Biosensors & Bioelectronics lO (1995) 831-839
The modification of enzyme electrode
properties with non-conducting
electropolymerised films
S. Eddy, K. Warriner, I. Christie, D. Ashworth, C. Purkiss & P. Vadgama
University of Manchester, Department of Medicine, (Clinical Biochemistry), Hope Hospital, Eccles Old Road,
Salford M6 8HD, UK.
Tel: 0161 787 5991 Fax: 0161 787 7432.
Abstract: Phenol and several phenol derivatives have been electropolymerised
on to platinum anodes. The selective properties of the modified electrodes
were dependent on the final polymeric structure. Although essentially nonconducting, dual phenolic films could be deposited on electrode surfaces. This
was achieved by the initial deposition of a porous polymer formed from,
phenol red, followed by the more diffusion limiting film of oxidised phenol.
The resulting composite film showed the combined selective characteristics of
the two component polymers. Attempts to enhance polymeric film selectivity
via the incorporation of charged or neutral surfactants are outlined. The
characteristics of glucose oxidase incorporated into (poly)phenol films are
discussed.
Keywords: amperometry, enzyme entrapment, glucose determination, modified
electrodes, phenols, selectivity, surfactant
INTRODUCTION
Amperometric enzyme electrodes have received
considerable attention in recent years (Yacynych,
1992). Enzyme incorporation to form a highly
selective biological recognition layer considerably
extends the analytical range of the base electrochemical transducer offering a route to the
reagentless analysis of many solutes of biological
interest including glucose, lactate, and acetaminophen. Practical realisation has involved several
approaches including the use of membrane technology to modify solute access to the enzyme
layer (Vadgama, 1990; Koochaki et al., 1993),
provide a biocompatible surface (Turner et al.,
1991; Davies et al., 1992; Higson et al., 1993),
0956-5663/95/$09.50
and confer a reduction in interference (PaUeschi
et al., 1986). In this way direct whole blood assay
has been possible with minimum sample dilution
and preparation. Membrane materials commonly
used by our group for a range of diffusion control
and selectivity function have included polyaryl
sulphone, cellulose acetate, and microporous
polycarbonate, and polyurethane (Christie &
Vadgama, 1994). Many such preformed membranes present significant diffusion distances for
solutes, up to 10/xm, and therefore can add
significantly to response time. For most purposes
resulting time to steady state is acceptable, but
it is valuable to extend the technology to the
use of thinner membrane phases. Furthermore,
coatings would be of possible advantage in
831
S. Eddy et al.
diminishing diffusion of passivating species to the
underlying electrode in blood (Higson et al.,
1993).
Electropolymerised films based on polyphenol
(Bartlett & Whitaker, 1987), polyaniline (Cooper
& Hall, 1992; Pud, 1994), polyindole and polypyrrole (Fortier et al., 1990) have been seen as an
alternative to conventional membranes (Wang et
al., 1989). The oxidation of species at an anode
can lead to modified electrode behaviour with
beneficial properties, including optimised selectivity (Sasso et al., 1990; Groom & Lvong, 1993)
and protection of the electrode surface from
passivation, in the past this oxidation was seen
as disadvantageous and referred to as electrode
fouling. Interest in modified electrodes has tended
to centre on electron conducting or redox polymers (Foulds & Lowe, 1986; Pud, 1994), but
non-conducting polymers are an ideal membrane
equivalent (Christie & Vadgama, 1993). Because
the growth of non-conducting polymers is selflimiting, the resulting films formed are very thin
(10-100 nm; Bartlett & Cooper, 1993). The
response time of these modified electrodes can
in principle, approach that of a bare electrode
(Christie & Vadgama, 1993). Phenol has been
especially studied in this regard with a mechanism
for electrochemical polymerisation proposed
based on polymerisation through simple radical
initiation (Bartlett & Cooper, 1993). Other advantages are that such films are usually free from
defects such as pinholes, and are potentially
robust, indeed they were originally used for their
anti-corrosion properties (Subramanian, 1980).
Phenol films have been shown to have favourable
perm-selective properties for hydrogen peroxide
over interferents of clinical significance in amperometric assays, notably ascorbate, acetaminophen, and uric acid (Christie & Vadgama,
1993). This selectivity appears to be based
predominantly on size exclusion, the film thus
acting as a molecular sieve.
Such films can also be used to immobilise
enzymes (Bartlett & Whitaker, 1987; Bartlett &
Whitaker, 1987; Bartlett et al., 1992), moreover
with mild conditions for electropolymerisation
entrapment, enzyme activity can be retained
more readily (Bartlett & Cooper, 1993). Electrochemical polymerisation is a simple and attractive
means of enzyme immobilisation at an electrode
surface. The process requires simply electrochemical oxidation of a suitable monomer from
solution containing enzyme. The process more832
Biosensors & Bioelectronics
over can be governed by polarisation potential
and duration which can allow accurate control
of the film thickness and the amount of enzyme
entrapped (Bartlett & Cooper, 1993). Precise
confinement of an enzyme at an electrode without
cross-immobilisation at a neighbouring electrode,
would be a particularly favourable aspect in the
production of microelectrode arrays (Bartlett &
Caruana, 1992; Bartlett & Caruana, 1994).
The present study was concerned with a
comparative examination of phenolics notably
phenol, phenol red and 4-aminophenol. Polymer
formation on platinum, subsequent selectivity,
and ability to retain enzyme, using glucose
oxidase (GOx) as a model, is discussed. GOx
was chosen for entrapment as it is a very robust
enzyme and therefore provides a more stable
system to study. Glucose is also an important
analyte both in medicine and the food industry.
EXPERIMENTAL
Apparatus
The electrochemical cell used was obtained from
Rank Bros. (Bottisham, Cambs., UK). This
consisted of a 2 mm diameter platinum anode,
surrounded by a 12 mm diameter annular Ag/
AgC1 pseudoreference. Polarisation at +0.85V
vs. Ag/AgCl was achieved with a variable voltage
source, also equipped to measure current in the
range 0.1 nA to 2.0 mA (Department of Chemistry Workshop, University of Newcastle-UponTyne). The output was recorded using a Goertz
Metrawatt SE120 (Austria) strip chart recorder.
Membranes used to cover the electrode surface
were secured with an O-ring held in place by the
sample chamber when the cell was assembled.
Membrane fabrication
Cellulose acetate, 37.8% acetyl content (Aldrich,
Gillingham, UK), membranes were formed from
1 ml of 2% w/v solution in acetone, cast on a
5 × 5 cm glass plate, manually rotated for several
minutes while the solvent evaporated, and then
left for at least 2 h before use. PVC membranes
were cast from solutions of 0.06 g PVC (200,000
Daltons, BDH) and 150/xl isopropyl myristate
(Fluka, Buchs, Switzerland) in 5 ml tetrahydrofuran poured into a Petri dish, (covered and left
Biosensors & Bioelectronics
at room temperature for the solvent to evaporate;
- 4 days).
Coating and measurement procedures
Experiments were performed in buffered solution
containing, per litre, 2.44 g NaH2PO4.H20, 7.5 g
Na2HPO4, 3 g NaCI, and 0.6 g disodium EDTA
adjusted to pH 7.4 with 1 M HCI. Phenol (Anal.
grade) and phenol red were obtained from Sigma
Chem Co (Poole, Dorset), 4-aminophenol from
Fluka. All solutions were prepared in buffer.
Electrodes were cleaned by scrubbing with 0.3/zm
alumina then a drop of concentrated nitric acid
was placed on the anode for 15 min followed by
rinsing in distilled water. The cell was conditioned
for several hours in buffer at +0.85V vs. Ag/
AgCI until a constant baseline was achieved
( - 5 nA). To prevent damage to the films from
the action of a rotating stirrer bar, an overlying
high permeability cellulosic dialysis membrane
from a haemodialysis cartridge (Gambro, Lund,
Sweden) was employed. Coatings were formed
through the dialysis membrane by continued
polarisation of the anode (+0.85V vs Ag/AgC1)
in the presence of a 5 mM buffered solution of
the coating species, 0.5 mM for phenol red. A
potential of +0.85V vs. Ag/AgCI was found to
electropolymerise all the phenolics used, without
causing raised background currents due to electrolysis of water. Coating was initiated by the
placement of 1 ml of the coating species in the
cell chamber, and terminated by its removal and
replacement with buffer. Coating times were
between 1-24 h depending on the phenolic species
used. The response to 0.1 mM ascorbate was
used to assess the integrity of the resulting films.
The surfactants used in order to modify phenolic films were deoxycholic acid, cholic acid, Noctadecyl-N,N-dimethyl-3-ammonio-2propanesulphonate, and n-decyl-b-D-maltopyranoside, purchased from Sigma. Surfactant was
present at a concentration of 10 mM in the
phenolic solution, and the coating procedure
as above performed. Cyclodextrin (Sigma) was
present at 1% (w/v) in the phenol solution.
Enzyme entrapment
Glucose oxidase (E.C. 1.1.3.4, Type VII, 180,
000 U/g) from Aspergillus niger was obtained
from Sigma. Varying enzyme quantities were
dissolved in 1 ml of the phenolic solutions, and
Modification of enzyme electrode properties
the coating procedure followed as above. After
completion a cellulosic dialysis membrane was
carefully laid over the film to prevent damage
by the action of the stirrer.
Enzyme laminate
GOx solutions were made up containing 30 mg/
ml enzyme (Sigma) and 200 mg/ml BSA (Sigma).
10/xl of this solution was combined with 5/zl 5%
w/v glutaraldehyde when required for deposition
in enzyme laminates. The procedure for laminate
formation was common to all polymer membranes. 5 txl of enzyme/BSA/glutaraldehyde solution was sandwiched between two 1.5 × 1.5 cm
membranes. The laminate was then compressed
between two microscope slides for 10 min until
the cross linking was complete, then rinsed in
buffer before being placed in the electrochemical
cell.
Responses to glucose, hydrogen peroxide, and
interferents were determined by adding stock
solutions to buffer solution in the cell. All
solutions were prepared daily except glucose
which was prepared at least 24 h in advance to
allow for mutorotation and then stored at 4°C.
The pH of buffer was altered by the addition
of 1 M HC1 or NaOH solution, to obtain solutions
with a pH range between pH 2-8 for the
investigation of the effect of pH on enzyme
entrapped within a phenolic film.
RESULTS
Electropolymerised film studies
The following study was initiated to demonstrate
the properties of phenolic films, the intention
was not to optimise procedures for specific
applications.
Monophenol deposition in stirred solution gave
current decay curves which confirmed that electropolymerisation was a self-limiting process (Fig.
1). Similar curves were seen at microporous
membrane protected platinum anodes. The
anodic current observed with phenol shows a
rapid initial increase followed by a decrease until
a stable baseline current was reached ( - 5 nA).
Current vs. time profiles were similar irrespective
of the oxidisable phenolic derivative employed.
In addition to the loss of response to the
modifying species due to film formation there
833
S. Eddy et al.
Biosensors & Bioelectronics
trode (Table 1). This latter effect applied to
modifier species with two or more hydroxy groups
or both hydroxy and amine substituents of the
aromatic ring. Application of 4-AP films did not
affect linearity of response up to at least 1.6 mM
hydrogen peroxide (Fig. 2). Response times were
similar to that of the bare electrode (<20 s).
Also phenol responses were retained enabling
later work to include a subsequent electropolymerisation.
A more complex charged phenolic monomer
gave a different behaviour on electropolymeris-
lOO
80
.~= 60
~ 4o
2O
0
5
10
15
Time
20
25
30
i
i
35
40
(rain)
60
4-AP
Fig. 1. Current vs. time profile during coating of Pt
anode from 5 mM phenol solution (+0.85V vs. Ag/
AgCI, pH 7.4 phosphate buffer, electrode overlaid by
dialysis membrane).
Uncoa'(ed
coated
50
40
~esponse [~A) 3.0
was a strong solute selectivity shown for some
polyphenolic layers (Table 1). With the phenol
film, both ascorbate and acetaminophen signals
are greatly attenuated compared to that of
hydrogen peroxide.
With some films however, ascorbate and acetaminophen responses were not decreased and the
hydrogen peroxide response was significantly
increased compared with that of the bare elec-
20
1.0
0
04
08
12
I6
Modified electrode responses expressed as % of unmodified
response to each analyte (0.1 mM)
Phenol
Acetaminophen
Dopamine
1,4-Dihydroxybenzene
1,3-Dihydroxybenzene
1,2-Dihydroxybenzene
Hydrocaffeic acid
4-Aminophenol
1,3,5
Trihydoxybenzene
1,2,3
Trihydoxybenzene
834
24
Fig. 2. Responses of hydrogen peroxide at uncoated
and 4-AP coated Pt anode (+0.85V vs. Ag/AgCl, pH
7.4, electrode overlaid by dialysis membrane).
TABLE 1 Effects on electrode responses of 1-h duration electropolymerisation
from 5 mM solution (+0.85 V vs. Ag/AgC1, pH 7.4, electrode overlaid by dialysis
membrane).
Modifier
2C
[H2021 (m~Al
Ascorbate
Acetaminophen
Hydrogen
peroxide
4Aminophenol
0.13
2
2
95
21
70
99
54
70
0.12
60
30
121
84
143
148
100
156
26
90
146
182
177
179
167
205
223
25
75
96
105
107
120
135
107
123
94
94
140
119
Biosensors & Bioelectronics
ation. Phenol red appeared to discriminate on
the basis of solute charge, such a resolution of
solute diffusion is shown for 0.1 mM solutions
of hydrogen peroxide and interferents at an
electrode modified by a 24 h electropolymerisation period (Fig. 3). The results clearly show
that acetaminophen, a neutral species, and 4-AP
a cation at pH 7.4, permeate freely through
phenol red whereas anionic ascorbate does not.
Baseline currents obtained after extensive phenol
red polymerisation were higher than that with
phenol films.
An electrode modified by a phenol red polymeric layer following extensive polymerisation
could still be further modified by the subsequent
electropolymerisation of phenol. However phenol
red could not be deposited after a phenol film
had formed. The former produced a dual film
modified electrode (Fig. 4), where response to
hydrogen peroxide is exceptionally high but
response to ascorbate and acetaminophen are
both reduced substantially, though not to the
extent found with 4-AP/phenol dual coatings - H202 ascorbate being 139:1 for the phenol red/
phenol whereas a ratio of 346:1 was found for
4-AP/phenol, despite the H202 response for
phenol red/phenol being larger by a factor of
two.
500400-
300-
Response(nA)
200-
Modification of enzyme electrode properties
ELECTRODE RESPONSES FOR SUCCESSIVE PHENOL RED AND PHENOL
800 ~
I
750 ~
I
,oot
650
,-%
J
i
"-°°°t
~
Hydrogen peroxide
"~550
o~.250 T
J,~
I,
Ace,tammophen
rr200
~o I ~
'°°1
O
I
ll~
~
......... I \
20
40
60
80
100
T i m e {rain)
Phenol red coating
I Phenol coating
Fig. 4. Electrode responses during interrupted coating
of phenol, after initial phenol red coating (+0.85V
vs. Ag/AgCI, p H 7.4, electrode overlaid by dialysis
membrane, 0.1 mM solutions).
A series of surfactants were included in the
prepolymer solution in order to achieve possible
co-entrapment of high molecular weight surfactant for film modifying. Whether for charged or
neutral surfactants there was little or no significant
effect on permeability of coatings towards the
model charged/neutral diffusing species (Table
2). These surfactants did increase polymerisation
time and in the cases of N-dodecyl-n, N-dimethyl3-ammonio-l-propanesulfonate and n-decyl b-Dmaltopyranoside totally inhibited film formation
(Table 2). This effect was likely to be the result
of surface adsorption of surfactant on the anode
because in the case of cholic acid exposure
of the electrode to surfactant prior to phenol
electropolymerisation led to identical I-t profiles.
Interestingly addition of cyclodextrin enabled
discrimination of ascorbate and urate (Table 2).
Enzyme electrode studies
100-
0-
8
Fig. 3. Responses at a Pt anode (+0.85V vs. Ag/AgCI,
pH 7.4, electrode overlaid by dialysis membrane), to
0.1 mM solutions after coating of anode by 24-h
exposure to 5 mM phenol red (+0.85V vs. Ag/AgCI,
pH 7.4, electrode overlaid by dialysis membrane).
(a) Enzyme/membrane laminate
Because of the enhanced hydrogen peroxide responsiveness of 4-AP modified
electrodes, these were chosen for use with
subsequent prolonged phenol electropolymerisation in order to effect selectivity.
Table 3 shows favourable selectivity
towards glucose when an enzyme laminate
is placed above the films, compared with
an electrode with only a phenol film,
comparison is also shown for a more
conventional enzyme electrode with the
835
S. Eddy et al.
Biosensors & Bioelectronics
TABLE 2 Effect on phenolic film formation of the present of modifier species in
the prepolymer solution. Responses after 1-h electropolymerisation (+0.85 V vs.
Ag/AgCI pH 7.4).
Modified electrode responses expressed as % of unmodified
response to each analyte (0.1 mM)
Modifier
Cyclodextrin
Deoxycholic acid
Cholic acid
N-Dodecyl-N,Ndimethyl-3-ammonio-1propanesulfonate
n-decyl/3-dmaltopyranoside
Ascorbate
Acetaminophen
Hydrogen
peroxide
Urate
7
41
11
103
20
39
2.6
107
20
77
26
104
138
10
8
99
91.5
106
107
94
TABLE 3 Selectivity ratios of glucose biosensors for
1 mM solutions acetaminophen, ascorbate and 5 mM
glucose.
Selective barrier
Glucose :
Acetaminophen
Cellulose acetate
Electropolymerised
phenol
Electropolymerised 4Aminophenol then
phenol
(b) Enzyme in electropolymerised film
Enzyme could be entrapped in both single
4-AP and double layer (4-AP and phenol)
(Fig. 6) films on electrodes. A very rapid
initial linear response phase was found,
decaying to a reduced but finite slope after
approximately 12 s. These kinetics were
seen with all enzyme electrodes, irrespective of phenolic monomer, single or double
layers, where the enzyme was entrapped
in electropolymerised film. For the conventional electropolymerisation of phenol
Glucose :
Ascorbate
2:1
100 : 1
100 : 1
30 : 1
>600 : 1
>600 : 1
(a)
enzyme immobilised between preformed,
polymeric microporous polycarbonate and
cellulose acetate membranes (laminates
shown in Fig. 5). Table 3 shows the
selectivity of the dual electropolymerised
film structures for glucose vs. ascorbate
and acetaminophen. For both latter species
selectivities were superior to a conventional
cellulose acetate membrane.
001urn PCM
001pro PCM
Enzyme
Enzyme
Cellulose acetate
Electrode
0 01!ira PGM
Enzyme
0 05#m PCM
0 05urn PCM
Phenol coating
Phenol coating
II
4-AP coating
E~ectrode
Electrode
Fig. 5. Membrane and film structures of enzyme electrodes for glucose.
836
40
30
c
(b)
2o
lO
0
~
0
4
-,
8
i
,
,
12
16
20
Time (sec)
Fig. 6. Current vs. time profiles for (a) 20 mM and
(b) 10 mM glucose. Enzyme entrapped in 4-AP film
with subsequent phenol polymerisation (no covering
membrane). Maximum rates of response 2300 and
1200 nA/min, respectively.
Biosensors & Bioelectronics
Modification of enzyme electrode properties
the presence of FAD in the cell chamber at
neutral pH. This resulted in a calibration curve
for glucose very similar to that seen before
exposure to acid pH, with also the same time
dependent behaviour. No change in ascorbate
and acetaminophen exclusion was noted after
acid treatment and similarly the permeability of
the enzyme/phenol film towards H202 remained
unchanged.
3(10
250200Response (after 5rain nA)
150100500
0
1'0
2'0
3'0
4'0
50
IGlucosel (mM)
DISCUSSION
Fig. 7. Responses to glucose obtained with glucose
oxidase entrapped within a phenol film, either before
(n = II) or after (m = 0), exposure to p H 2 phosphate
buffer (+ 0.85V vs. Ag/AgCl, p H 7. 4 phosphate buffer).
alone in the presence of GOx, an arbitrary
5 min current was used to construct the
calibration curve shown in Fig. 7.
The effect of solution pH on the behaviour of
the phenol entrapped enzyme system was also
investigated; Fig. 8 (n = II) shows the pH profile
between pH 2-8. The optimum pH was 6.
However if the enzyme electrode was pre-exposed
for 5-15 min to pH 2 buffer, the pH curve was
altered with no apparent optimum observed (Fig.
8 (m = O). The signal to 10 mM glucose remained
constant between pH 3 to pH 8. Furthermore
the stir dependence of the electrode was entirely
eliminated. Lost activity could be regained by
300
250200Response (nA)
15010050-
o!
i
i
i
i
3
4
5
6
pH
Fig. 8. Response to 10 m M glucose at different p H
values (n = II) before and (m = (3) after the electrode
incorporating Gox in a phenol film was exposed to p H
2 phosphate buffer (+0.85V vs. Ag/AgCI).
Electropolymerised film studies
The non-conductive polymer film formed on
electrode surfaces imparts advantageous characteristics which can be influenced by use of the
appropriate phenol derivative. That is, basic
phenol films give a degree of selectivity against
electroactive species such as ascorbate and acetaminophen which is thought to be predominantly
via a size exclusion effect (Christie & Vadgama,
1993) more so than charge exclusion. In contrast
amino phenols and di-phenolics are less selective,
probably due to a more porous structure related
to polymer branch chain formation. Where
additional enhancement of the response to hydrogen peroxide occurs (Fig. 2), this phenomenon
may be explained by modification of the platinum
oxide by the presence of the phenolic coating
(Christie et al., in press). Hydrogen peroxide
anodic reactions have been reported to be strongly
influenced by the nature of the platinum oxide
layer (Conway & Novak, 1979).
Films formed from phenol red (tri-aromatic)
show generally greater responses to hydrogen
peroxide than phenol. In addition phenol red
films were also found to discriminate between
acetaminophen and anionic ascorbate. This selectivity probably resides in the cationic nature of
the polymer film. The porous nature of phenol
red polymer permits the formation of dual films
with probably the phenol monomer being able
to freely permeate to the underlying platinum
electrode enabling a further polymerisation reaction. Phenol red/phenol film combinations demonstrated much of the selectivity of the basic
polyphenol but also had the maintained hydrogen
peroxide response attributed to the phenol red
polymer. Such characteristics may be due to the
formation of a less dense phenol film as a
consequence of an open phenol red structure.
837
S. Eddy et al.
Enzyme electrode studies
The co-immobilisation of GOx during the polymerisation process is favoured due to the mild
reaction conditions employed (Bartlett & Cooper,
1993). It is reasonable to assume that GOx
enzyme is located within the film at multiple
depths in the polyphenol matrix and the surface.
Upon exposure of the enzyme electrode to acidic
solutions the surface G O x becomes inactivated
which permits dominance of the internal matrix
entrapped GOx. The inner polymer matrix
located enzyme is clearly protected from H ÷,
indicated by the p H independence (Fig. 8), and
by its survival in pH 2 solution. The response in
this instance is comparable to that observed with
GOx immobilised in membrane laminates, being
steady state and stir-independent (Vadgama,
1990). The deactivation of surface enzyme may
be marginally due to denaturation but loss of the
prosthetic group is the most probable important
factor; indeed exposure to pH 2 is the basis for
the formation of apo-GOx (Bergmeyer, 1985).
The lack of proton permeability in GOx loaded
phenolic films contrasts access to glucose, this
therefore warrants further study, and suggests
phenol may have some charge discriminating
properties when the film is formed in the presence
of enzyme. Any contribution to extended operational lifetime as a result of enzyme protection
from adverse bulk solution matrices remains to
be ascertained.
CONCLUSION
This study has illustrated the ease with which
polyphenol (and derivatives) can modify electrodes that demonstrate responses that are selective, yet exceptionally fast, and of magnitude
similar to that of the bare electrode. The electrodes are also stir independent and immune
from pH changes. Non-conducting films provide
an alternative to standard polymeric membranes
with the advantageous one step process of enzyme
immobilisation.
ACKNOWLEDGEMENT
The authors wish to express their gratitude to
EPSRC for their generous financial support
during this study.
838
Biosensors & Bioelectronics
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