Carmen Rizzo1*, Giuseppa Genovese1, Marina Morabito1,
Caterina Faggio1, Maria Pagano1, Antonio Spanò1, Vincenzo Zammuto1,3, Simona Armeli Minicante2, Antonio Manghisi1, Rosalia Maria Cigala1, Francesco Crea1, Fabio Marinoand Concetta Gugliandolo1

1Department of Chemical, Biological, Pharmaceutical and Environmental Sciences, University of Messina, Italy, V.le Ferdinando Stagno d’Alcontres, 31, 98166, Messina,Italy.
2National Research Council, ISMAR, Arsenale Castello, 2737/F, 30122 Venezia, Italy.
3Department of Earth and Marine Sciences, University of Palermo, via Archirafi 18, Palermo, Italy.

Abstract:

The exploitation of macroalgal biomass, as a source of antibacterial drugs, would result into the valuable transformation of waste into an economic resource. Ethanol and water extractsor polysaccharides, from nine DNA-barcoded macroalgae (2 Chlorophyta, 5 Ochrophyta and 2 Rhodophyta) collected from Italian coastal environments, were screened for antibacterial activity against ten bacterial pathogens with relevance for aquaculture and human health. All extracts have not cytotoxic effects on molluscan digestive gland cells and mammalian red blood cells. As resulted by agar diffusion assays, water extracts showed broader and higher inhibitory activity than ethanol extracts against the tested pathogens. Polysaccharides from Fucus virsoides (Ochrophyta) possessed the strongest inhibitory activity against Aeromonas salmonicida subsp. salmonicida and Photobacterium damselae subsp. damselae, an emergent pathogen for humans.Polysaccharides from Undaria pinnatifida (Ochrophyta)were the most active against V. harveyi, the major pathogen responsible for diseases in aquaculture, and also against a multiresistant, clinical strain of Pseudomonas aeruginosa. Our results suggest that these polysaccharides could represent a novel source of compounds active against bacterial pathogens relevant for eco-sustainable aquaculture and human health.

Keywords:

algae; antibacterial activity; aquaculture; DNA barcoding; fish pathogens; polysaccharides.

INTRODUCTION

Marine macroalgae represent a great source of biomolecules with a wide spectrum of effects useful in different biotechnological fields, such as in food and textiles industries, biochemistry, pharmacology and in human and veterinary medicine. Green, brown and red algal crude extracts, and their fractioned or purified components, have been reported to exhibit anticoagulant, antibacterial, antiviral, antioxidant and anticancer activities [1-4]. Several studies have reviewed the antimicrobial properties of extracts from marine algae for food and pharmaceutical purposes [5-6]. Since diseases of bacterial origin are cause of considerable economic losses in aquaculture activities, the search for novel metabolites active against pathogens relevant in aquaculture has increased during the recent years [4, 7, 8].

Some species belonging to Aeromonas and Vibrio genera, which are ubiquitous in freshwater and marine environments, have been recognized as pathogenic for a variety of economically important fish and shellfish species, and also for humans, causing enteric pathologies, primary and secondary septicaemia, and wound infections [9, 10]. A. hydrophila, frequently isolated from seafood and shellfish, is often associated with diseases of aquatic animals and also is primary or opportunistic pathogen in humans [11]. A. salmonicida subsp. salmonicida is the causative agents of furunculosis, a bacterial septicaemia of salmonid and turbot [12]. Several vibrios, such as Listonella anguillarum (formerly Vibrio anguillarum), V. harveyi, V. parahaemolyticus and V. vulnificus are responsible for the most common vibriosis in fish and shellfish [13]. On the other hand, V. cholerae and non-epidemic vibrios, including V. parahaemolyticus and V. vulnificus, have been implicated in human diseases associated with the consumption of raw or undercooked shellfish, or the exposure of skin wounds to contaminated fish and waters [14]. V. harveyi is considered a serious pathogen of marine fish, the diseases include vasculitis, gastro-enteritis and eye lesions, and of invertebrates, particularly penaeid shrimps and abalone(Haliotistuberculata) of which it is often cause of mortality [15]. Among members of the Vibrionaceae family, Photobacterium damselae subsp. piscicida has been recognized as the causative agent of fish photobacteriosis, and Photobacterium damselae subsp. damselae has been considered a primary pathogen of a variety of marine animals (including crustaceans, molluscs and cetaceans) and of fish species of economic importance in aquaculture [16]. The isolation of this pathogen from diseased marine fish of new cultured species, suggested that Ph. damselae subsp. damselae can be considered as an emerging pathogen in marine aquaculture [17]. Most of the reported infections caused by Ph. damselae subsp. damselae in humans have their primary origin in wounds exposed to salt or brackish water, inflicted during fish and tools handling, that may evolve into necrotizing fasciitis with lethal effects [18 and references therein].

Bioactive compounds from marine algae with antimicrobial activity have been ascribed to a variety of metabolites, such as polysaccharides, polyunsaturated fatty acids, phlorotannins and other phenolic compounds, and carotenoids [1]. Marine algae contain large amounts of polysaccharides, notably cell-wall structural and storage polysaccharides, such as alginates, carrageenans, laminarans, fucoidans and ulvans, accounting from 4% to 76% of dry weight [19-21]. Polysaccharides of algal origin are polymers composed of various monosaccharides linked together by glycosidic bonds, and they have numerous commercial uses, such as stabilisers, thickeners, emulsifiers, food, feed, etc. [22].

The variability in the production of antimicrobial compounds by seaweeds, also within the same algal genus, may depend on different ecological factors, such as biogeographical distributions and seasonality, and physiological conditions [1, 4]. Since algal taxonomy is highly convoluted, molecular methods based on DNA barcoding sequencing represent the preferred tools to univocally identify algalspecies with promising applications [23]. Macroalge thrinving in transitional environments, such those of Venice and Cape Peloro coastal lagoons (Italy) produce large amount of biomass, which needs to be periodical removed and treated as a waste, stored in landfills, and finally incinerated.

In order to verify a possible exploitation of algal biomass as a source of antibacterial drugs, with the aim of transforming waste into a valuable resourcein the present study the in vitro antibacterial activity of algal extracts obtained from DNA barcoded marine macroalgae was evaluatedagainst bacterial pathogens concomitantly relevant for aquaculture and human health. In consideration of the relevance of the tested pathogens, the cytotoxic effects of extracts were investigated on isolated digestive gland cells of Mytilus galloprovincialis and on mammalian red blood cells.

Materials and Methods
Sample collection

Samples of Chlorophyta (green algae), Ochrophyta (brown algae) and Rhodophyta (red algae) were collected from different sites in two Italian transitional environments, namely Venice lagoon and lake Ganzirri in Cape Peloro lagoon (Table 1).

Fresh samples were washed with sterile seawater, manually cleaned of epiphytes. From each sample, a part was dried in silica gel and stored at -20 °C for molecular identification, while the rest was lyophilised for serial ethanol and polysaccharidic extractions.

 

Algal extracts

Collected samples of red, green and brown macroalgae were washed with clean water and lyophilised (FreeZone® 2.5 Liter Freeze Dry Systems 76705 S, Labconco, USA) and processed to obtain serial extracts of crude ethanol and polysaccharide fractions as detailed in Armeli Minicante et al. [3], with modifications. Each lyophilised sample was soaked in absolute ethanol (about 1:1 v:v) at room temperature for 48 h in a flask and then centrifuged at 4000 g to separate residual thalli. Supernatant was dried with a Rotavapor® at low temperature (35 °C) to preserve volatile compounds from evaporation (crude ethanol extracts).

Subsequently, residual thalli were soaked in distilled water (about 1:3 v:v) at 70 °C for 24 hours in order to extract the polysaccharide fraction. Polysaccharides were precipitated adding an equal volume of absolute ethanol to the mixture and dried at 40 °C overnight.

 

DNA barcoding

Identification of algal species was performed following standard procedures of DNA barcoding as reported in Saunders and McDevitt [23] and Leliaert et al. [24]. Sequences of the mitochondrial COI-5’ region were used as marker for red and brown algae, while sequences of the tufA gene were determined for the green alga Ulva, and the partial 28S ribosomal gene for the green alga Chaetomorpha.

Sequencing reactions were performed by an external company (Macrogen Europe, The Netherlands) or at the Muséum National d’Histoire Naturelle (Paris, France). Obtained DNA barcodes were contrasted with the Barcode of Life Data Systems (BOLD, http://www.boldsystems.org) and with GenBank through the BLAST platform (http://blast.ncbi.nlm.nih.gov/Blast.cgi) to define species attributions. Specimen data and sequences were deposited in BOLD and GenBank.

 

Antibacterial study

Bacterial strains

Both crude ethanol and polysaccharide extracts were tested against the following lab strains of fish and shellfish pathogenic bacteria Aeromonas hydrophila (AA5), Aeromonas salmonicida subsp. salmonicida (13M), Photobacterium damselae subsp. damselae (Pd), Pseudomonas aeruginosa (Pa), Salmonella sp. (2sp), Staphylococcus aureus (Sa), Vibrio anguillarum (Van), Vibrio cholerae Non-O1 (Vc), Vibrio harveyi (G5) and Vibrio parahaemolyticus (L12G). The strains were previously isolated from local marine and brackish environments and identified using standard biochemical and physiological characterization and phylogenetic analysis as reported in Gugliandolo et al. [25, 26]. Lab strains are maintained at -20 °C in Tryptone Soy Broth (TSB, Difco) supplemented with 1% (w/v) NaCl (TSB1) and 50% (v/v) glycerol. Clinical strains of Pseudomonas aeruginosa (Pa) and Staphylococcus aureus (Sa) were chosen on the basis of their strong antibiotic resistance [27].

 

Antibacterial tests

Antibacterial activity was evaluated by using the standard disk diffusion method (Kirby Bauer test), as accepted by the National Committee for Clinical Laboratory Standards (NCCLS 2000). Strains were overnight grown onto plates of Tryptone Soya Agar (TSA, Oxoid) amended with 1% (w/v) of NaCl (TSA1), for 24 h at 25 °C. Each strain was suspended in 3 ml of 0.9% NaCl solution with turbidity optically comparable to that of the 0.5 McFarland standard (1.5 × 108 bacteria ml-1) and aliquots of each suspension (100 µl) were inoculated onto triplicate plates of TSA1.

Each extract (100 mg, equivalent to 3 g of lyophilised algal sample) was dissolved in 1000 µl of absolute ethanol or sterile distilled water, and 20 µl were applied to sterile filter paper disks (6 mm in diameter, Oxoid). After solvent evaporation, the disks (containing each 2 mg of the extract) were placed onto the inoculated plates. Disks soaked with ethanol and submitted to evaporation were used as negative control, and disks containing chloramphenicol (30 µg) and tetracycline (30 µg) (Difco, Becton Dickinson and Company, USA) were used as positive control. Plates were incubated overnight at 25 °C. The diameter of complete inhibition zones was measured and means and standard deviations (n= 3) were calculated.

Minimum inhibitory concentration (MIC) values were determined for the most active extracts by using the serial dilution assay as accepted by the European Committee for Antimicrobial Susceptibility Testing (EUCAST) of the European Society of Clinical Microbiology and Infectious Diseases [28]. Serial dilutions of each extract (16, 8, 4, 2, 1, 0.5, and 0.25 mg ml-1) were prepared in tubes of TSB1 and then inoculated with suitable aliquots (10 ml) of an overnight culture (comparable to 0.5 McFarland standard)of each strain in TSB1. To confirm the inhibition activity of each extract, 100 mL from all tubes without visible growth were plated onto TSA1, and incubated overnight at 25 °C.

 

Cytotoxicity assays

Mytilus galloprovincialis specimens (7–8 cm shell length) were collected from the Faro Lake (Messina, Italy). Samples were transferred to laboratory in sterile bags and kept in tanks containing seawater (1100 mOsm/kg; pH= 8.0 ± 0.1; salinity ppm= 37 ± 1) at least for 7 days at 18 ± 1 °C until processing. The digestive gland cells of M. galloprovincialis were isolated according to Pagano et al. [29, 30], and suspended in saline solution (NaCl 550 mM; KCl 12.5 mM; MgSO4 8 mM; CaCl2 4 mM; glucose 10 mM, Hepes 20 mM) at a final concentration of 5 x 106 cells ml-1.

In order to define viability, cells were counted by using the Trypan blue exclusion method after 30, 60, 90 and 180 min of incubation, with each algal extract (2 mg ml-1) and in control condition (without algal extract).

The stability of lysosomal membrane was measured by neutral red retention assay (NR), after 30 and 60 min incubation, according to Matozzo et al. [31]. Digestive cells of M. galloprovincialis incubated in saline solution without algal extracts represented the negative control. All experiments were carried out in triplicate.

Cytotoxic effects were also investigated by incubating mammalian red blood cells for 180 min in physiological solution (0.9% NaCl) [32] containing algal extracts (final concentration of 2 mgml-1). A control test with mammalian red blood cells incubated in saline solution without algal extracts [33] was performed. Cell viability was determined by Trypan blue exclusion method and the percentage of unstained cells, considered as viable cells, was calculated. All experiments were performed in triplicate.

 

Determination of carbohydrates in algal extracts

Hydrolysis of polysaccharides was performed with 0.5 N trifluoroacetic acid at 120 °C for 2 h [34]. The standard stock solutions of carbohydrates were prepared by dissolving appropriate amount of their pure product in ultrapure water. NaOH solution used as eluent was prepared by diluting standard carbonate free concentrated solution. All the carbohydrates (minimum purity 98-99%) and reagents were Fluka or Aldrich products (Sigma-Aldrich Fine Chemicals, Missouri, USA). All the solutions were prepared using grade A glassware and ultrapure water (conductivity <0.1 µS), filtered on Millipore 0.45 µm (Pall Corporation Ann Arbor, Michigan, USA) and then ultrasonicated for 20 min. The chromatographic system was a DX500 ion chromatographic analyser (Dionex Sunnyvale, CA, USA) equipped with Dionex ED40 amperometric cell. Separations were carried out according to the Dionex technical note 21 [35] for the analysis of carbohydrates, that are electrocatalytically oxidized at the surface of the gold electrode by application of a positive potential.

The system was equipped with a pre-column (DionexcarboPac PA1, 4 ´ 50mm) and an analytical column (Dionexcarbopac PA1, 4 ´ 250 mm). The anion trap (ATC-1 Dionex) and amino trap (P/N 46122 Dionex) were used to remove the dissolved carbonate and the aminoacids.

The eluent was pumped in isocratic condition at 1.0 mL/min; the injection system was a 25 mL Loop. The system was controlled by DionexPeaknet 4.10 chromatographic software. The measurements were carried out in a temperature controlled room at 22 °C.

The carbohydrates taken into account were: D- (+)-cellobiose, D- (-)-fructose; D- (+)-galactose; D- (+)-glucose; D- (+)-maltose; D- (+)-mannitol; D- (+)-mannose; D- (+)-ribose; D- (+)-sucrose; D- (+)-trehalose dehydrate; D- (+)-xylose; L- (+)-fucose L- (+)-rhamnose.

The calibration plots (peak area vs carbohydrate concentration) were recovered for a wide concentration range between: 1 × 10-7 ≤ Cmol l-1r ≤ 1 × 10-4. The samples solution, obtained after hydrolysis of the polysaccharides extracted from algae, were previously diluted with ultrapure water in a ratio v/v of 1:10 and 1:150, and then injected.

 

Results
DNA barcoding

The DNA barcode regions were successfully sequenced for all studied specimens and specific attributions are reported in Table 1 together with accession numbers (BOLD).

 Antibacterial activity

Antibacterial activity ofboth crude ethanoland polysaccharideextracts is reported in Table 2. Algal extracts which did not show any activity against the tested pathogens were not included.

None of the crude ethanol extracts from Chlorophyta showed antibacterial effects against all the studied bacteria. Among the crude ethanol extracts, those obtained from Cystoseira barbata (Ochrophyta) against V. cholerae Non-O1 showed the highestactivity (inhibition zone of 10.0 mm in diameter), while those from Gracilaria gracilis showed only weak antibacterial activity (7.0 ± 0 mm) (Table 2A). Polysaccharides from Ulva fasciata (Chlorophyta) were active (10.0 ± 0 mm) against A. salmonicida subsp. salmonicida (13M), and they showed also weak inhibitory activity against A. hydrophila (AA5), Ph. damselae subsp. damselae (Pd), V. cholerae (Vc) and V. harveyi (G5) (Table 2B). Polysaccharides from Dictyopteris polypodioides (Ochrophyta) resulted active against V. anguillarum (Van), Salmonella sp. (2sp),and S. aureus (Sa). The polysaccharidic extracts from Fucus virsoides (Ochrophyta) were active against most of the tested pathogens, and exhibited the highest inhibition activity against Ph. damselae subsp. damselae (Pd) (inhibition zone of 13.0 ± 0 mm), followed by A. salmonicida subsp. salmonicida (13M) (11.0 ± 0 mm). Polysaccharides obtained from F. virsoides produced an inhibition zone against A. salmonicida (13M) equivalent to that of tetracycline (11.0 ± 0 mm) but lower than that of chloramphenicol (30.0 ± 0 mm), used as controls (Table 2B).

Polysaccharides from Undaria pinnatifida (Ochrophyta)showed the highest inhibition activity against V. cholerae (Vc) and V. harveyi (G5) (inhibition zone of 12.0 mm), and they were the only extracts activeagainst P. aeruginosa (Pa) (10.0 ± 0 mm).

Within Rhodophyta group, polysaccharides from Hypnea cornuta resulted weakly active against V. anguillarum (Van) (8.0 ± 0 mm) and those from G. gracilis exhibited weak antibacterial activity against V. harveyi (G5) (7.0 ± 0 mm).

The minimum inhibitory concentration was determined for polysaccharides obtained from F. virsoides and U. pinnatifida, as the most active extracts. The MIC values of F. virsoides extracts were 2 mg ml-1against A. salmonicida subsp. salmonicida (13M) and Ph. damselae subsp. damselae (Pd). Extracts from U. pinnatifida showed MIC values of 4 mg ml-1against P. aeruginosa (Pa), V. cholerae (Vc) and V. harveyi (G5).

Table 1 List of the algal samples used in this study

Phylum Voucher Species Collection date Collection site BOLD accession number
Chlorophyta PHL672 Chaetomorpha aerea March 2016 Lake Ganzirri (Messina, Italy) GRAPP001-17
SAM029 Ulva fasciata March 2010 Lake Ganzirri (Messina, Italy) ITGRE003-11
   
Ochrophyta SAM531 Cystoseira barbata May 2011 Certosa Island (Venice Lagoon, Italy) BRAPP004-17
SAM539 Sargassum muticum May 2011 Celestia (Venice Lagoon, Italy) BRAPP005-17
SAM099 Fucus virsoides March 2010 Ottagono S.P. Volta (Venice Lagoon,Italy) BRAPP002-17
SAM069 Undaria pinnatifida March 2010 Celestia (Venice Lagoon, Italy) BRAPP001-17
SAM303 Dictyopteris polypodioides June 2010 Certosa Island (Venice Lagoon, Italy) BRAPP003-17
   
Rhodophyta PHLCB358 Gracilaria gracilis January 2010 Lake Ganzirri (Messina, Italy) ITRED096-13
PHLCB221 Hypnea cornuta July 2009 Lake Ganzirri (Messina, Italy) ITRED087-13

 

 

 

Cytotoxicity assays

All algal extracts resulted not cytotoxic in the tested conditions. The viability of digestive gland cells of M. galloprovincialis and of mammalian red blood cells was on average 85% in all experiments. There were no statistical differences after exposition to different algal extracts (data not shown).

Table 2 Antibacterial activity of algal crude ethanol (A) and polysaccharides (B) extracts (2 mg/disc) in agar diffusion assay (inhibition zone is expressed in mm) against bacterial pathogens. Values are mean ± standard deviation of three replicates Ochrophyta

A) Crude ethanol extract Aeromonas hydrophila (AA5) Aeromonas salmonicida (13M) Photobacterium damselae (Pd) Pseudomonas aeruginosa (Pa) Salmonella sp.(2sp) Staphylococcus aureus(Sa) Vibrio anguillarum (Van) Vibrio cholerae Non-O1        (Vc) Vibrio harveyi (G5) Vibrio parahaemolyticus (L12G)
Ochrophyta Cystoseira barbata 7.0 ± 0.0 10.0 ± 0.0 7.0 ± 0.0
   
Rhodophyta Gracilaria gracilis 7.0 ± 0.0 7.0 ± 0.0 7.0 ± 0.0
   
B) Polysaccharidesextract                  
Chlorophyta Chaetomorpha aerea  7.0 ± 0.0
Ulvafasciata  8.0 ± 0.0 10.0 ± 0.0  8.0 ± 0.0  8.0 ± 0.0  8.0 ± 0.0
   
Ochrophyta Cystoseira barbata  –  8.0 ± 0.0  –  –  8.0 ± 0.0  –  –
Dictyopteris polypodioides 10.0 ± 0.0 10.0 ± 0.0 10.0 ± 0.0
Fucus virsoides  9.0 ± 0.0  11.0 ± 0.0 13.0 ± 0.0 10.0 ± 0.0  8.0 ± 0.0  9.0 ± 0.0
Sargassumuticum        8.0 ± 0.0
Undariapinnatifida 10.0 ± 0.0  12.0 ± 0.0  12.0 ± 0.0
   
Rhodophyta Gracilaria gracilis  7.0 ± 0.0  7.0 ± 0.0
Hypnea cornuta  8.0 ± 0.0
   
Chlorampheanicol(30µg) 13 ± 0.0 30 ± 0.0 30 ± 0.3 23 ± 0.0 20 ± 1.5 20 ± 0.0 28 ± 0.0 29 ± 0.0 27 ± 0.0
Tetracycline (30µg) 13 ± 0.0 11 ± 0.0 37 ± 2.8 33 ± 0.0 21 ± 1.4 27 ± 0.0 26 ± 0.0 29 ± 0.1 20 ± 0.0

 

 

 

Determination of carbohydrates in algal extracts

The determination of carbohydrates content was performed on the most active extracts obtained from F. virsoides and U. pinnatifida. After the chromatographic separation, carried out at least in duplicate and taking into account the retention time of the analytes and the dilution of the samples, the qualitative and quantitative results were obtained as reported in Table 3.

Table 3 Carbohydrates composition of polysaccharide extracts from Fucus virsoides and Undaria pinnatifida

Carbohydrate Fucus virsoides (ppm)a Undaria pinnatifida (ppm)a
D-(+)-cellobiose
D-(-)-fructose 295.3
D-(+)-galactose 17.4 57.9
D-(+)-glucose 4.0
D-(+)-maltose
D-mannitol 3.7 51.9
D-(+)-mannose
D-ribose
D-(+)-sucrose
D-(+)-trehalose dihydrate 54.4 269.0
D-(+)-xylose 34.1
L-(-)-fucose 512.4 48.5
L-(+)-rhamnose monohydrate 344.5
a ppm= mg/L (mg of solute/liter of solution)

 

In order to verify the correctness of the attribution of the peaks to the carbohydrates investigated, the samples were also spiked with known amounts of carbohydrates and once again analysed; we observed an increase of the peak area proportional to carbohydrate added to sample. This is a clear indication of the correct attribution of the retention time to each carbohydrate, even if the retention time of each analyte was previously determined by injection in the chromatographic system of the pure chemicals (Sigma-Aldrich Fine Chemicals, Missouri, USA) dissolved in ultrapure water.

The preliminary chemical characterization showed that, other than fucose, the most abundant sugars were trehalose and galactose in the polysaccharidic extract from F. virsoides, and rhamnose, fructose and trehalose in that from U. pinnatifida.

Analysis of the chromatograms highlights the presence in the samples of other components, namely carbohydrates and/or amino sugars, but the unavailability of standards did not allow to perform further qualitative and quantitative determination.

 

Discussion

Marine algal compounds able to inhibit the growth of bacterial pathogens may represent future alternatives to common antibiotics. The increasing resistance of pathogens to antibiotics represents a priority for exploring and developing effective natural antimicrobial agents with better potential, good bioavailability, minimal toxicity and less-side effects than antibiotics on humans, farmed organisms and environments.

In this study, both crude ethanol and polysaccharide extracts from nine marine algae (2 Chlorophyta, 5 Ochrophyta and 2 Rhodophyta), collected from different sites in two Italian transitional environments, have been evaluated for their antibacterial effects against pathogens of fish, shellfish and humans. Polysaccharide extracts showed a broader inhibitory activity against the tested pathogens than their ethanol counterparts. Our data revealed that all polysaccharides were active against one or more pathogens, and 67% were active against two or more targeted microorganisms. In contrast, only 22% of crude ethanol extracts from the studied macroalgae were active against one or more pathogens. Extraction protocols,used to test the biological activity of seaweeds, mainly involve different solvents which, depending on their polarity, provide a different efficiency in extracting the active compounds responsible for antimicrobial effects [1]. Moreover, the synthesis of antimicrobial compounds by seaweeds may depend on several factors, including geographical location, environmental factors and algal physiological conditions (active growth or sexual maturity). As reported in our previous study, crude ethanol extracts of Asparagopsis taxiformis, collected from the Straits of Messina (Italy) in different sampling periods, exhibited significantly different antimicrobial activity against fish pathogenic bacteria, probably due to a different content of active biomolecules [4]. Indeed, the crude ethanol extracts obtained in late spring showed the broadest activity against the whole panel of studied bacteria, especially against V. alginolyticus and V. vulnificus, followed by A. salmonicida subsp. salmonicida.

Seaweed polysaccharide constituents (including alginic acid and alginates, carrageenans and agar, laminarans, fucoidans, ulvans, and derivatives) usually represent the main components of algal cell walls and have important structural functions.

In this work, polysaccharides obtained from the green alga Ulva fasciata, and the brown algae Dictyopteris polypodioides, Fucus virsoides and Undaria pinnatifida, were the most active against the studied bacterial pathogens. Extracts from U. fasciata showed antibacterial activity against A. salmonicida subsp. salmonicida (13M), a well-known pathogen able to severely impact salmonid ichthyic stocks [12]. The antimicrobial activity of polysaccharides from U. fasciata has not been extensively investigated until now, whereas solvent extracts has been reported active against several Gram-positive and Gram-negative bacteria [36], including V. parahaemolyticus and V. alginolyticus [37], and have been demonstrated as non-specific defence factors against pathogens of shrimps [38].

Polysaccharidesfrom Dictyopteris polypodioides were the most active against V. anguillarum (Van), Salmonella sp. (2sp) and the multiresistant strain of S. aureus (Sa),that is a well-known human pathogen and also an occasionally fish pathogen [39]. Despite its worldwide distribution, very few data are available on the bioactive properties of compounds from D. polypodioides and their potential use.

Polysaccharides from Fucus virsoides showed inhibitory activity against most of the tested bacteria (6/10), including fish and human pathogens. Interestingly, these extracts were the most active against A. salmonicida subsp. salmonicida, exhibiting an inhibition zone equivalent to tetracycline used as control, andalso against Ph. damselae subsp. damselae (Pd), a member of Vibrionaceae family widely distributed in aquatic environments, and recognized as pathogen of a variety of sea animals. Similarly to its closest related strain Ph. damselae subsp. piscicida, Ph. damselae subsp. damselae is also considered resistant to most of the antibiotics used in the treatment of fish pseudotuberculosis [40-42]. Ph. damselae subsp. damselae was recently reported as an emergent pathogen for humans, causing infections in wounds exposed to marine or brackish waters and typically associated with fish handling [18 and references therein listed]. Necrotizing fasciitis due to Ph. damselae subsp. damselae have demonstrated to have more serious complications and higher mortality rate in humans than those caused by V. vulnificus [43, 44]. More recently, cases of severe wound infection in humans exposed to coastal waters have been referred to both Ph. damselae subsp. damselae and V. harveyi [45, 46]. A preliminary chemical characterization of polysaccharides extracts from F. virsoides showed that the most abundant carbohydrate was fucose, followed by trehalose and galactose, with a global composition close to the commercial fucoidan, a complex sulfated polysaccharide derived from F. vesiculosus. Sulfated polysaccharides extracted from different brown algae have been previously evaluated for their activity against both Gram-negative and Gram-positive bacteria, and differences in antimicrobial activities have been mainly related to the sulfate content [47, 48]. The commercially available fucoidan from F. vesiculosus has been reported active also against V. alginolyticus, however its antibacterial activity was mainly referred to the methanol extracted fraction, rather than to the entire fucoidan content [49].

Polysaccharides from U. pinnatifida resulted the most active against V. cholerae Non-O1 (Vc) and V. harveyi (G5),and were the only extracts active against P. aeruginosa (Pa),a multi-resistant strain susceptible only to fosfomycin [27]. Other than fucose, the main components of polysaccharides obtained from U. pinnatifidawere rhamnose, fructose and trehalose. Despite fucoxanthins, fucoidans and laminarans have been previously reported as active compounds from U. pinnatifida against pathogenic bacteria for humans [50-53], no results are actually available against fish pathogens or their potential applications in aquaculture.

The antibacterial activity (evaluated as inhibition zones and minimum inhibitory concentration values) of extracts here reported was overall lower than that of antibiotics used as control, with the only exception of polysaccharides of F.virsoidesagainst A. salmonicida. Although the exact mode of antimicrobial action of polysaccharides is still not clear, it was proposed that polysaccharides disrupt the bacterial cell wall and cytoplasmic membrane, leading to the dissolution of the protein and the leakage of essential molecules, resulting in cell death [54]. However, further investigations should attempt to purify active compounds from crude extracts and to elucidate their antimicrobial mechanisms.

All the studied polysaccharides have not cytotoxic effects on both molluscan digestive gland cells and mammals red blood cells, indicating a potential use for both aquaculture and human health.

 Conclusions

Our results extend previous observations on the antibacterial activity of macroalgae against pathogens of fish, shellfish and humans. Polysaccharides from nine barcoded macroalgae (2 Chlorophyta, 5 Ochrophyta and 2 Rhodophyta) showed broader and higher inhibitory activity than ethanol extracts against the tested pathogens. Indeed, the ethanol extracts showed a weak inhibitory activity against three of the pathogens (V. cholerae, V. harveyi,A. hydrophila). Our findings suggest that polysaccharides from the barcoded brown algae F. virsoides and U. pinnatifida could represent a novel source of antimicrobial compounds against Ph. damselae subsp. damselae and V. harveyi, recently recognized as bacterial pathogens concomitantly relevant for aquaculture and human health. As alternative compounds to common antibiotics for the control of fish infection they could be further investigated also as dietary supplements of farmed fish, in a modern and eco-sustainable aquaculture.The exploitation of algal biomass, as a source of antibacterial drugs, would result into the valuable transformation of waste into an economic resource.

 

Acknowledgements

The research has been carried out under the financial support obtained from the project PON INNOVAQUA (PON02_00451_3362185) from Italian Ministry of University and Research (MIUR). This work was supported by grant from the project FORINNOVAQUA (PON02_00451_3362185/F1) to Dr Carmen Rizzo. Acquisition of molecular data of samples from Venice was carried out at the Service de Systématique Moléculaire (CNRS-UMS 2700), Muséum National d’Histoire Naturelle, Paris, France, courtesy of dr. Line Le Gall.

 

References

[1] Pérez, M.J., Falqué, E., Domínguez, H. Antimicrobial action of compounds from marine seaweed. Mar. Drugs, 2016; 14:52. doi:10.3390/md14030052.

[2] Marino, F., Di Caro, G., Gugliandolo, C., Spanò, A., Faggio, C., Genovese, G., Santulli, A. Preliminary study on the in vitro and in vivo effects of Asparagopsis taxiformis bioactive phycoderivates on teleosts. Front. physiol., 2016; 7.

[3] Armeli Minicante, S., Michelet, S., Bruno, F., Castelli, G., Vitale, F., Sfriso, A., Morabito, M., Genovese, G. Bioactivity of phycocolloids against the Mediterranean protozoan Leishmania infantum: an incentive study. Sustainability, 2016; doi:10.3390/su8111131.

[4] Genovese, G., Faggio, C., Gugliandolo, C., Torre, A., Spanò, A., Morabito, M., Maugeri, T.L. In vitro evaluation of antibacterial activity of Asparagopsis taxiformis from the Straits of Messina against pathogens relevant in aquaculture. Mar. Environ. Res., 2012; 73:16.

[5] Abu-Ghannam, N., Rajauria, G. Antimicrobial activity of compounds isolated from algae. In Domínguez, H. (ed), Functional ingredients from algae for foods and nutraceuticals, Woodhead Publishing, Cambridge UK; 2013. pp 287–306.

[6] Eom, S.H., Kim, Y.M., Kim, S.K. Antimicrobial effect of phlorotannins from marine brown algae. Food Chem. Toxicol., 2012; 50:3251–3255.

[7] Bansemir, A., Blume, M., Schröder, S., Lindequist, U. Screening of cultivated seaweeds for antibacterial activity against fish pathogenic bacteria. Aquaculture, 2006; 252:7984.

[8] Vatsos, I.N., Rebours, C. Seaweed extracts as antimicrobial agents in aquaculture. J. Appl. Phycol., 2015; 27:2017–2035.

[9] Thompson, J.R., Marcelino, L.A., Polz, M.F. Diversity sources and detection of human bacterial pathogens in the marine environment, in Belkin S. & R.R. Colwell (eds), Oceans and Health: Pathogens in the Marine Environment, Springer, New York; 2005. pp 29–68.

[10] Toranzo, A.E., Magarinos, B., Romalde, J.L. A review of the main bacterial fish diseases in mariculture systems. Aquaculture, 2005; 246:37–61.

Janda, J.M., Abbott, S.L. The Genus Aeromonas: taxonomy, pathogenicity, and infection. Clin. Microbiol. Rev., 2010; 23:35–73.

[12] Daly, J.G., Kew, A.K., Moore, A.R., Olivier, G. The cell surface of Aeromonas salmonicida determines in vitro survival in cultured brook trout (Salvelinus fontinalis) peritoneal macrophages. Microb. Pathog., 1996; 21:447461.

[13] Austin, B., Austin, D.A. Bacterial fish pathogens: disease of farmed and wild fish, fourth ed., Springer-Praxis, Godalming England; 2007.

[14] Nishibuchi, M., De Paola, A. Vibrio species, in Fratamico PM, Bhunia AK, Smith JL (Eds), Foodborne Pathogens: Microbiology and Molecular Biology, Caister Academic Press, Norfolk UK; 2012. pp 251–271.

[15] Austin, B., Zhang, X.H. Vibrio harveyi: a significant pathogen of marine vertebrates and invertebrates. Lett. Appl. Microbiol., 2006; 43:119124.

[16] Romalde, J.L. Photobacterium damselae subsp. piscicida: an integrated view of a bacterial fish pathogen. Int. Microbiol., 2002; 5:39.

[17] Labella, A., Berbel, C., Manchado, M., Castro, D., Borrego, J.J. Photobacterium damselae subsp. damselae, an emerging pathogen affecting new cultured marine fish species in Southern Spain, in Aral F and Doğu Z (Eds), Recent Advances in Fish Farms, InTech, New York; 2011. pp 135–152.

[18] Rivas, A.J., Lemos, M.L., Osorio, C.R. Photobacterium damselae subsp. damselae a bacterium pathogenic for marine animals and humans. Front. Microbiol., 2013; 4:283.

[19] Murata, M., Nakazoe, J. Production and use of marine algae in Japan. Jpn. Agr. Res. Q, 2001; 35:281–290.

[20] Kumar, C.S., Ganesan, P., Suresh, P.V., Bhaskar, N. Seaweeds as a source of nutritionally beneficial compounds a review. J. Food Sci. Technol., 2008; 45:1–13.

[21] Holdt, S.L., Kraan, S. Bioactive compounds in seaweed: functional food applications and legislation. J. Appl. Phycol. 2011; 23:543–97.

[22] Tseng, C.K. Algal biotechnology industries and research activities in China. J. Appl. Phycol. 2001; 13:375–380.

[23] Saunders, G.W., McDevit, D.C. Methods for DNA barcoding photosynthetic protists emphasizing themacroalgae and diatoms, in Kress, W.J.,& D.L. Erickson (eds), DNA Barcodes: Methods and Protocols, Springer Science, New York; 2012. pp 207222.

[24] Leliaert, F., De Clerck, O., Verbruggen, H., Boedeker, C., Coppejans, E. Molecular phylogeny of the Siphonocladales (Clorophyta: Cladophorophyceae). Mol. Phylogenet. Evol. 2007; 44:1237–1256.

[25] Gugliandolo, C., Irrera, G.P., Lentini, V., Maugeri, T.L. Pathogenic Vibrio,Aeromonas and Arcobacter spp associated with copepods in the Straits of Messina (Italy). Mar. Poll. Bull., 2008; 56:580606.

[26] Gugliandolo, C., Lentini, V., Spanò, A., Maugeri, T.L. Conventional and molecular methods to detect bacterial pathogens in mussels. Lett. Appl. Microbiol., 2011; 52:1521.

[27] Spanò, A., Laganà, P., Visalli, G., Maugeri, T.L., et al. In vitro antibiofilm activity of an exopolysaccharide from the marine thermophilic Bacillus licheniformis T14. Curr. Microbiol., 2016; 72:518–528.

[28] European Committee for Antimicrobial Susceptibility Testing (EUCAST) of the European Society of Clinical Microbiology and Infectious Diseases (ESCMID), 2003. Determination of minimum inhibitory concentrations (MICs) of antibacterial agents by broth dilution. Clin Microbiol Infect doi: 10.1046/j.1469-0691.2003.00790.x.

[29] Pagano, M., Capillo, G., Sanfilippo, M., Palato, S., Trischitta, F., Manganaro, A., Faggio, C. Evaluation of functionality and biological responses of Mytilus galloprovincialis after exposure to quaternium-15 (Methenamine 3-Chloroallylochloride). Molecules 2016; 21:144. doi: 10.3390/molecules21020144.

[30] Pagano, M., Porcino, C., Briglia, M., Fiorino, E., Vazzana, M., Silvestro, S., Faggio, C. The influence of exposure of cadmium chloride and zinc chloride on haemolymph and digestive gland cells from Mytilus galloprovincialis. Int. J. Environ. Research, 2017; 11(2): 207-216.

[31] Matozzo, V., Pagano, M., Spinelli, A., Caicci, F., Faggio, C. Pinna nobilis: a big bivalve with big haemocytes? Fish Shellfish Immunol., 2016; 55:529–534.

[32] Faggio, C., Morabito, M., Armeli Minicante, S., Lo Piano, G., Pagano, M., Genovese, G. Potential use of polysaccharides from the brown alga Undaria pinnatifida as anticoagulants. Braz. Arch. Biol. Techn., 2015; 58:798–804.

[33] Pagano, M., Faggio, C. The use of erythrocyte fragility to assess xenobiotic cytotoxicity. Cell Biochem. Funct., 2015; 33:351–355.

[34] Boual, Z., Kemassi, A., Khelil, A.O.E.H., Michaud, P., Hadj, M.D.O.E. Partial characterization and hydrolysis procedure of water soluble polysaccharides extracted from one Saharian medicinal plant: Malva aegyptiaca. L Int. J. Biosci. Biochem. Bioinforma., 2012; 2:100–103.

[35] Roher, J. Optimal settings for pulsed amperometric detection of carbohydrates using the Dionex ED40 electrochemical detector. Thermo Fisher Scientific, Sunnyvale; 2013. CA USA.

[36] Osman, M.E.H., Abushady, A.M., Elshobary, M.E. In vitro screening of antimicrobial activity of extracts of some macroalgae collected from Abu-Qir bay Alexandria Egypt. Afr. J. Biotechnol., 2010; 9:7203–7208.

[37] Chakraborty, K., Lipton, A.P., Raj, R.P., Vijayan, K.K. Antibacterial labdane diterpenoids of Ulva fasciata Delile from Southwestern coast of the Indian Peninsula. Food Chem., 2010; 19:1399–1408.

[38] Selvin, J., Manilal, A., Sujith, S., Kiran, G.S., Lipton A.P. Efficacy of marine green alga Ulva fasciata extract on the management of shrimp bacterial diseases. Lat. Am. J. Aquat. Res., 2011; 39:197204.

[39] Lin, B., Chen, S., Cao, Z., Lin, Y., Mo, D., Zhang, H., Xu, A. Acute phase response in zebrafish upon Aeromonas salmonicida and Staphylococcus aureus infection: striking similarities and obvious differences with mammals. Mol. Immunol., 2007; 44:295–301.

[40] Chiu, T.H., Kao, L.Y., Chen, M.L. Antibiotic resistance and molecular typing of Photobacterium damselae subsp. damselae isolated from sea food. J. Appl. Microbiol., 2013; 114:1184–1192.

[41] Jun, J.W., Kim, J.H., Han, J.E., Shin, S.P., Gomez, D.K. Jr, Oh, C.C., Oh, K.S., Park, S.C. Isolation of Photobacterium damselae subsp damselae from the giant grouper Epinephelus lanceolatus. J. Vet. Clin., 2010; 27:618–621.

[42] Stephens, F.J., Raidal, S.R., Buller, N., Jones, B. Infection with Photobacterium damselae subspecies damselae and Vibrio harveyi in snapper Pagrus auratus with bloat. Austr. Vet. J., 2010; 84:173–177.

[43] Perez-Tirse, J., Levine, J.F., Mecca, M. Vibrio damselae a cause of fulminant septicemia. Arch. Intern. Med., 1993; 153:1838–1840.

[44] Yuen, K.Y., Ma, L., Wong, S.S.Y., Ng, W.F. Fatal necrotizing fasciitis due to Vibrio damselae. Scand. J. Infect. Dis., 1993; 25:659–661.

[45] Akram, A., Stevens, R.P., Konecny, P. Photobacterium damselae and Vibrio harveyi hand infection from marine exposure. Med. J. Aust., 2015; 203:224–225.

[46] Hundenborn, J., Thurig, S., Kommerell, M., Haag, H., Nolte, O. Severe wound infection with Photobacterium damselae ssp damselae and Vibrio harveyi following a laceration injury in marine environment: A case report and review of the literature. Case Rep. Med., 2013; doi:10.1155/2013/610632.

[47] Asker, M.M.S., Mohamed, S.F., Ali, F.M., El-Sayed, O.H.E. Chemical structure and antiviral activity of water-soluble sulfated polysaccharides from Sargassum latifolium. J. Appl. Sci. Res., 2007; 3:1178-1185.

[48] Li, L.Y., Li, L.Q., Guo, C.H. Evaluation of in vitro antioxidant and antibacterial activities of Laminaria japonica polysaccharides. J. Med. Plants Res., 2010; 4:2194–2198.

[49] Nishiguchi, T., Jiang, Z., Ueno, M., Takeshita, S., Cho, K., Roh, S.W., Kang, K.H., Yamaguchi, K., Kim, D., Oda, T. Reevaluation of bactericidal, cytotoxic, and macrophage-stimulating activities of commercially available Fucus vesiculosus fucoidan. Algae, 2014; 29:237–247.

[50] Al Hazzani, A.A., Shehata, A.I., Moubayed, N.M.S., Al Houri, H.J. Antimicrobial and biochemical properties of selected edible brown and red marine macroalgae. J. Pure Appl. Microbiol., 2014; 8:1275–1282.

[51] Hoffman, R., Paper, D.H., Donaldson, J., Alban, S., Franz, G. Characterisation of a laminarin sulphate which inhibits basic fibroblast growth factor binding and endothelial cell proliferation. J. Cell Sci., 1995; 108:3591–3598.

[52] Plaza, M., Cifuentes, A., Ibáñez, E. In the search of new functional food ingredients from algae. Trends Food Sci. Tech., 2008; 19:31–39.

[53] Wang, S.K., Li, Y., White, W.L., Lu, J. Extracts from New Zealand Undaria pinnatifida containing fucoxanthin as potential functional biomaterials against cancer in vitro. J. Funct. Biomat., 2014; 5:2942.

[54] He, F., Yang, Y., Yang, G., Yu, L. Studies on antibacterial activity and antibacterial mechanism of a novel polysaccharide from Streptomyces virginia H03. Food Control, 2010; 21:1257–1262.