Upload
s-sharma
View
216
Download
2
Embed Size (px)
Citation preview
Tropical Medicine and International Health
volume 3 no 1 pp 46–51 january 1998
© 1998 Blackwell Science Ltd46
Secretory acetylcholinesterase of Setaria cervi microfilariae andits antigenic cross-reactivity with Wuchereria bancrofti
S. Sharma, S. Misra and S. Rathaur
Department of Biochemistry, Faculty of Science, Banaras Hindu University, Varanasi, India
Summary Setaria cervi, a bovine filarial parasite, secretes acetylcholinesterase during in vitro cultivation. A significant
amount of enzyme activity was detected both in culture media and somatic extracts of different
developmental stages of the parasite. The microfilarial stage showed a higher level of AChE activity than
adult worms, with females being considerably more active than males. The secretory enzyme from
microfilariae preferentially utilized acetylthiocholine iodide as substrate and showed two electrophoretically
distinct isoforms in native PAGE. Secretory enzyme was purified from the excretory/secretory products of
microfilariae using edrophonium chloride linked to epoxy-activated sepharose. Analysis of purified
acetylcholinesterase by SDS-PAGE revealed the existence of two proteins of 75kD and 45kD under non-
reducing conditions. These secretory enzymes are antigenic and cross-reactive with Wuchereria bancrofti-
infected asymptomatic microfilaraemic human sera when tested by enzyme linked immunosorbent assay and
immunoblotting. The secretory AChE(s) from S. cervi microfilariae may be utilized for diagnosis of early
filarial infections.
keywords AChE, S. cervi, W. bancrofti, diagnosis
correspondence Dr. S. Rathaur, Department of Biochemistry, Faculty of Science Banaras Hindu
University, Varanasi-221 005, India
Introduction
The secretion of acetylcholinesterase (AChE) by nematode
parasites is well established (Rhoads 1981). A number of
filarial parasites release AChE into the culture medium when
maintained in vitro (Rathaur et al. 1987, 1992b), representing
an active secretory process. Setaria cervi, a bovine filarial
parasite homologous with Wuchereria bancrofti (Kaushal et
al. 1987), releases a significant amount of AChE during in
vitro culture. However, the role of secretory AChE is still
speculative (Rhoads 1984, Lee 1996).
The success of serological diagnosis with
excretory/secretory (ES) antigens in several parasitic
infections, e.g. Toxocara canis (Hogarth-Scott 1966, Brunello
et al. 1986) prompted substantial recent interest in the use of
ES antigens for serological diagnosis of lymphatic filariasis
and onchocerciasis. Microfilarial, L3 or adult ES antigens have
been used in the diagnosis of bancroftian (Harinath et al.
1984, Malhotra & Harinath 1984) and brugian filariasis by
Kaushal et al. (1984). There have been several reports of
experiments detecting circulating antigens in filarial
infections using polyclonal (Hamilton et al. 1984) and
monoclonal antibodies (Dissanayke et al. 1984, Sutanto et al.
1985). Recently, circulating parasite AChE was detected in
human filariasis (Rathaur et al. 1992a, Misra et al. 1993).
Detection of antibodies against ES antigens, together with
identification of circulating parasite ES product, may in
combination provide the best serological test for diagnosis of
filarial infections.
We purified AChE from the microfilarial excretory/
secretory product and studied its cross-reactivity with
W. bancrofti infection. Secretory AChE from S. cervi
microfilariae (mf) cross-reacted with the W. bancrofti-
infected asymptomatic microfilaraemic human sera as studied
by ELISA and immunoblotting. We suggest that the detection
of AChE antibodies or circulating AChE using S. cervi AChE
antigen or antibody could be used for the diagnosis of early
filarial infection.
Materials and methods
Acetylthiocholine iodide (ATCH). butyrylthiocholine iodide
(BTCH). eserine. edrophonium chloride, epoxy-activated
sepharose 6B, anti-human immunoglobulin peroxidase
Tropical Medicine and International Health volume 3 no 1 pp 46–51 january 1998
S. Sharma et al. Antigenic cross-reactivity of Setaria cervi and Wuchereria bancrofti
© 1998 Blackwell Science Ltd 47
conjugate, orthophenylenediamine chromogen (OPD) and
diaminobenzidine hydrochloride (DAB) were purchased from
Sigma (St. Louis, MO, USA). All other chemicals used were of
analytical grade purity.
Adult S. cervi were recovered from the peritoneal folds of
freshly slaughtered water buffaloes. Worms were washed with
saline and stored in Krebs Ringer bicarbonate buffer
supplemented with 1% glucose, 100 mg/ml penicillin, 100
mg/ml streptomycin and 2mm fresh glutamine. Microfilariae
(mf) were obtained by dissecting the distal portion of the
uterus of adult females and incubated with supplemented
KRB buffer for 2 h at 37 8C under sterilized conditions for the
collection of ES products. For enzymatic studies, pooled ES
material was concentrated 4–5 times and dialysed against
0.1M phosphate buffer pH 7.6 at 4 8C. Worm extract was
prepared by homogenizing adult worms at 4 8C in PBS pH
7.6, centrifuging at 10,000 3 g and recovering the clear
supernatant. Microfilariae were sonicated using a MSE150W
ultrasonic disintegrator MK2 at 20 KC for 15 min with 2 min
interval after every 2 min in cold PBS pH 7.6. Protein
estimation was done by the method of Lowry (1951).
Acetylcholinesterase was assayed according to the method of
Ellman et al. (1961), with ATCH and BTCH as substrates.
The ES enzyme was resolved under non-denaturing
conditions by electrophoresis in 6% polyacrylamide gels in
Tris-borate EDTA (TBE) buffer pH 8.0 and enzyme activity
detected according to the direct colouring thiocholine method
of Karnovsky & Roots (1964).
W. bancrofti-infected human sera were collected from
Chiraigaon, an endemic area near Varanasi (India). Filarial
cases were divided into asymptomatic microfilaraemic (mf
carrier) and symptomatic amicrofilaraemia (elephantiasis).
Of the total population in Chiraigaon, 8% were found to be
asymptomatic microfilaraemic. Sera were collected from 25
such patients aged 20–45 years with 200–300 mf/mm3 of
blood. Healthy persons devoid of any infections living in the
endemic area were treated as endemic normal and those
living in a non-endemic area as non-endemic normal. Serum
was separated by keeping the blood at 4 8C for a few hours
and centrifuged at 10,000 rpm for 20 min in a refrigerated
centrifuge and stored at 270 8C till further use.
For the purification of acetylcholinesterase by affinity
chromatography, edrophonium sepharose was prepared
according to the method of Hodgson and Chubb (1983) and
washed in sequence with 10 volumes each of 0.1m sodium
acetate pH 4.5, 0.012 m sodium borate pH 10.0 and distilled
water. A 5ml column was prepared at 4 8C and the flow rate
adjusted to 12ml/h. Concentrated ES (5 mg) from S. cervi mf
was applied and the column sequentially washed with 50 mmphosphate buffer pH 8.0 and 50mm phosphate buffer
containing 0.5 m NaCl. Bound AChE was eluted with 50 mmphosphate buffer containing 0.5 m NaCl and 12 mmedrophonium chloride. Fractions of 2 ml were collected and
edrophonium removed by dialysis against 5 3 1 litre changes
of phosphate buffer pH 8.0 prior to the enzyme and protein
assays. Homogeneity of enzyme active peak fractions was
checked by 10% SDS-PAGE and silver staining of an aliquot
of the sample.
ELISA was performed following the procedure of Rathaur
et al. (1987). NUNC plates were coated with 2 mg/ml of
affinity purified enzyme and incubated overnight at 40 8C,
followed by the addition of 1:100 dilution of W. bancrofti-
infected asymptomatic microfilaraemic human sera as
antibody and anti-human IgG peroxidase conjugate (1:4000
dilution). Immunoblotting of secretory AChE was performed
according to Lunde et al. (1988) utilizing infected human sera
as antibody (1:20 dilution) and anti-human IgG peroxidase
conjugate (1:1000). Bands were stained by carrying out DAB
reaction.
Results and discussion
Our study demonstrates that both adult and microfilarial
stages of S. cervi contain acetylcholinesterase activity. Mf
secrete several forms of the enzyme actively when maintained
in vitro. Table 1 shows the specific activity of AChE in
extracts of adult worms, mf and ES product of the
microfilarial stage. On the basis of units/mg of protein, mf of
Enzyme activity Specific activity
Stage (units/ml) (units/mg)
Adult male 0.0275 6 0.005 0.0100 6 0.005
Adult female 0.1393 6 0.032 0.0366 6 0.0025
mf 1.4016 6 0.120 0.2922 6 0.021
ES product 0.2446 6 0.008 0.0466 6 0.001
The enzyme activity was measured according to the procedure of Ellman et al. (1961), using
ATI as substrate with 1 enzyme unit being expressed in mmoles of substrate hydrolysed per
minute. The data represent mean values 6 SD for 5 different determinations.
Table 1 AChE activity in adult worm
homogenate, microfilarial extract and
microfilarial ES product of S. cervi
Tropical Medicine and International Health volume 3 no 1 pp 46–51 january 1998
S. Sharma et al. Antigenic cross-reactivity of Setaria cervi and Wuchereria bancrofti
© 1998 Blackwell Science Ltd48
S. cervi showed significantly higher activity than the adult
stage, with females being considerably more active than male
worms. The secretory AChE from mf preferentially utilized
ATCH over BTCH as substrate (data not shown). Greater
AChE activity per unit weight of protein in female worm
extracts than in males confirms the reported heterogeneity
between species (Rathaur et al. 1987).
We observed a considerable quantitative difference between
developmental stages, with microfilariae showing
approximately 8 times the activity of female adults. Similarly,
Hemonchus contortus larvae (Hart & Lee 1966), Brugia
malayi mf (Rathaur et al. 1987) and fourth-stage larvae of
Trichostrongylus colubriformis and Oesophagostomum
radiatum (Ogilvie et al. 1973) also show greater AChE
activity than adults. Lawrence & Pritchard (1993) found that
Heligmosomoides polygyrus secreted AChE with maximum
production of the enzyme occurring in the secretions from
the fourth-stage larvae. In contrast to this, there is marked
increase in enzyme activity of Nippostrongylus brasiliensis
during development.
The nematode secretory cholinesterases characterized so
far are either present as a single protein (Rothwell et al. 1973)
or in multiple molecular forms as in N. brasiliensis.
Blackburn & Selkirk (1992) showed that the
excretion/secretions of adult N. brasiliensis contain 3 major
forms of AChE and these were equivalent to forms A, B and
C identified by Edwards et al. (1971); 2 minor forms of AChE,
B1 and B2 were also sometimes present. McKeand et al.
(1994b) demonstrated that adults of the cattle lungworm
Dictyocaulus viviparus secrete 5 isoforms of the enzyme. In
our case, microfilarial secretory AChE resolved into two
distinct bands under 6% non-denaturing gel electrophoresis,
suggesting that S. cervi mf secrete at least two electromorphic
variants of AChE (data not shown).
The purification of AChE on edrophonium sepharose was
effected using the conditions described in Materials and
Methods with 53-fold enrichment of enzyme activity and
relatively low recovery of 9%. The loss in enzyme activity
may be attributed to dialysis during desalting of peak
fractions, as AChE is unstable to physical processes. The
purification of AChE from other parasites using this method
has been achieved with Necator americanus by Pritchard et
al. (1991) and T. colubriformis by Griffith & Pritchard
(1994).
Unfractionated microfilarial ES, detected using non-
reducing 10% SDS-PAGE on silver staining, shows several
bands ranging from 15 to 200 kD (Figure 1). The purified
enzyme from the edrophonium column was resolved only in
two proteins: a major component of 45kD and a very faint
band of 75 kD. Similar results have been found in other
invertebrates. Blackburn & Selkirk (1992) found isoforms of
AChE of 74 kD and 39 kD, both secreted by 4-day-old
worms, but there was a switch to predominant secretion of
the 39 kD form by day 8 of infection. They suggested that
this change may be related to maturation of the nematodes.
Nakazawa et al. (1995), with SDS-PAGE under non-reducing
conditions, detected only a 74 kD form of the enzyme in the
E/S of adult Nippostrongylus.
Cross-reactivity with heterologous antigens is common in
many tropical diseases (Kaliraj et al. 1979) but the degree of
specificity describes the suitability of such an antigen in
detecting the disease by immunological methods. Using
techniques of diagnostic potential, such as ELISA and
immunoblotting, circulating parasite antigens have been
detected in both human (Dasgupta et al. 1984, Hamilton et
al. 1984, Sugunan & Kaleysa Raj 1990) and animal
(Dasgupta et al. 1984) filariasis by polyclonal sera. In
humans, AChE activity has been found in immune complexes
obtained from filarial patients (Rathaur et al. 1992a).
Espinoza et al. (1988) reported antibodies against
Schistosoma AChE in the sera of mice and of human patients
infected with this parasite. McKeand et al. (1994a)
demonstrated that sera from calves infected naturally and
experimentally with D. viviparus contained antibodies which
Figure 1 Purification of S. cervi microfilarial secretory
acetylcholinesterase. Samples were run on 10% SDS-PAGE and silver-
stained. A, Fraction unabsorbed on edrophonium sepharose column;
B, crude ES originally loaded on column; C, AChE fraction eluted
with edrophonium chloride from same column.
Tropical Medicine and International Health volume 3 no 1 pp 46–51 january 1998
S. Sharma et al. Antigenic cross-reactivity of Setaria cervi and Wuchereria bancrofti
© 1998 Blackwell Science Ltd 49
specifically recognized secretory AChE of the adult parasite.
Secretory acetylcholinesterase purified from S. cervi
microfilarial ES, when reacted with W. bancrofti-infected
asymptomatic microfilaraemic human sera, showed
significantly higher activity in ELISA than endemic and non-
endemic normals (Figure 2). The mean OD of 10 non-
endemic normal sera evaluated was 0.127 (SD 5 0.017), so
the values above 0.161 were considered to have significantly
greater reactivity towards the secretory AChE in ELISA. The
mean OD for the endemic normal (n 5 10) was 0.183 (SD 5
0.010), which is slightly higher than normal. Significantly
higher reactivity was observed for human microfilaraemic
sera; the mean OD for 10 sera was 0.505 (SD 5 0.042). These
results clearly indicate that the AChE from S. cervi
microfilarial secretion is cross-reactive to W. bancrofti-
infected human sera and showed more than 3 times greater
activity than sera from non-filarial healthy humans. This
cross-reactivity of secretory AChE from S. cervi microfilariae
against sera from human filarial patients is in accord with the
view that homologous antigens are produced by related
species – as in this case between S. cervi and W. bancrofti.
Similar cross-reactivity has been shown by Sugunan and
Kaleysa Raj (1990) by S. digitata ES antigen.
Evidence for cross-reactivity was further provided by
immunoblotting. To check the cross-reactivity, we examined
the binding of W. bancrofti-infected human sera to the S.
cervi secretory AChE by immunoblotting. As shown in Figure
3, IgG antibodies in infected human sera recognized 45 kD
and 75 kD proteins specifically. Ott et al. (1975) and
Rosenberry (1977) reported that catalytic subunits of AChE
are typically around 75–80kD. Nakazawa et al. (1995)
reported that in immunoblotting analysis of ES product of N.
brasiliensis, a 74 kD AChE molecule is recognized by IgE and
IgG antibodies in nematode-infected rat sera. A report by
Blackburn & Selkirk (1992) showed that N. brasiliensis
secretory AChEs fall in two distinct proteins of 39 & 74 kD
with a high degree of structural identity, which appear to
derive from a single primary translation product. All AChEs
Figure 2 Reactivity of S. cervi secretory AChE in ELISA with
endemic normal (EN), non-endemic normal (NEN) sera and
W. bancrofti-infected asymptomatic microfilariaemic human sera
(Inf) from Chiraigaon (India). Horizontal bars represent mean OD
and dashed line indicate normal. Number of sera in each case was
10.
Figure 3 Immunoblot analysis of the affinity purified secretory
AChE of S. cervi mf. The purified enzyme was run on 10% SDS-
PAGE and transferred onto a nitrocellulose membrane. The
membrane was incubated with normal (Lane A) and W. bancrofti-
infected asymptomatic microfilaraemic human sera (Lane B). The
membrane was then incubated with anti-human IgG peroxidase
conjugate and the DAB reaction was carried out.
Tropical Medicine and International Health volume 3 no 1 pp 46–51 january 1998
S. Sharma et al. Antigenic cross-reactivity of Setaria cervi and Wuchereria bancrofti
reported so far are heavily glycosylated and this could
account for the multiple isoforms seen under non-denaturing
PAGE, particularly as differing carbohydrate side-chains are
known to account for the 5 electrophoretically variant forms
of human enythrocyte AChE (Ott et al. 1975). Selkirk &
Blackburn (1992) proposed that resistance of native N.
brasiliensis AChE to trypsin digestion may be due to
extensive glycosylation.
Recognition of S. cervi secretory AChEs by W. bancrofti-
infected asymptomatic microfilaraemic human sera suggests
that clear cross-reaction between the two genera and the
recognition of this enzyme may be an interesting component
of the immune response in natural infection. Naturally
evoked serum antibodies to parasitic cholinesterase have also
been observed in animal infections with N. brasiliensis (Jones
& Ogilvie 1972), O. radiatum (Bremner et al. 1973),
Stephanurus dentatus (Massouli & Bon 1982) and in the
serum of infected humans. This cross-reactivity might be the
result of the presence of a common antigenic determinant
such as the carbohydrate moiety of these glycoprotein
enzymes or a common tertiary or quarternary structure of
the enzyme in the two species (Tarrab-Hazdai et al. 1984).
The conservation of AChE secretion among parasitic
helminths is indicative of an important role in the host-
parasite relationship. Lee (1996) proposed that these secretory
AChEs from parasitic nematodes may have an important role
in modulation of the host’s inflammatory and/or immune
response. Further experimental investigations are required for
assessing the role of S. cervi microfilarial secretory AChE in
the host-parasite relationship. In order to evaluate the
diagnostic potential of S. cervi secretory AChE under field
conditions in early filarial infections, work is in progress to
identify its amino-acid sequence, which could then be used to
produce recombinant protein.
Acknowledgements
S. Sharma is grateful to UGC (GATE) and S. Misra thanks
CSIR for providing financial assistance.
References
Blackburn CC & Selkirk ME (1992). Characterization of the
secretory acetylcholinesterases from adult Nippostrongylus
brasiliensis. Molecular and Biochemical Parasitology 53, 79–88.
Bremner KC, Ogilvie BM, Keith RK & Berrie DA (1973).
Acetylcholinesterase secretion by parasitic nematodes III.
Oesophagostomum spp. International Journal for Parasitology 3,
609–618.
Brunello F, Falagiani P, Genchi C & Ospedale S (1986). ELISA for the
detection of specific immunoglobulin antibodies to Toxocara canis
excretory antigens. Bulletin dell Instituto Sieroterapico Milanese
65, 54–60.
© 1998 Blackwell Science Ltd50
Dasgupta A, Bala S & Dutta SN (1984). Lymphatic filariasis in man:
demonstration of circulating antigen in W. bancrofti infection.
Parasite Immunology 6, 341–348.
Dissanayake S, Forsyth KP, Ismail MM & Mitchell GE (1984).
Detection of circulating antigen in bancroftian filariasis by using a
monoclonal antibody. American Journal of Tropical Medicine and
Hygiene 33, 1130–1140.
Edwards AJ, Burt JS & Ogilvie GM (1971). The effect of host
immunity upon some enzymes of the parasitic nematode
Nippostrongylus brasiliensis. Parasitology 62, 339–347.
Ellman GL, Courtney KD, Andres V & Featherstone RM (1961). A
new and rapid colorimetric determination of acetylcholinesterase
activity. Biochemical Pharmacology 7, 88–95.
Espinoza B, Tarrab-Hazdai R, Silman I & Arnon R (1988).
Acetylcholinesterase in Schistosome mansoni is anchored to the
membrane via covalently attached phosphatidylinositol. Molecular
and Biochemical Parasitology 29, 171–179.
Griffiths G & Pritchard DI (1994). Purification and biochemical
characterization of AChE from the excretory/secretory products of
Trichostrongylus colubriformis. Parasitology 108, 579–586.
Hamilton RG, Hussain R & Ottesen EA (1984). Immunoradiometric
assay for detection of filarial antigen in human sera. Journal of
Immunology 133, 2237–2242.
Harinath BC, Malhotra A, Ghirnikar SN, Annadate SD, Isaacs VP &
Bharti MS (1984). Field evaluation of ELISA using Wuchereria
bancrofti mf ES antigen for bancroftian filariasis. Bulletin of the
World Health Organization 62, 941–944.
Hart RJ & Lee RM (1966) Cholinesterase activities of various
nematode parasites and their inhibition by the organophosphate
anthelmintic Haloxon. Experimental Parasitology 18, 332–337.
Hodgson AJ & Chubb IW (1983). Isolation of the secretory form of
soluble acetylcholinesterase using affinity chromatography on
edrophonium sepharose. Journal of Neurochemistry 41, 654–662.
Hogarth-Scott RS (1966). Visceral Larval migrans – an immuno-
fluorescent examination of rabbit and human sera for antibodies
to the ES antigen of the second stage larvae of Toxocara canis,
Toxocara cati and Toxascaris leonina (Nematoda). Immunology
10, 217–233.
Jones VE & Ogilvie BM (1972). Protective immunity to
Nippostrongylus brasilensis in rat III. Modulation of worm
acetylcholinesterase by antibodies. Immunology 22, 119–129.
Kaliraj P, Ghirnikar SN & Harinath BC (1979). Detection of
circulating filarial antigen in bancroftian filariasis. Indian Journal
of Experimental Biology 17, 1148–1149.
Karnovsky MJ & Roots L (1964). A direct colouring thiocholine
method for cholinesterases. Journal of Histochemistry and
Cytochemistry 12, 219–221.
Kaushal NA, Hussain R & Ottesen EA (1989). Excretory/secretory
and somatic antigens in the diagnosis of human filariasis. Clinical
and Experimental Immunology 56, 567–576.
Kausahl NA, Kaushal DC & Ghatak S (1987). Identification of
antigenic proteins of Setaria cervi by immunoblotting technique.
Immunological Investigations 16, 139–149.
Lawrence CE & Pritchard DI (1993). Differential secretion of
acetylcholinesterase and proteases during the development of
Heligmosomoides polygyrus. International Journal for
Tropical Medicine and International Health volume 3 no 1 pp 46–51 january 1998
S. Sharma et al. Antigenic cross-reactivity of Setaria cervi and Wuchereria bancrofti
© 1998 Blackwell Science Ltd 51
Parasitology 23, 309–314.
Lee DL (1996). Why do some nematode parasites of the alimentary
tract secrete acetylcholinesterase? International Journal for
Parasitology 26, 499–508.
Lowry OH, Rosebrough NJ, Farr AL & Randall RJ (1951). Protein
measurement with the Folin-phenol reagent. Journal of Biological
Chemistry 193, 265–275.
Lunde ML, Paranjape R, Lawley TJ & Ottesen EA (1988). Filarial
antigen in circulating immune complexes from patients with
Wuchereria bancrofti filariasis. American Journal of Tropical
Medicine and Hygiene 38, 366–371.
Malhotra A & Harinath BC (1989). Comparative efficiency of
Wuchereria bancrofti microfilarial and larval excretory/secretory
antigens in ELISA for the diagnosis of tropical eosinophilia and
bancroftian filariasis. Indian Journal of Experimental Biology 22,
520–522.
Massoulie J & Bon S (1982). The molecular forms of cholinesterase
in vertebrates. Annual Review of Neuroscience 5, 366–371.
McKeand JB, Knox DP, Duncan JL & Kennedy W (1994a). Genetic
control of the antibody repertoire against excretory/secretory
products and acetylcholinesterases of Dictyocaulus viviparus.
Parasite Immunology 16, 251–260.
McKeand JB, Knox DP, Duncan JL & Kennedy W (1994b). The
immunogenicity of the acetylcholinesterase of the cattle
lungworm, Dictyocaulus vivparus. International Journal for
Parasitology 24, 505–510.
Misra S, Mohapatra TM & Rathaur S (1993). Identification of
parasitic acetylcholinesterase in microfilariae infected human
serum. Tropical Medicine Parasitology 44, 75–78.
Nakazawa M, Yamada M, Uchikawa R & Arizono N (1995).
Immunocytochemical localization of secretory acetylcholinesterase
of the parasitic nematode Nippostrongylus brasiliensis. Cell and
Tissue Research 280, 59–64.
Ogilvie BM, Rothwell TLW, Bremner KC, Schnitzerling HJ,
Nolan J & Keith RK (1973). Acetylcholinesterase secretion by
parasitic nematodes: I Evidence for secretion of the enzyme by a
number of species. International Journal for Parasitology 3,
589–597.
Ott P, Jemmy B & Brodbeck U (1975). Multiple molecular forms of
purified human erythrocyte acetylcholinesterase. European
Journal of Biochemistry 57, 469–480.
Pritchard DI, Leggett KV, Rogan MT, McKean PG & Brown A (1991)
Necator americanus secretory acetylcholinesterase and its
purification from excretory-secretory products by affinity
chromatography. Parasite Immunology 113, 187–199.
Rathaur S, Robertson BD, Selkirk ME & Maizels RM (1987).
Secretory acetylcholinesterase from Brugia malayi adult and
microfilarial parasites. Molecular and Biochemical Parasitology
26, 257–265.
Rathaur S, Muller S, Maizels RM & Walter RD (1992a).
Identification of circulating parasitic acetylcholinesterase in
human and rodent filariasis. Parasitology Research 78, 671–676.
Rathaur S, Misra S, Mohapatra TM & Tancja V (1992b). A
comparative study of acetylcholinesterase activity in bovine (S.
cervi) and human (B. malayi, W. bancrofti) filaria. Lymphology
25, 159–165.
Rhoads ML (1981). Cholinesterase in the parasitic nematode,
Stephanurus dentatus, characterization and sex dependence of a
secretory cholinesterase. Journal of Biological Chemistry 256,
9316–9323.
Rhoads ML (1984). Secretory cholinesterase of nematodes: possible
functions in the host-parasitic relationship. Tropical Veterinarian
2, 3–10.
Rosenberry TL & Richardson JM (1977). Structure of 18S and 14S
acetylcholinesterase. Identification of collagen tailed subunits that
are linked by disulfide bonds to catalytic subunits. Biochemistry
16, 3550–3558.
Rothwell TLW, Ogilvie BM, & Love RJ (1973). Acetylcholinesterase
secretion by parasitic nematodes II. Trichostrongylus spp.
International Journal for Parasitology 3, 599–608.
Sugunan VS & Kaleysa Raj R (1990). Excretory/secretory antigens
from a bovine filarial parasite cross-react with human antifilarial
antibodies. Indian Journal of Experimental Biology 28, 1124–1127.
Sutanto I, Maizels RM & Denham DA (1985). Surface antigens of a
filarial nematode: analysis of adult Brugia pahangi surface
components and their use in monoclonal antibody production.
Molecular and Biochemical Parasitology 15, 203–214.
Tarrab-Hazdai R, Levi-Schaffer F, Gonzalez G & Arnon R (1984).
Acetylcholinesterase of Schistosoma mansoni molecular forms of
the solubilized enzyme. Biochemica Biophysica Acta 790, 61–69.