THYROID
Volume 15, Number 7, 2005
© Mary Ann Liebert, Inc.
Thyroid Sialyltransferase mRNA Level and Activity
Are Increased in Graves’ Disease
Jacek Kiljański,1 Michal Ambroziak,2 Janusz Pachucki,1 Krystian Jaz·dz·ewski,3 Wieslaw Wiechno,4
Elżbieta Stachlewska,5 Barbara Górnicka,6 Magdalena Bogdańska,6 Janusz Nauman1,7 and
Zbigniew Bartoszewicz1,7
[
[
Sialylation of cell components is an important immunomodulating mechanism affecting cell response to hormones and adhesion molecules. To study alterations in sialic acid metabolism in Graves’ disease (GD) we measured the following parameters in various human thyroid tissues: lipid-bound sialic acid (LBSA) content, ganglioside profile, total sialyltransferase activity, and the two major sialyltransferase mRNAs for sialyltransferase-1
(ST6Gal I) and for sialyltransferase-4A (ST3Gal I). Fragments of toxic thyroid nodules (TN), nontoxic thyroid
nodules (NN) and nontumorous tissue from patients with nodular goiter or thyroid cancer were used as a control (C). The LBSA content and sialyltransferase activity were the highest in the GD group (164 ⫾ 4.44 versus
120 ⫾ 2.00 nmoL/g, p ⬍ 0.005 and 1625 ⫾ 283.5 versus 324 ⫾ 54.2 cpm/mg of protein, p ⬍ 0.005 compared to
control group C). Ganglioside profile in the GD group was similar to that in control tissues. Sialyltransferase1 mRNA and sialyltransferase-4A mRNA levels were significantly higher in the GD group than in the control
group (12.52 ⫾ 6.90 versus 2.54 ⫾ 1.24 arbitrary units, p ⬍ 0.005 and 2,49 ⫾ 1.16 versus 1.23 ⫾ 0.46 arbitrary
units, p ⬍ 0.05, respectively). There was a positive correlation between the increased sialyltransferase-1 mRNA
level and the TSH-receptor antibody titer determined by the TRAK test. These results indicate that sialyltransferases expression and activity are increased in GD. Exact mechanism of this upregulation remains unknown,
though one of possible explanations is the activation of the thyrotropin (TSH) receptor.
Introduction
I
t IS WELL KNOWN that altered glycosylation of glycolipids
and glycoproteins affects structure and function of the key
pathogenic elements of many diseases. Similarly, changes in
the amount, linkage, and acetylation of sialic acids were reported in various pathologic conditions (1,2). Sialic acid is
usually the last glycosyl group transferred into glycoconjugates and therefore has a potential for changing protein-toprotein interactions (3). Sialylation of cell components is an
important mechanism for the regulation of immune response
and hormone-receptor interaction (3,4). Gangliosides, sialic
acid containing glycosphingolipids, are structural elements
of such a cell membrane components like receptors and ligands for adhesion molecules. Their impact on differentiation, signal transduction, cell-to-cell communication, im-
munogenicity, neoplastic transformation, and ability to form
metastases has been shown by numerous studies (5–8). However, there are only few studies focusing on sialic acid metabolism in thyroid tissue. Several groups studied thyroid
ganglioside profiles and their role in health and disease.
Most data came from studies on the bovine thyroid (9,10),
yet the ganglioside content and profile of the human thyroid
differs considerably from the bovine (11). Moreover, there is
evidence for the existence of several cell populations of thyroid cells showing a distinct profile of glycosphingolipids
(12). Early studies, based on thyrotropin (TSH) affinity chromatography, suggested that gangliosides were structurally
and functionally an important element of thyrothropin receptor (TSHR) affecting TSH binding and thyrocyte function
(13–18). One may speculate that potential changes of its immunogenicity might modify the course of Graves’ disease.
1Department
of Internal Medicine and Endocrinology, Medical University of Warsaw, Warsaw, Poland.
of Biochemistry, Medical Centre for Postgraduate Medical Education, Warsaw, Poland.
3Department of Hypertension and Diabetes, Medical University of Gdańsk, Gdańsk, Poland.
4Department of General and Thoracic Surgery, Medical University of Warsaw, Warsaw, Poland.
5Division of Endocrine Surgery, Institute of Oncology, Warsaw, Warsaw Poland.
6Department of Pathology, Medical University of Warsaw, Warsaw, Poland.
7Department of Endocrinology, Medical Research Centre, Polish Academy of Science, Warsaw, Poland.
2Department
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646
On the other hand, sialic acid metabolism in the thyroid is
regulated by thyrotropin (19). Sialylation is a late posttranslational modification of thyroglobulin that can affect synthesis and secretion of the thyroid hormone (19) and the thyroid hormone itself may control sialic acid content of various
glycoproteins and glycolipids (20,21).
The synthesis of glycolipids and glycoproteins depends on
the activity of specific glycotransferases. Sialyltransferases
belong to the family of glycotransferases catalysing the transfer of sialic acid from cytidine monophosphosialic acid
(CMP)-sialic acid to terminal position of sugar chains of glycolipids and glycoproteins. The nomenclature of sialyltransferases similarly to other glycotransferases is quite confusing. It is becoming clearer that the rule of one enzyme one
activity is not always obvious (22). Until now more than a
dozen of distinct sialyltransferases have been characterized
and their genes have been cloned in various species (23,24).
Among them sialyltransferase-1 (-galactoside ␣-2,6-sialyltransferase, previously known as ST6Gal I or CD75) and sialyltransferase-4A (-galactoside ␣-2,3-sialyltransferase, previously known as ST3Gal I) are well defined in many species
including humans. Their corresponding human genes were
cloned and named SIAT1 and SIAT4A, respectively. Changes
in their expression and cell distribution in organs, other than
the thyroid, were found in some pathological conditions including: various kinds of cancer (25–28), liver cirrhosis (28),
and von Willebrand disease (29).
The presented results showed that the sialic acid content
and metabolism is altered in Graves’ disease. To analyze
sialic acid metabolism we measured lipid-bound sialic acid
(LBSA), namely, ganglioside content, ganglioside profile, total sialyltransferase activity, and the two sialyltransferase
mRNA levels for sialyltransferase-1 and for sialyltransferase4A. Further studies are needed to address potential effects
of the changes in sialic acid metabolism on thyroid function
and pathophysiology of Graves’ disease.
Material and Methods
Patients and tissue samples
The material consisted of 103 tissue samples obtained from
80 patients (56 females, 24 males; ages 13 to 71, mean, 37
years). Twenty-five specimens came from patients with
Graves’ disease (GD). Twenty-eight samples came from 19
patients with toxic nodular goiter (19 from nodules (TN) and
9 from the nontumorous part of the same thyroid [TC]).
Thirty-six samples came from 22 patients with nontoxic
nodular goiters (22 from benign nodules [NN] and 14 from
the nontumorous surrounding tissue [NC]). Nontumorous
tissues (9 from toxic goiters, 14 from nontoxic nodular goiters, and 14 from patients with thyroid papillary carcinoma)
were used as a control group, C. In some assays this group
was split into subgroups: normal thyroid control tissue coming from toxic nodular goiter (TC) and from nontoxic nodular goiter (NC). All patients were diagnosed on the basis of
physical examination, hormone level measurements (TSH,
free thyroxine [FT4] and free triiodothyronine [FT3]), ultrasonography, iodine scyntygraphy, and/or fine-needle aspiration biopsy of the thyroid nodule if needed. The thyrotropin binding inhibitory immunoglobulin (TBII) level was
measured in some patients with GD using the LumiTest
TRAKhuman kit (Brahms, Hennigsdorf bei Berlin, Germany).
KILJA ŃSKI ET AL.
FT3, FT4, and TSH were measured on the Axsym system automatic analyzer (Abbott Laboratory, Abbott Park, IL) using
Abbott assays based on the microparticle enzyme immunoassay technology. The ultrasensitive hTSH II assay has
analytical sensitivity of 0.03 uIU/mL. Normal value ranges
for FT3 were 1.64 to 3.45 pg/mL, for FT4 were 0.71 to 1.85
ng/dL and for TSH were 0.49 to 4.67 U/mL. The laboratory is controlled by The Randox International Quality Assessment Scheme (RIQAS) of Immunoassay Programme
(Randox Laboratories Ltd, Crumlin, Co., Antrim, UK).
Patients with GD and toxic nodular goiter were treated
before operation with thiamazol (methimazol) and -adrenolitic agent, propranolol in doses 10 to 30 mg or 30 to 160 mg
per day, respectively. The duration of pharmacologic treatment ranged from 3 weeks to 2 months, according to the
amelioration of hyperthyroidism. All but four patients with
GD were treated with iodine solution. They received 170 mg
of iodine daily, 5 to 7 days before thyroidectomy. FT4 level
ranged from 0.76 to 1.87 ng/dL, mean 1.12 (normal range,
0.71–1.85). The TSH level ranged from the value below analytical sensitivity (0.03 uIU/mL) to 4.93 uIU/mL, mean 2.81
(normal range, 0.49–4.67). FT3 ranged from 0.68 to 3.28
pg/mL, mean, 2.84 (normal range, 1.64–3.45). Based on the
clinical signs the patients were euthyroid at the time of surgery.
The study was approved by the Ethical Committee of the
Medical Research Centre of Polish Academy of Sciences.
Tissue preparation for estimation of LBSA, ganglioside,
and sialyltransferase activity
After removal of a thyroid gland, samples were immediately put on ice and transported to a pathologist who selected proper fragments for scientific purposes and for a routine anatomopathologic examination. Tissue samples were
homogenized with 3 volumes of water on ice bath. Homogenates were used for the estimation of the total sialyltransferase activity (ST) and after the addition of the
complete protease inhibitors cocktail (Roche Diagnostics,
Mannheim, Germany) for measurement of protein content
and for extraction of gangliosides. Thyroid gangliosides
were extracted using the following method published by
Svennerholm (11) and Phillips et al. (30). Briefly, tissue lipids
were extracted over 24 hours at 4°C with methanol and chloroform in a final chloroform: methanol: water ratio of 4:8:3.
After centrifugation and reextraction of the pellet (12 hours
at 4°C) combined extracts were evaporated to dryness,
dissolved in a final volume of 20 mL of chloroform: methanol (4:1), sonicated, filtered, and applied to a 5 mL G 60
silica gel columns filled with the same solvent. Gangliosides were eluted with 11 mL of chloroform: methanol: water mixture (3:6:2 by volume). Eluent was subsequently purified on DEAE-Sephadex A-25 columns (BioRad, Hercules,
CA) packed with a mixture chloroform:methanol:water
30:60:8. Acidic lipids were eluted with methanol/0.2 M
NaOAc and solubilized at 37°C in 1 M methanolic NaOH.
The samples were then lyophilized and reconstituted in
water. The solution was acidified with 3 M AcOH to pH
4.5–4.6. Samples were then desalted on Sep-Pak C18
columns (Waters, Milford, MA) (31). Gangliosides were
eluted with methanol and solution chloroform/methanol
2:1. Eluents were dissolved in a small volume of chlo-
SIALYLTRANSFERASES IN GRAVES’ DISEASE
roform:methanol 4:1 and applied to small-volume silica gel
columns (0.5–1.0 mL). Gangliosides were eluted with chloroform:methanol:water 3:6:2. The samples were lyophilized
again, dissolved in chloroform:methanol. 2:1 and used for
thin-layer chromatography (TLC) or measurement of LBSA
content.
Measurement of LBSA content in ganglioside samples
The estimation of LBSA content was based on the method
published by Suzuki et al. (32) modified for small quantities
of material studied. Briefly: ganglioside fractions were
lyophilized and subsequently sonicated in 0.2 mL of distilled
water. Then, 0.4 mL of resorcinol reagent was added and
samples were incubated at 37°C for 15 minutes and cooled
down. Mixture of butyl acetate and n-butanol at an 85:15 ratio was added. After vortexing and centrifugation absorption of the upper phase was measured at 620 nm.
TLC of thyroid gangliosides
TLC was performed along with standards on silica gel
60 glass-backed HPTLC (high-performance thin layer chromotography) plates (Merck, Darmstadt, Germany) suitable
for small samples (nano-TLC) with chloroform:methanol:
aqueous 0.25% CaCl2 60:25:4 or with chloroform:methanol:
aqueous-0.2 % CaCl2 60:40:9. Gangliosides were visualized
with resorcinol reagent and the bands were scanned with a
Shimadzu Model CS-910 dual-wavelength scanning densitometer at 580 nm. Immunostaining of TLC thin-layer plates
(33) was done to confirm identification of ganglioside
FucGM1. Briefly, after pretreatment with 0.1% solution of
polyizobutylmetakrylate in hexane and blocking with 1%
bovine serum albumin (BSA) in phosphate-buffered saline
(PBS) strips of plates were incubated overnight at 4°C with
specific primary antibody dissolved 1:100 in 1% BSA in PBS.
After incubation with peroxidase-linked secondary antibodies (1:500) staining was developed using 4-chloro-1-naphthol.
Total sialyltransferase activity (ST) in tissue samples
The total ST activity in homogenized thyroid tissues was
measured according to Delannoy et al. (34) using [3H] CMPNANA and asialofetuin (Roche Diagnostics) or asialoglycophorin (Sigma, St. Louis, MO) as exogenous acceptors.
Asialofetuin and asialoglycophorin are highly glycosylated
glycoproteins, carrying diversity of N- and O-linked glycans
and both are good high molecular weight acceptors for
␣2-3 (e.g., sialyltransferase-4A), ␣2-6 (e.g., sialyltransferase1) and ␣2-8 sialyltransferases. Incubations were performed
for 1–5 hours at 37°C in a sodium cacodylate buffer. The reaction was stopped with phosphotunstic acid and centrifuged 14000g for 10 min at 4°C. The pellet was washed 3
times with 1 mL of ice–cold 5% trichloroacetic acid, water,
and ethanol, centrifuged as above and processed for counting in 1 mL of OptiPhase SuperMix scintillation fluid (Fisons
Chemicals, Loughborough Leics, UK) using MicroBeta
Trilux counter (Wallac, Turku, Finland). 0.2 mU of 2.6 sialyltransferase from rat liver (Roche Diagnostics) was used as
a positive control in assay instead of thyroid homogenate.
90% of radioactivity is incorporated to the exogenous acceptor in this condition. Homogenate of normal thyroid incubated 1 minute in 95°C was used as a negative control.
647
RNA isolation and Northern blots
Total RNA was isolated from tissue samples by Chomczynski’s method (35) using TRIzol reagent (Invitrogen,
Carlsbad, CA). The RNA concentrations in all samples were
measured by light absorptymetry (Wallac). Northern blots
were prepared from 0.9% agarose-formaldehyde gels
(1⫻MOPS, 0.9% agarose, 3% formaldehyde with 10 g total
RNA per line) by overnight osmotic transfer onto Gene
Screen Plus membranes (New England Nuclear, Boston, MA)
using 10 ⫻ SSPE buffer (3 M NaCl, 0.2 M NaH2PO4-H2O, 0.02
M ethylenediaminetetraacetic acid [EDTA]; pH 7.4). Clones,
used for preparation of specific probes, were obtained from
IMAGE Consortium. Clone IMAGE 2371549 (corresponding
to EST GeneBank sequence GI 5234676) was used for SIAT1
probe and clone IMAGE 360422 (corresponding to EST
GeneBank sequence GI 1476738) was used for SIAT4A probe.
The specific SIAT1 probe was made using a 480-bp fragment
of IMAGE clone 2371549 (corresponding to fragment between nucleotides 52 and 530 of human SIAT1 cDNA,
X17247) by PCR reaction using M13-forward and M13-reverse primers. Single labeled probe was made by linear PCR
using 10 ng of human SIAT1 cDNA, 3 fmol of specific antisense primer ACTCCCTTTCTTCTTTTCCTTCC, 10 fmol of
[␣-32P]-dCTP (3000 Ci/mmol; Gene Screen Plus; New England Nuclear) and 4 units of Taq polymerase (MBI Fermentas, Vilnius, Lithuania) in 20 L standard Taq polymerase buffer supplemented with (-dCTP)dNTP (final
concentration, 0.05 mM) and Mg2⫹ (final concentration, 1.5
mM) (36). The SIAT4A probe was made from the 420-bp fragment of IMAGE clone 360422 (corresponding to fragment between nucleotides 339 and 757 of human SIAT4A cDNA,
NM_003033) by PCR reaction using M13-forward and M13reverse primers. SIAT4A probe labeling was made by the
random primer method, using Prime-It Random Primer Labeling kit (Stratagene, La Jolla, CA) with random primers,
Klenow fragment (MBI Fermentas, Vilnius, Lithuania) and
[␣-32P]-dCTP (3000 Ci/mmol). All probes were purified after labeling on a Sephadex G50 column chromatography. The
percentage of [␣-32P]-dCTP incorporation was checked in the
Wallac Microbeta counter (Wallac). Membranes were hybridized for 16 to 24 hours at 42°C in hybridisation buffer
(5⫻ SSPE, 50% deionized formamide, 5⫻ Denhardt’s solution, 1% sodium dodecyl sulfate [SDS], 10% dextran sulfate)
supplemented with salmon sperm DNA (50 g/mL) and
with labeled, temperature-denaturated probe (1 million
cpm/mL).
Prehybridization was performed without probe for 2
hours at 42°C. Blots were washed after hybridization twice
for 15–30 minutes in 2 ⫻ SSC, 0.5% SDS at 50°C and twice
for 15–30 minutes in 0.1 ⫻ SSC, 0.1% SDS at 50°C. After 3 to
10 days of long exposure, autoradiographs were scanned using a Sharp JX-330 scanner and signals were quantified by
densitometry. The results were corrected to the total amount
of RNA transferred, which was determined by ethidium bromide staining.
Statistical analysis
All data are reported as mean ⫾ standard deviation (SE).
Groups were compared using the Mann-Whitney test, Student’s t test, and the correlation between variables was assessed using the Spearman test.
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KILJA ŃSKI ET AL.
Sialyltransferase activity and mRNA
levels in thyroid tissue
FIG. 1. Lipid-bound sialic acid (LBSA) content in Graves’
goiter. LBSA content was measured in samples coming from
control thyroid tissues (C), Graves’ goiters (GD), and benign
thyroid nodules: nontoxic (NN) and toxic (TN). The LBSA
content in the GD group was significantly higher from the
LBSA content in other groups, C, NN, or TN (p ⬍ 0.005 by
Student’s t test). LBSA content in all samples from the GD
group, in contrast to control tissues, was higher from 145
nmol/g. The sample numbers (n) is shown below the graph.
Results
LBSA content and ganglioside profile in thyroid tissues
The LBSA content was the highest in Graves’ thyroid tissues (mean value was 164 ⫾ 4.44 nmol/g, p ⬍ 0.005 when
compared to all other groups studied Fig. 1). There were no
significant differences in LBSA content between C, TN, and
NN groups (mean values, 120 ⫾ 2.00, 126 ⫾ 6.95 and 116 ⫾
3.12 nmol/g, respectively). There were no major differences
in ganglioside profiles between various groups (Table 1).
GM3 was found to be the predominate ganglioside in all
groups of tissues (over 50% of total ganglioside content).
Gangliosides GM3 and GD3 constituted 60%–80% of gangliosides present in all analyzed tissues (Table 1). To evaluate less abundant FucGM1 content we used TLC-immunooverlay. However we did not observe significant expression
of this ganglioside in any tissue studied.
Because of the relatively small weight of tissue samples
we could estimate only total sialyltransferase activity without differentiating into specific isoenzymes. The highest sialyltransferase activity was found in GD (1625 ⫾ 283.5
cpm/mg of protein, Fig. 2). The activity in GD group was
significantly higher from the control group, C (324 ⫾ 54.2
cpm/mg of protein, p ⬍ 0.005) or from the nontoxic thyroid
nodules, NN (607 ⫾ 101.0 cpm/mg of protein, p ⬍ 0.05). The
difference between the GD group and the toxic nodules (TN)
was not statistically significant (mean value for TN was 1153
cpm/mg of protein, p ⫽ 0,09). Sialyltransferase activity in the
TN group was also significantly higher than in the control
group, C (p ⬍ 0.005).
Northern blot for sialyltransferase-1 (SIAT1 gene product) and sialyltransferase 4A (SIAT4A gene product)
showed single mRNA signal of the expected size in all
tested groups (approximately 4 kb and 7 kb, respectively;
Fig. 3) (37–39). There were no obvious additional bands that
might have suggested the existence of exon splice variants
or different transcription sites. The sialyltransferase-1
mRNA level was the highest in Graves’ thyroid tissues
(12.52 ⫾ 6.90 arbitrary units[AU]) and statistically different
from control tissues, C (2.54 ⫾ 1.24 AU, p ⬍ 0.005 in MannWhitney test), or nontoxic nodules NN (3.14 ⫾ 3.61 AU, p ⬍
0.05, Fig. 4A). The sialyltransferase-1 mRNA level in the TN
group was not statistically different from the other groups.
Similar results were found for sialyltransferase-4A mRNA
(Fig. 4B), where the mRNA level was the highest in Graves’
thyroids (means were for GD 2,49 ⫾ 1.16 AU, for C 1.23 ⫾
0.46 AU, p ⬍ 0.05). The expression level found in the TN
group was significantly higher than in their counterpart the
TC group (1.37 ⫾ 0.09 versus 1.00 ⫾ 0.12 U, p ⬍ 0.05). Surprisingly, we found extreme variability in mRNA content
for both mRNAs within the same groups (Fig. 3) reaching
85-fold in the case of sialyltransferase-4A mRNA level in
Graves’ disease. We also found a significant, positive correlation between increased sialyltransferase-1 mRNA level,
but not sialyltransferase-4A mRNA level, and TSH-receptor antibody titer determined by the TRAK test (p ⫽ 0,029;
R ⫽ 0,6017).
TABLE 1. GANGLIOSIDE PROFILES
IN
THYROID TISSUES
Major ganglioside content in thyroid tissues
(% of total ganglioside content ⫾ ranges)
Ganglioside
Control (C)
(n ⫽ 14)
GM3
GM1
3⬘LM1
GD3
GD1a
GD1b
GT1 ⫹ GQ1
55 ⫾
⬍2
4.5 ⫾
17.5 ⫾
7.5 ⫾
3⫾
3.5 ⫾
5
1.5
2.5
2.5
1
1.5
Benign thyroid
nodules (NN ⫹ TN)
(n ⫽ 13)
55 ⫾ 5
⬍2
2.5 ⫾ 0.5
15 ⫾ 5
7.5 ⫾ 2.5
⬍2
3.5 ⫾ 1.5
Graves’ goiter (GD)
(n ⫽ 12)
60 ⫾
⬍2
⬍2
10 ⫾
12.5 ⫾
⬍2
2.5 ⫾
5
5
2.5
0.5
Values represent the percent of the total ganglioside content (mean ⫾ ranges). Each sample was measured in duplicates. Number of samples tested (n) is shown above. All ganglioside symbols are derived from Svennerholm classification (49).
SIALYLTRANSFERASES IN GRAVES’ DISEASE
FIG. 2. Total sialyltransferase activity in Graves’ goiter.
Total sialyltransferase activity was significantly higher in
Graves’ disease (GD) than in control nontumorous thyroid
tissues, C (1625.14 ⫾ 283.48 and 324.08 ⫾ 54.21, respectively). The difference between GD and nontoxic nodules
group NN (631.93 ⫾ 101.04; p ⬍ 0.05) was also significant,
in contrast to toxic thyroid nodules, TN (1153.00 ⫾ 190.88,
p ⫽ NS).
Discussion
GD is one of the most common thyroid pathologies affecting up to 1% of general population in the United States
and in many countries of the European Community (40). It
is well accepted that anti-TSH-R autoantibodies are the key
pathogenic factor responsible for the alteration in the thyroid function and morphology (40). However, little is known
about the initiation and the modulation of the autoimmune
process during the waxing and waning course of this disease. Prior studies done before TSHR cloning suggested that
gangliosides are components of the TSHR (13–16). In cultured rat thyroid cell line, FRTL-5 or bovine and human primary thyroid cell culture gangliosides modulate TSHR signal transduction and cyclic adenosinemonophosphate
(cAMP) synthesis (13–16). In FRTL-5 cells glycosphingolipid
moiety associated with TSHR was shown to belong to the
ganglioteratose family with both galactose molecules sialylated (18). Although these data need to be confirmed, one
may speculate that changes in the ganglioside amount or
profile might work as negative or positive feedback for the
TSHR activation. Our study has shown that LBSA content in
Graves’ thyroids was not only 30% higher than in any other
group but the single separating line can be drawn between
its level in individual tissue samples coming from Graves’
thyroids or control thyroids. This suggests that the observed
changes are not only meaningless statistically significant differences between groups but are rather important changes
affecting every individual Graves’ thyroid tissue. Measurements of Graves’ thyroid total lipid content can be potentially affected by morphological changes associated with
TSHR activation (relatively smaller follicles, containing less
colloid and more cellular components). As a result one can
expect a higher total lipid content in Graves’ thyroid than in
normal thyroid tissue.
Therefore, further studies might be needed to verify our
results in cellular compartment of Graves’ thyroid. Despite
the slightly higher content of ganglioside GM3 in Graves’
thyroids, profiles of the major thyroid gangliosides seem to
be unchanged. This suggests that the sialyltransferase activ-
649
ity is not restricted to a specific lipid product but rather affects all lipids equally. However, for an unknown reason
ganglioside profiles varied significantly from patient to patient in all studied groups. It has been suggested that ganglioside FucGM1 is occasionally a target of autoimmune reaction in GD (41) and in thyroid cancer (42). Interestingly we
were unable to detect significant expression of FucGM1 in
thyroid tissue.
The increased content of LBSA in Graves’ thyroid might
reflect its increased synthesis or decreased degradation.
However, the increased content of sialic acid correlated with
the increased sialyltransferase activity and their mRNA level.
This suggests that increased sialic acid content is mostly the
result of its increased incorporation into lipids rather than
decreased degradation of LBSA. Similar to LBSA content,
morphologic changes in Graves’ thyroid might potentially
alter sialyltransferase activity measurement because of contamination of thyroglobulin. However, because of scarcity of
the thyroid tissue samples, to obtain uniform results from
the same sample, we decided to homogenize the thyroid tissue samples first followed by dividing them into three parts
for estimation of LBSA, ganglioside composition, and sialyltransferase activity using different procedures. We did not
measure either specific sialoprotein level (like thyroglobulin) or total protein bound sialic acid. Nevertheless the same
sialyltransferase activity is responsible for sialic acid transfer into lipids and proteins (3). The same sialyltransferase activity is also responsible for sialic acid transfer into various
gangliosides (3). Lack of changes in ganglioside profiles also
FIG. 3. Northern blots showing specific SIAT1 and SIAT4A
gene transcripts in thyroid tissues. Total RNA was extracted
from 10 different thyroid tissues coming from 10 different
patients. Four samples came from patients with Graves’ disease (GD), 4 from patients with papillary thyroid cancer
(PTC; from surrounding normal tissues, C and 2 from tumor, PTC) and 2 from nodules of toxic nodular goiters, TN.
Upper panel represents the top part of Northern blot hybridized with specific human sialyltransferase-4A (SIAT4A)
probe. Single signal approximately 7 kb in size was seen
much above 28S ribosomal bound. Middle panel shows specific sialyltransferase-1 (SIAT1) signal approximately 4 kb in
size (below 28S ribosomal bands) and bottom panel shows
ribosomal RNA stained with ethidium bromide.
650
FIG. 4. Sialyltransferase-1 (SIAT1) and sialyltransferase-4A
(SIAT4A) mRNA levels in Graves’ goiter. Specific SIAT1 (A)
or SIAT4A (B) mRNA levels were measured by Northern
blots using the same techniques as for Figure 3. Two control
groups, either from macroscopically normal tissues of nontoxic nodular goiter (NC) or from toxic nodular goiter (TC)
are parts of a larger control group C. In the Graves’ goiters
(GD) SIAT1 and SIAT4A mRNA levels were significantly
higher than in the C group. SIAT1 but not SIAT4A mRNA
levels were significantly different between the GD group and
tissues of nontoxic and toxic nodules (NN and TN, respectively). Sample number (n) is shown below the graphs.
suggests that the increase in LBSA content is more likely to
result from the increased sialyltransferase activity rather
than from the changes in substrate profile. In one of the earliest studies on human thyroid ganglioside profile in cultured thyrocytes of patients with GD Lee et al. (43) observed
qualitative differences between samples coming from
Graves’ disease, toxic adenoma, and normal thyroid. However, conditions used for primary cell cultures are quite different from those seen in tissues.
The increased sialyltranferase-1 mRNA and sialytransferase-4 mRNA suggest that the increased sialyltransferase
activity in Graves’ thyroid is at least partially the result of
pretranslational mechanisms. Because activation or deactivation of the TSHR by autoantibodies present in Graves’ thyroid disease switch transcriptional machinery of many hu-
KILJA ŃSKI ET AL.
man thyroid genes it is tentative to postulate that TSHR activation was responsible for transcriptional changes in sialyltransferase gene expression. However, we did not measure the transcription directly and mRNA level, similarly to
protein level, could be affected by both synthesis and degradation. The results suggest that mechanisms for gene transcription activation of two sialyltransferases are not the
same, since there was no correlation in sialyltransferase-1
and sialyltransferase-4A mRNA levels in some tissues (Fig.
3). Interestingly the sialytransferase-1 mRNA level correlated with the TSHR antibodies titer. It must be emphasized
that patients with GD were treated with antithyroid medication and large doses of iodine before surgery. Both factors
can potentially affect gene expression. Hormonal status at
the time of the surgery was an unlikely factor affecting the
observed changes, because all patients were clinically euthyroid at least few weeks before and only few had decreased
TSH with normal thyroid hormone suggesting subclinical
hyperthyroidism. However, it is well known that changes
associated with long-standing severe thyrotoxicosis can persist for several weeks after normalization of thyroid hormone
levels. Because of the missing data we were unable to correlate the length of euthyroid state prior to surgery with sialyltransferase activity or mRNA levels. We believe that it is
more likely that TSHR activation by autoantibodies is responsible for observed changes in sialyltransferase activity
and mRNA levels. It would be of value to evaluate if sialylation of TSHR can affect thyroid autoimmune process
and/or TSHR responsiveness to autoantibodies.
The differences in sialyltransferase activity and sialic acid
content were not observed in toxic nodular goiter. It was recently postulated that, similar to toxic thyroid adenomas, activating mutation in TSHR is also present in toxic nodules
of multinodular goiter (44). Indeed in 3 of 6 tissues coming
from toxic nodule the sialyltransfease-1 mRNA was higher
than in any control tissue tested, although the statistical analysis is hampered by small sample size.
Studies on TSH-dependent regulation of thyroid glycosyltransferases used different experimental models, species,
and led to contradictory conclusions. Most of them focused
on thyroglobulin as one of major products of thyroid cells
and a protein well characterized in terms of glycan structure.
Unfortunately, most studies used cell culture as an experimental model. It has been demonstrated that glycosylation
of proteins in cell culture differs from their native forms (45).
Franc and colleagues (46) found that TSH stimulated several
thyroid glycosyltransferases in cultured porcine cells, among
them sialyltransferases. In cell culture TSH increased sialylation of thyroglobulin shifting terminal glycosylation from
␣-galactose to sialic acid (45). In rats the TSH-evoked increase
in glycosylation was exemplified by results of an in vivo
study demonstrating that propylthiouracyl treatment increased mannosyltransferase and galactosyltransferase levels (47). On the other hand, Grollman and colleagues (48) reported marked TSH-evoked decrease not only in the level of
␣2,6-bound sialic acid but also decreased other core monosaccharide constituents of thyroglobulin in FRTL-5 cells.
There are no prior data concerning the TSH effect on glycosyltransferase expression and activity in human thyroid tissue.
This study has shown that in GD increased sialic acid content correlated with increased sialyltransferase activity and
SIALYLTRANSFERASES IN GRAVES’ DISEASE
increased mRNA level. While more data and alternative
methodological approaches are needed to draw the definite
conclusion, it is possible that the changes in sialic acid metabolism may affect the thyroid function and the autoimmune process and may be an important part of pathophysiology of Graves’ thyroid disease. Further work is needed to
elucidate the exact mechanism for observed changes of sialic
acid metabolism in Graves’ thyroid.
651
17.
18.
19.
Acknowledgments
The study was supported by the State Committee for Scientific Research grant number 4 P05B 042 15.
20.
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Address reprint requests to:
Dr Jacek Kiljanski
Department of Internal Medicine and Endocrinology
Medical University of Warsaw
ul. Banacha 1a
02–097 Warsaw
Poland
E-mail: kiljan@amwaw.edu.pl