluidic samples, measure-
ments through a similar path length of liquid have been carried
out previously. Snyder and coworkers41 used a bespoke high-
optical-quality Brewster’s angle flow cell with a volume of 10 mL
and an optical path length of 300 mm to achieve a detection limit
of 6.2 6 1024 cm21 at 470 nm. Using the same flow cell, Bechtel
and coworkers42 further improved the detection limit to 7.8 61026 cm21 by replacing the pulsed 470 nm laser source used to
excite the cavity with a single-mode continuous wave laser source
operating at 488 nm, thus reducing noise on the signal associated
with shot-to-shot fluctuations in the laser intensity. Our
detection limit is somewhat higher than those reported by
Snyder and Bechtel, which can be ascribed primarily to the fact
that our simple microfluidic chip is not manufactured from high
optical quality components, and almost certainly suffers from
small scattering losses at the surfaces. There is scope to improve
the optical quality of the microfluidic chip, and therefore to
lower our detection limit, but even so, the integrated microfluidic
chip CRDS system provides a good general platform for
chemical analysis, with the potential for probing smaller sample
volumes than the flow cell arrangement.
The detection limit obtained here within a two-mirror cavity
can also be compared to that obtained using fibre-loop CRDS
techniques. Rushworth et al.34 recently reported a detection limit
of 0.11 cm21 using a cavity comprising a 3.08 m loop of 365 mm
core diameter optical fibre. The path length through the sample
was 180 mm, corresponding to a total probed sample volume of
19 nL. Using a similar technique,53 Waechter et al. recently
reported a detection limit of 4.6 6 1022 cm21 in a slightly
smaller volume (100 nL compared to 132 nL), but with a
significantly longer path length (800 mm compared to 466 mm). In
this case, the fibre-loop cavity comprised a 9.25 m loop of
400 mm core diameter optical fibre. While fibre-loop cavities
have a number of advantages for measurements on microfluidic
samples, being well size-matched to microfluidic channels and
inherently able to support a broad range of wavelengths, the
detection limits achievable are currently several orders of
magnitude poorer than for two-mirror arrangements due to the
unavoidably higher cavity losses associated with coupling light
into and out of the loop and introducing a sample region.
3.2 pH measurements
As explained in Section 2.2.2, CRDS measurements of the
optical absorption by phenolphthalein indicator were used to
Fig. 4 Typical ringdown traces recorded for a cavity containing a
thiolene glass microfluidic chip: reference ringdown recorded when the
channels are filled with water (grey trace); ringdown recorded when the
channels are filled with 50 mM aqueous KMnO4 solution (black trace).
Fig. 5 Measured absorbance as a function of concentration for a series
of aqueous solutions of KMnO4 over the concentration range from
100 nM to 100 mM.
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track the pH of a series of buffer solutions as they flowed
through the microfluidic chip. Fig. 6 shows the measured
absorbance as a function of pH over this range for the CRDS
measurements over the pH range 7.0 to 11.0. The measured
absorbance is directly proportional to the concentration of
deprotonated indicator, and follows the typical titration curve of
a weak acid, and the CRDS measurements are in good
agreement with single pass measurements made on a bulk
sample contained in a 1 cm cuvette.
For a known indicator concentration, the measured absor-
bance may be converted directly into a pH value using eqn (9).
Throughout the steepest part of the titration curve (pH range
y 9–10.5), the error on our experimental measurements allows
the pH to be measured to ¡ 0.028 of a pH point. Outside of this
range, the titration curve levels off and the absorbance is only
weakly dependent on pH, leading to much greater uncertainty.
These measurements demonstrate that provided an indicator can
be found whose colour change matches the pH region of interest,
and a probe wavelength identified that does not overlap with
absorption by the sample, introducing a low concentration of an
indicator compound to a sample and tracking its absorption
provides a general method for pH monitoring on a microfluidic
chip.
3.3 Oscillations of the Belousov–Zhabotinsky reaction
To demonstrate the potential use of CRDS for monitoring the
progress of chemical reactions occurring on microfluidic chips,
the Belousov–Zhabotinsky reaction was performed in the
thiolene-glass chip within the cavity, and the ringdown time
was monitored as a function of time from reaction initiation. The
reaction was carried out with a series of different concentrations
of the Ferroin indicator (3.125 6 1025 M to 5 6 1024 M) in
order to determine the optimum concentration for monitoring
the reaction both in CRDS and bulk absorption measurements.
Fig. 7 shows example data sets for an indicator concentration of
2.5 6 1024 M.
Under our reaction conditions, the oscillation period of the
reaction carried out on-chip is similar to that found in bulk
solution, around 70 s in both cases. However, the functional
forms of the oscillations in the absorption signal are quite
different for the two setups, indicating that the detailed kinetics
of the reaction are affected considerably by the shape and size of
the reaction vessel. After several oscillations, bubbles of CO2
(one of the reaction products) begin to form within the
microfluidic channels, degrading the ringdown signal; however
the bubbles do not appear to affect the period of oscillation.
These results demonstrate that CRDS measurements are easily
able to track the kinetics of reactions occurring on a timescale of
seconds. In principle, it should be possible to track events
occurring on the ms timescale, with even shorter timescales being
possible if a time-varying concentration is allowed when fitting
the ringdown traces. However, the time resolution of the
instrumentation used in this demonstration is limited by the
data transfer rate from the oscilloscope to around 250 ms.
3.4 Monitoring droplets in microfluidic systems
In our final demonstration, the CRDS setup was used to follow
the flow of droplets or ‘slugs’ of an aqueous phase seeded in a
toluene carrier phase, within a microfluidic channel. Fig. 8(a)
and 8(b) clearly show the change in ringdown time for two
different sets of flow conditions as the slugs of Rhodamine
solution pass through the laser beam. To acquire these data, the
toluene carrier phase was injected into the chip shown in Fig. 1
through port A at a flow rate of 0.003 mL min21 (Fig. 8(a)) or
Fig. 6 Absorption measurements as a function of pH for buffered
solutions of phenolphthalein indicator. Two different buffers were used
to cover the range from pH 7.0 to 11.0.
Fig. 7 Absorption signal recorded as a function of time for the
oscillating Belousov–Zhabotinsky reaction. The grey trace shows the
single-pass absorption recorded at 532 nm when the reaction was carried
out in a 1 cm cuvette, while the black trace shows the absorption
measured by CRDS when the reaction was carried out on the
microfluidic chip shown in Fig. 1(b).
Fig. 8 Droplet flow analysis using CRDS on a microfluidic chip. The
ringdown time t is tracked as droplets of 1 6 1026 M R6G solution in a
toluene carrier phase are flowed through a thiolene-glass chip at a total
flow rate of (a) 0.008 mL min21 and (b) 0.075 mL min21.
5382 | RSC Adv., 2012, 2, 5376–5384 This journal is � The Royal Society of Chemistry 2012
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0.05 mL min21 (Fig. 8(b)), and a 1026 M aqueous solution of
Rhodamine 6G was flowed through port B at 0.005 mL min21
(Fig. 8(a)) or 0.025 mL min21 (Fig. 8(b)).
The behaviour of t has several notable features. A clear
change in ringdown time is seen as the aqueous (droplet) and
toluene (carrier) phases pass through the laser beam. For the
data shown in Fig. 8(a), for example, the ringdown time switches
from y 220 ns for the toluene phase to y 260 ns for the aqueous
phase. As described earlier, the mounting angle of the chip
within the cavity has been optimised for measurements on
aqueous phases. The refractive indices of water (n = 1.333) and
toluene (n = 1.496) differ sufficiently that the ringdown time is
longer for the aqueous phase than for the toluene phase, even
though Rhodamine absorbs light at the wavelength of the laser.
For experiments in which quantitative absorption analysis of
droplets is the goal, the chip mounting angle should be optimised
to achieve the greatest difference in ringdown time between the
droplet and carrier phases. This was the case for the data shown
in Fig. 8(b), in which the ringdown times are y240 ns for the
toluene phase and y340 ns for the aqueous phase.
At low flow rates, a sharp reduction in t is observed as the
boundaries of each droplet pass through the laser beam. This is
caused by the meniscus at the droplet/carrier phase boundary
forming a lens that scatters the incident laser light out of the
cavity, dramatically reducing the ringdown time. The consistent
form of these scattering signals suggests that the topology of the
interface between the two immiscible solutions is identical for
each droplet, and a quantitative analysis of the signals could
even be used to study droplet morphology. This structure is
much less visible in Fig. 8(b), mostly due to the fact that the
droplet flow rate in this experiment was close to the limiting time
resolution imposed by our current fairly slow data acquisition
system.
These results demonstrate the ability of the two-mirror CRDS
system to interrogate and distinguish between individual
droplets. The acquisition time of the ringdown is of the order
of hundreds to thousands of nanoseconds. With an improved
data transfer system (currently limited at 4Hz), measurements at
kHz or even MHz data rates should become possible, allowing
the spatio-temporal resolution of fast moving droplets, com-
mensurate with kHz microfluidic label-free droplet production
systems.
4 Conclusions and future work
Thiolene-glass microfluidic chips have been integrated into a
two-mirror cavity ringdown spectrometer. By placing a chip at
an angle of 59u to minimise reflective and refractive losses, a
detection limit of 1.0 6 1023 cm21 has been achieved in a sample
volume of 132 nL, corresponding to a 214 nM minimum
detectable concentration of KMnO4. To illustrate the potential
of the system for monitoring a variety of different processes on
microfluidic chips, we have presented a number of proof-of-
concept demonstrations, including the measurement of pH,
reaction monitoring, and droplet flow monitoring. A number of
improvements are planned for the future, including minimising
the laser ‘footprint’ on the chip to allow smaller microfluidic
channels to be probed, expanding the method to probe at
multiple wavelengths or across a continuum of wavelengths,54
and upgrading the data acquisition system to allow measure-
ments at rates exceeding the kHz range.
Acknowledgements
This work was funded by the United Kingdom Engineering and
Physical Sciences Research Council through grant EP/G027838/
1.
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