Ulososides and urabosides--triterpenoid saponins from the Caribbean marine sponge Ectyoplasia ferox.

Three new triterpene glycosides, named ulososide F (1), urabosides A (2) and B (3), together with the previously reported ulososide A (4), were isolated from the Caribbean marine sponge Ectyoplasia ferox. Their structures were elucidated using extensive interpretation of 1D and 2D-NMR data, as well as HRESIMS. The aglycon of all compounds is a rare 30-norlonastane and the sugar residues were identified after acid hydrolysis and GC analyses. Cytotoxicities of the isolated compounds were evaluated against Jurkat and CHO cell lines by a MTT in vitro assay as well as a hemolysis assay. Unexpectedly, all these saponin derivatives showed very low activity in our bioassays.

1. Introduction

Secondary metabolites play critical roles in the chemical defense systems of many marine organisms and they are frequently involved in the organization of benthic communities. Marine sponges are already well known as producers of such secondary metabolites with ecological roles, especially in the Caribbean region, where they can dominate some ecosystems [1]. The high structural diversity of these secondary metabolites has been associated to the lack of physical defenses forcing them to develop chemical defenses to be used, for example, to deter predation [2]. The original chemical diversity of these metabolites have also found applications in the therapeutic field and this research is still in its infancy with the first marketing of the sponge-inspired eribulin mesylate as an anticancer agent by the Eisai company in 2011 [3].

We decided to embark on a program aiming at describing the pharmaceutical potential of secondary metabolites produced by dominant sponges of the South-Eastern Caribbean Sea, a region with a difficult access and thus rarely studied in this context. Ectyoplasia ferox (Duchassaing & Michelotti, 1864) (Poecilosclerida, Raspailiidae) was selected for a full chemical study due to its high abundance in the Urabá Gulf, our region of interest. This species has also been described at sites in the Northern part of the Caribbean, like Florida or even the Bahamas, and our chemical study will therefore also shed light on some possible differences in the secondary metabolome induced by geographical and/or environmental factors. The place of E. ferox in the order Poecilosclerida has been demonstrated, but the absence of guanidinic alkaloids was intriguing, as they are usually recognized as chemotaxonomic markers of this group [4,5,6]. This common sponge has also been proven as a good model for studies concerning the transfer of the microbial communities during the reproduction [7,8]. From the four species described so far within this genus, chemical studies have only been undertaken on E. ferox and this point also raised our interest. Triterpenoid saponins, named ectyoplasides and feroxosides, were identified as major chemical components of this species [9,10], but polar lipids were also reported [11,12,13]. These compounds were suggested to possess ecological roles, but also to have pharmaceutical potential.

Triterpenoid and steroidal glycosides are mainly found in the marine environment in echinoderms where they can act as chemical defense. However, few chemical studies have also underlined their presence in marine sponges, mostly from the genera Erylus, Mycale, Melophlus [14,15] and more recently from a Pandaros species (Poecililosclerida, Microcionidae) [16,17,18]. We report herein the results of our chemical study on a specimen of Ectyoplasia ferox collected in the Urabá Gulf (Colombia) and the isolation and structure elucidation of four triterpenoid saponins 1–4 which clearly differ from the previously isolated ectyoplasides and feroxosides (Figure 1).

Figure 1

Structures of saponins 1–4 from E. ferox.

2. Results and Discussion

2.1. Isolation and Structure Elucidation

The sponge specimen was lyophilized, ground, and repeatedly extracted with a 1:1 CH2Cl2/MeOH mixture. The combined extracts were filtered, concentrated under vacuum and fractionated by reversed phase column liquid chromatography with solvents of decreasing polarities (H2O, MeOH and CH2Cl2). The methanol fraction was further subjected to repeated HPLC purifications yielding the new ulososide F (1) and urabosides A (2) and B (3), together with the known compound uloloside A (4) (Figure 1). These compounds were identified by combined spectroscopic methods and comparisons of NMR data with literature [10,19,20,21].

Compound 1 was isolated as a white amorphous solid, with a molecular formula assigned as C44H71NO16 on the basis of combined HRESIMS (m/z 892.46222 [M+Na]+) and 13C-NMR data. The saponin nature of this compound was evidenced in the 1H-NMR spectrum of 1 by the presence of characteristic terpenoid methyl singlets (δH between 0.6 and 1.5) together with sugar residues (δH between 3.1 and 5.0). The portion of the 1H-NMR spectrum corresponding to the aglycon evidenced seven methyl signals that were reminiscent of a 29-functionalized 24-methyl-30-norlanostane at δH 0.67 (s, H3-18), 0.85 (d, H3-241), 0.93 (d, H3-21), 0.95 (d, H3-26), 0.96 (d, H3-27), 1.01 (s, H3-19), 1.34 (s, H3-28) (Table 1) [22]. The presence of a fused double bond at C-8/C-9 was mainly inferred from the key H3-19/C-9 HMBC correlation. Two alcohols and a methyl were placed at C-22, C-23 and C-24 of the side-chain respectively after inspection of the COSY spectrum and characteristic signals at δH 3.51 (m, H-22), 3.68 (dd, H-23), 1.56 (m, H-24) and δC 73.4 (CH, C-22), 72.2 (CH, C-23), 41.0 (CH, C-24). The structure was then very similar to the previously isolated ulososides isolated from an Ulosa sp. sponge collected in Madagascar [19,20,21]. In fact, 1 shares exactly the same aglycon as ulososides A, C, D and E due to very close chemical shifts, even if all NMR spectra were reported in C5D5N in the literature. We just changed the numbering replacing the C-28 methyl described in the literature by a C-241 methyl at C-24, thus respecting the IUPAC recommendations for this family of triterpenoids. The relative configuration of the tetracycle was confirmed by NOESY correlations and 3J scalar coupling interpretation [23]. We decided to assess the relative configuration of the asymmetric centers at C-22, C-23 and C-24 of the side-chain using a close inspection of the NMR data reported for the closely related and well known brassinosteroids [23,24,25].

Table 1

1H (500 MHz) and 13C-NMR (125 MHz) data for the aglycon of 1, 2, and 3 (in CD3OD).

Position	1		2		3
	δH, mult. (J in Hz)	δC, mult.	δH, mult. (J in Hz)	δC, mult.	δH, mult. (J in Hz)	δC, mult.
1a	1.86, m	37.4, CH2	1.83, m	38.2, CH2	1.87	37.8, CH2
1b	1.32, m		1.27, m		1.35
2a	2.38, qd (13.5, 2.5)	28.2, CH2	2.57, m	28.1, CH2	2.23, d (12.0)	28.0, CH2
2b	2.05, m		2.01, m		2.06, m
3	3.28 ª	89.8, CH	3.80, m	81.3, CH	4.00, dd (12.0, 4.0)	87.5, CH
4		50.5, C		55.9, C		63.8, C
5	1.33, m	53.2, CH	1.78, m	44.6, CH	1.98, m	50.6, CH
6a	1.94, m	21.2, CH2	1.92, m	20.8, CH2	2.13, m	23.8, CH2
6b	1.66, m		1.54, m		1.54, m
7a	2.07, m	29.8, CH2	2.08, m	28.8, CH2	2.01, m	29.8, CH2
7b	1.93, m		2.01, m		1.92, m
8		129.1, C		128.9, C		129.8, C
9		137.3, C		137.5, C		136.3, C
10		38.5, C		38.7, C		37.7, C
11a	2.17, m	23.3, CH2	2.15, m	23.2, CH2	2.14, m	23.1, CH2
11b	2.08, m		2.08, m		2.10, m
12a	2.00, m	38.4, CH2	1.98, m	38.4, CH2	1.98, m	38.3, CH2
12b	1.43, m		1.43, m		1.43, m
13		43.4, C		43.4, C		43.5, C
14	2.11, m	53.3, CH	2.09, m	53.2, CH	2.10, m	53.2, CH
15a	1.63, m	24.8, CH2	1.63, m	24.7, CH2	1.63, m	24.8, CH2
15b	1.37, m		1.34, m		1.34, m
16a	1.92, m	29.1, CH2	1.91, m	29.1, CH2	1.90, m	29.1, CH2
16b	1.36, m		1.36, m		1.33, m
17	1.57, m	52.5, CH	1.22, m	56.1, CH	1.22, m	56.1, CH
18	0.67, s	11.8, CH3	0.67, s	11.7, CH3	0.68, s	11.8, CH3
19	1.01, s	18.9, CH3	1.02, s	18.9, CH3	0.98, s	18.9, CH3
20	1.89, m	37.9, CH	1.99, m	34.2, CH	1.99, m	34.2, CH
21	0.93, d (6.8)	12.4, CH3	0.93, d (6.8)	20.3, CH3	0.93, d (6.8)	20.3, CH3
22a	3.51, br d (9.5)	73.4, CH	2.49, dd (16.0, 3.5)	51.0, CH2	2.49, dd (16.0, 3.5)	51.0, CH2
22b			2.17, m		2.17, m
23	3.68, dd (9.5, 1.5)	72.2, CH		213.8, C		213.8, C
24	1.56, m	41.0, CH	2.30, d (6.8)	53.6, CH2	2.30, d (6.8)	53.6, CH2
241	0.85, d (6.9)	10.0, CH3
25	1.62, m	32.2, CH	2.08, m	25.8, CH	2.08, m	25.8, CH
26	0.95, d (6.6)	21.6, CH3	0.90, d (6.6)	22.8, CH3	0.90, d (6.6)	22.8, CH3
27	0.96, d (6.6)	21.2, CH3	0.92, d (6.6)	22.8, CH3	0.92, d (6.6)	22.8, CH3
28a	1.35, s	24.8, CH3	3.96, d (11.0)	60.7, CH2		b
28b			3.89, d (11.0)
29		177.8, C		176.9, C		175.2, C

a Overlapped with the CD3OD residual peak; b Not seen.

It appears that 1H and 13C-NMR data are fully consistent with a 22R, 23S and 24R configurations assuming a usual absolute configuration at C-20 (Figure 2). Additionally, we then propose to change the configurations for ulososides A, C, D and E that were tentatively assigned as 22S, 23R and 24S.

Figure 2

Comparison of NMR data of the aglycon side-chain.

NMR spectra indicated the disaccharide nature of compound 1. For the glycosidic part of the molecule, two sugar residues were evidenced by the signals corresponding to two anomeric carbons at δ 104.8 (CH, C-1′), and 105.1 (CH, C-1′′) and protons at δH 4.56 (d, J = 8.1 Hz, H-1′) and 4.49 (d, J = 7.8 Hz, H-1′′), with coupling constants at J = 8.1 and 7.8 Hz suggesting a β anomeric configuration (Table 2). The first sugar residue was identified as a N-acetylglucosamine on the basis of the 13C chemical shifts and coupling constant values, as well as a comparison with ulososide D-NMR data [19]. A H-1′/C-3 HMBC correlation placed this sugar at C-3. Compared to ulososide D an additional glucuronic acid was branched at C-6′ on the basis of a H-1′′/C-6′ HMBC correlation. The glucuronic acid was ascertained by interpretation of coupling constant values and the presence of a H-5′′/C-6′′ HMBC correlation. The D absolute configurations of both sugar residues were determined by GC after derivatization and comparison with standard sugars [26].

Table 2

1H (500 MHz) and 13C-NMR (125 MHz) data for the sugars of 1, 2, and 3 (in CD3OD).

Position	1		2		3
	δH, mult. (J in Hz)	δC, mult.	δH, mult. (J in Hz)	δC, mult.	δH, mult. (J in Hz)	δC, mult.
1′	4.56, d (8.1)	104.8, CH	4.56, d (7.9)	105.3, CH	4.51, d (7.6)	104.6, CH
2′	3.61, dd (8.1, 9.5)	58.0, CH	3.90, m	74.3, CH	3.70, t (7.8)	79.8, CH
3′	3.53, t (9.5)	75.5, CH	3.79, m	86.7, CH	3.55, m	77.5, CH
4′	3.28 ª	72.1, CH	4.15, br d (3.0)	70.3, CH	3.56, m	73.0, CH
5′	3.49, ddd (9.4, 6.3, 1.6)	77.0, CH	3.53, m	76.1, CH	3.80, d	76.6, CH
6′a	4.11, dd (11.8, 1.8)	70.2, CH2	3.73, m	62.6, CH2		172.2, C
6′b	3.79, dd (11.8, 6.4)
-CO-CH3	1.93, s	23.0, CH3
-CO-CH3		173.5, C
1′′	4.49, d (7.8)	105.1, CH	5.59, d (3.2)	100.2, CH	4.57, d (8.1)	104.6, CH
2′′	3.26, dd (9.3, 7.8)	74.8, CH	3.78, m	70.4, CH	3.60, dd (9.3, 8.1)	73.7, CH
3′′	3.40, t (9.3)	77.5, CH	3.82, m	70.8, CH	3.44, dd (9.3, 3.0)	75.1, CH
4′′	3.53, m	73.2, CH	3.76, m	70.3, CH	3.76, d (3.0)	71.2, CH
5′′a	3.78, d (9.6)	76.6, CH	4.07, d (12.8)	64.9, CH2	3.53, m	76.9, CH
5′′b			3.42 (m)
6′′a		172.5, C			3.88, dd, (11.7, 7.6)	63.0, CH2
6′′b					3.65, dd, (11.7, 3.5)
1′′′			4.50, d (7.8)	106.1, CH
2′′′			3.61, m	72.9, CH
3′′′			3.46, m	75.1, CH
4′′′			3.82, m	70.4, CH
5′′′			3.53, m	76.8, CH
6′′′			3.70, m	62.6, CH

a Overlapped with the CD3OD residual peak.

Compound 2 was isolated as a white, amorphous solid with a molecular formula of C46H74O19 on the basis of the pseudomolecular ion at m/z 953.47165 [M + Na]+ by HRESIMS analysis. The aglycon of 2 differed from 1 in two main sites. First, changes in the 1H and 13C-NMR chemical shifts of the signals corresponding to C-3, C-4 and C-5 indicated a change in the substitution pattern at C-4. In the 1H-NMR spectrum, the methyl at C-28 for 1 was replaced by an AB system in 2 at δH 3.96 (d, J = 11.0 Hz, H-28a) and 3.89 (d, J = 11.0 Hz, H-28b) which was reminiscent of a methylene oxy at C-4 (Table 1). This assumption was confirmed by comparison with the corresponding signals found for ulososide B [20]. Comparison of the chemical shifts between both compounds and a clear H-29/H-3 NOESY correlation allowed us to assign the relative configuration at C-3 and C-4. The second modification was observed for the signals corresponding to the side-chain protons and carbons. Indeed, the signals corresponding to the vicinal diol of 1 were clearly absent as well as the one corresponding to the methyl at C-24. In contrast, a ketone was unambiguously placed at C-23 due to the 13C-NMR signal at δC 213.8 (C, C-23) and the key H-22a, H-22b, H-24/C-23 HMBC correlations. Interestingly, this side-chain was identical to the one of some pandarosides, steroidal saponins found in another Poecilosclerida sponge of the genus Pandaros [18,27].

The osidic part of this saponin was shown to contain three sugar residues as evidenced by the signals of three anomeric proton doublets at δH 4.56 (d, H-1′), 5.59 (d, H-1′′) and 4.50 (d, H-1′′′) and the corresponding anomeric carbons at δC 105.3 (CH, C-1′), 100.2 (CH, C-1′′) and 106.1 (CH, C-1′′′) observed in the HSQC spectrum. The three sugar residues were confidently located at C-3, C-2′ and C-3′ on the basis of H-1′/C-3, H-1′′/C-2′ and H-1′′′/C-3′ HMBC correlations. Two hexoses were deduced from the signals at δH 3.73 (m, H-6′), 3.70 (m, H-6′′′) and δC 62.6 (CH2, C-6′ and C-6′′′). The third sugar residue was found to be a pentose due to the presence of the signals at δH 4.07 (d, H-5′′a), 3.42 (m, H-5′′b) and δC 64.9 (CH2, C-5′′).

The ring sizes and identity of these sugar residues were determined by 2D-NMR experiments and by comparison of chemical shifts of protons and carbons of each monosaccharide with literature citations [28,29]. After the assignment of the individual NMR signals for these sugar units by extensive COSY, TOCSY, and HSQC analyses, HMBC experiments showed long-range correlations at H-1′/C-5′, H-5′/C-1′, H-5b′′/C-1′′, H-1′′′/C-5′′′, and H-5′′′/C-1′′′, thus revealing the pyranose nature of all three residues. The large coupling constant values for the doublets assigned to H-1′ and H-1′′′ (J = 7.9 and 7.8 Hz) implied that these hexoses were connected through β-glycosidic linkages, while the smaller coupling constant value for H-1′′ (J = 3.2 Hz) suggests also a β linkage for this arabinose residue. The absolute configurations of these three residues was ascertained after acidic hydrolysis, derivatization into chiral butylated derivatives and GC analysis which indicated a D-galactose at C-3, a D-arabinose at C-2′ and a second D-galactose at C-3′.

Compound 3 was obtained as a white, amorphous powder. The positive ion at m/z 849.38367 [M+Na]+ in HRESIMS and 13C-NMR data indicated an empirical molecular formula of C41H62O17. The signals corresponding in the NMR spectra of 3 were closely related with the signals of 2 indicating a close relationship between these two compounds. The sole difference appears for the signals corresponding to the positions C-3, C-4 and C-5 (Table 1). The absence of the AB system assigned to the primary alcohol of 1 at C-4 suggested a diverse functionalization at this position. Even if the corresponding signal was not observed in the 13C neither in the HMBC NMR spectra, the molecular formula was only consistent with a presence of a second carboxylic acid at this position. This is the first example of such a substitution pattern at C-4 for a terpenoid and then no comparison with literature data was available. Nevertheless, NMR modeling with ChemDraw was fully consistent with the observed chemical shifts in 1H-NMR and more importantly in 13C-NMR, especially for δC 63.8 (C, C-4), thus confirming this assumption.

Two hexose residues were observed in 3 which were identified as a first glucuronic acid linked at C-3 to the aglycon due to the presence of a H-1′/C-3 HMBC correlation. Coupling constant values and a clear H-5′/C-6′ HMBC correlation confirmed the β-glucuronic acid. The second sugar residue was linked at C-2′ to this first residue on the basis of a H-1′′/C-2′ HMBC correlation. This second residue was found to be a galactose unit due to the coupling constant values of the signal at δH 3.76 (d, J = 3.0 Hz, H-4′′). Furthermore, the value of J = 8.1 Hz for the coupling constant of H-1′′ ascertained a β linkage with the first residue. Using the same process used for 2 we confirmed the relative configurations and proposed a D absolute configuration for both residues.

2.2. Bioactivity

No significant cytotoxicity against two cell lines (Jurkat and CHO cells) or hemolytic activity was detected below 50 µM for any of the isolated compounds. Only compound 3 exhibited a low cytotoxicity, with an IC50 value of 100 µM. Other compounds were considered inactive, with IC50 > 100 µM, and with cytotoxicities below 30% up to 100 µM. Interestingly, compounds 1 to 4 did not induce hemolysis, which is the major known adverse effect of this kind of molecules and the major obstacle for clinical trials progress. Previous studies on the bioactivities of triterpene glycosides from E. ferox reported moderate cytotoxicity against J774 (murine monocyte-macrophage), WEHI164 (murine fibrosarcoma), and P388 (murine leukemia) cell lines at IC50 ranging from 8.5 to 19 μg/mL [9,10]. The biological activities of our new derivatives are significantly lower than those exhibited by the previously isolated ectyoplasides and feroxosides and consequently it suggests a key role of the aglycone in the cytotoxicity of these compounds. The assessment of detergent-like properties by the hemolysis assay demonstrated that there is no significant effect of our compounds.

3. Experimental

3.1. General Procedures

Optical rotations were measured on Perkin Elmer 343 polarimeter equipped with a 10 cm microcell. IR spectra were obtained with a Perkin–Elmer Paragon 1000 FT–IR spectrometer. High resolution mass spectra (HRESIMS) were obtained from a LTQ Orbitrap mass spectrometer (Thermo Finnigan). NMR experiments were performed on a Bruker Advance 500 MHz spectrometer. Chemical shifts (δ in ppm) are referenced to the carbon (δC 49.0) and residual proton (δH 3.31) signals of CD3OD, the solvent with multiplicity (s singlet, d doublet, t triplet, m multiplet). Column chromatography was performed using RP18 stationary phase (40–63 μm, Merck). HPLC separation and purification were carried out on an Agilent1100 system equipped with an Agilent UV detector and coupled with a Varian 385-ELSD. For GC-MS analysis of the derivatized sugar residues an Agilent 6890N GC interfaced to a 5975B MSD was used. TLC was performed with Kieselgel 60 F254 (Merck glass support plates) and spots were detected after spraying with 10% H2SO4 in EtOH reagent and heating. The OD570 nm absorbance for cytotoxicity evaluation was measured with a Thermo Scientific Multiskan® Spectrum instrument.

3.2. Biological Material

The marine sponge was collected off Caribbean Sea, Colombia, in October 2008 by SCUBA diving (Urabá Gulf 8°40′14′′N, 77°21′28′′W). A voucher specimen (INV-POR 0335) identified by Sven Zea, has been deposited in the sponge collection of Museo de Historia Natural Marina de Colombia, Invemar. The sponge was kept frozen from collection until the extraction process.

3.3. Extraction and Isolation

The frozen sponge (350 g wet) was cut into pieces of about 1 cm3 and extracted with 1:1 MeOH/CH2Cl2 (600 mL, 24 h) at room temperature yielding 3.6 g of crude extract after solvent evaporation. The crude extract was fractionated by RP-C18 column chromatography (elution with a decreasing polarity gradient of H2O/MeOH from 70:30 to 0:100, then MeOH/CH2Cl2 from 100:0 to 0:100). The third fraction (175.5 mg) from 10 collected (MeOH 100%) was then subjected to RP semi-preparative HPLC (Phenomenex, Gemini C6-phenylhexyl 110 Å, 250 × 10 mm, 5 μm) with a gradient of H2O/acetonitrile/TFA (flow 3.0 mL·min−1 from 60:40:0.1 to 45:55:0.1) to yield pure compound 2 (tr: 23.1 min; 1.4 mg); whereas the second fraction (122.5 mg) was purified with an isocratic mobile phase of H2O/Acetonitrile/TFA (flow 3.0 mL·min−1, 55:45:0.1) to afford pure metabolites 1, 4 and 3 (tr: 15.2, 16.8 and 24.1 min; 4.5, 3.6 and 2.9 mg, respectively).

3.4. Isolated Compounds

(22R,23S,24R)-3β-O-(β- (Ulososide F, 1). White amorphous solid; [α]20D −4.0 (c 0.036, MeOH); IR (thin film): γmax 3392, 2956, 2874, 1721, 1669 cm−1; 1H-NMR and 13C-NMR see Table 1, Table 2; HRESIMS (+): m/z 892.46222 [M+Na]+ (calcd for C44H71NNaO16, 892.46651, Δ −4.8 ppm).

3β-O-[β- (Uraboside A, 2). White amorphous solid; [α]20D −330 (c 0.013, MeOH); IR (thin film): γmax3392, 2988,1625, 1072 cm−1; 1H-NMR and 13C-NMR see Table 1, Table 2; HRESIMS (+): m/z 953.47327 [M+Na]+ (calcd for C46H74NaO19, 953.47165, Δ −1.7 ppm).

3β-O-[β- (Uraboside B, 3). White amorphous solid; [α]20D−130 (c 0.027, MeOH); IR (thin film): γmax 3409, 2920, 1712, 1674 cm−1; 1H-NMR and 13C-NMR see Table 1, Table 2; HRESIMS (+): m/z 849.38367 [M+Na]+ (calcd for C41H62O17Na, 849.38792, Δ −5.0 ppm).

(22R,23S,24R)-3β-O-(β- (Ulososide A, 4). White amorphous solid; [α]20D −9.5 (c 0.23, MeOH); IR (thin film): γmax 3425, 1715, 1648 cm−1; 1H-NMR (500 MHz, CD3OD) 1.84 (m), 1.36 (m), 2.41 (m), 2.03 (m), 3.30 (m), 1.34 (m), 1.97 (m), 1.71 (m), 2.07 (m), 1.93 (m), 2.17 (m), 2.08 (m), 1.99 (m), 1.46 (m), 2.11 (m), 1.64 (m), 1.34 (m), 1.99 (m), 1.44 (m), 1.57 (m), 0.67 (s), 1.01 (s), 1.90 (m), 0.93 (d, 6.9 Hz), 3.51 (m), 3.66 (dd, 1.6 Hz, 9.7 Hz), 1.55 (m), 1.62 (m), 0.97 (d, 6.6 Hz), 0.95 (d, 6.6 Hz), 0.85 (d, 6.9 Hz), 1.44 (s), 4.32 (d, 7.8 Hz), 3.25 (m), 3.47 (m), 3.27 (m), 3.53 (m), 4.08 (s, b), 3.77 (m), 4.47 (d, 7.8 Hz), 3.25 (m), 3.39 (m), 3.51 (m), 3.81 (d, 9.6 Hz); 13C-NMR (125 MHz, CD3OD) 37.7 (C-1), 28.5 (C-2), 89.4 (C-3), 50.7 (C-4), 53.6 (C-5), 21.3 (C-6), 29.9 (C-7), 129.3 (C-8), 137.1 (C-9), 23.2 (C-11), 38.5 (C-12), 43.3 (C-13), 53.3 (C-14), 24.8 (C-15), 29.1 (C-16), 52.5 (C-17), 11.9 (C-18), 18.6 (C-19), 38.0 (C-20), 12.3 (C-21), 73.2 (C-22), 72.2 (C-23), 41.0 (C-24), 32.2 (C-25), 21.6 (C-26), 21.2 (C-27), 10.0 (C-28), 179.0 (C-29), 24.3 (C-30), 107.2 (C-1′), 75.3 (C-2′), 77.0 (C-3′), 71.7 (C-4′), 73.2 (C-5′), 70.2 (C-6′), 105.1 (C-1′′), 74.9 (C-2′′), 77.9 (C-3′′), 73.5 (C-4′′), 76.8 (C-5′′), 171.2 (C=O); HRESIMS (+): m/z 851.43524 [M + Na]+ (calcd for C42H68NaO16, 851.43996, Δ −5.6 ppm).

3.5. Acidic Hydrolysis and GC-MS Analysis of the Butylated Sugar Derivatives

D- and L- determination was performed using combined gas chromatography/mass spectrometry (GC/MS) of the butylated derivatives of the monosaccharides produced from the compounds 1–4 by acidic hydrolysis. The sample materials were placed into individual test tubes. To this, aqueous 2 M TFA (400 µL) was added. The tubes were then placed at 121 °C for 1.5 h. Once cooled, the sample was dried under nitrogen. The dried samples were then re-N-acetylated with pyridine and acetic anhydride in methanol. After drying, the samples were butylated using S-(+)-2-butanol or R-(+)-2-butanol (Sigma) for 16 h at 80 °C. The samples were per-O-trimethylsilylated by treatment with Tri-Sil (Pierce) at 80 °C (0.5 h). GC/MS analysis of the butylated derivatives was performed using a Supelco EC-1 fused silica capillary column (30m × 0.25 mm ID). Individual standards of all the detected residues were analyzed in parallel with each sample. Comparison of retention times allowed for the elucidation of the specific conformation of each monosaccharide in the compounds. All residues were of D configuration.

3.6. Cell Cultures

Jurkat and CHO-K1 cells were cultured at 37 °C in a humidified 5% CO2 atmosphere in 24 cm2 cell culture flasks in RPMI 1640 medium supplemented with 5% heat inactivated fetal bovine serum, 2 mM L-glutamine, free of antibiotics.

3.7. MTT Test

The purity of all tested compounds was found to be higher than 96% based on HPLC-ELSD analysis. Compounds at final concentrations of 1 and 10 μM was added to 100 μL of the CHO and Jurkat cells suspension (1.0 × 104/well for Jurkat cells and 8.0 × 103/well for CHO cells in RPMI 1640 medium with 5% of FBS) onto wells. Cells were treated with each sample for 24 h at 37 °C in 5% CO2. After treatment, the viability of cells was evaluated by the MTT assay. MTT reagent was added to each plate, and after 4 h of incubation, 100 µL of acidic isopropyl alcohol mixture (50 mL Triton X-100, 4 mL of 30% HCl and 446 mL of isopropyl alcohol) was added to dissolve the water-insoluble formazan salt for overnight. The OD570 nm absorbance was measured. Each concentration was tested by triplicated and unexposed cells were regarded as 100% viable [30].

3.8. Hemolysis Assay

The method was adapted from van Duick et al. [31] and from Taniyama et al. [32]. Blood was obtained from healthy young male donors. The red blood cells (RBCs) were washed three times and resuspended in sterile RPMI 1640 medium (S&A) PBS to give about 15 × 106 cells per mL and further processed [31]. The erythrocytes were incubated with compounds in a range 100–200 μM for 1 h at 37 °C. After centrifugation of the nonhemolysed erythrocytes (800 rpm, 5 min), the absorbance of the released hemoglobin in the wavelength 540 nm was measured. The percentage of hemolysis was determined by comparing the absorbance of hemoglobin at 540 nm released from the RBCs in the presence of each compound. The positive control (100% hemolysis) was determined by the amount of hemoglobin released from 15 × 106 RBCs after 1h of incubation with 0.1% of Tween-20.

4. Conclusions

The structures of glycoconjugates found in some marine invertebrates are used as chemotaxonomic markers at different taxonomic levels (species, genus, and subfamily) [14]. As established earlier, glycoside terpenoids belonging to the same taxon show characteristic structural features that were found to be independent of the collection site and season. Glycosides from E. ferox collected in different geographic areas demonstrate structural similarity to each other. They contain related carboxylated aglycons of the lanostane type and their carbohydrate chains often include galactose and glucuronic acid units. It is interesting to note that the structures of the triterpenoid saponins isolated in this study differed from those isolated from the same species, but collected earlier in the Northern Caribbean. The most distinguishing feature is undoubtedly the presence of carboxy groups at C-4 of the aglycon. Difficulties in the isolation and structure elucidation of these compounds may also explain our finding in a previously studied species. Saponins are then confirmed as common compounds in marine sponges and especially in sponges belonging to the order Poecilosclerida. This can be of taxonomical significance and should trigger further chemical studies in this group.