Open Access

Arachidonic acid increases matrix metalloproteinase 9 secretion and expression in human monocytic MonoMac 6 cells

  • Tiina Solakivi1,
  • Tarja Kunnas1,
  • Satu Kärkkäinen2,
  • Olli Jaakkola2 and
  • Seppo T Nikkari1, 3Email author
Lipids in Health and Disease20098:11

DOI: 10.1186/1476-511X-8-11

Received: 17 February 2009

Accepted: 30 March 2009

Published: 30 March 2009



Dietary fatty acids may modulate inflammation in macrophages of the atherosclerotic plaque, affecting its stability. The n-6 polyunsaturated fatty acid (PUFA) arachidonic acid (AA) generally promotes inflammation, while the PUFAs of the n-3 series eicosapentaenoic acid (EPA), docosapentaenoic acid (DPA) and docosahexaenoic acid (DHA) are considered anti-inflammatory. We determined how these PUFAs influence MMP-9 expression and secretion by the human monocytic cell line (MonoMac 6) at baseline and after 24-hour exposure. MMP-9 protein was measured by zymography and relative levels of MMP-9 mRNA were determined using quantitative real time PCR.


Supplementation with AA (but not the n-3 fatty acids) increased, in a dose-dependent manner, expression of MMP-9 protein. This stimulation was regulated at the mRNA level. MMP-9 secretion started after 1 h of incubation and could not be prevented by simultaneous presence of n-3 series fatty acids. Finally, the secretion could be attenuated by LY 294002, a specific phosphatidylinositol-3-kinase (PI3K) inhibitor and by SH-5, a selective Akt inhibitor, suggesting that activation of PI3K by AA leads to augmented and sustained MMP-9 production.


This study shows that of the PUFA studied, AA alone influences the expression of MMP-9, which might have implications in MMP-9 induced plaque rupture.


Dietary fatty acids are known to modulate the metabolism of lipids and lipoproteins and therefore also to be involved in cardiovascular and metabolic diseases [1, 2]. Dietary polyunsaturated fatty acids (PUFA) are classified into two families, the n-6 and n-3 series. Although both families are substrates for the same enzymes in many cellular processes, the affinity of enzymes is greater for the n-3 family than that for the n-6 family. As an example, arachidonic acid (20:4n-6, AA), a metabolite of linoleic acid (18:2n-6), is the substrate of cyclooxygenases and lipoxygenases in the production of potent inflammatory eicosanoids. The polyunsaturated fatty acids of the n-3 series (eicosapentaenoic acid 20:5n-3, EPA; docosapentaenoic acid 22:5n-3, DPA; and docosahexaenoic acid 22:6n-3, DHA) limit the synthesis of these mediators from AA, and enhance the synthesis of less inflammatory eicosanoids from EPA [3]. Recent studies have identified novel groups of powerful EPA and DHA derived anti-inflammatory mediators which are produced during the resolving phase of an acute inflammatory response [4].

The propensity of atherosclerotic plaques to rupture is influenced by their lipid content and the distribution of lipid within the plaque as well as by the extent of infiltration of macrophages at the shoulder regions of the plaque and by the thickness of the fibrous cap [5]. A thin fibrous cap and a substantial presence of macrophages and other inflammatory cells in the shoulder region indicate a vulnerable plaque likely to rupture. Matrix metalloproteinases (MMPs) are a group of enzymes whose major functions are directed toward remodelling of extracellular matrix (ECM) components. Gelatinase B (MMP-9) is a very complex enzyme in terms of domain structure or regulation of its activity and expression. MMP-9 activity is controlled at different levels: transcriptional activation of the gene by cytokines and other factors, activation of the pro-enzyme by various enzymes like serine proteases and regulation by specific tissue inhibitors of the matrix metalloproteinases (TIMPs). MMP-9 has been shown to be up-regulated in unstable angina pectoris. It is mainly expressed by macrophages located especially in vulnerable regions of the atherosclerotic plaque [6]. Published results thus suggest that localized increase in MMP-9 associated with an inflammatory process in the vascular wall has the potential to weaken the tissue structure thus increasing the risk for plaque rupture. Still, the signalling pathways that lead to induction of expression of MMP-9 are incompletely understood.

Dietary n-3 fatty acids have a variety of anti-inflammatory and immuno-modulating effects that may be of relevance to atherosclerosis and its clinical manifestations of myocardial infarction, sudden death and stroke [1]. There is epidemiological evidence that consumption of fish or n-3 PUFA protects against cardiovascular disease [7]. However, more critical meta-analyses regarding the clinical importance of n-3 PUFA have also demonstrated no clear effect on combined cardiovascular events [8]. The effects of n-3 PUFA have been variously ascribed to anti-arrhythmic or anti-thrombotic actions of n-3 PUFA but might as well be linked to their anti-inflammatory effects [1]. Some of these effects are brought about through modifications in gene expression since long chain fatty acids also serve as ligands for several nuclear transcription factors [9]. In a recent study, patients who were scheduled to carotid endarterectomy were randomly allocated to receive either placebo, sunflower oil or fish oil. It was shown that the n-3 PUFAs were readily incorporated into plaques and were associated with reduced numbers of macrophages and signs of inflammation [10]. Inflammatory prostaglandins and leukotrienes derived from arachidonic acid have previously been shown to induce MMP production [1113]. Human MonoMac 6 monocytes appear to be a useful cellular model to investigate effects of compounds on plaque vulnerability through MMP-9 activity [14]. In this study we sought to clarify relationships between arachidonic acid and the polyunsaturated n-3 fatty acids in regulation of MMP-9.


To investigate the impact of long chain fatty acids with different characteristics on MMP-9 secretion we incubated MonoMac 6 cells in the presence of 1 μM and 10 μM AA, EPA or DPA (Fig. 1A). The secretion of MMP-9 to the medium increased in the presence of 1 μM AA as shown by the greater activity of MMP-9 in zymography (2.3 ± 0.2-fold, n = 10) and was further enhanced by 10 μM AA (6.7 ± 1.0-fold, n = 14). EPA and DPA had no effect, neither did DHA (result not shown). The effect of PMA (1.3 nM), a known activator of monocytes and also of MMP-9 secretion [15] was about ten-fold greater than that of 10 μM arachidonic acid Addition of 1 μM and 10 μM AA, EPA or DPA along with PMA did not affect MMP-9 production (Fig. 1B).
Figure 1

Effect of polyunsaturated fatty acids and PMA on the production of MMP-9. MonoMac 6 cells (0.8 × 106/ml in serum-free medium X-Vivo 15) were stimulated with 1 or 10 μM arachidonic acid (AA), eicosapentaenoic acid (EPA) or docosapentaenoic acid (DPA) without (1A) or in the presence of 1.3 nM PMA (1B). The culture media were harvested after 24 h incubation and analysed for MMP-9 by gelatin zymography. The media of PMA-treated cells were diluted (1:10) to preserve the linearity of response in image analysis.

Fatty acid analysis of the cells showed that all the long chain polyunsaturated fatty acids were readily taken up by the cells and metabolized further. The amount of AA in cellular lipids increased in the presence of 1 μM AA from 1.3 ± 0.037 μg/1.0 × 106 cells to 2.2 ± 0.23 μg/1.0 × 106 cells, and in the presence of 10 μM AA to 7.4 ± 1.29 μg/1.0 × 106 cells. In addition, fatty acid analysis showed that AA was efficiently elongated to 22:4n-6. Similarily, EPA was taken up by the cells and was elongated to 22:5n-3, since the amount of this fatty acid increased from 0.5 ± 0.046 μg/1.0 × 106 cells to 2.2 ± 0.28 μg/1.0 × 106 cells when the cells were exposed to 10 μM EPA for 24 h. Furthermore, when the monocytes were incubated in the presence of DPA this fatty acid was metabolized to 22:6n-3, which was further retroconverted to EPA. These results show that the fatty acids were taken up and were available at least to the enzymes in endoplasmic reticulum and peroxisomes.

We then looked at the concentration-dependency of arachidonic acid-induced secretion of MMP-9. We incubated MonoMac-6 cells for 24 h in the presence of increasing concentrations of AA (0–40 μM). Analysis of the zymograms by image analysis gave a logarithmic dose response curve (Fig. 2A). Examination of the cells after incubation in the presence of 40 μM AA revealed large clumps of clustered cells. This phenomenon was associated with a slightly lowered cellular protein concentration suggesting some undesirable effects of higher concentrations of AA on cellular well-being.
Figure 2

Dose- and time-dependent stimulation of MMP-9 secretion by arachidonic acid. 2A. MonoMac 6 cells (0.8 × 106 cells/ml in X-Vivo 15) were treated for 24 h with increasing concentrations of arachidonic acid. The media were collected and analysed for MMP-9 by zymography. Data are shown as means ± SEM of 3 to 4 independent experiments. The increase of MMP-9 secretion was statistically significant from 2.5 μM AA and upwards. 2B. MonoMac 6 cells (0.8 × 106 cells/ml in X-Vivo 15) were pre-exposed to 10 μM arachidonic acid for 1, 2, 4 or 6 hours where after the culture medium was changed to X-Vivo without arachidonic acid for 24 h. The media were analysed for MMP-9 by zymography. Results are shown as means ± SEM of three independent experiments. A statistically significant increase in MMP-9 secretion was evident after 1 h preincubation in comparison with cells incubated in the presence of vehicle only.

To investigate the time course of AA-induced MMP-9 secretion we took small samples of medium at 1, 2, 4, 8, 16 and 24 h after adding 10 μM AA or 1.3 nM PMA. MMP-9 activity became evident in zymograms of the media after 6 h to 8 h incubation with AA but was already discernible after 4 h incubation with PMA. We then pre-exposed the cells to 10 μM AA for different periods of time after which the medium was discarded. The incubation was then carried on with culture medium without AA for 24 h for MMP-9 activity to be detectable in zymograms. As shown in Fig. 2B, MMP-9 activity was augmented already after 1 h incubation with AA and increased for at least 6 h.

Since EPA, DPA or DHA by themselves had no effect on MMP-9 secretion, we looked at their effect on AA-induced production of MMP-9. Co-incubation of 5 μM AA with increasing concentrations of EPA, DPA or DHA for 24 h did not diminish or increase the secretion of MMP-9 (Fig. 3).
Figure 3

Effect of docosapentaenoic acid (DPA) on arachidonic acid (AA) stimulated production of MMP-9. MonoMac 6 cells (0.8 × 106 cells/ml in X-Vivo 15) were incubated in the presence of 5 μM arachidonic acid and increasing concentrations of DPA (1, 5, 10 μM) for 24 h. The presence of MMP-9 activity in the media was determined using zymography.

We then tested the hypothesis that AA could increase the secretion of MMP-9 by modulating its gene expression. In Fig 4 we show that MMP-9 mRNA expression was increased 6- to 8-fold when stimulated with 10 μM AA for 24 h; it was only slightly up-regulated in the presence of n-3 fatty acids and 1 μM AA (Fig. 4). Predictably, PMA treatment stimulated MMP-9 expression to a much greater extent than 10 μM AA (results not shown).
Figure 4

Effect of polyunsaturated fatty acids on MMP-9 mRNA expression. MonoMac 6 cells (4 × 106 cells/5 ml X-Vivo 15 on Nunclon 60 mm dishes) were treated with 1 or 10 μM arachidonic acid (AA), eicosapentaenoic acid (EPA) or docosapentaenoic acid (DPA) for 24 h. Then the cells were pelleted by centrifugation (400 × G, +4°C) and washed with ice-cold PBS. Total cellular RNA was isolated, reverse transcribed and the resulting cDNA was amplified as described in the methods. The MMP-9 expression was demonstrated by real-time PCR. Results represent the means ± SEM of four independent experiments. Only 10 μM AA increased the expression of MMP-9 mRNA statistically significantly.

In an endeavour to understand further the mechanism through which arachidonic acid acts, we investigated whether it affected the activity of phosphatidylinositol 3-kinase (PI3K). For this end we incubated MonoMac 6 cells with LY 294002, an inhibitor of PI3K for 30 min before adding 10 μM AA or 1.3 nM PMA for 24 h. As shown in Fig 5, Ly 294002 blocked the induction of MMP-9 by AA and PMA in a dose-dependent manner. However, if the inhibitor was removed from the incubation medium before the addition of AA or PMA the inhibitory effect was lost. These results indicate a role for PI3K activation in the signalling of both AA and PMA to produce MMP-9. To test the phophatidylinositol signalling system downstream of PI3K we treated the MonoMac 6 cells for 30 min with various concentrations of phosphatidyl inositol analog, SH-5, an inhibitor of Akt. This was followed by stimulation of the cells with 10 μM AA for 24 h. A concentration dependent decrease of AA-induced MMP-9 secretion was seen in zymographic analysis. The decrease was 20% (± 4%, n = 4) for 2.5 μM, 35% (± 3%, n = 4) for 5 μM and 53% (± 2%, n = 4) for 10 μM SH-5. These results further point to phosphatidylinositol lipids as mediators of AA stimulation.
Figure 5

Inhibition of arachidonic acid (AA) and PMA induced stimulation of MMP-9 secretion by LY294002. Dose- and time-dependent stimulation of MMP-9 secretion by arachidonic acid. MonoMac 6 cells (0.8 × 106 cells/ml in X-Vivo 15) were treated with various concentrations of LY294002 in DMSO for 30 min. Then 10 μM arachidonic acid (5A) or 1.3 nM PMA (5B) was added and the incubation was continued for 24 h. The media were analysed for the presence of MMP-9 using zymography and image analysis. Results (mean ± SEM) for 4 to 5 independent experiments are shown. All concentrations of LY294002 decreased the AA or PMA induced secretion of MMP-9 statistically significantly.


In the present study we show that incubation of human leukaemia Mono Mac 6 cells in the presence of AA (20:4n-6) in serum-free medium is associated with increased secretion of MMP-9 to the growth medium in comparison with control cells incubated without added AA. The response was concentration-dependent and intensified considerably as the level of AA rises from 1- to 40-μM. Since the composition and content of cellular fatty acids changed in accordance with fatty acids added to the incubation medium, the fatty acids obviously entered the cells either by diffusion or by membrane transport proteins. It is possible that the effect of AA on MMP-9 secretion was mediated via binding to a membrane receptor, since a family of G-protein coupled free fatty acid receptors has been recently identified [16]. However, none of these receptors has been shown to be specific to arachidonic acid.

EPA, DPA or DHA, fatty acids of the n-3 series, which are considered to be anti-inflammatory, had no effect on basal secretion of MMP-9. Since the n-3 series of polyunsaturated fatty acids are known to compete for the same enzymes as the n-6 series fatty acids in a multitude of cellular processes, and the enzymes seem to prefer n-3 series, we tested whether the effect of arachidonic acid on secretion of MMP-9 could be controlled or even prevented by increasing concentrations of EPA, DPA or DHA. However, the AA-induced activity of MMP-9 did not diminish in the presence of n-3 fatty acids, although the cellular fatty acid content revealed an ample availability of n-3 fatty acids after incubation. It is possible, though, that the intracellular pathways of n-6 and n-3 fatty acids differ in ways that give advantage to AA [17, 18]. On the other hand, it is also possible that a prolonged exposure of cells to n-3 fatty acids is necessary for inhibition of AA-triggered MMP-9 activity [19].

Experiments where MonoMac 6 cells were pre exposed to AA for increasing periods of time (Fig. 2B) showed that the system delivering MMP-9 to the medium was activated already after 1 h incubation and increased for at least 6 h. Given that a quantity of pro-MMP-9 is stored in intracellular vesicles it is possible that the activity detected during the first hour of incubation was in fact due to degranulation of existing vesicles. Degranulation of storage vesicles has been shown to occur quickly in response to less than 1 h treatment with IL-8 in neutrophils, where the activity of MMP-9 increased 2.5-fold but then declined [20]. It is not known whether AA causes degranulation in MonoMac 6 cells, but the continued accumulation of MMP-9 in the incubation medium speaks for additional mechanisms. The increases in AA-induced secretion of MMP-9 was blocked by co-treatment of MonoMac 6 cells with 1–10 μM of the protein synthesis inhibitor cycloheximide (data not shown), indicating further that the AA effect requires de novo protein synthesis.

The transcriptional regulatory mechanism was confirmed by the increase of MMP-9 mRNA by AA treatment. We could show in repeated experiments that the expression level of MMP-9 mRNA increased in response to AA, whereas EPA or DPA did not produce such amplifications. The response with AA was somewhat variable as can be seen from Fig. 4, but it was well associated with the results of enzyme activity as measured using zymography. It is notable that the level of mRNA was persistently elevated after 24-h incubation in the presence of the AA in comparison with basal conditions.

Production of MMP-9 by macrophages has been shown to occur through a prostaglandin E2/cAMP-dependent mechanism. It has been shown that production of MMP-9 is induced by prostaglandin E2 (PGE2), the predominant eicosanoid of macrophages [21]. PGE2 is produced from AA by the coupled actions of cyclooxygenase and prostaglandin E synthase [22]. Cylooxygenase 1 (COX-1) is constitutively expressed but cyclooxygenase 2 (COX-2) is induced by inflammatory cytokines, growth factors or phorbol esters. PGE2 acts in an autocrine or paracrine manner and activates adenylate cyclase. The increased cAMP leads to activation of PKA, and the expression of MMP-9 [23]. Studies using human monocytes have shown that induction of COX-2 protein production and concomitant PGE2 increase occur at 4 h – 16 h after stimulation with LPS [24]. In contrast, in our experiments the secretion of MMP-9 was enhanced after 1 h incubation in AA containing medium, speaking for a faster mechanism. Also, it has been shown that PGE2 alone does not stimulate MMP-9 synthesis in MonoMac 6 cells but needs a simultaneous presence of an effective primary stimulus such as TNFα [25].

The n-3 series fatty acids are competitive inhibitors of cyclooxygenase-catalysed catabolism of AA and show a preference for the COX-2 over the COX-1 forms [26], but could not prevent the effect of AA in our experiments. Therefore, we felt that AA by itself could trigger the events that lead to MMP-9 secretion. Earlier studies by Hii et al. [27] have shown that AA or its metabolites can activate PI3K-mediated pathways. On the other hand, studies of Lu et al. [28] show that in LPS-activated human peripheral blood monocytes MMP-9 production resulted through the stimulation of PI3K signalling pathway. Indeed, when we blocked the capability of PI3K to generate PIP3 in MonoMac 6 cells by Ly 294002 (a specific inhibitor of PI3K), MMP-9 production was inhibited in both AA and PMA stimulated cells. The result indicates that the PI3K pathway has a central role in regulation of monocyte MMP-9 production following stimulation with AA. This outcome accords with the results of Sato and co-workers, where the secretion of MMP-9 could be prevented by nobiletin (a flavonoid) or LY294002 in fibrosarcoma cells [29]. Activation of PI3K leads to phosphorylation of inositol lipids, in response to activation and membrane translocation of Akt/Protein kinase B. Inhibition of Akt by SH-5 was associated with attenuation of MMP-9 secretion in AA stimulated MonoMac 6 cells. This result further points to the involvement of PI3K signalling system in AA-induced MMP-9 production. Activated Akt in turn phosphorylates several proteins that regulate cell survival, including Bad and caspase 9 [30]. This activation is important for monocyte survival and therefore the results using PI3K or Akt inhibitors should be considered very carefully. It is possible that MonoMac 6 cell viability was affected and therefore the cells stopped secreting MMP-9. However, no evidence of increased cell death could be seen in Trypan Blue exclusion tests. MMP-9 production in response to LPS-induced PI3K stimulation has also been reported to occur through IKKα/NFκB pathway in human monocytes [28]. Whether AA also acts through this pathway remains to be examined.

AA concentrations in tissues and for example in inflammatory cells are dictated in part by the concentration of AA that these cells are exposed to and partly by local formation from linoleic acid [31]. AA is distributed to the cells as albumin-bound FA or lysophospholipid and as a component of various lipoprotein particles. Extracellular and intracellular concentrations of free AA are kept low, but in stressful situations like inflammation the extracellular concentration of AA can reach up to a level of a hundred μM [32]. This means that the fatty acid concentrations that were used in our in vitro incubations were well within the in vivo range. The primary pathway leading to AA release is the hydrolysis of phospholipids by enhanced activity of either secretory or cytoplasmic phospholipase A2. Relevant to the study of atherogenesis is the finding in human THP-1 monocytes that native LDL elicited a rapid, dose-dependent release of AA which was further increased when LDL was modified by secretory phospholipase A2 (PLA2) [33]. Also, it was recently reported by Namgaladze et al. [34] that sPLA2-modified LDL activated the PI3K pathway, thus increasing monocyte survival. The active ingredient was shown to reside in the lipid fraction and was suggested to be AA since this fatty acid reproduced the effect. Our results further establish the important role of AA in intracellular communications system and as a pro-atherogenic factor by linking it to the production of matrix degrading protease MMP-9 by way of PI3K.


In summary, MonoMac 6 cells secreted MMP-9 in response to increasing clinically relevant concentrations of AA in the medium. The secretion increased due to increased expression of MMP-9 mRNA. MMP-9 secretion started fairly rapidly and could not be prevented by simultaneous presence of n-3 series fatty acids. The secretion could be attenuated by LY 298002, a specific phosphatidylinositol-3-kinase inhibitor and by SH-5, a selective Akt inhibitor, which suggests that activation of phosphatidylinositol-3-kinase by AA leads to augmented and sustained MMP-9 production.


Cell culture

MonoMac 6, an established human monocytic cell line that grows in suspension, was obtained from the German Collection of Microorganisms and Cell Cultures (DSMZ ACC 124; Braunschweig, Germany). Cell cultures were maintained in RPMI-1640 medium (BioWhittaker, Belgium) supplemented with 2 mM L-glutamine, 5 ml/l non-essential amino acids, penicillin (50 IU/ml), streptomycin (100 μg/ml), 1 mM sodium pyruvate, 1 mM oxaloacetate, 0.2 U/ml bovine insulin (OPI Media Supplement, Sigma Chemicals Co) and 10% heat-inactivated fetal bovine serum (FBS). The cells were cultured at a density of 0.3 – 1 × 106 cells/ml in humidified 5% CO2 at 37°C. Fresh medium was added to the cultures twice weekly replacing one third of the suspension which was either reseeded or discarded. For the experiments, cells were harvested, washed with phosphate buffered saline (PBS), pH 7.4, and seeded on 12-well Nunclon plates (Nunc A/S, Denmark) at 0.8 × 106 cells/ml in serum-free medium X-Vivo 15 (BioWhittaker, Belgium) supplemented with penicillin-streptomycin. The cells were incubated in the presence of indicated concentrations of fatty acids (AA, EPA, DPA, DHA, all from Cayman Chemical), PMA (Sigma), LY 294002 (Cayman Chemical) or SH-5 (Alexis Biochemicals) for 24 h unless otherwise stated. Cell viability was checked with the Trypan Blue exclusion test. Cellular protein concentrations were determined by the method of Lowry.


Gelatin zymography was essentially done as described [35]. Media from MonoMac 6 incubations were diluted in electrophoresis sample buffer [36] and subjected to electrophoresis in a 10% SDS-polyacrylamide gel embedded with 1 mg/ml gelatin (Sigma) in nonreducing conditions. We used the Mini-PROTEAN II apparatus at 4°C (Bio Rad). After electrophoresis the enzymes were renatured with two 30 min washes in 0.25% Triton X-100, and then the enzyme reaction was allowed to proceed in activation buffer (50 mM Tris-HCl, pH 7.5, containing 15 mM CaCl2, 1 μM ZnCl2 and 1% Triton X-100) at 37°C for 18 h. Thereafter the gels were stained for 1.5 h with 0.1% (w/v) Coomassie Brilliant Blue in 40% (v/v) isopropanol and destained in 7% acetic acid for a minimum of 3 h. As a molecular weight marker we used BenchMark™ Protein Ladder from Invitrogen.

Image analysis

The degree of gelatin digestion was quantified using an Epson Perfection 3200 Photo scanner interfaced to a computer. Gels were scanned using Epson Scan software (version 1.00E) in transparency option and gray scale mode. The density of each pixel is encoded on a scale ranging from 1 (clear) to 255 (opaque). The scanner was calibrated using the Stouffer Graphic Arts step tablet. The images were analysed with Scion Image software (Scion Corporation). The density measurements were linearized using the Rodbard curve-fitting function within the Scion Image program. The images were digitally inverted so that integration of bands is reported as positive values. The pixel density was determined after background density subtraction and used to calculate the integrated density of a selected band. The integrated density values of gelatinolytic activity of MMP-9 are reported in volume units of pixel intensity per mm2 and adjusted for cellular protein concentration.


Total RNA was isolated from fresh cells using a commercial kit (Invitrogen Ltd, Paisley, UK). After isolation, RNA was incubated with DNAse I to remove genomic DNA. To determine the concentration and purity of RNA, the absorbance was measured at 260 nm and 280 nm in a spectrophotometer from an aliquot of the samples. Before cDNA synthesis, the integrity and size distribution of total RNA was checked by agarose gel electrophoresis and ethidium bromide staining.

cDNA synthesis and RT-PCR

Total RNA was reverse transcribed to cDNA using TagMan reverse transcription reagents (Roche Molecular Systems, Inc, Branchburg, NJ, USA).

Relative quantification of MMP-9 mRNA levels was done using real time PCR (AbiPrism 7000, Applied Biosystems, Foster City, CA, USA) with TagMan Assays-on-demand probe process (assay ID Hs00234579-m1). Eukaryotic translation elongation factor (EEF-2) mRNA was used as an endogenous RNA control (assay ID Hs00157330-m1). Relative quantification of the target MMP-9 mRNA levels in comparison to the reference gene EEF-2 (ratio) was calculated using the comparative CT method. The results were expressed as N-fold differences in MMP-9 expression relative to EEF-2 expression.

Analysis of cellular fatty acid composition

All organic solvents were redistilled. Chloroform, methanol, toluene (all analytic grade) were purchased from Merck (Darmstadt, Germany). Petroleum spirit (b.p. 60–69°C) was from Neste Oy (Finland).

The cells were stored under nitrogen at -70°C until analysis. Lipids were extracted from approximately 1.2 × 106 cells with chloroform-methanol, partitioned, and the chloroform phase was dried under N2 [37]. Tripentadecanoic acid was added as an internal standard. Saponification of lipids was carried out by boiling in 33% KOH in ethanol at 85°C for 2 h. The nonsaponifiable lipids were extracted into petroleum spirit. The lower phase was acidified with HCl, and the fatty acids were extracted into petroleum spirit. After evaporation of the solvent in a stream of nitrogen, the residue was dissolved in toluene and the fatty acids were esterified with 2% H2SO4-methanol at 80°C for 2 h. The methyl esters of fatty acids were extracted into petroleum spirit. The fatty acids were analysed with Hewlett-Packard 5890A gas chromatograph equipped with a flame ionisation detector using a Nordion NB 351 capillary column (25 m, 0.32 mm I.D., 0.20 μm).

Data analysis

Results are expressed as mean ± SEM. Statistical comparisons were made by one-way analysis of variance using SPSS software, version 16.0. Post hoc comparisons of means were made using Dunnett's test. A p value < 0.05 was taken to be statistically significant.



We appreciate the expert technical assistance of Ulla Saarijoki. This study was supported by grants from Competitive research funding of the Pirkanmaa Hospital District and the Finnish Cultural Foundation.

Authors’ Affiliations

Department of Medical Biochemistry, University of Tampere Medical School
Institute of Medical Technology, University of Tampere
Department of Clinical Chemistry, Tampere University Hospital


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