Nitrogen eutrophication particularly promotes turf algae in coral reefs of the central Red Sea

Study site and environmental conditions

The experiments were conducted at Abu Shoosha reef (22°18′15″N, 39°02′56″E) on the west coast of Saudi Arabia in the central Red Sea from late January until late March 2018. The reef assessed in this study does not fall under any legislative protection or special designation as a protected area. Under the auspices of KAUST (King Abdullah University of Science and Technology, Thuwal, Saudi Arabia), sailing permits to the reef were granted that included the collection of corals and other reef benthos. This reef is characterized by generally high levels of herbivory and small fluctuations in ambient dissolved inorganic nitrogen (DIN) concentration during this period (Roth et al., 2018). For example, in January to March of the previous year (i.e., 2017), sea water concentrations of ammonium (NH₄⁺) ranged from 0.16 to 0.17 μM, nitrate (NO₃⁻) from 0.25 to 0.40 μM, nitrite (NO₂⁻) from 0.03 to 0.06 μM, phosphate (PO₄³⁻) from 0.02 to 0.21 μM and the resulting DIN(NO₃⁻ + NO₂ + NH₄⁺)/PO₄³⁻ ratio from 2.9:1 to 20:1 (Roth et al., 2018, Table S4). Abu Shoosha reef features turf algae (37%) and hard corals (29%) as most abundant functional groups (Table 1).

Key environmental variables were monitored every 2–3 weeks at the sampling site, as described in a related study by Roth et al. (2018). Briefly, water temperature was measured with continuous data loggers (Onset HOBO Water Temperature Pro v2 Data Logger—U22-001; accuracy: ±0.21 °C) and are given in 3-day means (72 h). For background measurements of dissolved NO₃⁻, NO₂⁻ and PO₄³⁻, water samples were taken in triplicates at the study site at least 2 m away from any fertilizer source (see “Experimental Design and Sampling Strategy” for more details). Water samples were filtered on the boat (Isopore™ membrane filters, 0.2 μm GTTP) and stored dark and cool until they were frozen to −50 °C in the lab. Nutrient concentrations were determined with a continuous flow analyzer (AA3 HR, SEAL). The limits of quantification (LOQ) for NO₃⁻, NO₂⁻ and PO₄³⁻ were 0.084 μmol L⁻¹, 0.011 μmol L⁻¹ and 0.043 μmol L⁻¹ respectively. Five mL subsamples for NH₄⁺ were filtered into separate acid washed centrifuge tubes. A total of 1.2 mL ortho-phthalaldidehydesolution (OPA) was added, and samples were incubated >4 h with OPA in the dark. NH₄⁺ concentrations were determined fluorometrically within 8 h (Trilogy^® Laboratory Fluorometer; Turner Designs Inc., San Jose, CA, USA). The LOQ for NH₄⁺ was 0.094 μmol L⁻¹. The sum of NO₃⁻, NO₂⁻ and NH₄⁺ concentrations reflect DIN.

Experimental design and sampling strategy

Eight distinct patches of reef communities, each surrounded by patches of reef sand, were chosen in the back reef of Abu Shoosha at a water depth of approximately 5 m. The chosen communities, which represented the surrounding reef in composition (Table 1), were exposed to simulated eutrophication for 8 weeks in total. More specifically, each of the replicate communities was surrounded by four pins with approximately 70 g of slow release fertilizer granulate (Osmocote^® Plus (15-9-12)) (Fig. 1). Being one of the most commonly used fertilizers for eutrophication experiments (Wheeler, 2003; Russell et al., 2009; Falkenberg, Russell & Connell, 2013; Stuhldreier et al., 2015), this approach provides a fast and high supply of macronutrients (15% total N (8% nitrate N, 7% ammoniacal N), 9% available phosphate, 12% soluble potash) from the 1st day of fertilization under local temperature regimes (Adams, Frantz & Bugbee, 2013). Osmocote^® Plus (15-9-12) provides a balanced fertilization of N and phosphorus (P), however, only the fate of N was considered in this experiment as particularly N effects were of interest. The fertilizer was renewed every 2–3 weeks to assure a continuous nutrient supply (Adams, Frantz & Bugbee, 2013). To test whether the nutrient addition was effective locally, water samples for nutrients were taken directly at the fertilizer pin, and 25 cm towards the manipulated communities according to the protocol outlined above.

The effect of eutrophication was then assessed at the major functional groups (in terms of benthic reef cover in the central Red Sea) that were present in the selected communities. Specifically, we chose autotrophic hard corals (Pocillopora cf. verrucosa), soft corals (Xeniidae), turf algae and reef sand (sediments). These groups covered ~80% of the sampled reef (Roth et al., 2018). Turf algae were defined as dense and flat (less than 2 cm in height) assemblages of filamentous algae of different species, including small individuals of macroalgae and cyanobacteria.

Manipulated specimens (“treatment”) were sampled from within a close radius (~25 cm) of the fertilizer tubes. As the in-situ communities were also needed in other experiments investigating their C chemistry (F. Roth, 2018, unpublished data) and N fluxes (Y. El-Khaled, 2018, unpublished data), specimens for natural conditions at the beginning (“start”) of the experiment were collected in the surrounding reef. Additional samples in replicates of eight were collected in the surrounding non-fertilized reef at the end (“control”) of the experiment, to reflect non-fertilized control conditions. For start and control data, a distance of at least 10 m from any fertilizer pin was maintained and the same depth as well as light conditions were given.

Samples were acquired with hammer and chisel. Hard coral and turf fragments (their substrate) were of approx. 10 cm in length. Sediments were collected using a Petri dish, which was dragged into the sediment upside-down (max. depth 14 mm) and the sediment was fixed to the dish from underneath. The samples were stored at −80 °C until further preparation. Hard corals, soft corals and turf algae were rinsed with Milli-Q to remove excess salt. Epilithic turf algae were scraped off from their surface with a scalpel and tweezers.

Elemental and stable isotopic compositions of C and N

Turf algae, soft corals and sediments were dried for 48 h (sediments: 72 h) at 40 °C. Following Jessen et al. (2013b), hard coral tissue was removed using an airbrush, and the resulting tissue slurry was weighed, homogenized (MicroDisTec 125) and centrifuged for 10 min (Eppendorf Centrifuge 5,430 R, 4 °C, 3,220 rcf) to separate algae (“zooxanthellae”) from animal “tissue”. The supernatant was filtered (Whatman, GF/F) and for each sample two filters were generated. Filters for N and inorganic C analysis were dried for 24 h at 40 °C. Filters for C_org measurements were exposed to HCl fumes (from 37% HCl) and dried for 24 h. The remaining zooxanthellae pellet was dried for 48 h at 40 °C.

Sub-samples of all groups were ground using an agate mortar and pestle. A mill grinder (Retsch, PM 200, 4 min) was used for the sediments. For preparation of C_org samples, 5–10 g of ground sediment were placed in an Erlenmeyer flask and covered with Milli-Q. Drops of HCl (37%) were added until the reaction ceased. The acidified liquid was transferred to 50 mL Falcon tubes which were filled up with Milli-Q, to stepwise wash the sample pellet and raise the pH up to neutrality, and subsequently centrifuged for 10 min (Eppendorf Centrifuge 5,430 R, 4 °C, 7,200 rcf). The liquid supernatant was discarded and tubes were then refilled with Milli-Q for 3–4 times to raise pH. The pellets were dried in the Falcon tubes for 48 h at 40 °C.

The dry, homogenous powder was analyzed for: (a) N and inorganic C quantities; and (b) C_org as in Roth et al. (2018). C_org/N ratios, fractions of organic and inorganic C and isotope ratios were measured as in Rix et al. (2018) using a Flash 1112 EA coupled to a Delta V IRMS via a ConfloIV-interface (Thermo Scientific, Waltham, MA, USA). Isotopic ratios are shown as δ¹³C or δ¹⁵N (‰) = (R_sample/R_ref − 1) × 1,000. There, R is the ratio of heavier:lighter isotope (¹³C:¹²C or ¹⁵N:¹⁴N). As reference, Vienna Pee Dee Belemnite was used for C (R_ref = 0.01118) and atmospheric nitrogen for N (R_ref = 0.00368).

Zooxanthellae cell density and mitotic index

For hard corals, zooxanthellae cell density and the mitotic index were analyzed following the described sampling strategy (start, control and treatment), whereby “start” and “control” were from the surrounding reef. Aliquots of 20 µL homogenized tissue sample and 80 µL Milli-Q were vortexed (Gilson, GVLab) directly before taking 10 µL on an improved Neubauer Levy hemocytometer (0.0100 mm deep). Pictures were taken with a ZEISS Primovert microscope via Labscope (Version 2.5) from the 5 × 5 grid in 40-fold and randomly in 20-fold magnification. Manual counts of zooxanthellae and the mitotic index were related to the total amount of airbrushed slurry per individual. Here, clumps and inhomogeneous patches were not considered. For normalization to the coral surface area, 3D models for all coral skeletons were generated using the software AutodeskReCap Photo (v18.2.0.8).

Data analysis

Nitrogen uptake by functional groups was assessed using stable isotope analysis. N utilization was assessed by elemental analysis, and C_org/N ratios served to identify nutrient limitations (Lapointe, Littler & Littler, 1992; Hillebrand & Sommer, 1999; Sterner & Elser, 2002; Lapointe et al., 2005), along with zooxanthellae cell density and mitotic index (for hard corals). Statistical analysis was conducted with RStudio (R Core Team, 2017). Xeniidae and Pocillopora cf. verrucosa were not abundant in all eight communities (only in 5 and 6, respectively). Due to logistical constraints, “start” data of soft corals was not available. A two-way ANOVA (factors: treatment, dominant functional group) showed no significant effect of community composition on our response parameters under N eutrophication, therefore data from more coral and more algae dominated communities were pooled. Significant differences between “start” and “control” as well as between “control” and “treatment” were checked with two-sample t-tests (test statistic: t) if test assumptions were fulfilled, otherwise Mann–Whitney–Wilcoxon Tests (test statistic: W) were applied. A similar approach was conducted for cell density of zooxanthellae and mitotic index per treatment. Tissue homogenization of the “start” samples was visually much worse than for “treatment” and “control” samples, but is shown for completeness and homogeneity.

Environmental parameters and N availability

During the study period, water temperature increased from 25 °C to 28 °C (Table S1). The mean background concentration in sea water for DIN was 0.34 ± 0.07 μM N and 0.10 ± 0.02 μM PO₄³⁻ during the time of the experiment (measured after 2, 4 and 6.5 weeks). Accordingly, the environmental background DIN/PO₄³⁻ ratio was 3.4 (±0.08):1 on average. The manipulation of nutrients increased DIN concentrations (measured after 2, 4 and 6.5 weeks) on average 3-fold and to a maximum of 7-fold directly at the communities relative to background concentrations (Fig. 2). Namely, manipulated NO₃⁻ was 1.05 ± 0.09 μM and manipulated NH₄⁺ was 0.22 ± 0.06 μM. PO₄³⁻ remained at ambient condition, despite being present in the fertilizer (Table S1). As such, the mean DIN/PO₄³⁻ ratio at the manipulated communities was 15.1 (±3.46):1.

Uptake of excess N by benthic functional groups

Pure Osmocote^® fertilizer was enriched in ¹⁵N (δ¹⁵N = 16.326 ± 0.257, Table S2). Hard corals (tissue), turf algae and soft corals took up excess N, as indicated by significantly (t₁₂ = 2.553, p = 0.025; t₁₃ = 3.228, p = 0.007; t₉ = 6.705, p < 0.001, respectively) increased δ¹⁵N (Fig. 3A). The δ¹⁵N values in manipulated functional groups were 8% (Pocillopora tissue), 27% (Xeniidae) and 28% (turf algae) higher compared to untreated controls after the same time.

Utilization of excess N by benthic functional groups

Nitrogen content was highest in hard coral zooxanthellae both before and after eutrophication (Fig. 3B). In the eutrophication treatment, N content was significantly higher in the tissues of Xeniidae (t₉ = 5.667, p < 0.001) and turf algae (W = 49, p = 0.014). Their tissues contained 85% (Xeniidae) and 39% (turf) more N compared to untreated controls. Increases in the other groups were not significant.

To investigate whether N was utilized to produce C_org under a metabolically stable ratio, the C_org content and C_org/N ratio are presented. The hard coral components showed the highest C_org content ranging from 50.39 ± 1.83% to 55.05 ± 1.49% in the tissue and between 42.64 ± 1.39% and 45.78 ± 1.49% in zooxanthellae (Fig. 3C). Minimum C_org content was observed in reef sediments, ranging between 0.09 ± 0.01% and 0.11 ± 0.01%. Only turf algae and sediments showed a significant change in C_org content (t₁₄ = 2.568, p = 0.022; t₁₄ = 2.537, p = 0.023, respectively). This represents an increase in C_org content by 33% in turf algae and 24% in sediments in the treatment compared control specimen.

The C_org/N ratio for treated Xeniidae was significantly lower (t₈ = −6.405, p < 0.001) than for Xeniidae in the surrounding reef (8.520 ± 0.320 compared to 4.132 ± 0.566, Fig. 3D). In sediments of the eutrophication “treatment” the C_org/N ratio was significantly higher than in controls (W = 53, p = 0.028), however it did not increase compared to start values. In hard coral zooxanthellae, C_org/N ratio declined over time but was not significantly different in treatment data compared to controls. C_org/N remained constant in hard coral tissue and turf algae.

Cell density of hard coral zooxanthellae (Pocillopora cf. verrucosa) doubled over the 8 weeks, while their mitotic index halved (Figs. 4A and 4B). However, zooxanthellae density and mitotic index in fertilized and control corals remained similar. After 8 weeks, cell densities ranged from 1.324 ± 0.147 Mio. cells cm⁻² (treatment) to 1.373 ± 0.172 Mio. cells cm⁻² (control), whereas the mitotic index ranged from 4.718 ± 0.445% to 4.901 ± 0.244% in organisms under control and N enrichment conditions, respectively.

Uptake of excess N by major benthic functional groups

In-situ N enrichment resulted in an uptake of N in the tissues of turf algae, soft corals and hard corals, but not in sediments and hard coral zooxanthellae. The fact that turf algae exhibited the lowest δ¹⁵N at the start of our experiment suggests considerable assimilation of N from N₂ fixation (Yamamuro, Kayanne & Minagawao, 1995; Rix et al., 2015; Tilstra et al., 2017; Y. El-Khaled, 2018, unpublished data). Biological fixation of atmospheric N₂ leads to a depletion in ¹⁵N in the N compounds of the fixer (Carpenter et al., 1997; Karl et al., 2002). After the experiment, turf algae showed one of the strongest uptakes of N from the fertilizer among the benthic reef functional groups, as indicated by significantly higher δ¹⁵N values (Fig. 3A), which concurs with Den Haan et al. (2016). The low DIN/PO₄³⁻ ratio in ambient waters at the reef further suggests a relatively low degree of P-limitation under ambient conditions, which may help to explain the strong uptake of N when available. Concordantly, Lapointe et al. (2019) showed that in the eutrophic waters of the Florida Keys, the N:P ratio of turf algae (293:1) increased to a much greater extent than that of macroalgae (71:1) as DIN concentrations increased over a 3-decade period. Also soft corals incorporated fertilizer N and reached higher δ¹⁵N values than typical for soft corals that are exposed to industrial and urban run-off in the central Red Sea (Kürten et al., 2014).

In the present experiment, the uptake of excess N was not noticeable in the sediment δ¹⁵N, in contrast to a study by Miyajima et al. (2001). There, sediment microflora took up NO₃⁻ and NH₄⁺ in bottle incubations (Miyajima et al., 2001), and assimilation as well as adsorption of N compounds on carbonate reef sands were observed (Erler, Santos & Eyre, 2014). This would suggest fast nutrient uptake, especially in microalgae on the sediments, and high uptakes into pore water, as reported by Rasheed, Badran & Huettel (2003) and Erler, Santos & Eyre (2014). Pore water was not targeted in our study and a change of isotopic signature in the sediment could take longer than the current experimental period, as previously suggested by Cook et al. (2007) who did not find clear δ¹⁵N patterns in N manipulated sediments. This would account for the integration time of isotopic signatures through the food-web (Rolff, 2000; O’Reilly et al., 2002). In agreement to our study, Koop et al. (2001) also did not find high δ¹⁵N uptake in sediments. Potentially, organisms on and in the sediments are not N-limited, given that sediments are active sites of microbial N transformations (Capone et al., 1992) and remineralization (Tribble, Sansone & Smith, 1990) allowing for N recycling.

Within the hard coral holobiont, the zooxanthellae did not incorporate excess N significantly. This generally agrees with Koop et al. (2001) and Den Haan et al. (2016) showing that hard corals (i.e., Madracis mirabilis (now Madracis myriaster)) take up less excess nutrients than turf or macroalgae. Most studies, however, report stronger δ¹⁵N enrichment in the zooxanthellae fraction compared to host tissue (Grover et al., 2002; Pernice et al., 2012; Kopp et al., 2013). There are several possibilities why this was not observed in our study. Firstly, NO₃⁻ uptake in zooxanthellae can be highest under low NH₄⁺ availability (Grover et al., 2003; Tanaka et al., 2017), however, NH₄⁺ was elevated ~5-fold compared to the environmental background in our experiment (Table S1). Secondly, P can be a limiting factor to zooxanthellae’s N uptake (Godinot et al., 2011). Unlike the highly increased N availability, the P provided by our fertilizer did not alter the PO₄³⁻ concentration 25 cm away from the source (Table S1). The resulting increased DIN/PO₄³⁻ ratio at the communities underlines a stronger P-limitation under manipulation. Potentially, reef sediments (Millero et al., 2001) or organisms in the water column and the surrounding benthos took up PO₄³⁻ too quickly as P was stated crucial (Cuet et al., 2011) and limiting (Lapointe, Littler & Littler, 1992; Eyre, Glud & Patten, 2008; Kürten et al., 2014) for primary production in coral reefs. However, we acknowledge dissimilar findings on the limiting roles of N and P in the central Red Sea (Peña-García et al., 2014). The understanding of P cycling and limitation in coral reef environments is still in its infancy (Ferrier-Pagès et al., 2016), but PO₄³⁻ could have been limiting for significant N uptake in zooxanthellae (Godinot et al., 2011). In contrast to other findings (Grover et al., 2003; Tanaka et al., 2006), coral tissue incorporated more available N than the symbionts. This suggests that the host tissue was less P-limited than the zooxanthellate fraction, and hence took up relatively more N. This is corroborated by the low DIN/PO₄³⁻ ratio of 3.4 in ambient waters of the studied reef that indicates N-rather than P-limitation, confirming Al-Farawati, El Sayed & Rasul, (2019).

Utilization of excess N by benthic functional groups

Due to eutrophication, tissue N content significantly increased in turf algae and soft corals but not in hard corals and sediments. C_org content remained constant in hard and soft corals but increased in sediments and turf algae. Thus, turf algae and hard coral tissue remained at constant C_org/N ratio, while it decreased in soft corals and showed unclear trends in hard coral zooxanthellae and sediments.

For turf algae, N and C_org content were significantly higher under nutrient addition compared to controls, which contrasts findings by Stuhldreier et al. (2015) reporting no such eutrophication effects on turf algae dominated settlement communities. In the present study, relatively similar increases in N content (+39%) and C_org content (+33%) occurred and the C_org/N ratio stayed constant (between 9.1 and 9.3). Hence we interpret N to be a limiting nutrient (Hecky, Campbell & Hendzel, 1993) for turf algae growth, which also corroborates other studies (Hatcher & Larkum, 1983; Williams & Carpenter, 1988; McCook, 1999). Turf algae are strong opponents to corals (Airoldi, 1998; Roth et al., 2018), and their competitiveness under high-nutrient availability has been documented in Hawaii (Smith, Smith & Hunter, 2001), the Caribbean (Vermeij et al., 2010), Brazil (Costa et al., 2000), Australia (Gorgula & Connell, 2004) and in the Red Sea (Naumann et al., 2015). As turf algae are also rapidly taking over bare substrates (Stuhldreier et al., 2015; Roth et al., 2018) and are very resistant to disturbances (Airoldi, 1998), their monitoring should be on regional management agendas. Cover data was not documented in the present study but turf algae growth could be speculated upon based on increases in C_org content.

Nitrogen was taken up by soft corals while the C_org content did not increase, resulting in an altered elemental stoichiometry (C_org/N ratio). The strong decline in the soft corals’ C_org/N ratio could be explained by an uptake of excess N as so-called “luxury consumption” (Sterner & Elser, 2002), describing on-going uptake while a different nutrient (e.g., P) might limit growth and productivity. We interpret that in our eutrophication experiment P rather than N was the limiting nutrient for soft corals, which may limit chlorophyl a content and photosynthesis in Xeniidae (Bednarz et al., 2012). Our data from elemental analysis and non-documented visual observations support the hypothesis of Fabricius et al. (2005) that soft corals could react more timely and strongly to water quality gradients than hard corals.

Our results further correspond to other studies (Capone et al., 1992; Rasheed, Badran & Huettel, 2003; Wild et al., 2004b) finding low C_org content in carbonate dominated reef sands (0.18–0.36%), which were even lower in our study (0.1%). We acknowledge that the utilized acid wash-out processing may underestimate C_org contents due to C_org losses to the liquid acid of 4–52% (Yamamoto, Kayanne & Yamamuro, 2001) and as such lower the C_org/N ratio. However, this is a commonly used method in comparative studies (Rasheed, Badran & Huettel, 2003; Wild et al., 2004b). The observed 21% increase in C_org could be attributed to P-supported algae growth on the sediments (Fig. S1) as fertilizer N was not taken up (constant δ¹⁵N) but gross primary production significantly increased (Y. El-Khaled, 2018, unpublished data). A different source for the increased C_org content in sediments could be the export of C_org from turf algae (F. Roth, 2018, unpublished data) for example, as dissolved organic carbon (DOC) (Haas et al., 2011) and subsequent uptake by reef sediments, as suggested by Cárdenas et al. (2015). This, along with the low C_org/N ratio, corroborates the previous assumption that life in and on the sediments, as well as its increase in C_org content was not N limited.

Regarding the hard coral holobiont, our results suggest that the incorporation of excess N only to the host tissue did not result in its utilization in terms of C_org production. As such, C_org/N ratios for Pocillopora cf. verrucosa contrast a study conducted in 10 km distance to our study site further offshore at the same time of the year in 2012 (Ziegler et al., 2014). There, the natural host total C:N ratio was around 5, which makes our presented host material appear more N depleted in comparison. Over time, we observed an increase in symbiont cell density, which contrasts with other studies finding higher zooxanthellae cell densities in Pocillopora species in cooler and more nutrient rich phases (Stimson, 1997; Al-Sofyani & Floos, 2013; Sawall et al., 2014a). However, particularly the similarity between treatment and non-fertilized controls should be considered where cell density and mitotic index did not differ. Similar findings have been reported by Ferrier-Pagès et al. (2001) and Rosset et al. (2017) during pure N fertilization but contrast with other studies (Stambler et al., 1991; Muller-Parker, Cook & D’Elia, 1994; Fabricius, 2005). Increased zooxanthellae cell density in hard corals was found, for example, after only 18 days of eutrophication (Falkowski et al., 1993) or following a natural nutrient gradient (Sawall et al., 2011). Altogether, this suggests that N was not a limiting factor for zooxanthellae in our experiment. The production (Ezzat et al., 2016), health and density (Tanaka et al., 2017) of zooxanthellae cells was found to be P limited. Accordingly, high P availability resulted in higher increases of zooxanthellae density (Pocillopora damicornis and Euphyllia paradivisa (now Fimbriaphyllia paradivisa)) than availability of only N (Stambler et al., 1991; Rosset et al., 2017). As a consequence, we hypothesize that hard corals also did not shift in primary productivity, even though a significant increase in δ¹³C in hard coral zooxanthellae (Fig. S2) could be a sign of increased photosynthesis (Swart, Saied & Lamb, 2005) for example, following a seasonal pattern (F. Roth, 2018, unpublished data). However, gross primary production did not increase in our manipulated hard corals (Y. El-Khaled, 2018, unpublished data). The increased δ¹³C in the zooxanthellae (Fig. S2) could also be an indicator for a negative effect on hard coral health which was also found in relation to bleached Favia favus (now Dipsastraea favus) corals in the Northern Red Sea (Grottoli, Tchernov & Winters, 2017) but not Montastraea faveolata (now Orbicella faveolata) in Florida (Wall et al., 2019). Given our 8-week observation period and a comparatively cold water temperature, our study did not provide a setting to trace severe bleaching effects and for the Southern Red Sea it was speculated that higher nutrient availability might even benefit P. verrucosa to resist higher water temperature (Sawall et al., 2014a). This corroborates that effects of eutrophication on coral health are not always negative (Bongiorni et al., 2003; Sawall et al., 2011; Ezzat et al., 2019) and do not necessarily harm or kill individual coral colonies but get outcompeted or overgrown over time (reviewed in Fabricius, 2005). Longer (3 years; Vega Thurber et al., 2014), and both longer and stronger (1 year, 36.2 μM NH₄⁺; Koop et al., 2001) N manipulation could, however, lead to increased coral mortality (Koop et al., 2001). In particular, reviewed findings (Morris et al., 2019), natural long-term observations (Lapointe et al., 2019) and laboratory experiments (Wiedenmann et al., 2013; Rosset et al., 2017) with high N (>3 μM and 38 μM N, respectively) and low P supply (<0.07 μM and 0.18 μM P, respectively) increased susceptibility of corals to bleaching, which suggests negative effects. In agreement with Ezzat et al. (2016) and Ferrier-Pagès et al. (2016), we suggest increasing efforts investigating P cycling and limitation in current and future reef ecosystems. Besides this key role of nutrient ratios, Burkepile et al. (2019) highlight the importance to also account for varying effects of different forms of N. As N sources and pathways in corals and their reef environments are of major importance to better understand ecosystem functioning (Rädecker et al., 2015), the uptake and utilization of N (this study) should be compared to eutrophication effects on the N cycle.