Article | Open

Antifouling potential of Nature-inspired sulfated compounds

  • Scientific Reports 7, Article number: 42424 (2017)
  • doi:10.1038/srep42424
  • Download Citation
Received:
Accepted:
Published online:

Abstract

Natural products with a sulfated scaffold have emerged as antifouling agents with low or nontoxic effects to the environment. In this study 13 sulfated polyphenols were synthesized and tested for antifouling potential using the anti-settlement activity of mussel (Mytilus galloprovincialis) plantigrade post-larvae and bacterial growth inhibition towards four biofilm-forming bacterial strains. Results show that some of these Nature-inspired compounds were bioactive, particularly rutin persulfate (2), 3,6-bis(β-D-glucopyranosyl) xanthone persulfate (6), and gallic acid persulfate (12) against the settlement of plantigrades. The chemical precursors of sulfated compounds 2 and 12 were also tested for anti-settlement activity and it was possible to conclude that bioactivity is associated with sulfation. While compound 12 showed the most promising anti-settlement activity (EC50 = 8.95 μg.mL−1), compound 2 also caused the higher level of growth inhibition in bacteria Vibrio harveyi (EC20 = 12.5 μg.mL−1). All the three bioactive compounds 2, 6, and 12 were also found to be nontoxic to the non target species Artemia salina (<10% mortality at 250 μM) and Vibrio fischeri (LC50 > 1000 μg.mL−1). This study put forward the relevance of synthesizing non-natural sulfated small molecules to generate new nontoxic antifouling agents.

Introduction

The process of biofouling involves the attachment of a range of micro- and macroorganisms in natural and artificial underwater surfaces, constituting a diverse settled community that causes serious problems and large investments to maritime industry worldwide1,2,3. Short-term prevention of biofouling currently implies the use of biocide-based antifouling paints. After the ban of tributyltin (TBT) in several countries4, some booster biocides have been introduced based on Cu2+ paints as less toxic antifouling (AF) agents. However, significant environmental harm was also attributed to these AF active principals5. Recent international regulation (EU Regulation n° 528/2012) has been issued for biocides currently used in antifouling coatings, and many have been banned by individual initiative of many countries, through tight legislation.

Considering this, efforts have been applied on the development of alternative nontoxic and environmentally friendly AF agents. These agents should be capable to inhibit the settlement of selected biofouling species by acting in more specific signaling targets, somehow related with settlement processes, instead of inducing general toxicity6. Therefore, in the pursuit of an environmental friendly strategy for marine biofouling control, both effectiveness and toxicity of new AF agents need to be well established.

Sulfation of biomolecules is a metabolic strategy used by Nature to prevent toxicity in different physiological and pathological processes7. Some marine sulfated secondary metabolites, namely sulfated polyphenols, such as flavonoids, coumarins, cinnamic acids, and sulfated sterols, have been emerged as antifoulants with low or nontoxic effects to the environment8,9,10,11,12,13,14. Particularly, sulfated cinnamic acid (thereafter referred as zosteric acid), a natural metabolite from the sea grass Zostera marina, has been mentioned as a fully biodegradable and nontoxic natural AF agent14,15,16,17. Considering that commercial supply issues limit an effective implementation of natural products in AF coatings18,19, the aim of this study was to search for potential synthetic sulfated derivatives (Fig. 1, 113) as new relevant nontoxic AF agents. Different chemical classes were selected for sulfation (Fig. 1113) to represent the chemical diversity found in known marine antifoulants, namely xanthones20, flavonoids, including flavonols and one flavone11, coumarins12, and cinnamic acid derivatives14,15,16,17. This chemical diversity will allow structure-activity relationship (SAR) studies. Polysaccharides are a promising material for antifouling surfaces because their chemical composition makes them highly hydrophilic and able to form water-storing hydrogels. A number of recent studies showed that coatings with amphiphilic properties have a high potential for inert surface coatings, a property that can be established in the hydrophilic polysaccharides network via chemical modifications with hydrophobic molecules21. Therefore, flavonoids, xanthones, coumarins and other polyphenols with C-glysosyl and O-glycosyl linked to a diversity of saccharidic units, namely glucose, galactose, and rutinose were selected. The linkage between these two molecular moieties was also planned to contain a triazole group in order to mimic potent triazole-based biocides22. Furthermore, in order to develop an attractive protection against fouling from a bioenergetic point of view, a low cost synthesis of the potential biologically active compounds was guaranteed by the selection of raw materials such as diosmin, hesperidin, rutin, ethoxyrutin, resveratrol glucoside, gallic acid, and chlorogenic acid, which are readily available.

Figure 1: Sulfated compounds chemical structures.
Figure 1

1, diosmin 2″,2″′,3″,3″′,4″,4″′-hexasulfate; 2, rutin 2″,2″′,3′,3″,3″′,4′,4″,4″′,7-nonasulfate; 3, 3″,4″-bis(2-sulfate ethoxy)-7-(2-sulfate ethoxy)-rutin 2″,2″′,3′,3″′,4′,4″′,7-sulfate; 4, 3,7-di(β-D-glucopyranosyl)flavone persulfate; 5, mangiferin 2′,3,3′,4′,6,6′,7-heptasulfate; 6, 3,6-bis(β-D-glucopyranosyl)xanthone persulfate; 7, 3,6-bis(1-(1-(β-D-galatopyranosyl)-1H-1,2,3-triazole-4-yl)methoxy)xanthone persulfate; 8, trans-resveratrol 3-β-D-glucopyranoside persulfate; 9, salicin persulfate; 10, 4-methylumbelliferyl 7-β-D-glucopyranoside persulfate; 11, 4-methylumbelliferyl 7-β-D-galactopyranoside persulfate; 12, gallic acid persulfate; 13, chlorogenic acid persulfate.

To assess their AF effectiveness and toxicity, ecotoxicological bioassays towards the macrofouling organism Mytilus galloprovincialis using adhesive plantigrades and also antibacterial assays using several biofilm-forming marine bacteria (Cobetia marina, Vibrio harveyi, Pseudoalteromonas atlantica and Halomonas aquamarina) were conducted. Mytilus spp. are among the most common biofouling species with worldwide representatives. The larval phases responsible for the initial settlement of Mytilus galloprovincialis have produced consistent results in anti-settlement bioassays23,24,25,26,27. Marine bacterial biofilms are known to modulate in some degree the succession of colonization of macrofouling species28. Evidences show that the inhibition/induction of settlement is dependent on the nature of the bacterial biofilms regarding the production/absence of proteolytic enzymes29. Thus, biofilm inhibition assessment of different biofilm-forming marine bacteria can give valuable insights on the effectiveness and eventually mode of action of promising bioactive compounds.

Finally, compounds showing promising AF bioactivity were further tested in complementary bioassays to assess the viability of selected compounds as AF products. These complementary bioassays include: toxicity to sensitive non target species Artemia salina and Vibrio fischeri; the assessment of the anti-settlement activity of their chemical precursors (non-sulfated) to evaluate the influence of the sulfate groups in the AF activity; the bioaccumulation potential and the evaluation of possible mechanims of action related with adhesion and neurotransmission pathways.

Results

Syntheses and structure elucidation of sulfated compounds

Sulfated compounds 1–13 were obtained by reaction of the corresponding hydroxylated derivatives with triethylamine-sulfur trioxide adducts in moderate yields. For the new described derivatives, 3,7-di(β-D-glucopyranosyl)flavone persulfate (4), 3,6-bis(1-(1-(β-D-glucopyranosyl)-1H-1,2,3-triazole-4-yl)methoxy)xanthone persulfate (7), and 4-methylumbelliferyl 7-β-D-galactopyranoside persulfate (11), microwave assisted synthesis was successful in achieving persulfation. The complete structure elucidation of the new sulfated derivatives (4, 7, and 11) was possible to obtain by IR, NMR, and HRMS. The IR spectra of sulfated derivatives showed the presence of two strong bands corresponding to the S = O (ca 1250–1260 cm−1) and C-O-S (ca 1030–1070 cm−1) and a band around 800 cm−1 corresponding to the S-O. The HRMS allowed the elucidation of the number of sulfate groups. The assignments of the protonated carbons were achieved from HSQC experiments and the chemical shifts of the carbon atoms not directly bonded to proton atoms were deduced from HMBC correlations. The purity of the investigated compounds 1–13 was at least 95%.

Antifouling bioactivity

From the series of sulfated derivatives 1–13, four compounds (1, 2, 6, and 12) showed a significant inhibitory effect (p < 0.05) against the settlement of M. galloprovincialis plantigrades, and nine compounds were not significantly different from the negative control (Fig. 2). However, since compound 1 showed significant anti-settlement activity only for the highest concentration tested (250 μM), only three promising AF compounds (2, 6, and 12) were considered from this primary screening based on the significant anti-settlement responses at 50 μM (Fig. 2).

Figure 2: Anti-settlement activity of sulfated compounds 1–13 towards plantigrades of the mussel Mytilus galloprovincialis.
Figure 2

*Indicates significant differences (p < 0.05, Dunnett test) against the negative control (B: ultra-pure water); CuSO4 at 5 μM was used as positive control (C).

The concentration-response analysis using successive concentrations between 1.56–500 μM (Fig. 3) revealed that the most effective anti-settlement activity was observed for compound 12 (EC50 = 17.65 μM; 8.4 μg.mL−1), followed by compounds 2 (EC50 = 22.59 μM; 36.84 μg.mL−1) and 6 (EC50 = 23.19 μM; 31.74 μg.mL−1) (Table 1).

Figure 3: Concentration-response of anti-settlement activity of the promising AF compounds 2, 6, and 12 towards plantigrades of the mussel Mytilus galloprovincialis.
Figure 3

*Indicates significant differences at p < 0.05 (Dunnett test) ** at p < 0.001 (Dunnett test), against the negative control (B: ultra-pure water); CuSO4 at 5 μM was used as positive control (C).

Table 1: Antifouling effectiveness versus toxicity of sulfated compounds 2, 6, and 12 and the commercial AF compound ECONEA® towards the anti-settlement of mussel plantigrades.

Compound 12 showed significant anti-settlement activity in the range 12.5–500 μM when compared to negative control, while compounds 2 and 6 only showed significant bioactivity for higher concentrations (25–500 μM) (Fig. 3).

Regarding toxicity, none of the three selected compounds caused mortality to the target species M. galloprovincialis plantigrades at any of the tested concentrations, while the commercial eco-friendly AF agent ECONEA® showed some toxicity at the higher concentrations tested (LC50 = 107.78 μM) (Table 1). Therefore, LC50 values for sulfated compounds were considered as higher than 500 μM, and this value was used to estimate the therapeutic ratios LC50/EC50. Therapeutic ratios higher than 22.13, 21.56, and 26.61 μM were found for compounds 2, 6, and 12, respectively (Table 1).

From the obtained chromatograms (data not shown), a concentration of at least 95% of the initial one was detected for each compound, 2, 6, and 12, for the time period and temperature of the AF assay, warranty that the sulfated derivatives were stable in AF assay conditions.

Chemical precursors of compounds 2 and 12, rutin (14) and gallic acid (15) respectively, did not show significant anti-settlement activity when compared to the negative control (S1).

Acetylcholinesterase and tyrosinase activities

Acetylcholinesterase and tyrosinase activities were not inhibited by any of the three promising sulfated compounds 2, 6, and 12 (S2).

Antibacterial activity

Two compounds, 2 and 4, from the series of sulfated derivatives 1–13 showed a significant inhibitory activity against bacterial growth, namely against V. harveyi and H. aquamarina strains, respectively. The other eleven compounds either induced or had no effect on the bacterial growth when compared to the negative control (Fig. 4).

Figure 4: Antibacterial activity of sulfated compounds 1–13 towards four biofilm-forming marine bacteria Cobetia marina, Vibrio harveyi, Pseudoalteromonas atlantica and Halomonas aquamarina.
Figure 4

*Indicates significant diferences (p < 0.05, Dunnett test) against the negative control (B: ultra-pure water); penicilin-streptomycin-neomycin stabilized solution was used as positive control (C).

Regarding the concentration-response analysis of the two bioactive antibacterial compounds, compound 2 showed significant antibacterial activity against V. harveyi for the concentrations of 3.12 (27.9% growth inhibition) to 100 μM (15% growth inhibition) when compared to negative control, while compound 4 showed significant bioactivity against H. aquamarina from the concentrations of 12.5 (15.3% growth inhibition) to 100 μM (26.5% growth inhibition) (Fig. 5).

Figure 5: Concentration-response of antibacterial activity of the promising AF compounds 2 and 4 towards Vibrio harveyi and Halomonas aquamarina, respectively.
Figure 5

*Indicates significant differences at p < 0.05 (Dunnett test) against the negative control (B: ultra-pure water); penicilin-streptomycin-neomycin stabilized solution was used as positive control (C).

The percentages of growth inhibition reached, even at the higher concentrations tested, are below 30%. Thus, for both compounds the antibacterial efficacy only enabled the determination of the response concentrations that inhibited 20% of bacterial growth (EC20), being 7.69 and 42.3 μM (12.5 and 51.22 μg.mL−1) for compounds 2 and 4, respectively (Table 2).

Table 2: Bacterial growth inhibition activities of compounds 2 and 4.

Artemia salina ecotoxicity assay

The three compounds selected from the initial screening as potential AF compounds (2, 6, and 12) showed less than 10% mortality to A. salina nauplii at concentrations of 25, 50, and 250 μM (S1). The observed lethality was not significantly different (p < 0.01) from the negative control (filtered seawater) and thus these compounds showed no toxicity to this non target species (S3).

Luminescent Vibrio fischeri ecotoxicity assay (ISO11348)

Results from the Luminescent Vibrio fischeri assay revealed that the three compounds selected from the initial AF screening (2, 6, and 12) do not exert significant general ecotoxicity, as no inhibition of light radiation emitted was found, either after a contact time of 15 min or 30 min (LC50 > 1000 μg/mL) (S4).

In silico evaluation of bioaccumulation potential

In contrast to commercial AF agents, namely the toxic agent tributyltin oxide (TBTO), and two eco-friendly agents Sea-nine and ECONEA®, log Kow lower than 3 were obtained for compounds 2, 6, and 12 (S5), indicating the low bioaccumulation potential of the three hit compounds of the present study.

Discussion

Nature uses sulfation mainly to avoid potential toxicity, so synthesis of non-natural sulfated small molecules could be a way of giving Nature a helping hand in generating new nontoxic bioactive agents. Thus, in this work, a series of Nature inspired sulfated compounds 1–13 was synthesized and tested for the AF potential. This series of compounds was obtained by a simple and efficient synthesis, with yields exceeding 80%, with high scale-up potential, isolated with purity higher than 95% by a purification process under environmentally favorable conditions (Portuguese patent n° 104739)30.

From the AF screening, persulfated flavonoid 2, xanthone 6, and phenolic acid 12, showed therapeutic ratios (LC50/EC50) higher than 15, which is in accordance with the standard requirement for efficacy level of natural AF agents as established by the US Navy program31. Since chemical precursors tested, rutin (14) and gallic acid (15), were not active towards anti-settlement in the same conditions, the bioactivity of compounds 2 and 12 against mussel plantigrades can be associated with the presence of the sulfate groups. However, other sulfated compounds did not show notable activity. These results show that the nature of the scaffold plays a role in placing sulfate groups in favorable position for the activity: (i) while xanthone 6 was highly active, a structure related xanthone (compound 7) in which the O-linkage was replaced by a triazole linkage, was not active; (ii) while flavonoid 2 was highly active, other three flavonoids (compounds 1, 3, and 4) did not show notable activity, showing that sulfate groups at positions 5, 7, 3′, and 4′ on the flavonoid scaffold were crucial for the anti-settlement activity on this macrofouling species; and (iii) since compound 13, with an alkylcarboxy group was much less potent than compound 12, which contains an arylcarboxy group, the degree of acidity of the carboxylic group seems to influence the activity.

From the three promising compounds, a good level of effectiveness (defined by an EC50 value < 25 μg.mL−1) was only achieved for compound 12. Considering the effectiveness, compound 12 (EC50 = 8.4 μg.mL−1) was recognized to have the highest potential as effective AF agent. When comparing the structures of three most promising compounds, it is reasonable to hypothesize that a benzoic acid scaffold (compound 12) is associated with a more interesting AF activity. In fact, the importance of a benzoic acid moiety in the AF activity was previously observed32,33. It is interesting to point out that the hit compound in this study, gallic acid persulfate (12) is structurally-related to a previously described naturally-occurring AF agent, the zosteric acid, a metabolite from the sea grass Zostera marina. Zosteric acid has been found to prevent the attachment of bacteria14,15,16,34,35, fungus17,36 and higher-order organisms37 at nontoxic concentrations. The AF capability of zosteric acid was firstly attributed to the sulfate ester group14. More recently, the anti-biofilm activity of zosteric acid against E. coli was proven to be related to the cinnamic acid scaffold12,32.

When compared with the commercial eco-friendly AF agent ECONEA®, sulfated compounds presented lower levels of effectiveness, however have evidenced more potential as ecofriendly AF agents considering the nontoxic effects found.

The specific AF molecular targets and the mechanisms of action of booster biocides currently in used in marine paints remain largely unknown. AF compounds described in literature with known molecular targets mainly act on ion channels, enzymes, adhesive production and neurotransmission blocking6. Therefore, in this study, in vitro quantification of two enzymes (acetylcholinesterase and tyrosinase) having a metabolic role in the settlement of macrofouling organisms was performed to assess a possible mechanism of action for the promising synthesized compounds (S2). Acetylcholinesterase (AChE) has been suggested as being involved in the settlement of marine organisms, with AChE inhibitors being found to inhibit larval settlement38,39, while DOPA-containing adhesive plaques of mussels are thought to be produced by the action of tyrosinase on a protein precursor40. Nevertheless, no effect was observed in the activity of these enzymes indicating that at least these two pathways seem to remain unchanged after exposure to the synthesized compounds and the observed bioactivity seems to be not linked to these functions inhibition.

Considering the antibacterial activity, sulfated compounds did not present particular effectiveness, as results indicate that only compounds 2 and 4 had the ability to inhibit bacterial growth (less than 30% at all the concentrations tested) of one of the bacterial strains each (V. harveyi and H. aquamarina, respectively). The fact that low antibacterial activity was found and no consistent growth inhibition results were observed among all the tested bacterial strains seems to give an indication of sulfated compounds anti-settlement mode of action. In fact, the mode of action playing in M. galloprovincialis plantigrades seems to be organism-specific, more related with plantigrades metabolic pathways, rather than with the biofouling ecological succession cascade, which starts with the colonization of biofilms41. On the other hand, these results put in evidence the low toxicity of these sulfated compounds towards different bacterial strains, enhancing their potential as AF agents.

Concerning general ecotoxicity assessment, the standard lethality A. salina bioassay revealed that none of these promising compounds exerted significant lethal effects at the higher concentrations tested in anti-settlement assays (25, 50 and 250 μM), showing the low toxicity potential of these synthesized compounds. The nontoxic nature of the promising compounds 2, 6, and 12 was also confirmed by the lack of light radiation inhibition on the V. fischeri luminescent assay. Adding to the low toxicity potential, the bioactive sulfated compounds 2, 6, and 12, are highly water soluble, suggesting also a low bioaccumulation potential. Existing measurements of persistence, bioaccumulation and biodegradation are a cumbersome and expensive process, and thus not applied in the early stages of the product discovery and development. Nevertheless, in silico screening tools for the search for “environmentally-benign” antifouling biocides provide a valuable resource in early decision-making when applied with discretion42. Thus, log Kow (octanol-water partition coefficient) were calculated for the most promising compounds (compounds 2, 6, and 12) and compared with those calculated for some marketed AF agents and in contrast to the latter, compounds 2, 6, and 12 were shown to have low potential for bioaccumulation. In conclusion, new synthetic AF scaffolds were disclosed in this work, namely a polysulfated flavonoid, xanthone, and phenolic acid, with effective anti-settlement response towards M. galloprovincialis plantigrades, high seawater solubility, and general low toxicity and low potential for bioaccumulation. The viable synthetic process can predict their easy scale-up and future commercialization. Thus these results give important contributions for the future development of new environmental friendly AF coatings.

Material and Methods

All experiments were conducted in accordance with ethical guidelines of the European Union Council (Directive 2010/63/EU) and the Portuguese Agricultural Ministry (Portaria nr. 1005/92 of 23 October 2010) for the protection of animals used for experimental and other scientific purposes.

The starting materials for sulfation, diosmin (D 3525), rutin (R 2303), tri-hydroxyethylrutin (91950), mangiferin (M 3547), trans-resveratrol 3-β-D-glucopyranoside (572691), salicin (S 0625), 4-methyl 7-hydroxycoumarin 7-β-D-glucopyranoside (M 3633), 4-methyl 7-hydroxycoumarin 7-β-D-galactopyranoside (M 1633), gallic acid (D 3525), and chlorogenic acid (25700) were purchased from Sigma-Aldrich, Spain. The starting materials of compounds 4, 6, and 7, 3,7-di(β-D-glucopyranosyl)flavone, 3,6-bis(β-D-glucopyranosyl)xanthone, and 3,6-bis(1-(1-(β-D-galactopyranosyl)-1H-1,2,3-triazole-4-yl)methoxy)xanthone, respectively, were obtained following described procedures43,44 and their syntheses will be described elsewhere.

Melting points were obtained in a Köfler microscope and are uncorrected. Infrared (IR) spectra were recorded on a Perkin Elmer 257 in KBr. Nuclear magnetic resonance (NMR) spectra were taken in DMSO-d6 at room temperature, on Bruker DRX 300 instrument. Chemical shifts are expressed in δ (ppm) values relative to tetramethylsilane (TMS). High-resolution mass spectrometry (HRMS) results were obtained in CACTI services, Vigo, Spain.

High performance liquid chromatography with Diode-Array Detection (HPLC-DAD) analyses were carried out on a System SMI Pump Series II (Gloucester, UK) equipped with a Rheodyne 7125 injector fitted with a 20 μL loop, a TSP-UV6000LP detector, and a Chromquest for Windows NT integrator and using a C-18 Nucleosil column (5 μm, 250 × 4.6 mm I.D.), from Macherey-Nagel (Düren, Germany); acetonitrile was of HPLC grade from Merck. HPLC ultrapure water was generated by a Milli-Q system (Millipore, Bedford, MA, USA). The mobile phase used was water with tetrabutylammonium bromide (TBAB, 25 mM) and acetonitrile (38:62) at a constant flow rate of 1.0 mL.min−1. The mobile phase was filtered (45 μm) and degassed for 15 min in an ultrasonic bath before use.

Syntheses and structure elucidation of sulfated compounds

The following sulfated derivatives were synthesized according to previously described procedures (Fig. 1): diosmin hexasulfate (1), rutin persulfate (2), 3″,4″-bis(2-sulfate ethoxy)-7-(2-sulfate ethoxy)-rutin 2″,2″′,3′, 3″′,4′,4″′,7-sulfate (3), mangiferin 2′,3,3′,4′,6,6′,7-heptasulfate (5), 3,6-bis(β-D-glucopyranosyl)xanthone persulfate (6), trans-resveratrol 3-β-D-glucopyranoside persulfate (8), salicin persulfate (9), 4-methyl 7-hydroxycoumarin 7-β-D-glucopyranoside persulfate (10), gallic acid persulfate (12), and chlorogenic acid persulfate (13)45,46. Synthesis of new sulfated derivatives, compounds 4, 7, and 11, was achieved by sulfation of 3,7-di(β-D-glucopyranosyl)flavone, 3,6-bis(1-(1-(β-D-galactopyranosyl)-1H-1,2,3-triazole-4-yl)methoxy)xanthone, and 4-methyl 7-hydroxycoumarin 7-β-D-galactopyranoside, respectively, in microwave (MW) with triethylamine-sulfur trioxide adduct (8–10 equiv/OH) in dimethylacetamide. Generally, the reaction vessel was sealed, and the mixture was kept stirring and heated for 1 h at 100 °C under MW irradiation (2 cycles). After cooling, the mixture was poured into acetone (200 mL) under basic conditions (triethylamine until pH 8) and left at 4 °C for 24 h. The crude oil formed was washed with acetone and ether and then dissolved in aqueous solution of 30% sodium acetate (5 mL). The suspension was added dropwise in ethanol to precipitate the sodium salt of the sulfated derivative. In both syntheses of compounds 4 and 7, each solid obtained was further purified from other salts (monitored by IR) using a Spectra/Por 6 regenerated cellulose MWCO 1000. The purity of the investigated compounds was determined by HPLC-DAD analysis.

3,7-Di(2,3,4,6-tetrasulfate-β-glucopyranosyl)flavone (4)

Orange solid, mp 215–218 °C (methanol). IR (KBr, cm−1) υmax: 1627, 1066, 803. 1H NMR (DMSO-d6, 300.13 MHz) δ: 8.27 (2 H, d, J = 8.7 Hz, H-2′, H-6′), 8.07 (1 H, d, J = 8.7 Hz, H-5), 7.58–7.48 (3 H, m, H-3′, H-4′, H-5′), 7.30 (1 H, d, J = 2.2 Hz, H-8), 7.13 (1 H, dd, J = 8.7 and 2.2 Hz, H-6), 6.02 (1 H, d, J = 4.4 Hz, H-1″), 5.66 (1 H, d, J = 2.9 Hz, H-1″′), 4.76 (1 H, d, J = 4.4 Hz, H-2″), 4.72 (1 H, d, J = 4.0 Hz, H2″′), 4.65 (1 H, d, J = 1.7 Hz, H-3″), 4.62 (1 H, d, J = 2.4 Hz, H-3″′), 4.47 (1 H, t, J = 4.1 Hz, H-4″), 4.41 (1 H, t, J = 3.1 Hz, H-4″′), 4.20 (1 H, m, H-5″), 4.04–3.90 (5 H, m, H-5″′ and H-6″a, H-6″b, H-6″′a, H-6″′b). 13C NMR (DMSO- d6, 75.47 MHz) δ: 173.0 (C-4), 161.5 (C-9), 156.0 (C-7), 154.8 (C-1′), 143.6 (C-2), 136.5 (C-3), 130.4 (C-4′), 129.2 (C-2′, C-6′), 128.6 (C-3′, 5′), 126.8 (C-5), 118.1 (C-10), 115.5 (C-6), 103.3 (C-8), 98.8 (C-1″), 98.7 (C-1″′), 80.6 (C-2″), 76.2 (C-2″′), 76.1 (C-5″), 75.5 (C-5″′), 74.8 (C-3″), 74.2 (C-3″′), 72.0 (C-4″), 71.1 (C-4″′), 67.3–66.9 (C-6″, C-6″′). HRMS (ESI+) m/z calcd for C27H22Na9O38S8 [M + Na] 1416.66285, found 1416.66256.

3,6-Bis(1-(1-(2,3,4,6-tetrasulfate-β-D-galactopyranosyl)-1H-1,2,3-triazole-4-yl)methoxy)xanthone (7)

White solid, mp 205–208 °C (methanol). IR (KBr, cm−1) υmax: 1260, 1052, 805. 1H NMR (DMSO-d6, 300.13 MHz) δ: 8.24 (1 H, s, triazole), 8.08 (1 H, d, J = 8.9 Hz, H-1/H-8), 7.37 (1 H, brd, H-4/H-5), 7.18 (1 H, brdd, H-2/H-7), 5.92 (1 H, d, J = 8.5 Hz, H-1′), 5.35 (2 H, s, OCH2), 4.90 (1 H, s, H-2′), 4.83 (1 H, t, J = 8.8 Hz, H-4′), 4.53–4.49 (1 H, dd, J = 1.9 and 9.5, H-3′), 4.18 (1 H, J = 8.2, H -5′), 4.03–3.77 (2 H, m, H-6′a, H-6′b). 13C NMR (DMSO-d6, 75.47 MHz) δ: 174.2 (C-9), 163.5 (C-3, C-6), 157.5 (C-4a, C-10a), 141.2 (CH = C triazole), 127.4 (C-1, C-8), 124.4 (CH = C triazole), 115.1 (C-8a, C-9a), 113.9 (C-2, C-7), 101.5 (C-4, C-5), 86.3 (C-1′), 75.5 (C-5′), 75.0 (C-3′), 73.6 (C-2′), 72.1 (C-4′), 66.3 (C-6′), 62.0 (OCH2). HRMS (ESI+) m/z calcd for C31H26N6Na10O38S8 [M + H] 787.85091, found 787.85080.

4-Methyl-7-[(2S,3R,4R,5S,6R)-3,4,5-trisulfate-6-(methylsulfate)oxan-2-yl] oxychromen-2-one (11)

Pallid-yellow solid, mp > 340 °C (ethanol). IR (KBr, cm−1) υmax: 1617, 1257, 1032, 847. 1H NMR (DMSO-d6, 300.13 MHz) δ: 7.73 (1 H, d, J = 8.7 Hz, H-8), 7.04 (1 H, dd, J = 8.8 and 1.5 Hz, H-6), 6.93 (1 H, d, J = 1.5 Hz, H-5), 6.24 (1 H, s, H-3), 5.57 (1 H, d, J = 2.9 Hz, H-1′), 4.59 (2 H, m, H-2′ and H-4′), 4.42 (1 H, m, H3′), 4.00–3.88 (2 H, m, H-6′a/H-6′b), 1.16 (3 H, s, 4-CH3). 13C NMR (DMSO-d6, 75.47 MHz) δ: 160.2 (C-2), 160.2 (C-7), 154.4 (C-9), 153.6 (C-9/C-4), 113.6 (C-6), 103.6 (C-5), 111.8 (C-3), 114.3 (C10), 126.7 (C-8), 98.4 (C-1′), 75.2 (C-5′), 74.1 (C-2′/C4′), 73.9 (C-2′/C4′), 70.9 (C-3′), 67.1 (C-6′), 18.3 (4-CH3). HRMS (ESI+) m/z calcd for C16H14Na5O20S4 [M + Na] 768.84443, found 768.84443.

Mytilus galloprovincialis plantigrades collection and processing

M. galloprovincialis juvenile (0.5 cm shell length approximately) aggregates were collected from mussel beds from the intertidal rocky shore, during low neap tides at Memória beach, Matosinhos, Portugal (41°13′59″N; 8°43′28″W), and immediately transported to the laboratory. M. galloprovincialis plantigrade post-larvae (0.5–2 mm) were screened among the small mussel aggregates in a binocular magnifier (Olympus SZX2-ILLT), gently washed with filtered seawater to remove organic debris and sand particles and isolated in a petri dish with filtered seawater immediately before the bioassays.

Antifouling bioassays

For the screening bioassay, competent M. galloprovincialis plantigrades (showing exploring behavior, ie, moving their foot searching for the appropriate substrate to settle) were selected and exposed to the series of sulfated compounds 113 at two concentrations (250 and 50 μM) in 24-well microplates for 15 h, at 18 ± 1 °C, in the darkness. Bioassays time frame was selected based on preliminary bioassays to ensure that the response measured is reflecting the compounds effect. Test solutions were prepared in filtered seawater (previously treated by UV light, and carbon filters and mechanically filtered with 0.45 μM filter before use) and obtained by dilution of the compounds stock solutions (50 mM) in ultra-pure water. Four well replicates were used per condition with five plantigrades per well and 2.5 mL of test solution. A negative control, with ultra-pure water was included in all bioassays, as well as a positive control with 5 μM CuSO4 (a potent AF agent). At the end of the exposure period, the anti-settlement activity was determined by the presence/absence of byssal threads produced by each individual efficiently attached for all the conditions tested.

Compounds that have showed anti-settlement effectiveness at the concentration of 50 μM were selected for further testing at higher and lower successive concentrations (500, 250, 100, 50, 25, 12.5, 6.25, 3.12 and 1.56 μM) for the determination of the semi-maximum response concentrations that inhibited 50% larval settlement (EC50) and the median lethal dose (LC50). The commercial eco-friendly AF agent ECONEA® was also tested in the same experimental conditions for bioassay validation and to obtain comparable data regarding effectiveness and toxicity of sulfated compounds.

The seawater stability of the three most promising compounds 2, 6, and 12 in the time period (15 h) and temperature (18 °C) of the AF assay was evaluated by HPLC-DAD. Compounds were analyzed at 250 μM (final concentration) in filtered seawater (45 μm). Incubations were performed in glass HPLC vials and three independent samples plus respective blank (filtered seawater) and controls (time zero - freshly prepared solutions of compounds) were analyzed.

To test the hypothesis that the exerted antifouling activity is due to the molecular modification by sulfation, chemical precursors of promising AF compounds 2 and 12, rutin (14), and gallic acid (15), respectively, were also tested for AF activity at two concentrations (250 and 50 μM), at the same bioassay conditions as previously described, except for the negative control that in this case includes 0.1% DMSO, considering the low water solubility of the chemical precursors.

In vitro determination of acetylcholinesterase and tyrosinase activities

Acetylcholinesterase and tyrosinase inhibition were tested as potential AF mechanisms of action of compounds 2, 6, and 12.

The potential of compounds 2, 6 and 12 to inhibit acetylcholinesterases activity was evaluated using Electrophorus electric acetylcholinesterase Type V-S (SIGMA C2888, E.C. 3.1.1.7), according to Ellman et al.47 with some modifications48,49. Briefly, reaction solution containing phosphate buffer 1 M pH 7.2, dithiobisnitrobenzoate (DTNB) 10 mM (acid dithiobisnitrobenzoate and sodium hydrogen carbonate in phosphate buffer) and acetylcholine iodide 0.075 M was added to pure acetylcholinesterase enzyme (0.25 U/mL) and each test sulfated compound (final concentration of 50 μM) in quadruplicate. The optical density was measured at 412 nm in a microplate reader during 5 min at 25 °C. A negative control (B) with ultra-pure water and a positive control (C+) with 20 mM eserine also included.

Tyrosinase inhibition assays were conducted using Agaricus bisporus tyrosinase (EC 1.14.18.1) according to Adhikari et al.50 with slight modifications. The enzymatic reaction follows the catalytic conversion of L-Dopa to dopaquinone and the formation of dopachrome by measuring the absorvance at 475 nm. Briefly, tyrosinase (25 U/mL) is added to 50 mM fosfate buffer pH 6.5 and the sulfated compound at 50 μM. The enzymatic activity was triggered by the addition of L-dopa (25 mM). Kojic acid was included as positive control and ultra-pure water as negative control.

Antibacterial activity

Antibacterial activities were evaluated against four strains of marine biofilm-forming bacteria Cobetia marina CECT 4278, Vibrio harveyi CECT 525, Halomonas aquamarina CECT 5000, and Pseudoalteromonas atlantica CECT 570, all from Spanish Type Culture Collection (CECT). The bacteria were inoculated and incubated for 24 h at 26 °C in marine broth (Difco) at an initial density of 0.1 (OD600) in 96 well flat-bottom microtiter plates. Sulfated compounds stock solutions were prepared in ultra-pure water. For the initial screening, a final concentration of 12.5 μM was used in the bioassays, given the higher sensitivity of the bacteria when compared to mussel plantigrades. Bacterial growth inhibition in the presence of the test compounds was measured in quadriplicate by reading of optical density at 600 nm using a microplate reader (Biotek Synergy HT, Vermont, USA). Marine broth with ultra-pure water and penicilin-streptomycin-neomycin stabilized solution were used as negative (B) and positive (C) controls, respectively.

Compounds that showed significant inhibitory activity at this initial screening were selected for further bioassays. For the determination of maximal inhibitory concentrations (IC) a serial dilution of the stock solution was used to obtain final concentrations from 100 μM to 0.75 μM, the same range applied in antifouling bioassays plus one lower concentration, and the same procedure was applied.

Artemia salina ecotoxicity assay

Selected sulfated compounds with AF potential 2, 6, and 12 were tested for general toxicity to nontarget species using the brine shrimp (Artemia salina) nauplii lethality test51. Briefly, A. salina eggs were allowed to hatch in nutrient–enriched seawater as nauplii for approximately 48 h at 25 °C. Toxicity tests were performed in the darkness in 96-wells microplates with eight replicates per condition and 15–20 nauplii per well. Serial diluted test solutions of the most promising sulfated AF compounds (25, 50, and 250 μM) were prepared in filtered seawater. K2Cr2O7 (13.6 μM) was included as positive control and ultra-pure water as negative control. Percentage of mortality was determined at 48 h of exposure.

Luminescent Vibrio fischeri ecotoxicity assay (ISO11348)

Luminescent Vibrio fischeri ecotoxicity assessment (ISO11348) was performed by IK4 TEKNIKER accordingly to the EU hazard assessment of substances and European Ecolabel (ISO 113482). Luminescent Vibrio fischeri bacteria test (NRRL-B-11177) was used as a standard test to evaluate the ecotoxicity of the most promising AF compounds. Vibrio fischeri bacteria from HACH-LANGE GmbH were grown in laboratory in standard conditions according to guidelines and exposed to a dilution serial of each compound (1000, 500, 250, 125, 62.5 mg/L). After 5, 15 and 30 min of exposure, the light emitted as a by-product of Vibrio fischeri cellular respiration was measured at 490 nm. Any inhibition of cellular activity results in a decreased rate of respiration and a corresponding decrease in the rate of luminescence. The decrease of bacterial luminescence measured after 5, 15 or 30 min of exposition was used as test endpoint. Luminescence was measured using a LUMIStox photometer from DR LANGE, after a contact time of 15 min and 30 min at 15 ± 1 °C, taking into account a correction factor, fk, which is a measure of intensity change of control samples during the exposure time.

The pH of all samples was within the interval 6.0–8.5. A 2% solution of sodium chloride (NaCl) in deionized water (20 g/L) was used as dilution medium and K2Cr2O7 11.3μg.mL−1) was used as positive control.

In silico evaluation of bioaccumulation potential

KOWWIN™ v1.68 (log octanol-water partition coefficient calculation program)52 developed by Syracuse Research Cooperation jointly with the Environmental Protection Agency (EPA) was used for in silico calculation of log Kow (octanol-water partition coefficient) in order to evaluate the bioaccumulation potential of compounds 2, 6, and 12 when compared to other AF active principles in use. Compounds are considered potentially bioaccumulative if the log Kow (octanol-water partition coefficient) is higher than 3.

Data analysis

Data from the anti-settlement and antibacterial screenings were analyzed using a one-way analysis of variance (ANOVA) followed by a Dunnett test against the control (p < 0.05). Semi-maximum response concentration that inhibited 50% larval settlement (EC50), semi-maximum response concentration that inhibited 20% bacterial growth (EC20) and the median lethal dose (LC50) for each bioactive compound were assessed using Probit regression analysis. Pearson Goodness-of-fit (Chi-Square) significance was considered at p < 0.05 for all analyses, and 95% lower and upper confidence limits [95% LCL; UCL] were presented. Therapeutic ratio (LC50/EC50) was used to evaluate the effectiveness vs toxicity of compounds31,53,54. The software IBM SPSS Statistics 21 was used for statistical analysis.

Additional Information

How to cite this article: Almeida, J. R. et al. Antifouling potential of Nature-inspired sulfated compounds. Sci. Rep. 7, 42424; doi: 10.1038/srep42424 (2017).

Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

References

  1. 1.

    & Marine biofouling: a sticky problem. Biologist (London) 49, 10–14 (2002).

  2. 2.

    , , & Economic impact of biofouling on a naval surface ship. Biofouling 27, 87–98 (2011).

  3. 3.

    , & Antifouling technology - past, present and future steps towards efficient and environmentally friendly antifouling coatings. Progress in Organic Coatings 50, 75–104 (2004).

  4. 4.

    IMO. International Convention on the Control of Harmful Anti-fouling Systems on Ships. International Maritime Organization Adoption: 5 October 2001; Entry into force: 17 September 2008, (2008).

  5. 5.

    & The environmental fate and effects of antifouling paint biocides. Biofouling 26, 73–88 (2010).

  6. 6.

    , & Mini-review: Molecular mechanisms of antifouling compounds. Biofouling 29, 381–400 (2013).

  7. 7.

    , & In Natural Products: Chemistry, Biochemistry and Pharmacology (ed ) 392–416 (Narosa Publishing House, New Delhi, India, 2008).

  8. 8.

    , , , & Biological activity of Seaweed extracts from Cladophora clavuligera (Kutzing, 1843) and Sargassum wightii (Greville, 1995) against marine fouling bacteria. Indian Journal of Geo-Marine Sciences 40, 398–402 (2011).

  9. 9.

    , & Bioactive marine metabolites II. Halistanol sulfate, an antimicrobial novel steroid sulfate from the marine sponge halichondria cf. moorei bergquist. Tetrahedron Lett 22, 1985–1988 (1981).

  10. 10.

    et al. Chemical and Biological Investigation of the Polar Constituents of the Starfish Luidia clathrata, Collected in the Gulf of Mexico. Journal of Natural Products 58, 653–671 (1995).

  11. 11.

    , , & Evidence that a New Antibiotic Flavone Glycoside Chemically Defends the Sea Grass Thalassia testudinum against Zoosporic Fungi. Applied and Environmental Microbiology 64, 1490–1496 (1998).

  12. 12.

    , & Sulfation mediates activity of zosteric acid against biofilm formation. Biofouling 31, 253–263 (2015).

  13. 13.

    , , & Biologically-active sterol sulfates from the marine sponge Toxadocia zumi. Experientia 39, 759–761 (1983).

  14. 14.

    , , & The antifouling activity of natural and synthetic phenol acid sulphate esters. Phytochemistry 34, 401–404 (1993).

  15. 15.

    , , & Zosteric acid—An effective antifoulant for reducing fresh water bacterial attachment on coatings. Journal of Coatings Technology and Research 3, 69–76 (2006).

  16. 16.

    , , & Evaluation of toxicity of capsaicin and zosteric acid and their potential application as antifoulants. Environmental Toxicology 20, 467–474 (2005).

  17. 17.

    et al. Hindering biofilm formation with zosteric acid. Biofouling 26, 739–752 (2010).

  18. 18.

    et al. Structural optimization and evaluation of butenolides as potent antifouling agents: modification of the side chain affects the biological activities of compounds. Biofouling 28, 857–864 (2012).

  19. 19.

    , , & Anti-barnacle activity of novel simple alkyl isocyanides derived from citronellol. Biofouling 27, 201–205 (2011).

  20. 20.

    , , & Antifouling Compounds from the Marine-Derived Fungus Aspergillus terreus SCSGAF0162. Natural Product Communications 10, 1033–1034 (2015).

  21. 21.

    et al. Adhesion of Marine Fouling Organisms on Hydrophilic and Amphiphilic Polysaccharides. Langmuir 29, 4039–4047 (2013).

  22. 22.

    et al. Imidazole and Triazole Coordination Chemistry for Antifouling Coatings. Journal of Chemistry 2013, 23 (2013).

  23. 23.

    et al. Acetylcholinesterase in Biofouling Species: Characterization and Mode of Action of Cyanobacteria-Derived Antifouling Agents. Toxins 7, 2739–2756 (2015).

  24. 24.

    et al. Optimising settlement assays of pediveligers and plantigrades of Mytilus galloprovincialis. Biofouling 27, 859–868 (2011).

  25. 25.

    Effects of macroalgae and biofilm on settlement of blue mussel (Mytilus edulis l.) larvae. Biofouling 14, 153–165 (1999).

  26. 26.

    & The influence of natural surface microtopographies on fouling. Biofouling 20, 43–51 (2004).

  27. 27.

    , , & How effective is intermittent chlorination to control adult mussel fouling in cooling water systems? Water Research 37, 329–338 (2003).

  28. 28.

    Biofilms and Marine Invertebrate Larvae: What Bacteria Produce That Larvae Use to Choose Settlement Sites. Annual Review of Marine Science 3, 453–470, (2011).

  29. 29.

    , , , & Novel antifoulants: Inhibition of larval attachment by proteases. Marine Biotechnology 9, 388–397 (2007).

  30. 30.

    , , , & Xantonas sulfatadas e análogos xantónicos glicosilados sulfatados com actividade anticoagulante e processos para a sua preparação. Portugal patent (2011).

  31. 31.

    , & Natural products as antifouling compounds: recent progress and future perspectives. Biofouling 26, 223–234 (2010).

  32. 32.

    et al. Unravelling the Structural and Molecular Basis Responsible for the Anti-Biofilm Activity of Zosteric Acid. PloS one 10, e0131519 (2015).

  33. 33.

    & Incorporation of benzoic acid and sodium benzoate into silicone coatings and subsequent leaching of the compound from the incorporated coatings. Progress in Organic Coatings 56, 135–145 (2006).

  34. 34.

    et al. Evaluation of zosteric acid for mitigating biofilm formation of Pseudomonas putida isolated from a membrane bioreactor system. International Journal of Molecular Sciences 15, 9497–9518 (2014).

  35. 35.

    , , , & Altered expression level of Escherichia coli proteins in response to treatment with the antifouling agent zosteric acid sodium salt. Environmental Microbiology 14, 1753–1761 (2012).

  36. 36.

    et al. Efficacy of zosteric acid sodium salt on the yeast biofilm model Candida albicans. Microb Ecol 62, 584–598 (2011).

  37. 37.

    , , & Evaluation of the natural product antifoulant, zosteric acid, for preventing the attachment of quagga mussels-a preliminary study. Natural Product Research 26, 580–584 (2012).

  38. 38.

    , , , & Involvement of acetyl choline in settlement of Balanus amphitrite. Biofouling 19 Suppl, 213–220 (2003).

  39. 39.

    , & Acetylcholinesterase activity in juvenile Ciona intestinalis (Ascidiacea, Urochordata) after exposure to tributyltin. Caryologia 65, 18–26 (2012).

  40. 40.

    , & Phenoloxidase (EC 1.14.18.1) from the byssus gland of Mytilus edulis: Purification, partial characterization and application for screening products with potential antifouling activities. Biofouling 16, 235–244 (2000).

  41. 41.

    & Natural chemical cues for settlement and metamorphosis of marine invertebrate larvae. Marine chemical ecology. CRC Press, Boca Raton, FL, 431–461 (2001).

  42. 42.

    , , & Searching for “Environmentally-Benign” Antifouling Biocides. International Journal of Molecular Sciences 15, 9255 (2014).

  43. 43.

    et al. Polysulfated Xanthones: Multipathway Development of a New Generation of Dual Anticoagulant/Antiplatelet Agents. Journal of Medicinal Chemistry 54, 5373–5384 (2011).

  44. 44.

    & The copper(I)-catalyzed alkyne-azide cycloaddition (CuAAC) “click” reaction and its applications. An overview. Coordination Chemistry Reviews 255, 2933–2945 (2011).

  45. 45.

    et al. Flavonoids with an Oligopolysulfated Moiety: A New Class of Anticoagulant Agents. Journal of Medicinal Chemistry 54, 95–106 (2011).

  46. 46.

    et al. Dual anticoagulant/antiplatelet persulfated small molecules. European Journal of Medicinal Chemistry 46, 2347–2358 (2011).

  47. 47.

    , , & A new and rapid colorimetric determination of acetylcholinesterase activity. Biochemical Pharmacology 7, 88–95 (1961).

  48. 48.

    et al. Acetylcholinesterase in Biofouling Species: Characterization and Mode of Action of Cyanobacteria-Derived Antifouling Agents. Toxins 7, 2739 (2015).

  49. 49.

    , & Sea-urchin (Paracentrotus lividus) glutathione S-transferases and cholinesterase activities as biomarkers of environmental contamination. Journal of Environmental Monitoring 7, 288–294 (2005).

  50. 50.

    et al. Screening of Nepalese crude drugs traditionally used to treat hyperpigmentation: in vitro tyrosinase inhibition. International Journal of Cosmetic Science 30, 353–360 (2008).

  51. 51.

    et al. Brine shrimp: a convenient general bioassay for active plant constituents. Planta Medica 45, 31–34 (1982).

  52. 52.

    Estimation Programs Interface Suite™ for Microsoft® Windows, v 4.11. United States Environmental Protection Agency, Washington, DC, USA (2016).

  53. 53.

    & Natural antifouling compounds: effectiveness in preventing invertebrate settlement and adhesion. Biotechnology Advances 33, 343–357 (2015).

  54. 54.

    In Recent advances in marine biotechnology, Vol. 3. Biofilms, bioadhesion, corrosion, and biofouling. (ed. , , ) 245–257 (Enfield, USA: Science Publishers Inc, 1999).

Download references

Acknowledgements

The authors thank to Elisabete Silva from the FFCUL for the ECONEA® sample. This research was supported by Fundação para a Ciência e Tecnologia (FCT), Projeto 9471 – Reforçar a Investigação, o Desenvolvimento Tecnológico e a Inovação (RIDTI) and by Fundo Comunitário Europeu FEDER - PTDC/AAG-TEC/0739/2014 (POCI-01-0145-FEDER-016793) under the project PTDC/AAG-TEC/0739/2014 (POCI-01-0145-FEDER-016793), and through a postdoctoral scholarship to J.R.A. (SFRH/BPD/87416/2012), to M.C.d.S. (SFRH/BPD/81878/2011), and a PhD scholarship to J.A. (SFRH/BD/ 99003/2013).

Author information

Affiliations

  1. CIIMAR/CIMAR - Interdisciplinary Centre of Marine and Environmental Research, University of Porto, Terminal de Cruzeiros do Porto de Leixões Avenida General Norton de Matos P 4450-208 Matosinhos, Portugal

    • Joana R. Almeida
    • , Marta Correia-da-Silva
    • , Emília Sousa
    • , Jorge Antunes
    • , Madalena Pinto
    • , Vitor Vasconcelos
    •  & Isabel Cunha
  2. Laboratory of Organic and Pharmaceutical Chemistry, Department of Chemical Sciences, Faculty of Pharmacy, University of Porto, Rua Jorge Viterbo Ferreira, 228, 4050-313 Porto, Portugal

    • Marta Correia-da-Silva
    • , Emília Sousa
    •  & Madalena Pinto
  3. Department of Biology, Faculty of Sciences, University of Porto, Rua do Campo Alegre, P 4069-007 Porto, Portugal

    • Jorge Antunes
    •  & Vitor Vasconcelos

Authors

  1. Search for Joana R. Almeida in:

  2. Search for Marta Correia-da-Silva in:

  3. Search for Emília Sousa in:

  4. Search for Jorge Antunes in:

  5. Search for Madalena Pinto in:

  6. Search for Vitor Vasconcelos in:

  7. Search for Isabel Cunha in:

Contributions

Chemical contribution, including synthesis, structural elucidation, and chemical stability evaluation in the conditions of the AF assay, was accomplished by M.C.d.S. and E.S. In vivo antifouling bioassays, enzymatic determinations and Artemia salina bioassays were performed by J.R.A. and I.C. Antibacterial experiments were executed by J.A. and J.R.A. V.V. and M.P. were involved in all aspects of this study. M.C.d.S. and J.R.A. wrote this manuscript but all the authors gave an important contribution in the revision of the manuscript.

Competing interests

The authors declare no competing financial interests.

Corresponding author

Correspondence to Marta Correia-da-Silva.

Supplementary information

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.

Creative CommonsThis work is licensed under a Creative Commons Attribution 4.0 International License. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in the credit line; if the material is not included under the Creative Commons license, users will need to obtain permission from the license holder to reproduce the material. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/